Design and fabrication of scaffolds for cartilage ...
Transcript of Design and fabrication of scaffolds for cartilage ...
Design and fabrication of scaffolds for cartilage
applications through photopolymerization of hydrogels
A thesis submitted to the University of Manchester for the Degree of
Doctor of Philosophy in the Faculty of Science & Engineering
September 2019
Hussein H. M. Mishbak
Supervisor:
Professor Paulo Jorge Bartolo
Dr. Glen Cooper
School of Mechanical, Aerospace and Civil Engineering
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Table of Contents Table of Contents ....................................................................................................... 2
List of Figures ............................................................................................................. 6
List of Tables ............................................................................................................ 13
List of Abbreviations ............................................................................................... 14
List of Notations ....................................................................................................... 16
Abstract ..................................................................................................................... 17
Declaration ................................................................................................................ 19
Copyright .................................................................................................................. 20
Acknowledgements ................................................................................................... 21
Chapter 1 Introduction ............................................................................................ 25
1.1 Background .................................................................................................... 26
1.2 Research aims and objectives ....................................................................... 27
1.3 Thesis outlines ............................................................................................... 30
Chapter 2 State-of-art of Cartilage Tissue Engineering ....................................... 33
Biological perspectives and current strategies in osteochondral tissue
engineering ............................................................................................................ 34
Introduction .......................................................................................... 35
Composition of articular cartilage ........................................................ 36
Structure of osteochondral tissue ......................................................... 38
Zonal structure of articular cartilage .................................................... 39
Current osteochondral treatments ........................................................ 41
Tissue engineering: requirements and challenges ................................ 47
Conclusion and future perspectives ..................................................... 54
Engineering natural-based photocrosslinkable hydrogels for cartilage
applications ............................................................................................................ 56
Introduction .......................................................................................... 56
Articular cartilage................................................................................. 59
Engineering hydrogels for cartilage tissue engineering ....................... 64
Crosslinking mechanisms of hydrogels ............................................... 68
Biofunctionalization of hydrogels ........................................................ 69
Conclusions and future perspectives .................................................... 76
Chapter 3 Development and characterisation of a photocurable alginate bioink
for 3D bioprinting .................................................................................................... 78
Introduction ................................................................................................. 79
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Materials and methods ................................................................................. 81
Synthesis of methacrylate alginate ....................................................... 81
Characterisation of pre-polymerised methacrylate alginate ................. 81
Hydrogel formation .............................................................................. 82
Characterisation of photocrosslinked hydrogels .................................. 83
Results and discussion ................................................................................. 84
Alginate functionalization .................................................................... 84
Rheological behaviour of pre-polymerised alginate methacrylate
systems .............................................................................................................. 87
Rheological changes during the photopolymerization process ............ 92
Viscoelastic properties of formed hydrogels........................................ 93
Internal morphology of alginate hydrogels .......................................... 95
Mechanical characterisation ................................................................. 96
Swelling and degradation kinetics ....................................................... 97
Conclusion ................................................................................................... 98
Chapter 4 Photocurable alginate bioink development for cartilage replacement
bioprinting ................................................................................................................ 99
Introduction ............................................................................................... 100
Materials and methods ............................................................................... 101
Synthesis of methacrylated alginate ................................................... 101
HNMR ................................................................................................ 101
Rheological characterization .............................................................. 102
Cell viability and proliferation ........................................................... 102
Result and discussion ................................................................................ 102
Chemical modification through 1HNMR ........................................... 102
Rheological characterization of alginate methacrylate ...................... 104
Cell viability assessment .................................................................... 105
Conclusions ............................................................................................... 106
Chapter 5 Photocrosslinkable gelatin methacrylate (GelMA) hydrogels:
Towards 3D cell culture and bioprinting for cartilage applications ................. 107
Introduction ............................................................................................... 108
Experimental ............................................................................................. 109
Synthesis of methacrylated gelatin .................................................... 109
Photocurable hydrogel solutions ........................................................ 110
HNMR characterization ..................................................................... 110
Rheological characterization .............................................................. 110
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Scanning Electron Microscopy .......................................................... 111
Mechanical characterization............................................................... 111
Swelling and degradation characterization ........................................ 111
hADSCs Cell encapsulation ............................................................... 112
Data analysis ...................................................................................... 113
Results and discussion ............................................................................... 113
Characterization of gelatin and GelMA by HNMR ........................... 113
Rheological characterization ..................................................................... 115
Prepolymer rheology .......................................................................... 115
Morphological characterization ......................................................... 119
Mechanical characterization............................................................... 121
Swelling and degradation characterization ........................................ 121
Cell viability and proliferation ........................................................... 122
Conclusion ................................................................................................. 124
Chapter 6 Development and characterisation of a photocurable alginate-gelatin
for cartilage applications ....................................................................................... 125
Introduction ............................................................................................... 126
Materials and methods ............................................................................... 128
Photocrosslinkable polymer preparation ............................................ 128
Alginate methacrylate preparation (AlgMA) ..................................... 128
Hydrogel formation ............................................................................ 128
Structural conformation of the hybrid hydrogels ............................... 130
Rheological characterisation .............................................................. 130
Structure morphology and porosity .................................................... 131
Swelling and degradation kinetics of the hybrid hydrogels ............... 132
Mechanical assessment ...................................................................... 132
Biological assessment ........................................................................ 132
Histological analysis .......................................................................... 133
Glycosaminoglycan quantification..................................................... 135
Results and discussion ............................................................................... 136
Functionalisation confirmation and rheological characterisation ...... 136
Rheological Characterization ............................................................. 137
Structure morphology and porosity .................................................... 141
Swelling and degradation kinetics and hydrogel ............................... 142
Mechanical characterisation ............................................................... 143
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Hydrogel encapsulated chondrocyte viability and proliferation ........ 144
Histological assessment of hydrogel ECM formation ....................... 146
GAGs quantification .......................................................................... 151
Conclusion ................................................................................................. 152
Chapter 7 Hybrid PCL/Hydrogel scaffold fabrication and in-process plasma
treatment using PABS ........................................................................................... 153
Introduction ............................................................................................... 154
Materials and Methods .............................................................................. 157
Polycaprolactone (PCL) ..................................................................... 157
Hybrid hydrogel) methacrylate anhydride (Alg-Gel)MA preparation .....
............................................................................................................ 157
Plasma-assisted Bioextrusion System set up...................................... 158
Scaffolds printing strategies ............................................................... 160
Nuclear Magnetic Resonance characterisation .................................. 161
Rheological characterisation .............................................................. 161
Morphology Characterization ............................................................ 161
Wettability measurement ................................................................... 162
Biological tests ................................................................................... 162
Data analysis ...................................................................................... 163
Results ....................................................................................................... 163
Hybrid Scaffold Fabrication ............................................................... 163
Full-layer treated PCL scaffold .......................................................... 163
Wettability assessment of full-layer plasma modified scaffold ......... 164
Biological assessment of full-layer plasma modified scaffold .......... 166
Discussion ................................................................................................. 166
Conclusion ................................................................................................. 167
Chapter 8 Conclusion and future work ............................................................... 169
Conclusion ................................................................................................. 170
Future works .............................................................................................. 173
References ............................................................................................................... 175
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List of Figures
Figure 1.1: Framework structure of this thesis. ........................................................ 32
Figure 2.1: Comparison between the physiology and healing capacity of bone and
cartilage. Cartilage is avascular tissue so lacks ready access to a supply of circulating
stem cells and nutrients so relies on the synovial fluid for nourishment. This combined
with its largely acellular composition and low metabolic activity results in a nearly
complete lack of innate regenerative capacity. Consequentially, defects fail to heal,
and clinical interventions typically result in the formation of inferior fibrocartilage. In
contrast, bone has a greater ability for self-repair due to the constant tissue remodelling
by osteoblasts and osteoclasts. Bone is also a highly vascularised tissue which allows
a ready supply of nutrients and proteins that stimulate bone repair. Furthermore, there
is a large source of stem cells in the bone marrow and periosteum which are able to
differentiate into bone producing cells. This allows bone to heal defects up to a certain
critical size after which vascularisation becomes an issue. Image from reference. ... 36
Figure 2.2: Hierarchical and graded composition, structure, and properties of
osteochondral tissue. a) Procollagen polypeptides bind together to form collagen that
assemble into microfibrils and then fibrils which can be crosslinked together by
collagen type IX. Collagen fibrils exhibit a characteristic banding pattern of ~67 nm
due to the staggered packing arrangement of collagen. Image from reference . b)
Molecular composition and arrangement of the chondron depicting the pericellular,
territorial, and interterritorial matrix with increasing distance from the chondrocyte.
Image from reference. c) Zonal structure and properties of osteochondral tissue. Image
adapted from .............................................................................................................. 39
Figure 2.3: Current treatment options for cartilage regeneration. a) A full-thickness
chondral lesion (Grade III). b) Debridement of the lesion is used as precursor to more
invasive procedures as it removes damaged cartilage and bone to create a healthy
border which enables improved integration of neotissue with native tissue. In smaller
cartilage defects debridement may be used without further procedures as a minimally
invasive treatment option. c) Microfracture is treatment that drills into the subchondral
bone to create channels that allow MSCs to migrate into the defect. d) Autologous
chondrocyte implantation (ACI) uses a population of 12-48 million autologous
chondrocytes to which are inserted into the defect which is then covered with either a
periosteal patch or a collagen membrane. e) Matrix-induced autologous chondrocyte
implantation (MACI) is a development of the ACI technique. The autologous
chondrocytes are cultured in vitro and seeded onto an absorbable 3D scaffold (collagen
or hyaluronic acid) before being implanted into the defect and fixed to the defect with
fibrin glue. Image from reference. ............................................................................. 42
Figure 2.4: a) Discrete cartilage defect; b) End stage arthritis; c) Full thickness area
of cartilage loss. ......................................................................................................... 45
Figure 2.5: a) Normal cartilage; b) Fibrocartilage next to hyaline after microfracture.
.................................................................................................................................... 46
Figure 2.6: Tissue engineering strategies for articular cartilage regeneration. Image
from reference . .......................................................................................................... 48
Figure 2.7: 3D bioprinting technologies; a) Inkjet bioprinting; b) Laser-assisted
bioprinting; c) Extrusion bioprinting . ....................................................................... 50
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Figure 2.8: Bioink properties for successful 3D bioprinting require a suitable a)
biofabrication window which balances printability and biocompatibility whilst
providing a variety of b) suitable characteristics. ...................................................... 51
Figure 2.9: Schematic diagram of photocrosslinkable 3D hydrogel constructs and
approaches for use in cartilage tissue engineering. .................................................... 59
Figure 2.10: a) Articular cartilage covers the surfaces of bones in diarthrodial joints
(e.g. knee and elbow); b) Zonal structure and composition of articular cartilage .... 60
Figure 2.11: Stages of articular cartilage damage. 0) Healthy cartilage. I) Softening,
swelling and fissuring of the cartilage. II) Lesions <50% of cartilage depth. III)
Lesions >50% of cartilage depth but not through subchondral bone layer. IV) Severely
abnormal with penetration through the subchondral plate. Reproduced with permission
from the International Cartilage Regeneration & Joint Preservation Society (ICRS).
.................................................................................................................................... 62
Figure 2.12: Current techniques for articular cartilage repair and future scaffold-based
approaches. a) Debridement and microfracture; 1-4 debridement of damaged tissue, 5
microfracture into the subchondral bone, 6 blood clot formation containing
mesenchymal stem cells (MSCs), and 7 formation of inferior fibrocartilage. b) ACI; 1
cartilage biopsy from a non-load bearing site, 2 in vitro expansion of chondrocytes to
obtain sufficient numbers for implantation, 3 a second operation cleans the damaged
area and is covered with the periosteal flap and the expanded chondrocytes are injected
under this or the expanded chondrocytes are seeded into a matrix (e.g. collagen
membrane) and fixed with fibrin glue into the defect area (MACI/MACT). c) AMIC;
a microfracture is created and a membrane placed over the top and fixed with a fibrin
glue or sutures. The membrane protects the clot formation and allows chondrogenic
differentiation of the MSCs in the blood to aid the regeneration process. d)
Osteochondral auto/allograft transplantation; cylindrical plug of fresh cartilage and
subchondral bone is taken from the patient or a cadaver donor, 1 a guide pin is placed
perpendicular to the joint surface in the defect, 2 implantation of the graft plug, and 3
securing the plugs with the insertion of screws. e) Acellular scaffold only requiring a
single surgery and in vivo recruitment and stimulation of cells for tissue regeneration.
f) Cellular-based scaffold involving two surgeries of initial cartilage biopsy,
chondrocyte expansion, and seeding into the scaffold before implantation into the
defect. Adapted with permission from the ICRS ....................................................... 63
Figure 2.13: Engineering 3D hydrogels for cartilage application through a) cell-
encapsulation, b) optimizing crosslinking density, and c) functionalizing with
biomolecules (e.g. RGD) to guide cell behavior. ....................................................... 64
Figure 2.14: Hybrid hydrogel network systems. Multi-material bioink networks are
two different component polymers or more crosslinked together. Interpenetrating
networks (IPN) is a 3D structure of two or more polymeric networks, which are
partially or fully chemically bonded but not covalently bonded, or a network of
embedded linear polymers entrapped within the original hydrogel (semi-IPN).
Nanocomposites bioink network can be produced by adding nanoparticles to the
polymeric hydrogels. Supramolecular bioink network is composed of short repeating
units with functional groups that can interact non-covalently with other functional
units, forming large, polymer-like entanglements . ................................................... 66
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Figure 2.15: Crosslinking mechanisms using in physical and chemical gelation of
hydrogels. ................................................................................................................... 68
Figure 2.16: Influence of hydrogel stress relaxation on cartilage matrix production
and formation. Immunohistochemical staining of chondrocytes embedded within 3
kPa alginate hydrogels for 21 days (scale bar: 25 µm) . ............................................ 72
Figure 2.17: Effect of chondrocytes embedded within cell-degradable hydrogels. A)
Schematic illustration of cell-laden hydrogel formation with tethered MMP
fluorescent sensor (Dab‐ GGPQG↓IWGQK‐Fl‐AhxC), and TGF‐β1; hydrogels are
crosslinked using either an MMP‐degradable peptide sequence
(KCGPQG↓IWGQCK) or non‐degradable (3.5 kDa PEG dithiol) linker. B)
Determination of in situ cleavage of fluorescent sensor by chondrocytes. C) GAG
staining of sections from cell-laden hydrogels after 28 days of culture: nuclei stained
black and GAGs stained red. D) Collagen staining of sections obtained from cell-laden
hydrogels at day 28: nuclei stained black and collagen stained blue (scale bars: 100
μm). ............................................................................................................................ 76
Figure 3.1: Alginate showing a linkage between the mannuronic and guluronic acid.
.................................................................................................................................... 80
Figure 3.2: Schematic representation of the photopolymerization process of alginate-
methacrylate. a) After exposing the polymer solution to UV radiation, the
photoinitiators generated free radicals that react with the vinyl methylene starting the
crosslinking reaction; b) The reaction propagates with macro-radicals reacting with
unreacted carbon-carbon double bonds; c) At the end through a bimolecular
termination mechanism a 3D network of crosslinked hydrogel is formed. ............... 83
Figure 3.3: a) Non-functionalized alginate 1% w/v; b) Functionalized alginate 1% w/v
after 8 hours of reaction; c) Functionalized alginate 1% w/v after 24 hours of reaction.
The functionalization is confirmed by the presence of new peaks in the spectra at 5.63
ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82 ppm that
corresponds to the methyl group. ............................................................................... 85
Figure 3.4: a) Non-functionalized alginate 2% w/v, b) Functionalized alginate (2%
w/v) after 8 hours of reaction, c) Functionalized alginate 2% w/v after 24 hours of
reaction. The functionalization is confirmed by the presence of new peaks in the
spectra at 5.63 ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82
ppm that corresponds to the methyl group. ................................................................ 86
Figure 3.5: a) Non-functionalized alginate 3% w/v; b) Functionalized alginate 2% w/v
after 8 hours of reaction; c) Functionalized alginate 2% w/v after 24 hours of reaction.
The functionalization is confirmed by the presence of new peaks in the spectra at 5.63
ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82 ppm that
corresponds to the methyl group. ............................................................................... 87
Figure 3.6: Stress versus shear rate profiles for alginate-methacrylate solutions
containing different alginate-methacrylate concentrations, reacted for 8 hours. a) 1%
w/v of alginate; b) 2% w/v of alginate; c) 3% w/v of alginate, and d) comparison of
all compositions. ........................................................................................................ 88
Figure 3.7: Stress versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 24 hours. a) 1% w/v of alginate, b) 2% w/v of
alginate, c) 3% w/v of alginate, and d) comparison of all compositions. ................. 89
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Figure 3.8: Viscosity versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 8 hours. a) 1% w/v; b) 2% w/v; c) 3% w/v d)
comparison of all compositions. ................................................................................ 89
Figure 3.9: Viscosity versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 24 hours. a) 1% w/v; b) 2% w/v; c) 3% w/v
d) comparison of all compositions. ............................................................................ 90
Figure 3.10: 2% wt. Alginate solution reacted for 8 hours. a) Storage and loss modulus
vs strain b) Storage and Loss modulus vs frequency; c) Complex modulus vs
frequency; d) tan δ vs frequency. ............................................................................... 91
Figure 3.11: 2% wt. Alginate solution reacted for 24 hours. a) Storage and loss
modulus vs strain; b) Storage and Loss modulus vs frequency; c) Complex modulus
vs frequency; d) tan δ vs frequency. .......................................................................... 91
Figure 3.12: 2% wt. methacrylate alginate with different concentration of VA-086
photoinitiators functionalized for 8 hours a) 0.5% w/v of PI; b) 1% w/v of PI; c) 1.5%
w/v of PI; d) 0.05% w/v of PI. ................................................................................... 92
Figure 3.13: 2% wt. methacrylate alginate with different concentration of VA-086
photoinitiators functionalized for 8 hours a) 0.5% w/v of PI ; b) 1% w/v of PI; c) 1.5%
w/v of PI. .................................................................................................................... 93
Figure 3.14: 2% wt methacrylate alginate hydrogel with different concentration of
VA-086 functionalized for 8 hours a) 0.5% w/v of PI; b) 1% w/v of PI; C) 1.5% w/v
of PI. ........................................................................................................................... 94
Figure 3.15: 2% wt methacrylate alginate with different concentration of VA-086
functionalized for 24 hours. a) 0.5% w/v of PI; b) 1% w/v of PI; C) 1.5% w/v of PI.
.................................................................................................................................... 95
Figure 3.16: SEM images of crosslinked methacrylate-alginate hydrogel structures
obtained from alginate-methacrylate at different reaction times: 8 and 24 hours. ..... 96
Figure 3.17: Compression tests for alginate methacrylate samples (8h) with different
photoinitiator concentrations a) 0.5% w/v; b) 1% w/v; and c) 1.5 % w/v. ................ 96
Figure 3.18: Compression tests for alginate methacrylate samples (24h) with different
photoinitiator concentrations a) 0.5% w/v; b) 1% w/v; and c) 1.5 % w/v. ............... 97
Figure 3.19: Swelling and degradation rate for 2% wt. functionalized alginate (24 and
8) hours reaction time in a) distilled water b); degradation rate in distilled water; c)
DMEM; d) degradation rate in DMEM. ................................................................. 98
Figure 4.1: 1H NMR spectra of a) unmodified alginate and; b) 2% wt methacrylate
alginate (15 mL MA) after 8 hrs of reaction; c) 2% wt methacrylated alginate (25 mL
MA) after 8 hrs of reaction; d) 2% wt methacrylate alginate (15 mL MA) after 24 hrs
of reaction................................................................................................................. 103
Figure 4.2: Rheological characterization of 2 % wt methacrylate alginate samples. a)
Stress vs shear rate profile for samples functionalized for 8 hrs reaction time with
different methacrylate concentrations; b) Stress vs shear rate profile for samples
functionalized for 24 hrs reaction time with different methacrylate concentrations; c)
Viscoelastic behaviour low methacrylate concentration (15 mL); d) Viscoelastic
behaviour high methacrylate concentration (25 mL). .............................................. 105
Figure 4.3: Live/dead results at a) day 3, in AlgMA hydrogels; b) day 3, in the control;
c) day 7, in AlgMA hydrogels; d) day 7, in the control; and Alamar blue results e)
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Fluorescence intensity as a function of time for different time point (1, 3, 5 and 7 days).
Note: in the live/dead results green corresponds to live cells and red to dead cells.106
Figure 5.1: Schematic crosslinking mechanism of gelatin and methacrylate. ........ 110
Figure 5.2: 1H NMR spectra for non-functionalized and functionalized gelatin. (a)
Non-functionalized gelatin (b) GelMA functionalized for 2 hrs; c) GelMA
functionalized for 4 hrs; d) GelMA functionalized for 6 hrs. .................................. 114
Figure 5.3: Rheological behaviour of 10 and 15% wt of GelMA samples considering
2 and 6 hrs of functionalization time. (a)10% wt of GelMA functionalized for 2 hrs;
(b) 10% wt of GelMA functionalized for 6 hrs; (c) 15% wt of GelMA functionalized
for 2 hrs; (d) 15% wt of GelMA functionalized for 6 hrs. ...................................... 115
Figure 5.4: Oscillatory tests: storage and loss modulus of 10% wt GelMA for 2 and 6
hrs; (a) Amplitude sweep for 10 and 15% wt GelMA functionalized for 2hrs; (b)
Frequency sweep for 10 and 15% wt GelMA functionalized for 2hrs; (c) Amplitude
sweep for 10 and 15% wt GelMA functionalized for 6hrs (d) Frequency sweep for 10
and 15% wt GelMA functionalized for 6hrs. ........................................................... 117
Figure 5.5: Oscillatory results for GelMA hydrogel samples functionalized for 2 hrs
(a) Storage and loss modulus as a function of strain for 10 and 15% wt GelMA and
1% wt of PI; (b) Storage and loss modulus as a function of frequency for 10 and 15%
wt GelMA and 1% wt of PI; c) Storage and loss modulus as a function of strain for
10 and 15% wt GelMA and 1.5% wt of PI; d) Storage and loss modulus as a function
of frequency for 10 and 15% wt GelMA and 1.5% wt of PI. ................................ 118
Figure 5.6: Oscillatory results for GelMA hydrogel samples functionalized for 6 hrs
(a) Storage and loss modulus as a function of strain for 10 and 15% wt GelMA and
1% wt of PI; (b) Storage and loss modulus as a function of frequency for 10 and 15%
wt GelMA and 1% wt of PI; c) Storage and loss modulus as a function of strain for
10 and 15% wt GelMA and 1.5% wt of PI; d) Storage and loss modulus as a function
of frequency for 10 and 15% wt GelMA and 1.5% wt of PI. ................................ 119
Figure 5.7: Cross-section images of GelMA crosslinked structures considering
different GelMA concentrations, reaction times and PI concentration; (a) 10% of
GelMA, 2 hrs of functionalization time and 1% wt of PI; (b) 10% of GelMA, 6 hrs of
functionalization time and 1% wt of PI; (c) 10% of GelMA, 2 hrs of reaction time and
1.5% wt of PI; (d) 10% GelMA, 6 hrs of reaction time and 1.5% wt of PI; (e) 15% of
GelMA, 2 hrs of reaction time and 1% wt of PI; (f) 15% of GelMA, 6 hrs of reaction
time and 1% wt of PI; g) 15% of GelMA, 2 hrs of reaction time and 1.5% wt of PI; (h)
15% of GelMA, 6 hrs of reaction time and 1.5% wt of PI. ...................................... 120
Figure 5.8: Unconfined compression tests for gelatin methacrylate hydrogels samples
with different photoinitiator concentrations a) 10% wt GelMA functionalized for 2h
containing 1% wt of PI; (b) 10% wt GelMA functionalized for 2h containing 1.5% wt
of PI; (c) 10% wt GelMA functionalized for 6h containing 1% wt of PI; (d) 10% wt
GelMA functionalized for 6h containing 1.5% wt of PI. ......................................... 121
Figure 5.9: Swelling and degradation profiles as a function of functionalization time
for different functionalized gelatin methacrylate systems; a) Swelling in DMEM ; b)
degradation rate in DMEM. .................................................................................... 122
Figure 5.10: Live/dead images of adipose-derived mesenchymal stem cells
encapsulated in samples based on 10% wt GelMA dissolved at 1% wt of PI solution
and exposed to UV light (Light intensity of 8 mW/cm2) for 8 min a) After 3 days of
11
encapsulation; b) After 7 days of encapsulation; c) After 19 days of encapsulation.
Note: Green corresponds to live cells and red to dead cells. ................................... 123
Figure 5.11: Alamar blue fluorescence intensity at different time points (1, 3, 5 and 7
days) considering samples functionalized at two different reaction times (2 and 6 hrs)
.................................................................................................................................. 124
Figure 6.1: Photocrosslinking mechanism to form a) AlgMA and b) GelMA hydrogels
using UV irradiation. ................................................................................................ 129
Figure 6.2: Photocrosslinking of hybrid alginate-gelatin systems when exposed to UV
irradiation. ................................................................................................................ 130
Figure 6.3: Representative 1H NMR spectra of a) non-modified alginate, b) non-
modified gelatin, c) AlgMA, d) GelMA, and the hybrid Alg-Gel(MA) systems e)
75:25, f) 50:50, and g) 25:75. ................................................................................... 137
Figure 6.4: Viscosity vs share rate profiles of AlgMA, GelMA, and Alg-Gel(MA)
(25:75, 50:50, and 75:25) samples. .......................................................................... 138
Figure 6.5: Oscillatory results for pre-polymerized systems a) Storage and loss
modulus as a function of strain for AlgMA systems; b) Storage and loss modulus as a
function of frequency for AlgMA systems; c) Storage and loss modulus as a function
of strain for GelMA systems; d) Storage and loss modulus as a function of strain for
GelMA systems; e) Storage and loss modulus as a function of strain for hybrid
systems; f) Storage and loss modulus as a function of frequency for hybrid systems.
.................................................................................................................................. 139
Figure 6.6: Oscillatory results for polymerized systems a) Storage and loss modulus
as a function of strain for AlgMA systems; b) Storage and loss modulus as a function
of frequency for AlgMA systems; c) Storage and loss modulus as a function of strain
for GelMA systems; d) Storage and loss modulus as a function of strain for GelMA
systems; e) Storage and loss modulus as a function of strain for hybrid systems; f)
Storage and loss modulus as a function of frequency for hybrid systems. .............. 140
Figure 6.7: Cross-section images of different hydrogel systems a) AlgMA, b)
GelMA, c) Alg-Gel(MA) 75:25, d) Alg-Gel(MA) 50:50, and e) Alg-Gel (MA) 25:75.
Scale bar: 200 µm. ................................................................................................... 141
Figure 6.8: Swelling and degradation profiles of all hydrogel groups. a) Swelling ratio
profile and b) degradation (mass loss profile).......................................................... 143
Figure 6.9: Mechanical properties of different photocrosslinked hydrogel, a) stress-
strain curve; b) Young modulus. Legend: A-alginate; G-gelatin; H-Hybrid system.
.................................................................................................................................. 143
Figure 6.10: Cell viability of human chondrocytes encapsulated in AlgMA, GelMA,
Alg-Gel(MA) 50:50, and seeded on a TCP control at day 3, 7, and 16. Scale bar: 200
µm. ........................................................................................................................... 145
Figure 6.11: Fluorescence intensity indicating the metabolic activity of human
Chondrocytes in AlgMA, GelMA, Alg-Gel (MA) 50:50 and TCP control at days 1, 3,
5, 7 and 14. ............................................................................................................... 146
Figure 6.12: Histological analysis. a) Gomori; b) Aggrecan; c) Safranin-O production
at days 14, 21, 28 and 35 in Alginate methacrylate hydrogels, Gelatin methacrylate
hydrogels and hybrid system (50:50 Alg-Gel)MA. ................................................. 148
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Figure 6.13: Semi-quantification of the relative area of histological staining of the
AlgMA, GelMA, and Alg-Gel(MA) hydrogels at day 14, 21, 28, and 35 for a) Gomori
trichrome and b) aggrecan. ....................................................................................... 150
Figure 6.14: Assessment of GAG secretion in the photocrosslinked AlgMA, GelMA,
and Alg-GelMA hydrogels at day 7, 14, 21, 28, and 35. ......................................... 151
Figure 7.1: scaffold-based approach for tissue engineering. .................................. 155
Figure 7.2: a) Set-up of plasma-assisted bio-extrusion system; b) system diagram:
multi-extrusion system, plasma modification system and control system. .............. 159
Figure 7.3: a) Sequence of operations to fabricate hybrid PCL/hydrogel scaffolds; b)
Sequence of operations to fabricate full-layer plasma treated scaffolds. ................. 161
Figure 7.4: (a) Hybrid polycaprolactone (PCL)/hydrogel scaffold; (b) Scanning
electron microscopy (SEM) image of top view of PCL/hydrogel scaffold; (c) SEM
image of side view of PCL/ hydrogel scaffold; (d) photo of a full-layer N2 plasma-
treated PCL scaffold; (E) SEM image of top view of full-layer N2 plasma treated PCL
scaffold; (f) SEM image of filament surface of full-layer N2 plasma-treated PCL
scaffold. .................................................................................................................... 164
Figure 7.5: a) Temporal variation of fluorescence intensity of cell-seeded PCL
scaffolds with and without N2 plasma treatment; b) Confocal microscope images of
untreated and full-layer treated of cell seeded scaffolds, 1 day and 14 days after cell
culture. Scale bar 250 µm. ....................................................................................... 165
13
List of Tables
Table 2.1: Photocrosslinkable natural polymers used in cartilage tissue engineering.
.................................................................................................................................... 65
Table 3.1: Effect of reaction time on the modification degree of alginate methacrylate.
.................................................................................................................................... 85
Table 3.2: Rheological constants for solutions containing 15 mL of methacrylate and
different alginate concentrations, 24 h. ...................................................................... 88
Table 3.3: Rheological constants for solutions containing 15 mL of methacrylate and
different alginate concentrations, 8h. ......................................................................... 88
Table 4.1: Effect of reaction time on the degree of modification. .......................... 104
Table 5.1: Effect of reaction time on the degree of functionalization..................... 114
Table 5.2: Power law coefficients for different reaction time and GelMA
concentration. ........................................................................................................... 116
Table 6.1: Degree of functionalization for all functionalized group polymers. ...... 136
Table 6.2: Showing the hydrogel composition, experimental density, porosity, and the
average pore size. ..................................................................................................... 142
Table 7.1: Temporal variation of water contact angles for treated and untreated
scaffolds. .................................................................................................................. 165
14
List of Abbreviations
1D One dimension
2D Two dimensions
2PP Two-photon polymerisation
3D Three dimensions
3DP Three-dimensional printing
ASTM American Society for Testing and Materials
BASCs Brown adipose-derived stem cells
CAD Computer aided design
CaP Calcium phosphates
CGCaP Collagen–glycosaminoglycan
DAPI 4,6-diamidino-2-phenylindole
DEF Diethyl fumarate
ECM Extracellular matrix
FBS Fetal bovine serum
GelMA Gelatin methacrylate
hADSCs Human adipose-derived stem cells
hBMSCs Human bone marrow mesenchymal stem
cells
HCAECs Human coronary artery endothelial cells
hMSCs Human mesenchymal stem cells
hUVECs Human umbilical vein endothelial cells
hUVSMCs Human umbilical vein smooth muscle cells
IPN Interpenetrating Polymer Networks
MC Methylcellulose
MeCol Methacrylate collagen
MRI Magnetic resonance imaging
MSCs Mesenchymal stem cells
PBS Phosphate buffered saline
PBT Poly(butylenes terephthalate)
PCL Poly-ε-caprolactone
TGA Thermal gravimetric analysis
TGF Transforming growth factor
TIPS Thermally induced phase separation
15
TPU Thermoplastic polyurethane
UV Ultraviolet Light
VEGF Vascular endothelial growth factor
ACAN Aggrecan gene
ACI Autologous chondrocyte implantation
AlgMA Alginate methacrylate
DMEM Dulbello’s modified eagle medium
DMMB DMMB Dimethylmethylene blue
DNA Deoxyribonucleic acid
ECM Extracellular matrix
GAG Glycosaminoglycan
GelMA Gelatin-methacrylate
NMR (1H NMR) Nuclear magnetic resonance (Proton NMR)
FGF Fibroblast growth factor
HA Hyaluronic acid
HA-MA Hyaluronic acid methacrylate
Hep-MA Heparin methacrylate
KS Keratan sulfate
MAAh Methacrylic anhydride
MMP Matrix metalloproteinase
MSC Mesenchymal stromal cell
OA Osteoarthritis/osteoarthritic
PABS Plasma-Assisted Bio-extrusion System
PCL Polycaprolactone
16
List of Notations
�� Shear rate (s-1)
G' Storage modulus (Pa)
G'' Loss modulus (Pa)
ɳ Flow coefficient or consistency (Pa sn)
tanδ Loss factor
η Apparent viscosity (Pa∙s)
τ Shear stress (Pa)
17
Abstract
Articular cartilage is a load-bearing tissue that covers the ends of bone joints, acting
as a low-friction bearing surface and a mechanical damper for the bones. Articular
cartilage is a matrix-rich tissue with specialized cells (chondrocytes) that maintain the
structural and functional integrity of the extracellular matrix (ECM). An important
feature of cartilage is lacking self-repair ability and as a consequence, the zonal
structure and cartilage functions are often irreversibly lost following trauma and
disease. As a result, cartilage defects are prone to develop into predominant cartilage
disease osteoarthritis (OA), characterized by loss of cartilage, pain and debilitation.
The most common treatment for OA is joint replacement surgery, in which damaged
joint components are replaced by artificial prosthesis. This typically reduces the pain
and increases the mobility. However, over time such implants often fail and require
revision surgeries.
Tissue engineering has emerged as an alternative strategy to overcome the limitations
of traditional therapies by replacing the damaged part of cartilage tissue with a
biofabricated cartilage tissue for long-lasting periods and holds great promise as an
effective treatment for cartilage repair. However, most of the approaches in this field
focus on the use of single material structures, not able to mimic the real structure of
cartilage. This research project focus on the design and fabrication of novel multi-
material cartilage replacement by using two different hydrogels (alginate, gelatin) and
a hybrid system based on the combination of both alginate and gelatin. These
materials were successfully functionalized with methacrylate anhydride allowing them
to be processed through UV photopolymerization. The effect of polymer
concentration, methacrylated anhydride concentration and functionalization reaction
time was investigated allowing to tailor rheological and viscoelastic properties. Pre-
polymerized polymeric solutions were also prepared considering different
concentrations of photoinitiators. Mechanical, swelling and degradation
characteristics of these different systems were determined allowing to identify the
most suitable compositions for each single polymer system. Additionally, the ability
of each system to be used as a cartilage bioink was further investigated through
live/dead assay using human chondrocyte and mesenchymal stem cells. Finally, the
novel hybrid system proposed by this research was further investigated in terms of its
18
composition (ratio between gelatin and alginate) and a detailed biological study was
preformed not only to investigate the ability of this system to support cell growth and
cell-cell network formation but also the ECM formation through the quantification of
GAGs, Collagen and aggrecan. Results show that the developed systems can be used
as bioinks, their properties can be easily tailored and that the novel hybrid system,
which overcomes the main limitations of each individual system, is a promising bioink
material to support cartilage formation.
19
Declaration
I declare that no portion of the work referred to in the dissertation has been submitted
in support of an application for another degree or qualification of this university or
any other university or other institute of learning.
Hussein Mishbak
2019
20
Copyright
i. The author of this thesis (including any appendices and/or schedules to this
thesis) owns certain copyright or related rights in it (the “Copyright") and
she/he has given The University of Manchester certain rights to use such
Copyright, including for administrative purposes.
ii. Copies of this thesis, either in full or in extracts and whether in hard or
electronic copy, may be made only in accordance with the Copyright.
Designs and Patents Act 1988 (as amend) and regulations issued under it
or, where appropriate, in accordance with licensing agreements which the
University has from time to tie. This age must form part of such copies
made.
iii. The owner of certain copyright, patents, designs trademarks and other
intellectual property (the \Intellectual Property") and any reproductions of
copyright works in the thesis, for example graphs and tables
(\Reproductions"), which may be described in this thesis, may not be
owned by the author and may be owned by third parties. Such Intellectual
Property and Reproductions cannot and must not be made available for use
without the prior written permission of the owner(s) of the relevant
Intellectual Property and/or Reproductions.
iv. Further information on the conditions under which disclosure, publication
and commercialisation of this thesis, the Copyright and any Intellectual
Property and /or Reproductions described in it may take place is available
in the University IP Policy (see
http://documents.manchester.ac.uk/DocuInfo.aspx?DocID=487 ), in any
relevant Thesis restriction declarations deposited in the University Library.
The University Library’s regulations (see
http://www.manchester,ac,uk/library/aboutus/regulations) and in the
University’s policy on presentation of Theses.
21
Acknowledgements
First and foremost, I would like to express my gratitude to my advisor and supervisor
Prof. Paulo Jorge Bartolo. He has guide me through this PhD journey with lots of
support and patience. Taught me, both consciously and unconsciously, how great
experimental work is done and most importantly, how to take advantages of any
challenge that I experienced. In brief, I would consider myself very lucky to have such
a supervisor, not only for his tremendous academic support, but also for giving me so
many wonderful opportunities. Secondly, Special thanks goes to my co-supervisor,
Dr. Glen Cooper for his great support and encouragement. I was so fortunate to receive
their guidance, endless support and encouragement for all these years.
I’m also grateful to Dr. Carl Diver, Dr Liu, Dr Bo, Dr David and Ms. Svetlana
Kuimova for their support throughout these years
I would like to thank all members of staff at the University of Manchester for providing
me with a perfect working environment all these years. Special thanks to the
Manufacturing Centre in the School of MACE and those fantastic technicians: Eddie,
Kevin, Bill, Ross, Tony, Rus, Marie and Jack, and to the managers Stuart and Phil.
Special thanks goes to Stuart Mores, Maria and Louise from Materials School.
I am grateful to all colleagues in my research group: Cian, Salam, Enes, Mohammed,
Vag, Alex Pinar and Tom. Their daily support, friendship and our discussion helped
me to move forward. My time at Manchester was made enjoyable in large part because
of you, thanks for being part of my life. Big thanks to all my friends, old and new, who
have made the last few years so enjoyable.
I would like to acknowledge the support of the Government of Iraq for supporting this
PhD through a grant provided by Higher Committee for Development Education Iraq
(HCED). This work was also partially performed within the framework of the
SKELGEN project – Establishment of a cross continent consortium for enhancing
regenerative medicine in skeletal tissues (Marie Curie Action, International Research
Staff Exchange Scheme (IRSES) – Project reference: 318553).
Last but not least, I would like to acknowledge from the bottom of my heart the endless
love and support of small family, my lovely supportive wife (Najlaa) who was always
in my side in the good and bad days, my children (Bilal and Layaan). Special thanks
to my parents who supported me through my whole life during this journey since the
22
primary school till now. My brothers and Sisters and all my big family. They all kept
me moving forward and without them it would be very difficult to successfully
complete my PhD.
23
وثمرة إلحبيبة ، زوجتيإلغاليين وإلدي لى إ
بلال و ليان ولاديأ فؤإدي
24
Graphical abstract illustrating this research work focusing on material preparation and
characterization, and bioprinting of multi-material cell laden constructs for cartilage
tissue engineering.
25
Chapter 1 Introduction
26
1.1 Background
Millions of people around the world have experienced cartilage disease through
accidents, such as a tear to the anterior cruciate ligament (ACL), trauma, joint injuries
and abnormal joint loading, or due to ageing such as, degenerative joint diseases, that
can develop into osteoarthritis. Osteoarthritis (OA) is the most common disease
affecting cartilage tissue (1). When the hyaline cartilage is completely damaged, this
means that the joint surface may no longer be smooth to facilitate bone movement.
Despite new therapies have been developed to treat cartilage diseases, articular
cartilage repair is still a major clinical challenge. This is particularly critical since
cartilage presents very limited capacity to naturally heal due to its avascular nature
and relatively low cellular mitotic activity. Moreover, there are no available therapies
for long term treatment of articular cartilage damages. This is a very active field of
research and new therapeutic techniques are being developed not only to treat
damaged or diseased joint cartilage tissue but also to achieve and restore functional
normal cartilage that will give long-lasting improvements and allow patients to return
to a fully active lifestyle. Particularly relevant to this field is the concept of tissue
engineering (TE), combining the knowledge of engineers, biologists, material
scientists, and clinicians towards the development of biological substitutes that restore,
maintain, or improve the function of tissues (2). For cartilage applications, the
combined used of biodegradable and biocompatible materials, cells and growth factors
and the use of additive biomanufacturing systems, present high potential to create
customised cartilage replacements. In this case, three-dimensional biocompatible and
biodegradable structures (hydrogel-based scaffolds) are normally used and designed
considering the following requirements (3):
• The designed structure must allow cells to accommodate, proliferate and
differentiate.
• Support the metabolic activity of cells serving as a template for cells to
produce their own extra-cellular matrix (ECM);
• Provide an adequate mechanical and biological environment promoting tissue
regeneration.
In this context, the aim of hydrogel-based 3D constructs is to direct cartilage cells
(chondrocytes) to grow, mature, and build their own ECM mimicking the native
cartilage tissue (4, 5). Besides chondrocytes, non-differentiated stem cells are also
27
used together with specific growth factors (transforming growth factor beta
superfamily) to promote chondrogenesis (6).
Two approaches have been considered for cartilage tissue engineering, the use of
scaffolds seeded with cells or the use of bioinks (hydrogels encapsulating cells) (7).
Both approaches strongly depend on both the characteristics of the biomaterials being
considered and the fabrication processes. The scaffold-based approach is the most
commonly used but requires a pre-culture phase in a bioreactor before implantation,
while the fabrication of cell laden constructs allow the development of in situ printing
strategies (5).
The use of additive manufacturing for cartilage applications is a relatively new
approach. Most of the studies focused on the use of extrusion-based or pressure-
assisted additive manufacturing systems with or without cells (8, 9). Interesting results
were obtained in terms of the design of scaffolds (it is clear from the literature that
porous scaffolds for cartilage applications require small pores in comparison to bone
scaffolds) and cell differentiation (positive effect of hypoxia conditions) (9).
Additionally, most of these studies used hard materials (e.g. polycaprolactone) or very
soft materials (e.g. collagen), not able to completely simulate the mechanical
behaviour of cartilage and compromising the stability of any constructs. Besides this,
up till now, very few studies investigated the combined used of different materials to
create a structure mimicking cartilage. Naturally derived polymers such as alginate,
agarose, gelatin and collagen have been investigated as a single material system. Most
of these polymers are non-covalently crosslinked or ionically crosslinked, which could
be considered a major challenge since the produced hydrogels are weak and the gelling
conditions complex. Hybrid systems combining naturally derived and synthetic
polymers have also been investigated to overcome some mechanical and degradation
limitations of natural polymers (10, 11). Hybrid systems based on natural polymers
with tailored properties represents a novel area of research.
1.2 Research aim and objectives
The common problem with all available clinical strategies for cartilage repair is their
limitation to fully repair damaged cartilage providing long-term treatment. Usually,
they are expensive strategies and not appropriated to be applied in children. Thus,
tissue engineering is an alternative approach to overcome the problems of traditional
28
therapies by replacing the damaged part of cartilage tissue with a biofabricated
engineered cartilage tissue for long-lasting periods of time.
The aim of this research project is to design and evaluate a novel cell-laden multi-
hydrogel able to provide a temporospatial environment that could form
functional cartilage. This cell-laden, produced using additive manufacturing, is based
on biodegradable and biocompatible hydrogels resembling the structure of cartilage,
with tuneable mechanical and biodegradability properties able to support cells,
promote cell-cell interactions and the formation of ECM and processed under mild
and physiological conditions.
This construct is based on two different polymer materials (alginate and gelatin), one
for the superficial zone and the other for the deeper region of cartilage) and a hybrid
system obtained by mixing both alginate and gelatin for the transitional zone. Alginate
and gelatin were selected due to their biocompatibility, biodegradability properties,
easy to process under mild conditions and low cost.
Both alginate and gelatin were functionalized with methacrylate anhydride (MA) to
introduce photoreactive sites into the polymer backbone to produce
photocrosslinkable constructs. Ultraviolet (UV) photopolymerization was selected to
induce rapid gelation, allowing to control the polymeric network properties such as
crosslinking density, matrix stiffness and cell encapsulation by tuning the
photopolymerization parameters (e.g. light intensity, wavelength, photinitiator and
polymer concentration, and exposure time). Key research challenges considered to
design the cartilage constructs are related to the mechanical properties of produced
constructs, photoinitiator concentration, biological effect of the unsaturated degree,
cell exposure to UV radiation and cytotoxicity of both photoinitiators and unreacted
polymers.
To achieve the research aim, the following research objectives were considered:
✓ Objective 1: understand cartilage structure and its role, main clinical problems
and treatment strategies; investigate current biofabrication technologies,
suitable materials and design requirements to produce a bioink for cartilage
regeneration;
✓ Objective 2: select and functionalize polymeric materials and develop a
suitable approach for cartilage regeneration by investigating two different
hydrogels and the combination of both polymers into a hybrid system able to
functionally mimic the articular cartilage structure, composition and
29
properties. Variations in polymer concentration, methacrylate anhydride
concentration and degree of substitution can provide hydrogels with tunable
and controllable properties;
✓ Objective 3: establish a correlation between process conditions and
morphology, mechanical and biological properties of 3D polymeric constructs
and the capacity of producing a functional engineered cartilage replacement;
✓ Objective 4: quantify the optimal composition, conditions, biomechanical,
biophysical and biochemical properties of tailored polymeric constructs for
better ECM matrix production.
✓ Objective 5: develop a new tissue engineering approach to enable the
neocartilage formation fully anchored to the underlying subchondral bone.
In order to achieve the research aims and objectives four main research phases were
considered:
❖ Material design (phase 1) – Selected polymeric systems must be
functionalized in order to be photopolymerizable. Functionalization
corresponds to the introduction of unsaturations (C=C sites) into the hydrogel
structure through the use of methacrylate. Solutions containing different
concentrations of alginate or gelatin mixed with different concentrations of
methacrylate during different reaction times were prepared. Proton nuclear
magnetic resonance 1HNMR is used to assess the equivalent unsaturation level
and to confirm the functionalization process. The level of unsaturation has an
impact on the processability of these materials and crosslinked density, which
determines the mechanical properties and free volume available for cell
encapsulation, viability and proliferation.
❖ Photopolymerization process (phase 3) – Low light intensity values and low
concentrations of free-radical photoinitiators are considered. Photocurable
polymers prepared in phase 1 are mixed with different concentrations of
photoinitiator and polymerised at different light intensity values, by changing
the distance between the material and the light source. The curing kinetics and
mechanical properties are assessed as a function of light intensity and
photoinitiator concentration.
❖ Printing optimisation (phase 2) – The rheological and viscoelastic properties
of the prepared solutions are critical. High viscous materials and Newtonian
formulations require high pressures during the printing process, which might
30
induce significant shear stresses on encapsulating cells. During this phase a
general understanding on the effect of the material design characteristics on
the rheological properties is obtained.
❖ Biological assessment (phase 4) – Human chondrocytes and/or human
mesenchymal stem cells (hMSC) were encapsulated on those three different
bioink systems (alginate, gelatin and hybrid systems), before
photopolymerization. The production of glycosaminoglycan, Collagen
secretion, and the formation of cell networks were studied. Histological
analysis is used to semi quantify the gene expression in the deposited ECM in
the hydrogel constructs.
1.3 Thesis outlines
This thesis, based on published and submitted papers and book chapters, comprises
eight Chapters, which progress in accordance with the identified research objectives.
Besides this introductory Chapter, which presents the current research context,
research aims and objectives, the remaining chapters can be summarized as follows:
Chapter II: State-of-art in cartilage tissue engineering;
This Chapter, focusing on objective 1, comprises two sections. First, it overviews the
problem being addressed by this research, describing the cartilage structure and
composition, main clinical problems, and most commonly used clinical approaches. It
discusses also the concept of tissue engineering, presenting the key requirements of
cartilage tissue engineering constructs. The second Section provides an overview on
recent advances in the design and engineering of naturally derived photocrosslinkable
hydrogels for cartilage tissue engineering. Hydrogel properties, synthesis routes,
crosslinking methods, and strategies for hydrogel bio-functionalization are described
and future research perspectives discussed.
Chapter III: Development and characterisation of a photocurable alginate bioink
for 3D bioprinting
This Chapter, focusing on the research objectives 2 and 3, investigates the preparation
of alginate-based systems for UV bioprinting applications. The material is
characterised before and after the polymerisation (curing) process and the effect of
both functionalization time and photoinitiator concentration on the rheological,
mechanical, morphological, swelling and degradation properties are investigated.
31
Chapter IV: Photocurable alginate bioink development for cartilage replacement
bioprinting
This Chapter, focusing on the research objectives 2 and 3, investigates the use of the
photocurable alginate presented in Chapter 3 as a carrier of chondrocyte cells for
cartilage repair. Different methacrylate concentration and reaction times are
considered and their effects on the degree of substitution, rheological and biological
properties investigated. Alginate methacrylate cell laden constructs were produced,
and preliminary cytotoxicity and cell proliferation tests performed using the live/dead
assay.
Chapter V: Photocrosslinkable gelatin methacrylate (GelMA) hydrogels:
towards 3D cell culture and bioprinting for cartilage applications
This Chapter, focusing on the research objectives 2 and 3, investigates the use of
photocurable gelatin to encapsulate human adipose-derived stem cells. Gelatin is
functionalised and the level of functionalisation is investigated. Material preparation
and characterisation is discussed. The influence of the functionalisation time, polymer
concentration, degree of modification and viscoelastic behaviour on the mechanical
strength and cell viability is also discussed.
Chapter VI: Development and characterisation of a photocurable alginate-
gelatin bioink for cartilage applications
This Chapter, addressing the research objectives 2 and 4, investigate a novel hybrid
alginate/gelatin photocrosslinking hydrogel system. The synthesis, morphological,
rheological, mechanical and biological characterisation is detailed.
Chapter VII: Hybrid PCL/Hydrogel scaffold fabrication and in-process plasma
treatment using PABS;
This Chapter, addressing the research objectives 4 and 5, investigates the use of a novel
plasma-assisted bio-extrusion system (PABS), to produce multi-material scaffolds for
the interface between the subchondral bone and cartilage, consisting in a synthetic
biopolymer (polycaprolactone) and a hybrid natural hydrogel system (previously
described in Chapter 6). The Plasma-Assisted Bio-extrusion System (PABS),
developed at the University of Manchester, is also used for the scaffold surface
modification (N2 plasma modification).
Chapter VIII: Conclusions and future work.
32
This Chapter provides an overall summary of the thesis and the main conclusions that
can be drawn from the research work carried out. Possible future directions for
research following on from this thesis are also presented.
The structure of this thesis is illustrated in Figure 1.1
Figure 1.1: Framework structure of this thesis.
33
Chapter 2
State-of-the- art of
Cartilage Tissue
Engineering
34
This Chapter, which provides the current state-of-the-art on cartilage tissue
engineering comprises two main sections. The first section overviews the problem
being addressed by this research, describing the cartilage structure and composition,
and the most commonly used clinical approaches presenting their main advantages
and limitations. It discusses also the concept of tissue engineering, presenting the key
requirements of cartilage tissue engineering constructs. The second section provides
an overview on recent advances in the design and engineering of naturally derived
photocrosslinkable hydrogels for cartilage tissue engineering. Hydrogel properties,
synthesis routes, crosslinking methods, and strategies for hydrogel
biofunctionalisation are described and future research perspectives discussed.
Therefore, these two Sections covered the two main cartilage tissue engineering
approaches, scaffold-based and cell laden (bioprinting), covered by this research.
Biological perspectives and current strategies in osteochondral
tissue engineering †
Articular cartilage and the underlying subchondral bone are crucial in human
movement and when damaged through disease or trauma results in a severe impact on
quality of life. Cartilage has a limited capacity to regenerate due to the avascular
composition of the tissue and limited efficacy of current therapeutic interventions.
Worldwide the numbers of patients requiring therapy for osteochondral indications is
rising due to an ageing population, thus increasing the pressure on healthcare systems.
Subsequently, research into new therapies especially using the principles of tissue
engineering is increasing. However, a basic understanding of the biological
composition, structure, and mechanical properties is required. Furthermore,
consideration of material design, architecture, biomanufacturing strategies, and the
role of experimental standardisation is needed to help develop tissue engineering
therapies that can be successfully translated into the clinic.
This Section provides an overview of the biological properties of osteochondral tissue
and the role of tissue engineering principles in developing new therapies is provided.
† This Section is based on the paper: Hussein Mishbak, Cian Vyas, Glen Cooper, Ruben Pereira, Chris
Peach, Paulo Bartolo, “Osteochondral tissue: a biological and mechanical review for tissue
engineering”, Biomanufacturing Reviews, Springer, in Press.
35
Introduction
Osteochondral tissue is composed of articular cartilage, a specialized tissue that covers
the distal ends of the bones in articulating joints, and the subchondral bone which
anchors the cartilage to the underlying bone (12-16). Articular cartilage has a highly
flexible and lubricated surface to reduce frictional forces during movement and
facilitate smooth articulation. The tissue enables the transmission of mechanical loads
from movement to the skeleton (17-20). Osteochondral tissue is composed of distinct
regions with articular cartilage, comprising the majority of the structure, and an
underlying subchondral bone phase.
Articular cartilage is avascular and aneural with low metabolic activity and thus
trauma or diseases (e.g. osteoarthritis and rheumatoid arthritis) are difficult to treat
due to the inherent inability of articular cartilage to self-regenerate in comparison to
the greater healing capacity of bone (Figure 2.1) (20). A thorough understanding of
the composition and structure of the tissue will enable superior tissue engineering
approaches to be explored to solve the clinical challenges of osteochondral defects.
Current clinical approaches, typically palliative, are ineffective and the tissue either
continues to degrade, resulting in total replacement with an implant, or fibrocartilage
is formed. Tissue engineering approaches have been widely explored to develop new
approaches to repair and regenerate the tissue. However, to date these have been
unsuccessful in producing mature articular cartilage. The current fundamental
approaches based on scaffolds (acellular and cellular), biomaterials, and cells may
need to be revaluated to understand why these approaches consistently fail in
producing a relatively simple and thin tissue, although exhibiting a highly complex
hierarchical organisation (21). Adult articular cartilage tissue takes over 20 years to
mature and the tissue generated once produced does not turnover or regenerate unlike
other tissues in the body. The cartilage tissue produced during childhood is the same
throughout a person’s lifetime. Malda et al. suggest that new approaches must
appreciate this fundamental aspect of cartilage tissue physiology which may require
the incorporation of permeant non-degradable structures to support the major
mechanical properties required of the tissue and the restoration of the
microenvironment (cytokines, growth factors, and mechanical loading profiles) in the
early stages of development (fetal and childhood) to recapitulate the developmental
processes which generate the correct articular cartilage tissue (21). Furthermore,
elucidating the underlying processes of cartilage development will provide a
36
mechanistic understanding that can be utilised in tissue engineering approaches for
cartilage regeneration.
Figure 2.1: Comparison between the physiology and healing capacity of bone and
cartilage. Cartilage is avascular tissue so lacks ready access to a supply of circulating
stem cells and nutrients so relies on the synovial fluid for nourishment. This combined
with its largely acellular composition and low metabolic activity results in a nearly
complete lack of innate regenerative capacity. Consequentially, defects fail to heal,
and clinical interventions typically result in the formation of inferior fibrocartilage. In
contrast, bone has a greater ability for self-repair due to the constant tissue remodelling
by osteoblasts and osteoclasts. Bone is also a highly vascularised tissue which allows
a ready supply of nutrients and proteins that stimulate bone repair. Furthermore, there
is a large source of stem cells in the bone marrow and periosteum which are able to
differentiate into bone producing cells. This allows bone to heal defects up to a certain
critical size after which vascularisation becomes an issue. Image from reference (20).
Composition of articular cartilage
There are three forms of cartilage in the human body which are fibrocartilage (22),
elastic cartilage, and hyaline cartilage each with their own specific biological,
mechanical, and structural properties (23). Hyaline cartilage is a thin connective tissue
present at synovial joints such as the knee, elbow, shoulder, and hip where it covers
the bearing surface of the underlying bone and is termed articular cartilage (24). Thus,
37
hyaline cartilage provides an efficient load bearing surface that has a low friction
coefficient thus lubricating the movement of joints and can support load transfer of up
to six times the human body weight in the knees (17). The complex, nonlinear,
viscoelastic, anisotropic, and heterogeneous structure and composition of cartilage
enable these vital properties (25, 26).
Adult articular cartilage consists of predominately extracellular matrix (ECM),
approximately 95–99% of the total volume, which itself consists of 80% water and
20% solid contents (27). The solid content is mostly comprised of collagens (50-75%),
proteoglycans (15-30%), and a small amount of non-collagen proteins (24, 28). Cells
account for a small percentage of the total volume (1-5%) and consist of only a single
cell type, chondrocytes (29). The composition of articular cartilage changes as the
tissue matures from initial formation during embryogenesis to final maturation (18-21
years old) (30).
The mature tissue has a low density of chondrocytes in a low proliferative and
metabolic state, and are isolated from each other, so lack cell-cell interactions due to
being encapsulated in the pericellular matrix (19). This is partly responsible for the
low healing capacity of mature articular cartilage. However, the mature chondrocyte
has an important role in the tissue homeostasis by coordinating and producing the
ECM components. The morphology, orientation, and phenotypic expression of
chondrocytes are depth and biomechanically dependent as the cells are influenced
through mechanotransduction (31, 32). This results in the wide range of morphologies
observed, which range from rounded, elongated, flattened, and hypertrophic, all within
the same tissue (33).
The collagen network in articular cartilage is highly organised and primarily
composed of collagen type II (~50% dry weight of articular cartilage) (25). The
organisation is depth dependent in the tissue and is partly responsible for the
biomechanics, especially the tensile and compressive properties (26). The fibre
diameter increases from the articular surface through the depth of the tissue
(superficial zone ~ 55 nm, middle zone ~ 87 nm, and deep zone ~ 108 nm) (34).
Although collagen type II is the main collagen (95% of total collagen), there are other
collagens present such as type I, II, VI, IX, X, and XI. Collagen type I is present in
small amounts only in the superficial zone but can be found abundantly in
fibrocartilage so can be used as a useful indicator of fibrocartilage formation (35-37).
Subsequently, the ratio between collagen I and collagen II can be used as a marker to
38
assess the status of the cartilage tissue as chondrocytes cultured in vitro monolayer
express higher levels of collagen type I indicating that the chondrocytes have
undergone dedifferentiation (32). Collagen IX and XI are found throughout the tissue
in small amounts and are involved in crosslinking between fibrils, regulation of fibril
size, and interactions with other biomolecules (25). Collagen X is found in the deep
and calcified zones and is believed to have a role in the mineralisation between the
cartilage and the subchondral bone (38, 39). A major non-collagenous component of
the ECM is proteoglycans and glycosaminoglycan’s (GAGs) (17). Proteoglycans
consist of a core protein that is heavily bound with covalently attached polysaccharide
chains, GAGs. Aggrecan is a main proteoglycan within articular cartilage and is
covalently attached to negatively charged GAGs, keratan sulphate and chondroitin
sulphate. This is able to bind multiple times to a hyaluronic acid backbone to form
aggrecan-hyaluronan aggregates which are highly negatively charged (40, 41). The
negative charge on this proteoglycan aggregate, and other proteoglycans, causes an
osmotic pressure to be generated as water is taken in and entrapped which causes
swelling (38). This turgidity produced by the network of proteoglycans and combined
with the structural confinement caused by the organisation of collagen results in a high
compressive modulus (14, 32). Subsequently, as the concentration of proteoglycans
increases with depth in articular cartilage towards the subchondral bone region, the
water content and swelling pressure rises, thus the compressive modulus of the tissue
increases (42-45). This enables articular cartilage to have a high mechanical load
bearing capability which can transfer and distribute loads effectively (46).
Structure of osteochondral tissue
Articular cartilage has a hierarchical organisation from the nanoscale to the macroscale
with a distinct zonal structure. Each zone has its own specific ECM composition,
biomolecule orientation, chondrocyte shape and organisation (47), imparting specific
biomechanical characteristics (Figures 2.2 a, b and c). These zones are termed,
descending from the articulating surface, the superficial or tangential zone, the middle
or transitional zone, the deep or radial zone, and the calcified zone, before the articular
cartilage gives way to the subchondral bone region. Furthermore, there is a microscale
radial organisation surrounding the chondrocyte termed the chondron which has a
unique composition depending on the distance from the chondrocyte (Figure. 2.2b).
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Zonal structure of articular cartilage
On the articular surface and above the superficial zone is a thin layer, ranging from a
few hundred nanometres to a micrometre, termed the lamina splendens which is
acellular and composed of proteins (48). Although the structural role is unclear it is
thought that the gradual build-up of proteins from the synovial fluid acts as a protective
and low friction interface for the articular cartilage surface (35).
Immediately below the lamina splendens is the superficial zone (10-20% of cartilage
thickness) which comprises small diameter collagen fibres (predominately type II and
IX) that are organised parallel to the articular surface and densely packed. This allows
a low coefficient of friction, which enables smooth movement of the joint and imparts
the ability to withstand both the high tensile and shear stresses that the articular
cartilage encounters under loading. The chondrocytes are densely packed and arrange
themselves along the collagen fibres parallel to the surface, displaying a flattened
morphology. Chondrocytes also secrete proteins such as superficial zone protein (SPZ,
also known as lubricin or PGR 4) and collagen I which act as lubricants (25, 49-51).
Figure 2.2: Hierarchical and graded composition, structure, and properties of
osteochondral tissue. a) Procollagen polypeptides bind together to form collagen that
assemble into microfibrils and then fibrils which can be crosslinked together by
collagen type IX. Collagen fibrils exhibit a characteristic banding pattern of ~67 nm
due to the staggered packing arrangement of collagen. Image from reference (36). b)
Molecular composition and arrangement of the chondron depicting the pericellular,
territorial, and interterritorial matrix with increasing distance from the chondrocyte.
Image from reference (37). c) Zonal structure and properties of osteochondral tissue.
Image adapted from (52).
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SPZ is a potential marker to identify this zone. The amount of proteoglycans is low
compared to the other zones which increases the permeability, thus resulting in
compressive strains of up to 50% and high fluid flow which influences the
compressive properties of the entire cartilage tissue (25, 26, 40, 52).
Below the superficial zone is the middle zone (40–60% of cartilage thickness), which
is predominately composed of collagen II fibres randomly arranged and displaying a
larger diameter than the superficial zone. Chondrocytes are present at a lower density,
have a rounded morphology, and also express large quantities of collagen II and
aggrecan. A marker for this zone is the cartilage intermediate layer protein which is
expressed throughout this zone (39). This zone also has the highest concentration of
proteoglycans especially aggrecan (52, 53).
The deep zone (20-50% of cartilage thickness) is comprised of the largest diameter
collagen fibres that are oriented perpendicular to the subchondral bone region with the
chondrocytes organised along the collagen fibres in columns with an elongated
morphology. The cells themselves are present in lower density compared to the other
zones and express lower levels of collagen II (53, 54).
The final zone before the subchondral bone region is the calcified zone which is
distinguished from the deep zone by the presence of a tidemark which demarks the
boundary between calcified and non-calcified regions (55, 56). The zone anchors the
collagen fibres of the deep zone to the subchondral bone thus integrating the cartilage
to the underlying bone. This also provides an interface between the hard phase of bone
and the soft phase of cartilage since the presence of hydroxyapatite reduces the
mechanical gradient between the phases (25, 41, 57). The calcified zone also has the
highest number of chondrocytes which are in a hypertrophic state.
The final zone of the osteochondral tissue is the subchondral bone which lies directly
below the calcified zone and separates the articular cartilage from the bone marrow.
This zone consists of the bony lamella (cortical endplate) and the subarticular
spongiosa, the supporting trabeculae and bone components, which is separated from
the calcified zone of articular cartilage by a cement line (58, 59). The subchondral
bone differs markedly in composition and structure to the articular cartilage. The
subchondral trabeculae are highly vascularised which enables transportation of
nutrients, gases, and waste through channels which cross the subchondral bone plate
and enter the calcified zone, which is entirely reliant on the synovial fluid as a source
of nutrients if these channels are absent (58, 59). The main collagen is type I due to
41
the tissue being mineralised bone. These collagen fibres do not cross between the
calcified cartilage and subchondral bone so does not act as an anchor as occurs with
collagen fibres that cross the tidemark and connect the non-calcified and calcified
cartilage. Furthermore, the subchondral trabecular structure and mechanical properties
are anisotropic and can dynamically remodel itself to respond to applied forces (60-
62). The main function of the subchondral bone is to maintain joint shape and provide
mechanical support since it has a high compressive modulus and is impermeable so is
able to stabilise the tissue and distribute the applied mechanical forces (25, 40, 58, 63,
64). Furthermore, the subchondral bone acts as a nutrient source for articular cartilage
which is not vascularised itself (43).
Current osteochondral treatments
The zonal structure of osteochondral tissue and the innate inability of articular
cartilage for self-regeneration poses a problem for clinical interventions.
Subsequently, a variety of both clinical treatments are available with different degrees
of success and tissue engineering approaches are currently in clinical trials (65, 66).
The type of treatment used will depend on the defect category, stage, size, and
location. Osteochondral defects are commonly classified by the Outerbridge
classification system which indicates the severity of a lesion (67). This system
classifies defects from grade I-IV, where a grade 0 defect is normal healthy articular
cartilage; grade I indicates swelling and softening of the tissue; grade II indicates a
partial thickness defect with a diameter less than 1.5 cm; grade III defect has a
diameter greater than 1.5 cm and presents as a full thickness lesion up to the
subchondral bone; and grade IV is a full thickness defect that exposes the subchondral
bone.
The main treatments currently used clinically are classified into (1) microfracture, (2)
autologous chondrocyte implantation (ACI), (3) matrix-induced autologous
chondrocyte implantation (MACI), and (4) osteochondral auto- and allografts as
shown in Figure 2.3 (18, 44, 68). These approaches mainly utilise in vivo methods to
repair and regenerate the tissue in situ.
Microfracture is a technique that has been used clinically since the 1980s to produce
fibrocartilage in articular cartilage defects (69, 70). The technique recruits MSCs from
the bone marrow by drilling into the subchondral bone. The defect area is debrided to
ensure a clean and stable margin before drilling into the subchondral bone. This
42
induces bleeding into the defect area which forms a fibrin clot that contains MSCs
which subsequently remodels into fibrocartilaginous tissue over a period of 12-16
months. This long period of remodelling requires a lengthy postoperative
rehabilitation period with limited mechanical loading (51, 71).
Figure 2.3: Current treatment options for cartilage regeneration. a) A full-thickness
chondral lesion (Grade III). b) Debridement of the lesion is used as precursor to more
invasive procedures as it removes damaged cartilage and bone to create a healthy
border which enables improved integration of neotissue with native tissue. In smaller
cartilage defects debridement may be used without further procedures as a minimally
invasive treatment option. c) Microfracture is treatment that drills into the subchondral
bone to create channels that allow MSCs to migrate into the defect. d) Autologous
chondrocyte implantation (ACI) uses a population of 12-48 million autologous
chondrocytes to which are inserted into the defect which is then covered with either a
periosteal patch or a collagen membrane. e) Matrix-induced autologous chondrocyte
implantation (MACI) is a development of the ACI technique. The autologous
chondrocytes are cultured in vitro and seeded onto an absorbable 3D scaffold (collagen
or hyaluronic acid) before being implanted into the defect and fixed to the defect with
fibrin glue. Image from reference (37).
Although considered the gold standard by the FDA and some clinicians, the long-term
outcomes for joint functionality using microfracture technique show limited
improvement (49, 50). This is due to the inferior biomechanical and biochemical
properties of fibrocartilage compared to hyaline cartilage, which creates a mismatch
between the native tissue and the neotissue (52, 72). The treatment provides a short-
term benefit to the patient but only postpones cartilage degeneration as the repair tissue
typically deteriorates approximately 18-24 months after surgery (52). Subsequently,
five years after surgery the likelihood of treatment failure is high irrespective of the
cartilage defect (49, 50). This technique can also be combined with other treatment
43
methods and an advancement on the technique utilises a collagen matrix that is
inserted into the defect to promote MSC differentiation into chondrocytes (53).
In the early 1990s a new technique called autologous chondrocytes implantation (ACI)
was developed as an improvement on the microfracture technique (18, 44, 54, 73).
The technique is a two-stage surgical procedure that first involves harvesting
autologous chondrocytes from a minimal load bearing region through a biopsy punch
and expanding these cells in vitro to obtain a population of approximately 12-48
million cells. In the second surgery, the defect area is debrided, and the cell suspension
is seeded into the defect area and confined to the defect by membrane coverage. This
membrane is typically a periosteal patch; however, a major cause of treatment failure
is hypertrophy of the patch (56). Subsequently, synthetic collagen or hyaluronic acid
patches have been utilised, showing reduced failure rates (5 to 26%) due to patch
hypertrophy (57). However, these synthetic patches are considered as off-label in the
USA due to the sourcing of the material from allogenic sources which may increase
the chance of an immune response (44). ACI has been shown to be effective through
clinical trials which demonstrated positive long-term functional and clinical outcomes.
This is potentially due to the use of autologous chondrocytes which are having a
greater inherent ability to form hyaline cartilage than MSCs. However, the technique
has limitations as fibrocartilaginous tissue was shown to develop in the majority of
patients. This may be a result of the in vitro culturing stage as studies have
demonstrated that chondrocytes dedifferentiate into fibro chondrocytes in 2D culture
however other studies have shown that by culturing the cells in a 3D and hypoxic
environment this can be reversed (58, 59). There are further limitations to ACI which
include the need for two invasive surgical procedures combined with in vitro culturing
and the subsequent long recovery period (6-12 months) needed to ensure successful
neotissue formation.
A derivative of the ACI technique is MACI, which can be considered as a tissue
engineering approach as it utilises a scaffold to assist in cell attachment, distribution,
proliferation, and to guide matrix formation. MACI is similar to ACI in that it requires
the initial isolation of autologous chondrocytes from the patient, in vitro cell expansion
and seeding onto the scaffold, which can be made of collagen or hyaluronic acid. The
cell-seeded scaffold is then cultured in vitro before implantation into the debrided
defect and fixation with fibrin glue. The clinical advantage of MACI over other
techniques remains to be confirmed as current clinical trial data has shown that MACI
44
either has similar or better functional results. MACI however has the same limitations
as ACI in that two surgical procedures are required, slow tissue maturation, and long
recovery periods. However, the long recovery periods may happen with any treatment
due to the nature of the limited regenerative capacity of articular cartilage. There are
a number of benefits to using a scaffold based treatment such as easier fitting of the
graft into the defect, improved graft stability, and better control in preventing
dedifferentiation of the chondrocytes due to fact that cells are cultured in a 3D matrix
which reduces the formation of fibrocartilaginous tissue (44, 60).
A further treatment option is the use of osteochondral auto- and allografts,
mosaicplasty, which involves the transplantation of osteochondral tissue from either
patient (autograft) or a cadaveric donor (allograft) (61). A biopsy is taken from a non-
loading or minimal loading region, in an autograft transplant, which also includes a
portion of the subchondral bone. This is then transplanted into the defect, which has
been prepared with only healthy tissue remaining, and the graft is then aligned with
the native tissue. Mosaicplasty has been shown to have better results than
microfracture however there are a number of limitations to the technique (49, 62, 63).
The use of autografts is limited due to the need to restrict donor site morbidity which
results in only small defect sizes (<4 cm2) being treated. Furthermore, the use of
allografts raises the issue of disease transmission and immunogenicity which is
potentially an issue, however the size of defect treated can be larger as the tissue is
derived from cadavers. Finally, graft failure has been observed in 15-55% of patients
after 10 years due to poor integration with the host tissue which is also a major
limitation with the other techniques as well (64).
Although there are a number of clinical approaches none as of yet have fully repaired
either an articular cartilage defect or a full osteochondral defect over the long-term.
All the approaches have significant limitations which fail to recapitulate the native
structure and result in mechanical mismatch with failure over the long-term.
Subsequently, new tissue engineering approaches are required that enable rapid weight
bearing neotissue that develops into hyaline cartilage and that is fully anchored to the
underlying subchondral bone to enable vertical integration.
Patients with clinical conditions causing cartilage loss present either discrete cartilage
loss in a joint surface or full thickness cartilage degeneration as shown in Figure 2.4
(74). Discrete areas of cartilage loss e.g. osteochondritis dissecans, often caused by
trauma affects the younger population, whereas full thickness cartilage loss in the
45
whole joint affect more elderly patients and is a result of a systemic disease such as
rheumatoid or osteoarthritis (75).
When considering discrete small areas of cartilage loss, patient present with pain due
to exposed bone and mechanical symptoms (e.g. joint locking), due to the disruption
in the smooth low friction joint surface.
Figure 2.4: a) Discrete cartilage defect; b) End stage arthritis; c) Full thickness area
of cartilage loss.
Current solutions haven’t addressed the goal of restoration of the hyaline cartilage
surfaces of the joint (76). The most common surgical procedure to address small areas
of cartilage loss is arthroscopic (keyhole) surgery, called debridement, which uses
mechanical shavers to remove debris from the joint and loose cartilage material which
solves some of the mechanical symptoms (77). The aim of the surgery is to remove all
loose material and roughen the surface of the exposed bone enough to allow new tissue
to adhere and form in the base.
Due to the unpredictable results from debridement techniques were then developed to
create more biological healing in the cartilage defect. Microfracture, popularised by
Steadman (70), involves making 3mm perforations in the subchondral bone, ensuring
that the structural integrity of that bone is not compromised. This allows a super clot
to form in the space creating an environment for pluripotential marrow cells to
differentiate into stable tissue. In one study biopsies after microfracture treatment
noted that 11% had formed predominantly hyaline cartilage and 17% a mixture of
fibrocartilage and hyaline cartilage within them (Figure 2.5). The remaining patients
formed either predominantly fibrocartilage or no tissue at all (78, 79).
46
Figure 2.5: a) Normal cartilage; b) Fibrocartilage next to hyaline after microfracture.
With continued poor results from microfracture due to poor differentiation of new
tissue, allografting techniques were developed. Mosaicplasty involves tacking small
osteochondral allograft plugs from the periphery of weightbearing joints and
transplanted into the defect. There are issues of donor site morbidity with this
technique and the lack of integration of the periphery of the plugs with each other or
the native hyaline cartilage (80).
Lastly, autologous chondrocyte implantation techniques have been in use since the
first reported series in 1987 (81). Cartilage is harvested and at a second surgery,
culture-expanded autologous chondrocyte cells are injected into the cartilage defect
underneath a patch of periosteum that prevents cell migration from the site. Clinical
results are promising in the early years following this treatment and hyaline-like tissue
has been identified in some specimens. However, the tissue is not morphologically or
histochemical identical to normal hyaline cartilage and fibrocartilage is often found in
samples.
These are promising techniques however, rarely last more than 5 years and results
often gradually deteriorate over this period. However, as no other superior alternatives
are available to clinicians, these procedures continue to represent the mainstay of
management despite their failure to recreate the hyaline cartilage that has been
damaged.
Whole joint osteoarthritis represents a different clinical challenge. Not only is the
articular cartilage damaged, but the subchondral bone becomes deformed and the
periarticular capsule, muscles and tendons become affected. Current treatment
strategies are dominated by joint replacement surgery (82). Since the development of
the successful low friction arthroplasty by the late Sir John Charnley, the metal on
47
high molecular weight polyethylene bearing surfaces has been widely used in total
joint prostheses. In the UK over 160,000 hip and knee replacements are carried out
each year (83). However, the challenge continues to overcome the mechanical
loosening of these prostheses over time. In addition, cellular regeneration strategies
are unlikely to overcome the structural changes in all of the tissues types that are
involved (84). Revision surgery to replace failed prostheses causes not only significant
morbidity to the patient but also the results of the second or subsequent joint
replacement being significantly inferior to primary procedures. There is an associated
substantial financial burden to the healthcare system due to increased cost of peri-
operative investigations, blood transfusions, surgical instrumentation, implants and
operating time, as well as an increased length of stay in hospital which accounts for
most of the actual costs associated with surgery. Innovation has been able to reduce
the incidence of prosthetic failure by improving the techniques employed to ensure
good integration with the host bone, e.g. coating implants with hydroxyapatite and
using uncemented implants.
Tissue engineering: requirements and challenges
Tissue engineering is a multidisciplinary field of research conducted to meet clear
clinical requirements of therapies to promote the regeneration and repair of diseased
and damaged tissues. Tissue engineering approaches in cartilage regeneration and
repair has great potential and provides an alternative to current available therapies
which are inadequate, however, challenges remain (18, 20, 44, 85, 86). Engineered
cartilage constructs are comprised of biomaterials, cells, and stimulatory factors (e.g.
growth factors and biomechanical stimulation), which are considered key to the design
of functional cartilage tissue (Figure 2.6) (87, 88). However, the current paradigm still
lacks in the development of long-term phenotypically stable articular cartilage tissue
which exhibits integration with the surrounding tissue, mechanical stability, and
withstands inflammatory factors, especially in a diseased environment such as
osteoarthritis.
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Figure 2.6: Tissue engineering strategies for articular cartilage regeneration. Image
from reference (85).
2.1.6.1 Biomaterials design and selection
Biomaterials are the backbone of 3D engineered constructs and support tissue growth
and formation by providing a similar environment to the native tissue and structural
integrity during maturation to allow cell proliferation, cell to cell communication, and
ECM formation. The ideal design specifications of 3D tissue engineered scaffolds
from the biomaterials perspective include: i) biocompatibility, cell viability with a
desired cellular behaviour; ii) biodegradability, the scaffold degrades at a controlled
rate which matches tissue formation; iii) provides mechanical and biochemical cues to
promote a desired cellular response. An alternative strategy to the use of biomaterials
is cell self-assembly approaches such as spheroid formation which do not require
supporting materials.
Biomaterial scaffolds can be produced from different sources such as naturally derived
polymers, synthetic polymers and ECM derived materials.
Natural derived biopolymers have been explored extensively for cartilage tissue
engineering applications (86, 89, 90). The most associated advantages with naturally
derived polymer are their capacity of supporting cell attachment, viability,
proliferation, attachment, and differentiation, and, in some cases, maintenance of cell
phenotype (91). This is mediated in protein derived biopolymers through binding
motifs present in the polymer. Despite these key advantages, naturally derived
polymeric materials present significant limitations such as poor degradation kinetics
49
and mechanical properties, however, these limitations may be improved through the
modification of the backbone of the polymer chain or via crosslinking mechanisms
(91).
Naturally derived polymeric materials can be classified into two main categories:
1- Polysaccharides: gel forming polysaccharides such as alginic acid and
mucopolysaccharides (glycosaminoglycans), storage polysaccharides which include
starch and glycogen, and structural polysaccharides such as cellulose and chitin.
2- Protein based polymeric material composed of amino acid groups such as
collagen, gelatin, and silk fibroin. Proteins can be classified by their shape, size,
solubility, composition, and function.
Synthetic polymers have shown potential in tissue engineering due to their improved
mechanical and degradation properties with the capacity to be more easily chemically
modified or engineered to tune their properties (92-94). The hydrolytic and enzymatic
degradation of the polymer can be controlled through modification of the polymer
(95). However, due to lack of biologically functional domains, which can reduce the
risk of immune response, synthetic polymers may not facilitate cell phenotype
expression or cell attachment as occurs in naturally derived protein-based polymers.
Decellularized extracellular matrix (dECM) based biomaterials have also been
explored to create 3D constructs. The native ECM is ideal for tissue engineering as it
is identical to the desired matrix structure required and helps controls cell behaviour
(96-100). Thus, the use of dECM is suitable as it is biodegradable, does not produce
antagonistic immune responses, provides cues for cell differentiation, and presents
bioactive molecules that determine tissue homeostasis and tissue regeneration (101,
102). The decellularisation process comprises mechanical and chemical manipulation
to remove the cellular components (103). This protocol from harvesting,
decellularisation, and sterilisation to creating the dECM based scaffolds affects the
hydration status and 3D configuration of the proteins and ECM, and hence strongly
influences biomechanical and biological behaviour properties which may not be
suitable anymore (104, 105). The replication of the ECM microenvironment has
provided inspiration to use the ECM from articular cartilage as matrix for tissue
regeneration (101, 106). However, concerns remain about potential immunogenicity
and poor biomechanical and biological performance.
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2.1.6.2 Bioprinting cartilage tissue constructs
The advancement of 3D printing or additive manufacturing in tissue engineering has
allowed the fabrication of scaffolds and biological models that more accurately reflect
the complex organisational structure and material properties of tissues and organs
(107, 108). 3D bioprinting uses biomaterials, cells (encapsulated or seeded), and
biomolecules, typically referred to as a bioink, which are precisely deposited in a
layer-by-layer process to build-up a 3D structure. The ability to print multiple
biocompatible materials with greater design freedom compared with conventional
fabrication techniques has enabled the development of 3D structures that resemble the
complex 3D biophysical and biochemical environment in tissues. The use of 3D
bioprinting within cartilage tissue engineering is becoming widespread as an enabler
technology to fabricate complex multi-material structures that mimic the biological
and mechanical properties of cartilage tissue (109, 110). Currently, 3D bioprinting
predominately uses inkjet, extrusion, and laser-assisted systems to fabricate 3D
structures (Figure 2.7). However, stereolithography based systems are gaining
attention due to novel visible light photo crosslinkers with improved cytocompatibility
and advancements in the technology which promises faster fabrication times and
increased structure complexity (111, 112).
Figure 2.7: 3D bioprinting technologies; a) Inkjet bioprinting; b) Laser-assisted
bioprinting; c) Extrusion bioprinting (113).
The development of bioinks has become a key factor in 3D bioprinting in particular
biomaterials with controllable mechanical, biological, and biophysical characteristics
which can modulate cell behaviour combined with printability (Figure 2.8) (114, 115).
Printing resolution, structure fidelity, material viscoelasticity are crucial parameters in
determining the printability of bioinks and its relationship to the final mechanical and
biological properties of the structure. Developing advanced bioinks requires
51
consideration of pre-functionalisation processes to incorporate biological functional
groups and crosslinking moieties, the rheological behaviour of the bioink to ensure
printability and fidelity, and the crosslinking method to ensure rapid gelation of the
hydrogel (116-119). Depending on the biofabrication process and material properties,
the bioink polymers will have various chemical and physical characteristics that will
determine the corresponding application (120). These properties can be determined by
rheological characterization, mechanical assessment and crosslinking properties of the
hydrogel (120, 121). Shear-thinning behaviour, a decrease in the viscosity as a
function of increasing shear rate, is crucial for bioprinting applications, since the
material will flow with an applied force during printing and the lower the applied force
the higher the cell viability (119, 122, 123). The viscoelastic behaviour characterised
by the material response during printing needs to be optimised as low viscous materials
will deform and collapse during printing, unless a rapid crosslinking process can be
initiated. On the contrary high viscosity materials can be difficult to print as they can
block the printing nozzle, require high deposition force, and restrict cell attachment
and spreading which can negatively impact cell viability (124, 125).
Figure 2.8: Bioink properties for successful 3D bioprinting require a suitable a)
biofabrication window which balances printability and biocompatibility whilst
providing a variety of b) suitable characteristics (126).
2.1.6.3 Biochemical, biophysical and biomechanical stimulation
Biochemical, biophysical, and biomechanical stimulation of 3D bioengineered
constructs is crucial in the formation of functional neocartilage tissue. The stimulation
of cells can be achieved at specific stages: cell expansion, differentiation, and the
maturation of the tissue construct in vitro. This can be attained through
supplementation of the cell culture media, incorporation of biomolecules within the
52
3D structure, engineering the physical ECM environment, and mechanical stimulation
of the construct.
A key approach to direct cell behavior and facilitation of neocartilage tissue formation
is the use of biological signaling molecules (e.g. growth and transcription factors)
during cell culture, tissue maturation, and utilization via direct inclusion,
encapsulation or binding to the biomaterial matrix of the construct (127-132). A range
of growth and transcription factors have been identified and investigated including
transforming growth factors (TGFs), bone morphogenetic proteins (BMPs), insulin
growth factors (IGFs), fibroblastic growth factors (FGFs), platelet-derived growth
factors (PDGFs), and sex determining region Y (SRY)-box (SOXs).
Growth factors are proteins that have a key role in cell behavior and regulate cellular
growth, proliferation, differentiation, and migration and are grouped into families with
shared amino acid sequences and superfamilies with shared structural folds (130, 133).
In articular cartilage tissue engineering, 3D engineered constructs have been used to
deliver these biological factors (130). For instance, TGF-β1 stimulates the synthesis
of cartilage ECM, maintain chondrocytes phenotypes, synthesis of proteoglycans,
aggrecan and type II collagen and can enhance the repair of cartilage defects (134,
135). IGF-1 has been reported showing high anabolic effects and decrease in catabolic
responses in articular cartilage metabolism in vitro (135, 136). Other studies have
reported using different growth factors which were successful in producing several
features that resembled typical articular cartilage (137-139). Despite of the capacity to
promote cartilage matrix formation, growth factors have shown some drawbacks with
IGF-1 associated with a loss of chondrocyte phenotype and extracellular matrix
breakdown (136). Furthermore, IGF-1 in human MSCs inhibited collagen II
expression and overexpression can induce hypertrophic differentiation and
mineralization (140).
Biomechanical stimulation is key in the development and homeostasis of functional
cartilage tissue (141-145). The importance of mechanical loading and physical
movement on embryonic chondrogenesis has demonstrated in chicken embryos which
when physically impaired exhibited poor development of cartilage tissue (146-148).
Mechanical loading is required for healthy tissue; however, excessive loading can lead
to trauma and disease progression (141). Thus, mechanical stimulation of cells and
tissue constructs via compression, shear and hydrostatic pressure is important to
promote chondrogenic differentiation, maintain a chondrogenic phenotype, and
53
generation of functional tissue in vivo. Mechanical stimulation of MSCs under varied
loading regimes have been shown to increase the deposition and expression of
collagen II, GAG, TGF-1/3, and SOX9 and modulated secretory factors such as
stromal-derived factor-1 (SDF-1), matrix metalloproteinase-2 (MMP-2), FGF,
vascular endothelial growth factor (VEGF), activated leukocyte cell adhesion
molecule (ALCAM), nitric oxide, urokinase receptor (uPAR), macrophage
inflammatory protein 3 (MIP3). The advancement of bioreactors in tissue
engineering has enabled the use of mechanical stimulation as a key capability in
engineering cartilage tissue formation (149-151). Dual compressive and shear
mechanical stimulation of human articular chondrocytes encapsulated in gelatin
methacrylate and hyaluronic acid methacrylate hydrogel have been demonstrated by
Meinert et al (152). Cartilage specific marker genes and ECM were upregulated with
significant increase in collagen II synthesis. Combining compressive and shear
stimulation has been investigated using multi-axial loading bioreactor which mimics
the movement of articulating joint (153, 154). Vainieri et al investigated a chondrocyte
seeded hybrid fibrin-polyurethane scaffold implanted in an osteochondral defect
model that was mechanically stimulated using a joint mimicking bioreactor (154). The
results showed increased production of chondrogenic specific markers, proteoglycan
4 and cartilage oligomeric matrix protein, and the improved collagen II to I ratio.
Alternatively, tensile stimulation of a self-assembled scaffold-free neocartilage
construct has shown to increase the tensile strength and modulus of the construct and
once implanted in vivo in a mice model had similar mechanical properties and collagen
content of native tissue (155). The development of improved mechanically stimulating
bioreactors and osteochondral models will provide a valuable tool in understanding
cartilage development and will aid the screening of biomaterials and tissue
engineering.
Challenges remain in the use of stimulatory processes to guide cell behavior and tissue
development. A complete understanding of chondrogenic development is still
developing so the entire milieu of factors that influence tissue formation incomplete.
However, tissue engineering strategies will most likely, to be successful, use a
combination of growth factors, a controlled biophysical environment, and a
mechanical stimulation to promote tissue formation with phenotypic stability. As the
use of soluble factors alone in the differentiation of chondrocytes and MSCs in vitro
54
typically results in the expression of hypertrophic chondrocyte phenotype. The design
of these stimulatory environments will aim to recapitulate the native environment
during early stage development of the tissue. A successful strategy will need to
determine the combination, dosage, and delivery profile of growth factors. The design
of the physical matrix surrounding the cells by controlling parameters such as
crosslinking density, ECM protein selection, and oxygen tension. Finally, the timing,
type, and loading conditions of mechanical stimulation will be key in promoting an
ECM which is mechanically compliant. However, the complexity of this environment
and the actual implementation of a multi-stimulatory strategy is a serious challenge
for researchers.
Conclusion and future perspectives
This Section discusses articular cartilage structure, composition, and current clinical
therapies. Tissue engineering strategies are discussed with a focus on selection of
biomaterials, stimulatory factors, and bioprinting to provide an overview of
approaches to generate osteochondral tissue.
The clinical size and market of cartilage and osteochondral problems is expanding
due to the ageing worldwide population and the most common treatment approaches
are ineffective at stopping the progression of degeneration of the tissue. Thus, tissue
engineering strategies are key in solving this pressing clinical problem. The design
specification of any biomaterial-based 3D construct must fulfil a stringent criterion
requiring suitable biomaterial selection, scaffold architecture, fabrication technique,
stimulatory factors, and maturation of the tissue.
Key research challenges are the maintenance of phenotype in the engineered tissue
construct and the prevention of hypertrophic or fibrocartilage phenotypes being
expressed. The tissue constructs also require strategies to promote integration with
the surrounding healthy tissue in an osteochondral defect, although in total
replacement the strategy would primarily to be to anchor the neocartilage to
underlying bone. Furthermore, the underlying biological behaviour of the tissue, the
early-stage developmental biology, and haemostatic processes in adult tissue need
further understanding. This knowledge may unlock key aspects of the tissue which
may guide tissue engineering strategies. This could require a strategy of multiple
stimulatory factors (e.g. growth factors and mechanical stimulation) over an
extended maturation time of up to many years to mimic the underlying biological
55
development of the tissue and even then, the incorporation of permanent mechanical
structures may be necessary. Subsequently, future studies should focus on a multi-
stimulatory environment, long-term studies to determine phenotypic alterations and
tissue formation, and the development of novel bioreactor systems that can more
accurately resemble the in vivo environment. Finally, a clear and considered route
in the development process of the materials, structures, and strategy should be
evaluated prior and during the research phase to expedite clinical and regulatory
approval. This will allow faster and more successful access to animal trials and
eventually human clinical trials with the prospect of a successful therapy being
developed.
56
Engineering natural-based photocrosslinkable hydrogels for
cartilage applications †
Articular tissue is an avascular tissue at the ends of articulating joints which provides
lubrication and transmission of compressive forces during movement. The tissue has
poor regenerative capacity and low cellular metabolic activity thus disease or trauma
can result in significant clinical issues characterised by pain in the joints and restriction
of movement. This can affect patient’s quality of life and impose substantial
socioeconomic costs on society. Currently no treatment can prevent the long-term
degradation of the tissue, so new and improved therapies are required. Tissue
engineering based strategies are a promising approach to repair and regenerate
damaged tissue. Natural hydrogel-based scaffolds have been widely developed to
promote cartilage regeneration due to their biocompatibility, resemblance to the native
extracellular matrix, and capacity for cell encapsulation. However, a key challenge is
the engineering of biomimetic hydrogels to promote the development of articular
cartilage rather than fibrocartilage. Hydrogels can be designed through the selection
of appropriate materials, crosslinking mechanisms, mechanical properties and the
incorporation of biofunctional moieties that can regulate biodegradation, cell
attachment and differentiation, and the delivery of biomolecules. The range of
parameters to engineer provides the opportunity to fabricate biomimetic structures that
can facilitate cartilage regeneration. However, the complexity of the challenge is
daunting and requires an interdisciplinary approach to successfully fabricate hydrogel-
based scaffolds that can promote long-term regeneration of articular cartilage.
Introduction
The desire to regenerate and replace damaged or dysfunctional human tissues to
improve quality of life is as old as human history. This aspiration has been expressed
in numerous cultures throughout history such as the myth of Prometheus with his
eternally regenerating liver and Mary Shelley’s ‘Frankenstein’ in which the scientist
created new life from the rejuvenation of dead tissue. This human fascination to
regenerate the body has in recent decades developed into the rapidly expanding
scientific field of tissue engineering (TE). TE holds the promise to offer a paradigm
† This section is based on the book Chapter: Hussein Mishbak, Cian Vyas, Glen Cooper, Chris Peach,
Rúben F. Pereira, Paulo Bartolo, “Engineering natural-based photocrosslinkable hydrogels for cartilage
applications’’, in Bio-materials and Prototyping Applications in Medicine, Edited by B. Bidanda and
P.J. Bartolo, Springer, 2020 (ISBN: 978-3-030-35875-4).
57
shift in clinical treatment and understanding of a host of disease states. This shift will
enable a science fiction like prospect of infinite replacement human body parts which
will have tremendous positive impact on human health. The concept of TE has
developed into the currently accepted definition put forward by Langer and Vacanti in
1993 that states:
“Tissue engineering is an interdisciplinary field that applies the
principles of engineering and the life sciences toward the development
of biological substitutes that restore, maintain, or improve tissue
function.” (156).
Due to an ageing population worldwide and increasing numbers of age-related and
lifestyle linked diseases such as osteoarthritis, diabetes, and cardiovascular disease,
the importance of TE is enormous. TE will enable the development of superior clinical
treatments to the benefit of patients but also relieve the strain on healthcare systems.
Furthermore, TE has applications beyond tissue regeneration and replacement such as
the development of three-dimensional (3D) culture and tissue constructs that allow
pharmaceutical testing, disease modelling, toxicology testing, and improved
understanding of cell biology (157).
There are multiple strategies employed in TE to enable tissue regeneration and
replacement. A scaffold based or top-down approach, typically utilises a scaffold
which is a supporting construct that outlines the spatial requirement of the tissue,
enables cell attachment, and provides environmental cues to promote a desired cellular
response (158-160). This approach can be typically split into either acellular or cellular
techniques. Cellular approaches using a traditional in vitro TE strategy require cells to
be isolated, expanded in culture, and then seeded onto a scaffold in vitro to enable
maturation and remodelling of the construct before subsequent implantation into a
patient. An alternative method is to seed the scaffold with cells isolated at the point of
surgical implantation which avoids the in vitro maturation phase and requires a single
surgical intervention. The acellular in vivo TE scaffold approach bypasses the need for
cell seeding and maturation completely as a bio-functional scaffold is directly
implanted into the patient. This approach relies on the recruitment of cells in vivo to
initiate tissue repair and remodelling of the scaffold. An alternative approach is the
scaffold-free strategy which is a bottom-up process utilising cell spheroids, cell sheets,
and self-assembly to generate new tissue and typically does not require exogenous
scaffolds or cell seeding (161). These approaches utilise the ability of cells to fuse into
58
larger constructs and in self-assembly necessitates the recapitulation of embryonic and
developmental pathways of tissue and organ genesis (162-164). The scaffold-free
approach using cells, their own extracellular matrix (ECM) and signalling molecules
aims to generate new tissues and organs with high level of biomimicry, thus requiring
a deep understanding of the underlying biological and physical mechanisms of these
pathways. Finally, a new hybrid approach aims to combine both scaffold and scaffold-
free TE in a synergistic approach to benefit from the inherent advantages of both
techniques (165).
Hydrogels are a specific class of materials highly relevant for both the fabrication of
acellular scaffolds and cell-laden constructs. They are biocompatible and can be
designed to be biodegradable with a structure that closely mimics the native in vivo
ECM (166-168). This is a result of hydrogels typically being composed of a three-
dimensional (3D) polymer network which swells on contact with water (169). This
enables storage of large quantities of water which resembles soft biological tissues and
allows for encapsulation of cells and bioactive molecules. Furthermore, hydrogels are
typically biocompatible and allow for diffusion of oxygen, nutrients, and water-
soluble compounds. Hydrogel properties can be tuned through chemical, physical, and
biological modification which allows a variety of cell behaviours such as adhesion,
proliferation, and differentiation to be optimised. Moreover, hydrogels can be tuned
to respond to stimuli such as temperature, light, pH, and biomolecules which enables
hydrogels to have a variety of properties such as self-healing, controlled degradation,
and drug delivery (170). A pioneering example of a cell-responsive hydrogel is
Hubbell et al. demonstration that inclusion of specific peptides in a hydrogel could
enhance matrix metalloproteinases (MMP) activity and thus control the rate of
scaffold degradation (171). The ability to fabricate hydrogels with specific properties
has enabled precise control of cell behaviour which is a benefit in creating scaffolds
that will allow tissue engineering to be successfully translated.
Photocrosslinkable or photocurable hydrogels are particularly relevant for TE
applications due to the rapid gelation, control over spatiotemporal formation, and the
ability to tune polymer network properties such as crosslinking density and matrix
stiffness (172). This is often achieved by controlling operating parameters such as light
intensity, exposure time, and illumination area. When used in combination with
bioprinting techniques, photopolymerization enables the fast and automated
crosslinking of complex scaffold architectures during and post-printing. However,
59
photocrosslinking conditions need to be optimized to overcome concerns regarding
cell exposure to UV radiation and potential cytotoxicity from photoinitiators, by-
products, and unreacted reagents.
This Section outline the recent advances in the design of naturally derived
photocrosslinkable hydrogels for cartilage tissue engineering. A brief description of
the structure and composition of cartilage tissue will be firstly provided, followed by
an overview of hydrogel properties, synthesis routes, and strategies for hydrogel
biofunctionalisation within cartilage tissue engineering (Figure 2.9).
Figure 2.9: Schematic diagram of photocrosslinkable 3D hydrogel constructs and
approaches for use in cartilage tissue engineering.
Articular cartilage
Articular cartilage is a load-bearing and non-vascularised tissue that covers the ends
of bone joints (Figure 2.10a), acting as a low-friction bearing surface and a mechanical
damper for the bones (173, 174). It is a matrix-rich tissue with specialized cells
(chondrocytes) that maintain the structural and functional integrity of the ECM (175-
178). However, cartilage lacks inherent self-repair ability and remains a significant
clinical and economic challenge throughout the world, hence the zonal structure and
function are often irreversibly lost following trauma and disease. Thus, cartilage
defects are prone to develop into osteoarthritis (OA), which is a major disease
60
associated with cartilage tissue and is characterized by a loss of healthy and functional
cartilage tissue, pain, and debilitation thus is a significant clinical and economic
challenge (179, 180).
2.2.2.1 Composition and zonal organization
Cartilage is characterized by a distinct zonal structure comprising, in descending
order, the articular or superficial surface, the middle (or transitional) zone, the deep
zone, a tidemark (separates the non-calcified and calcified regions) (18, 181), and the
calcified zone (Figure 2.10b). These zones differ with respect to the molecular
composition and organization of the cartilage ECM, the shape, density, alignment of
the resident chondrocytes and the mechanical properties of each zone. The
subchondral bone acts as a shock absorber, the loading forces experienced by the joint
are transmitted to this region, and the bone tissue contains blood vessels that supply
nutrients, oxygen, and removes waste from the lower regions of the avascular cartilage
tissue (182). Surrounding each individual chondrocyte are three distinct ECM regions
which depending on the distance from the cells are termed the pericellular, territorial,
and interterritorial region. The highly organised and hierarchical properties of the
tissue are responsible for its remarkable mechanical properties (183-187).
Figure 2.10: a) Articular cartilage covers the surfaces of bones in diarthrodial joints
(e.g. knee and elbow); b) Zonal structure and composition of articular cartilage (40)
Articular cartilage is typically composed of:
Chondrocytes: responsible for production and maintenance of the cartilage ECM and
essential for tissue formation and functionality. They represent about 5-10% of the
total volume of cartilage (17, 187). However, they have limited proliferation capability
and low metabolic activity, which is partially responsible for the limited capacity of
cartilage to recover from trauma or disease (188, 189).
61
Collagen: the main component of cartilage with up to 60% of the dry weight being
collagen with type II the most common type representing 90-95% of total collagen in
the ECM which can form fibrils and fibres entwined with proteoglycan aggregates
(65).
Proteoglycans: molecules responsible for the resistance to compression of cartilage
tissue (190). Proteoglycans (PG), corresponding to around 35% of the cartilage dry
weight, are made up of repeating disaccharide units, glycosaminoglycans (GAGs),
with two main types; chondroitin sulphate and keratin sulphate (190). Proteoglycans
have a turnover rate of three months and weave between the collagen fibres creating a
mesh responsible for retaining water and providing elasticity to the tissue (191).
Water: represents 65-80% of the total cartilage mass (192). This content reduces with
aging and is linked to a reduction of strength and elasticity of the tissue (193).
Synovial fluid: a highly viscous liquid secreted by synovial lining cells, they are
responsible for secreting hyaluronic acid (the intrinsic component of synovial fluid)
(194, 195). The main function of the synovial fluid is to distribute nutrients and gases
to the upper regions of the cartilage tissue whilst providing lubrication at the interface
between articulating surfaces in the joint to allow facilitation of movement (196).
2.2.2.2 Clinical treatments and challenges
Cartilage disease and traumas are a serious clinical problem that can lead to
debilitating pain, swelling, inflammation, and can result in drastically impaired
mobility. An ageing worldwide population is resulting in increased number of patients
suffering from osteoarthritis, a leading cause of cartilage damage (197). Additionally,
tissue degeneration through disease or significant trauma results in steady degradation
of the tissue with limited successful clinical interventions to prevent this long-term
decline which eventually results in a total joint replacement (Figure 2.11). The limited
regenerative capacity of cartilage is due to the avascular nature of the tissue and low
metabolic activity of the resident chondrocytes and is in marked contrast to other
tissues such as bone and the liver which have remarkable healing properties in
comparison (163, 198). Current clinical interventions have limited success in
regenerating or replacing articular cartilage with most therapies producing inferior
fibrocartilage or only delaying the progression of tissue degeneration (199, 200).
62
Figure 2.11: Stages of articular cartilage damage. 0) Healthy cartilage. I) Softening,
swelling and fissuring of the cartilage. II) Lesions <50% of cartilage depth. III)
Lesions >50% of cartilage depth but not through subchondral bone layer. IV) Severely
abnormal with penetration through the subchondral plate. Reproduced with permission
from the International Cartilage Regeneration & Joint Preservation Society (ICRS)
(200).
The most commonly used cartilage repair strategies are debridement and
microfracture, autologous chondrocyte implantation (ACI), matrix-assisted
autologous chondrocyte transplantation/implantation (MACT/MACI), autologous
matrix-induced chondrogenesis (AMIC), and osteochondral auto- and allografts
(Figure 2.12) (201, 202). Each of these approaches has major disadvantages such as
the formation of inferior fibrocartilage, requirement of two surgeries, donor site
morbidity, and limited prevention of continued tissue degeneration. Therefore, new
approaches are required to address these unmet clinical challenges. TE has the
potential for a breakthrough approach by synergistically incorporating
chondrocytes/stem cells, biomaterials, 3D scaffolds, stimulatory growth factors,
mechanical stimulation, and bioreactors for the fabrication of tissue constructs. If this
approach is successful, then we will approach our final goal of the predictable
regeneration of articular cartilage (110, 203-207).
63
Figure 2.12: Current techniques for articular cartilage repair and future scaffold-based
approaches. a) Debridement and microfracture; 1-4 debridement of damaged tissue, 5
microfracture into the subchondral bone, 6 blood clot formation containing
mesenchymal stem cells (MSCs), and 7 formation of inferior fibrocartilage. b) ACI; 1
cartilage biopsy from a non-load bearing site, 2 in vitro expansion of chondrocytes to
obtain sufficient numbers for implantation, 3 a second operation cleans the damaged
area and is covered with the periosteal flap and the expanded chondrocytes are injected
under this or the expanded chondrocytes are seeded into a matrix (e.g. collagen
membrane) and fixed with fibrin glue into the defect area (MACI/MACT). c) AMIC;
a microfracture is created and a membrane placed over the top and fixed with a fibrin
glue or sutures. The membrane protects the clot formation and allows chondrogenic
differentiation of the MSCs in the blood to aid the regeneration process. d)
Osteochondral auto/allograft transplantation; cylindrical plug of fresh cartilage and
subchondral bone is taken from the patient or a cadaver donor, 1 a guide pin is placed
perpendicular to the joint surface in the defect, 2 implantation of the graft plug, and 3
securing the plugs with the insertion of screws. e) Acellular scaffold only requiring a
single surgery and in vivo recruitment and stimulation of cells for tissue regeneration.
f) Cellular-based scaffold involving two surgeries of initial cartilage biopsy,
chondrocyte expansion, and seeding into the scaffold before implantation into the
defect. Adapted with permission from the ICRS (200)
64
Engineering hydrogels for cartilage tissue engineering
Hydrogels are three-dimensional (3D) insoluble crosslinked polymer networks able to
retain a large amount of water and biological fluids (between 10-200%) in their
swollen state (208-211). The 3D network of the hydrogel (Figure 2.13) is maintained
by polymer crosslinking among the polymer chains, with water taken up and contained
within the polymeric structure (212, 213).
Figure 2.13: Engineering 3D hydrogels for cartilage application through a) cell-
encapsulation, b) optimizing crosslinking density, and c) functionalizing with
biomolecules (e.g. RGD) to guide cell behavior.
Hydrogels have a range of useful characteristics such as their hydrophilic capacity to
absorb a volume of water that is significantly beyond their weight when dehydrated
(214), potential printability and ability to create a self-supporting 3D structure to suit
various biological engineering needs (cell encapsulation, cell support and
biodegradability) (215), uniform cell distribution, as well as providing both chemical
and biological signalling (216). The ability of the 3D network to resist dissolution in
wate r is related to the presence of the crosslinked polymer molecules which will
determine the quality and stability of the hydrogel. Due to these properties and
characteristics, a wide range of different hydrogels have been used for ECM formation
and cartilage regeneration applications. Currently, natural based hydrogels represent
the most relevant group of materials to produce constructs for cartilage applications
(Table 2.1). Depending on the source, they can mimic the ECM structure and
composition of articular cartilage presenting relevant swelling, degradation,
mechanical and lubrication characteristics. Natural based hydrogel materials such as
alginate (217), agarose (218), gelatin (219), collagen (220-222), hyaluronic acid (HA)
(223), chitosan (224), and interpenetrating network/hybrid systems have been
extensively explored for cartilage applications (225).
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Table 2.1: Photocrosslinkable natural polymers used in cartilage tissue engineering.
Polymer Crosslinking conditions Biological properties Refs.
Alginate
Methacrylate anhydride, photoinitiators (VA-
086, Irgacure 2959) and 254-365 nm exposure wavelength. Simple preparation.
Chondrocytes showed ECM formation with ~80%
similarity to native cartilage. >85% viability
Stem cells/ MSCs/ hASCs: could be regulated via the
introduction of soluble factors and biophysical cues in 3D cell culture systems
(226-228)
Agarose
Typically, physical crosslinked (thermal),
however, can be functionalized with
methacrylate group,
Chondrocytes: no results reported (for chondrocyte
cells encapsulated in photocurable agarose).
hBMSCs: cell viability in agarose scaffolds decreased
from 75% at day 3 to 40% at day 90.
Fibrochondrocytes: 80% cell viability and maintains
chondrocyte phenotype
(229-231)
Gelatin
Methacrylate and acrylic anhydride,
photoinitiators (VA-086, Irgacure 2959) and 254-365 nm exposure wavelength. Simple
preparation.
Chondrocytes showed ECM formation similar to
native cartilage . >85-97% viability, cell morphology could be controlled by the stiffness of hydrogels.
Stem cells/ MSCs/ hASCs : could be regulated via the introduction of soluble factors and biophysical cues
in 3D cell culture systems
(232-235)
Hyaluronic
acid
Glucuronic acid carboxylic acid, the primary
and secondary hydroxyl groups, and the N -
acetyl group (following deamidation) thiols, methacrylate, tyramines
Photoinitiators (VA-086, Irgacure 2959) and
254-365 nm exposure wavelength
Chondrocytes, epithelial cells and murine fibroblasts
cells
For cartilage engineered tissue, ECM formation reached about 80% of those found in native cartilage.
>85% viability
Promoted the retention of chondrocyte phenotype and
matrix synthesis of encapsulated porcine
chondrocytes and enhanced cell infiltration and tissue repair in rabbit osteochondral defect model at 2-week
post-surgery
Stem cells/ MSCs/ hASCs: could be regulated via the
introduction of soluble factors and biophysical cues in 3D cell culture systems
(233)
Chitosan
(CS)
Vinylated CS Macromers, Azido-Functionalized CS azido, and (methyl)acrylated CS
Structurally analogous to cartilage glycosaminoglycans, Biocompatible, showed low
cytotoxicity at various concentrations for
chondrocytes, cell viability between 82-96%
(236, 237)
Dextran
Methacrylate groups (glycidyl methacrylate) introduced in dextran to prepare
photocrosslinkable dextran (photoinitiator
Irgacure 2959 to UV light. 254-365 nm
wavelength
Chondrocytes, endothelial cells and stem cells, the dextran-based IPN hydrogel provides cell-adhesive
and enzymatically degradable properties
Fibroblasts ~90% cell viability.
(238, 239)
Gellan Gum
Methacrylic anhydride, the aqueous solution of methacrylated gellan is added with 0.08 mg/mL
calcium chloride and 0.5% (w/v) Irgacure 2959
Human nasal chondrocytes: The gellan gum supports is their use as cells encapsulating agents to be used in
cartilage regeneration approaches
Exhibits good cell viability and chondrocyte morphology.
(240, 241)
Collagen
Collagen I: dual crosslinking with visible light,
Rose Bengal, and chemical crosslinking using 1-
ethyl-3-(3-dimethylaminopropyl) carbodiimide and N-hydroxysuccinimide.
Chondrocytes had ≥ 95% viability. Dual-crosslinked
gels showed greater resistance to collagenase
digestion.
(222)
Collagen II: amidation reaction between amino groups on the collagen lysine and methacrylic
anhydride resulting in collagen methacrylamide.
Irgracure 2959 used as photoinitiator and exposed to UV (8 W cm−2) for 30 s. Triple
helical structure of collagen was preserved after
functionalization.
BMSCs differentiated into a chondrogenic phenotype with lacuna-like cartilage formation. High cell
viability. Increase in chondrogenic gene expression
(AGG, SOX9, COL II, COL X). In vivo subcutaneous implantation in a mouse model
demonstrated the secretion and deposition of cartilage
specific matrix.
(220)
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Although pure natural hydrogels have been widely explored in cartilage applications,
they often have significant limitations relating to the suitability of their biomechanics,
degradation profiles, and cell-material biological interactions. Subsequently,
significant research into new hydrogel systems that have tuneable mechanical and
degradation properties, provide specific control over cellular behaviour, allow
incorporation of novel materials, and display suitable material processing properties
for different fabrication routes such as 3D printing have been developed (126, 242-
245). The incorporation of multiple materials, hybrid hydrogels, to produce a system
with a mixture of two or more of distinct classes of molecules (e.g. a blend of natural
and synthetic hydrogels) or different structures (e.g. blend of organic polymer
hydrogels and inorganic particles/metals or synthetic nanoparticles) have been
developed to improve single material-based systems (Figure 2.14) (246-249).
Figure 2.14: Hybrid hydrogel network systems (96). Multi-material bioink networks
are two different component polymers or more crosslinked together. Interpenetrating
networks (IPN) is a 3D structure of two or more polymeric networks, which are
partially or fully chemically bonded but not covalently bonded, or a network of
embedded linear polymers entrapped within the original hydrogel (semi-IPN) (97, 98).
Nanocomposites bioink network can be produced by adding nanoparticles to the
polymeric hydrogels (99). Supramolecular bioink network is composed of short
repeating units with functional groups that can interact non-covalently with other
functional units, forming large, polymer-like entanglements (100).
67
The use of photocrosslinkable hybrid hydrogels is a burgeoning research field
especially within tissue engineering. Photocurable hydrogels are particularly relevant
for biomedical applications due to the advantage of being able to encapsulate cells,
fast gelation time, tuneable mechanical properties and crosslinking density, and the
cytocompatibility processing conditions that allow their in situ crosslinking into the
defect site during a surgical procedure (250-252). The use of vat photopolymerization
and light curing processes in additive manufacturing also enables the fabrication of
high resolution and complex structures that are not possible through conventional
methods (111, 172). This approach facilities the development of more biomimetic
structures that can recapitulate the complexities of native tissues.
Typically, polymers are unable to initiate a photopolymerization reaction alone and
can require both functionalisation with photocrosslinkable groups and the addition of
light sensitive molecules, called photoinitiators. The photoinitiators typically used
within tissue engineering are normally excitable within the ultraviolet (UV) (e.g. 1-4-
(2-hydroxyethoxy)-phenyl-2-hydroxy-2-methyl-1-propane-1-one, Irgacure 2959, and
2,2'-azobis-2-methyl-N-(2-hydroxyethyl)propionamide, VA-086), UV-visible (e.g.
lithium phenyl-2,4,6-trimethylbenzoylphosphinate (LAP), and diphenyl(2,4,6-
trimethylbenzoyl) phosphine oxide, TPO), and visible light range (e.g. ruthenium,
Bengal rose, riboflavin, eosin-Y, and camphorquinone). Upon irradiation, an initiation
step begins and the photoinitiator undergoes an excitation mechanism which results in
the formation of highly reactive species (free radicals). The next step is propagation,
free radicals attach at specific sites on the monomer/oligomer structure (unsaturation
sites) starting a chain reaction that creates a permanent crosslinked network. Finally,
a termination step results in the completion of the polymer chain and crosslinking with
free radical extinction. The degree of photopolymerization (curing percentage) of the
resulted hydrogels is highly affected by the functionalisation process and polymer
solution concentration, light wavelength and intensity, photoinitiator type and
concentration, and curing time (253). The number of parameters to control also
provides an opportunity to highly engineer the resulting hydrogels properties and
when used in conjunction with bioprinting processes can result in tuneable and
biomimetic structures.
Photocrosslinking is an advantageous process, however, specific issues need to be
addressed especially in biomedical applications. The chemical processes used can
generate toxic by-products that can result in cytocompatibility residues in the hydrogel
68
(254). Thus, the hydrogel is usually subjected to a purification step prior to its
application, for example, the modified macromer may require dialysis prior to use.
Furthermore, the photoinitiators themselves can be toxic, Thus, specific care is
required when designing the photocuring system such as using a low concentration of
photoinitiator. Finally, the wavelength and intensity of light can induce genetic
damage within the cells resulting in reduced viability and function, thus this requires
careful consideration (255-259).
Crosslinking mechanism, biofunctionalization, controlled delivery of biochemical
factors and hydrogel physical characteristics are the most crucial parameters that
determine hydrogel suitability for the target application.
Crosslinking mechanisms of hydrogels
The crosslinking mechanisms of hydrogels are broadly classified into two categories
(Figure 2.15): chemically crosslinking (permanent crosslinking) and physical
crosslinking (reversible crosslinking) (260). Chemically crosslinking hydrogels are
formed by covalent bonding that creates a permanent 3D polymer network (261).
Physical crosslinking hydrogels are produced through the entanglement mechanism of
the polymer chains (262). For the fabrication of both scaffolds and cell-laden
constructs, chemical crosslinking is the most suitable mechanism (254, 263, 264).
Figure 2.15: Crosslinking mechanisms using in physical and chemical gelation of
hydrogels (265).
Crosslinking reactions can be induced by using a variety of stimuli such as light, pH
stimulation, ionic exchange, enzymes, and temperature (254). The crosslinking
density strongly determines the characteristics of the hydrogels, such as mechanical,
degradation, porosity, pore size, swelling and biological properties (266, 267).
69
Light initiated crosslinking reactions correspond to the most common approach,
allowing the fabrication of complex structures under relatively mild conditions. Two
different reaction mechanisms are being considered: free radical polymerisation and
click chemistry.
Free radical photopolymerization is a chain growth reaction started by the absorption
of light by photoinitiators. The photoinitiator concentration determines the
polymerisation kinetics and consequently the properties of the polymerised structures.
Radical photopolymerisable hydrogels can be functionalised with cell adhesive
moieties and degradation sites in a relatively easy and reproducible manner (268).
Major limitations are associated to the relatively poor control over the crosslinking
kinetics, the presence of unreacted double bonds which can react with biological
substances, and the generation of heterogeneities due to the random chain reaction
process. As an alternative, orthogonal click reactions (e.g. thiol-norbornene) proceed
under mild reaction conditions with higher efficiency and faster curing kinetics
compared to free radical photopolymerization (269). This step-growth reaction allows
high spatio-temporal control and the fabrication of 3D networks with minimal defects
(270).
Biofunctionalization of hydrogels
Hydrogels for cartilage tissue engineering must be designed to closely capture the
composition, architecture, biophysical properties and biochemical cues of the native
tissue. This is essential to provide a cell-instructive 3D microenvironment that guides
the fate of embedded cells and morphogenesis. In the case of acellular networks,
hydrogel characteristics such as mechanical properties and porosity must ensure
adequate load transfer and eventually promote cell recruitment. Multiple approaches
have been explored to develop photocrosslinkable hydrogels that perform fundamental
functions of the ECM, including the (i) material selection and hydrogel structure, (ii)
modulation of hydrogel viscoelasticity, (iii) bioconjugation of bioactive peptides, and
(iv) tethering of biochemical factors (271).
2.2.5.1 Hydrogel composition and structure
Important design criteria for hydrogels include appropriate mechanical properties,
ensuring nutrient/waste transport and maintenance of cell viability. Several studies
have modulated the mechanical properties of hydrogels by varying the macromer
concentration or crosslinker type/content using a single polymer network. These
70
works demonstrated that hydrogel stiffness has a tremendous impact on matrix
deposition with highly crosslinked networks restricting new tissue formation and
eventually leading to matrix calcification (272, 273). In addition to the matrix stiffness,
it was also reported that the molecular weight (50 to 1100 kDa) and macromer
concentration (2 to 20 % wt ) of methacrylated hyaluronic acid hydrogels determine
the amount and distribution of new ECM via modulation of the gel structure (e.g.,
compressive modulus, swelling ratio) (274). Another important consideration of
hydrogels is to balance the mechanical integrity and the degradation rate. Gel networks
should support tissue growth as the hydrogel degrades, maintaining the structural
integrity of the new ECM. One interesting approach to control the degradation rate of
hydrogels for cartilage applications involves the synthesis of photocrosslinkable
macromers bearing hydrolytically labile linkages. This strategy was explored to design
hydrolytically degradable hydrogels via thiol-ene photopolymerization of norbornene-
modified Poly(ethylene glycol) (PEG) containing caprolactone segments with
hydrolytically labile ester linkages and PEG dithiol crosslinker in the presence of a
photoinitiator (275). Although hydrogels based on a single polymer are relatively
simple to design, their limited mechanical properties and potential reduced cell
viability due to high crosslink density constitute important concerns. To tackle these
limitations, more complex hydrogels have been developed based on the combination
of multiple polymers. Depending on the selected materials and crosslinking
chemistries, different hydrogel structures have been designed, including
interpenetrating networks (IPNs) (276), semi-IPNs (277), double networks (278) and
guest-host networks (279). Wei et al (280) synthetized a two-component guest-host
hydrogel of adamantane-functionalized hyaluronan (HA) as guest polymers and
monoacrylated β-cyclodextrin as host monomers, rapidly crosslinked through UV
photopolymerization. Hydrogels displayed self-healing properties, supported robust
chondrogenesis of embedded human MSCs and stimulated cartilage formation in a rat
model. In addition to the dynamic nature of the network and/or superior mechanical
properties often achieved by more complex hydrogel systems, these gels can also
address key compositional and biological properties of the native tissue by the
incorporation of major components of the cartilage ECM (281). One strategy consists
of the chemical incorporation of ECM components bearing a photocrosslinkable
moiety into the hydrogel network via photopolymerization. This strategy was explored
by Wang et al (282) to evaluate the influence of methacrylated ECM molecules
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(chondroitin sulfate, heparan sulfate and hyaluronic acid) on the in vivo cartilage
formation using ECM-containing hydrogels with tuneable stiffness and controllable
biochemical composition. Methacrylated ECM molecules were incorporated into the
network of PEG dimethacrylate hydrogels through photopolymerization in the
presence of adipose derived stem cells and neonatal chondrocytes. Cellular hydrogels
with varying matrix stiffness and biochemical cues showed increased collagen type II
deposition in both chondroitin sulfate- and hyaluronic acid-containing hydrogels,
while heparan sulfate-containing hydrogels promoted a fibrocartilage phenotype and
failed to retain newly deposited matrix. This study revealed the importance of
biochemical composition of hydrogels and matrix stiffness on the phenotype of
neocartilage formation.
2.2.5.2 Hydrogel viscoelasticity
Traditional hydrogels obtained by photopolymerization reactions are made of strong
covalent bonds, leading to almost purely elastic gel networks. In contrast to native
cartilage tissue, which is viscoelastic and exhibit partial stress relaxation when a
constant strain is applied, chemical hydrogels store cellular forces and resist
deformation. Purely elastic hydrogels with embedded chondrocytes were found to
limit cell proliferation and restrict cartilage matrix deposition to the pericellular space,
probably due to the elastic nature of hydrogels (283). Recent findings have shown that
viscoelastic hydrogels, in which the stress is relaxed over time, support the spreading,
proliferation and differentiation of embedded mesenchymal stem cells in 3D culture
without requiring matrix degradation (284). It has also been reported that cell-laden
hydrogels exhibiting faster stress relaxation support significantly more new bone
growth in vivo when compared to slow stress-relaxing gel networks (285). As stress
relaxation is suggested as a key design parameter of hydrogels to both better
recapitulate the viscoelastic behaviour of natural ECM and perform important
biological behaviours, efforts have been focused on the design of viscoelastic
hydrogels with tuneable stress relaxation for cartilage tissue engineering. In a recent
work, Lee et al, (286), developed a series of viscoelastic alginate hydrogels exhibiting
tuneable stress relaxation to evaluate the effects of viscoelasticity on embedded
chondrocytes in 3D culture. Stress relaxation of calcium-crosslinked hydrogels was
controlled by varying the molecular weight of alginate and covalent coupling of short
PEG spacers. It was found that hydrogels with faster stress relaxation supported the
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formation of increased cartilage matrix with deposition of both collagen and GAGs
(Figure 2.16), while slower relaxing gel networks led to the up-regulation of genes
associated to cartilage degradation and cell death. An alternative approach to engineer
hydrogels with tuneable viscoelastic properties consists on the formation of covalent
adaptable networks with the ability to reorganize the network connectivity to dissipate
local stress. As an example, hydrazone crosslinked PEG hydrogels were synthesised
as viscoelastic gels for cartilage applications (287). After 4 weeks of culture, porcine
chondrocytes embedded within hydrogels exhibiting average relaxation times of 3
days secreted an interconnected articular cartilage-specific matrix with increased
deposition of collagen (e.g., collagen type II) and sulfated glycosaminoglycans (e.g.,
aggrecan) compared to predominantly elastic hydrogels with slow average relaxation
times (~ 1 month). The authors suggested that a balance between slow and fast relaxing
crosslinks is essential to preserve gel network integrity and support the formation of
high-quality neocartilaginous tissue.
Figure 2.16: Influence of hydrogel stress relaxation on cartilage matrix production
and formation. Immunohistochemical staining of chondrocytes embedded within 3
kPa alginate hydrogels for 21 days (scale bar: 25 µm) (170).
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2.2.5.3 Bioconjugation of bioactive peptides
Articular cartilage is an intricate meshwork rich in collagen and proteoglycans. Rather
than a static milieu, the ECM is a highly dynamic microenvironment that establishes
reciprocal interactions with neighbouring cells. Cartilage ECM components provide
biochemical motifs for cell adhesion and degradation sites for cell-mediated matrix
degradation, which are essential to allow cell adhesion, proliferation, migration and
tissue formation. As most cell types require adhesion sites to survive and perform their
functions, several bioconjugation strategies have been explored for the
functionalization of hydrogels with bioactive peptides that impart cell adhesion
domains (288). The fibronectin-derived adhesion peptide RGD (arginine-glycine-
aspartic acid) is often bond to the hydrogel network to promote integrin-mediated cell
binding and allow cell attachment and spreading (276, 289). Other sequences derived
from collagen and decorin have also been immobilized into hydrogels with beneficial
outcomes regarding chondrogenic differentiation of MSCs and matrix retention (290,
291). Since chondrocytes in native ECM display a round morphology, the benefit of
RGD functionalization in chondrocytes is still controversial. For example,
chondrogenesis of bone marrow stromal cells embedded within RGD-functionalized
alginate hydrogels was inhibited in response to TGF-β1 and dexamethasone regarding
gene expression and matrix synthesis (292). Another work showed that
photocrosslinked RGD-modified PEG hydrogels enhanced cartilage-specific gene
expression and matrix synthesis by bovine chondrocytes, but only in the presence of
dynamic mechanical stimulation (293). In fact, most of the hydrogel systems used for
chondrocyte encapsulation did not require cell-adhesion domains to support tissue
formation (277, 286). Overall, this data demonstrates that the immobilization of cell-
adhesion domains in hydrogels perform a key role in terms of cell phenotype and
chondrogenesis, further studies are necessary to elucidate the cell-specific influence
of peptide ligands.
Natural ECM is continuously remodelled by cell-secreted enzymes, which is required
to create space in the matrix for cell migration, proliferation and tissue deposition.
Thus, the development of hydrogels susceptible to hydrolytic and/or cell-driven
degradation is becoming increasingly recognized as a key feature to improve the ECM
biomimicry (294). Hydrolytic degradation of hydrogels is commonly obtained by
hydrolysis of ester linkages, leading to changes in the overall network properties.
While enzymatic degradation depends on the cell type and levels of circulating
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enzymes, hydrolytic degradation is spontaneous and occurs via bulk and/or surface
erosion mechanisms. Cell-driven hydrogel degradation via cleavage of protease-
sensitive peptides occurs in a more localized manner, at the pericellular space, better
recapitulating the remodelling of natural ECM. Hydrogels based on animal polymers
such as fibrin, collagen and hyaluronic acid are naturally degraded, whereas some
plant-based polymers (e.g., alginate, pectin) and synthetic polymers are often modified
to make them susceptible to enzymatic degradation (288). This has been accomplished
by the incorporation of peptide sequences recognized by specific proteases. These
peptides can be grafted into the polymer backbone or used as crosslinker agents with
a dual function – allow gel formation and promote matrix degradation. As an example,
MMP7-degradable hydrogels based on recombinant Streptococcal collagen-like 2
(Scl2) proteins and functionalized with peptides that bind to hyaluronic acid and
chondroitin sulphate were synthetized for cartilage tissue engineering (295). Cell-
degradable hydrogels with embedded hMSCs and functionalized with GAG-binding
peptides significantly enhanced chondrogenic differentiation and gene expression of
COL2A1, ACAN, and SOX9, compared to non-functionalized hydrogels.
2.2.5.4 Tethering and controlled delivery of biochemical factors
Cartilage formation is regulated by a coordinated spatiotemporal delivery of
biochemical factors that interact with cells to induce chondrogenesis. To this end, a
major role of ECM is to serve as a storage depot for growth factors, regulating their
spatiotemporal and tissue-specific presentation to the cells. Its ability to locally bind,
store, and release growth factors is essential to regulate their bioavailability,
bioactivity and stability in order to elicit a biological response (296). The binding of
growth factors to the ECM, for example, via electrostatic interactions to heparan
sulfate, is fundamental to enhance their activity in the vicinity of cells, prolong their
action and protect them from degradation (297).
To recreate the dynamic presentation of bioactive cues available to the cells in native
cartilage, hydrogels have been designed with the ability to sequester and/or deliver
biochemical cues such as growth factors. This has been achieved through different
strategies including the covalent immobilization (298), affinity binding (299), and
encapsulation within carrier vehicles (300). Members of the transforming growth
factor beta (TGF-β) superfamily such as TGF-β1 play a role in regulating
chondrogenesis during development. To allow the immobilization into the hydrogel
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network towards improved bioactivity and cell presentation, growth factors are usually
modified with photoreactive groups. In one example, TGF-β1 was reacted with 2-
iminothiolane, yielding thiolated TGF-β1 that can homogeneously bond throughout
the gel network of non-degradable PEG hydrogels during photopolymerization
without impairing its bioactivity (298). Thiolated TGF-β1 was covalently linked to the
norbornene end groups of PEG hydrogels crosslinked by photoinitiated step-growth
polymerization using an MMP-degradable peptide (KCGPQGIWGQCK) as a
crosslinker (301). The ability of chondrocytes to promote in situ hydrogel degradation
was firstly confirmed using a fluorogenic peptide sensor to determine the extent of
MMP‐sensitive sequence cleavage (Figure 2.17). In this hydrogel, GAG and collagen
deposition was found to be restricted to the pericellular space, which was attributed to
the limited chondrocyte degradation of the gel network to allow diffuse matrix
production. When hydrogels were used to co-encapsulate chondrocytes and hMSCs, a
higher degradation rate was observed, along with increased GAG and collagen
deposition at 14 days of culture compared to non-degradable hydrogels. This data
highlights the importance of cell-degradable motifs and localized presentation of
biochemical cues in photocrosslinked hydrogels to support the formation of cartilage
specific ECM.
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Figure 2.17: Effect of chondrocytes embedded within cell-degradable hydrogels. A)
Schematic illustration of cell-laden hydrogel formation with tethered MMP
fluorescent sensor (Dab‐ GGPQG↓IWGQK‐Fl‐AhxC), and TGF‐β1; hydrogels are
crosslinked using either an MMP‐degradable peptide sequence
(KCGPQG↓IWGQCK) or non‐degradable (3.5 kDa PEG dithiol) linker. B)
Determination of in situ cleavage of fluorescent sensor by chondrocytes. C) GAG
staining of sections from cell-laden hydrogels after 28 days of culture: nuclei stained
black and GAGs stained red. D) Collagen staining of sections obtained from cell-laden
hydrogels at day 28: nuclei stained black and collagen stained blue (scale bars: 100
μm) (185).
Conclusions and future perspectives
Naturally derived hydrogels are suitable materials for cartilage applications. They are
biocompatible and biodegradable with a chemical and physical structure that
resembles the ECM structure of natural tissues. Different light-mediated
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photopolymerization strategies have been explored for the fabrication of scaffolds
with micro- and nano-scale resolutions. These strategies proceed under biocompatible
conditions in the presence of cells and biochemical signals allowing the fabrication of
cell-laden bioconstructs. In order to improve the biological performance of both
scaffolds and cell-laden constructs different biofunctionalisation strategies have been
explored. Many naturally derived hydrogels degrade through enzymatic and/or
hydrolytic mechanisms, adding another layer of complexity to control their
degradation rate. This is an important limitation in terms of the design of suitable
constructs for cartilage tissue engineering.
Another critical challenge in cartilage tissue engineering is the integration and
engineering of hydrogels that are specific for each region of the osteochondral tissue.
The structure and properties of constructs for osteochondral applications must address
the characteristics of the two comprising tissues, articular cartilage and subchondral
bone, which still represents a major research challenge. The section of such constructs
related to the cartilage zone must present adequate mechanical properties to resist
mechanical loading and friction whilst promoting ECM formation and chondrogenic
expression of mesenchymal stem cells or chondrocytes, inhibiting hypertrophic
differentiation and mineralization of chondrocytes in the upper regions of the tissue.
Contrary, the section of the constructs corresponding to subchondral bone must
promote the formation of a blood vessel network, stimulate osteoblast proliferation,
and osteogenic differentiation of mesenchymal stem cells whilst remaining
biomechanically suitable until successful tissue regeneration is complete. How to
engineer hydrogels to promote or inhibit specific cellular behavioural pathways is a
major challenge, for example, a osteochondral hydrogel must promote hypertrophic
chondrocytes in the calcified zone and flatter and aligned chondrocytes in the
superficial surface. This will demand the development of multi-material and multi-
scale hydrogels that are specifically biofunctionalized to promote the complex
behaviour and organisation of chondrocyte cells. Furthermore, top-down fabrication
techniques will need to improve their resolution and multi-material processing
capabilities thus driving demand for hybrid biomanufacturing systems that incorporate
multiple fabrication technologies into a single system. Whilst bottom-up fabrication
processes will require further understanding of the fundamental developmental
biology of osteochondral tissue.
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Chapter 3
Development and
characterisation of a
photocurable alginate
bioink for 3D bioprinting†
† This Chapter is based on the paper: Hussein Mishbak, Glen Cooper, Paulo Bartolo, “Development
and characterisation of a photocurable alginate bioink for 3D bioprinting”, International Journal of
Bioprinting, 5(2): 189, 2019 http://dx.doi.org/10.18063/ijb.v5i2.189. A preliminary version of this
manuscript was also presented at the International Conference on Engineering Science and Applications
(Tokyo, Japan, 2017) and was awarded as the best paper.
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Alginate is a biocompatible material suitable for biomedical applications, which can
be processed under mild conditions upon irradiation. This Chapter investigates the
preparation and the rheological behaviour of different pre-polymerised and
polymerised alginate-methacrylate systems for 3D photopolymerisation bioprinting.
The effect of the functionalization time on the mechanical, morphological, swelling
and degradation characteristics of crosslinked alginate hydrogel is also discussed.
Alginate was chemically modified with methacrylate groups and different reaction
times considered. Photocurable alginate systems were prepared by dissolving
functionalized alginate with 0.5-1.5% photoinitiator solution and crosslinked by
ultraviolet (UV) light (8 mW/cm2).
Introduction
Three different approaches are being explored for tissue engineering applications
(302, 303). The first approach, cell therapy, is based on harvesting cells, sorting,
expanding and implanted them. This is a simple process but presents limited outcomes
as it is difficult to keep the cells in the desired region for clinically relevant periods of
time (289). The second approach, scaffold-based approach, is based on the use of
three-dimensional support structures that provide the necessary environment for cell
attachment, differentiation and proliferation (304). In this approach, scaffolds can be
directly implanted after fabrication or seeded with cells and pre-cultured in a
bioreactor before implantation (305). Finally, the third approach (bioprinting) uses
bioinks (hydrogels and cells) to create cell-laden constructs. This is a highly relevant
approach allowing in situ printing (172, 306). Techniques such as inkjet bioprinting,
extrusion-based and photopolymerization-based process are being explored. Among
them, photopolymerization is a very versatile method allowing a rapid crosslinking
under biocompatible reaction conditions without the use of solvents (172, 302).
Additionally, photocurable hydrogels are particularly relevant for biomedical
applications due to the advantage of being able to encapsulate cells and the mild
processing conditions that allow their in-situ crosslinking within a patient during a
surgical procedure
Suitable hydrogels for bioprinting must be biocompatible, biodegradable, present
appropriate mechanical properties, which depend on the type of tissue, good
printability (307) and shear thinning properties to facilitate the printing process (308).
In the case of photopolymerization bioprinting systems the amount and type of
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photoinitiator is also critical as determines the crosslinking density, cytotoxicity,
mechanical properties and biocompatibility (309). The increase of crosslinking density
is usually associated to an increase of printability and mechanical properties and a
decrease of biocompatibility due to the reduction of free space to accommodate cell
proliferation (310).
Alginate is a suitable material for bioprinting (311). It is a natural water-soluble linear
polysaccharide derived from alginic acid, extracted from several species of brown
algae, such as Laminaria Hyperborea, Ascophyllum Nodosum and Macrocystis
Pyrifera (312-314). Its structure contains 1,4-linked -D-mannuronic (M) and -L-
guluronic (G) acid residues (Figure 3.1), arranged in a non-regular and block-wise
fashion along the chain (315-317). Alginate shows good biocompatibility, low
cytotoxicity and high-water content (high swelling ratio), mimicking the structure of
the natural extra-cellular matrix (318-322). These properties make alginate a suitable
material for wound dressings, drug delivery systems and soft tissue engineering
applications (323).
This Chapter investigates the preparation of alginate-based systems for UV bioprinting
applications. The material is characterised both before and after the curing process and
the effect of functionalization time on the rheological, mechanical, morphological,
swelling and degradation properties investigated. The effect of photoinitiator
concentration in terms of rheological and mechanical properties is also assessed and
discussed.
Figure 3.1: Alginate showing a linkage between the mannuronic and guluronic acid
(324).
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Materials and methods
Synthesis of methacrylate alginate
Photocurable alginates were prepared through a functionalization mechanism with
methacrylate anhydride (MA) (325). Briefly, sodium alginate powder (W201502 ) 1%,
2% and 3% w/v (Sigma-Aldrich, UK) was dissolved in Dulbecco's Phosphate Buffered
Saline (DPBS) (Sigma-Aldrich, UK) and then mixed with methacrylate anhydride
(MA) (Sigma-Aldrich, UK) at 15 mL MA/g of alginate under vigorous stirring. The
pH of the solution was kept around 7.4-8.0 during the reaction time by adding 5M of
NaOH. Maintaining a higher pH during the reaction is crucial since higher pH
enhances the reaction among the amine and hydroxyl groups, which lead to higher
degree of modification (326). Two different reaction times (8 and 24 hours) were
considered to assess the effect of the reaction time on the degree of functionalisation.
After the chemical modification reaction, the polymeric solution was precipitated and
totally mixed in 100 mL of ethanol (100% ethanol) and dried in an oven overnight at
50 ºC. The precipitate polymer was dissolved in distilled water (diH2O), loaded in the
dialysis tubes membranes (SnakeSkin Dialysis Tubing 3.5K MWCO from Thermo
Fisher Scientific, UK), sealing both sides and dialyzed the solution against NaCl for 7
days with periodic water changes every day. The solution was freeze at -80ºC and the
polymer recovered by lyophilisation.
Characterisation of pre-polymerised methacrylate alginate
3.2.2.1 Nuclear magnetic resonance
The chemical structure of functionalized alginate was assessed through Nuclear
Magnetic Resonance Spectroscopy (1HNMR), using the B400 Bruker Avance III 400
MHz (Billerica, Massachusetts, USA). Polymeric materials were dissolved in
Deuterium oxide (D2O) (Sigma-Aldrich, UK), transferred to NMR tubes and the
spectra acquired with 128 scans.
3.2.2.2 Rheological characterisation
The rheological tests were performed to characterise the viscoelastic behaviour of both
pre-polymerised and polymerised alginate. The rheological assessment of pre-
polymerised alginate systems was carried out using the DHR2 TA Instrument (USA).
Samples were placed between two parallel plates and two different tests (rotational
and oscillation) were considered. Rotational tests were performed to evaluate the
viscosity and the material strength. In these tests it is assumed that the material flows
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by applying a stress, being the response measured alongside time (temperature was
not considered in this work). A controlled stress was applied, and the resulting
movement measured. Oscillation tests were considered to evaluate the viscoelastic
behaviour of the material and dynamic moduli. The viscoelastic behaviour was
characterized by measuring the energy stored (storage modulus, Gʹ) in the material
during shearing and the energy subsequently lost (loss modulus, Gʺ). Shear strain was
controlled by varying the oscillation amplitude.
To assess the rheological changes during the photopolymerization process, the
rheological tests were carried out using the Bohlin Gemini system (Malvern
Instruments) equipped with the OmniCure® S1000 light source irradiating in the range
of 254-450 nm wavelength, and oscillation tests were considered. The light intensity
was 10 mW/ cm2.
The rheological behaviour of the materials is described by the following equation:
τ = ɳ ��n (3.1)
where τ is the shear stress (Pa), �� is the shear rate (s-1), ɳ the consistency index or
equivalent viscosity (Pa. s) and n is the power law index (dimensionless) that varies
as follows:
n<1: shear-thinning system;
n=1: Newtonian system;
n>1: shear-thickening system.
Hydrogel formation
Photocrosslinked alginate methacrylate hydrogels were prepared by dissolving 2%
w/v alginate-methacrylate with different photoinitiator concentration solutions 0.5%
w/v, 1% w/v and 1.5% w/v of VA-086 photoinitiator solution (2,2'-Azobis[2-methyl-
N-(2-hydroxyethyl) propionamide azo initiator (Wako Pure Chemical Industries,
USA). Crosslinked disks were produced by pipetting the alginate solution in an acrylic
mould with 8 mm diameter and 4 mm height. Photopolymerization was conducted
using a 365nm UV light (Model Dymax 2000-EC, Dymax Europe GmbH, Wiesbaden,
Germany) irradiating at 8 mW/cm2 during 8 min.
The photopolymerization process of alginate-methacrylate is a radicular
polymerization process started by the absorption of UV light by the photoinitiators,
followed by the generation of free radicals and a crosslinking chain reaction (327).
The mechanism is briefly presented in Figure 3.2.
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Figure 3.2: Schematic representation of the photopolymerization process of alginate-
methacrylate. a) After exposing the polymer solution to UV radiation, the
photoinitiators generated free radicals that react with the vinyl methylene starting the
crosslinking reaction; b) The reaction propagates with macro-radicals reacting with
unreacted carbon-carbon double bonds; c) At the end through a bimolecular
termination mechanism a 3D network of crosslinked hydrogel is formed. Adapted
from (328).
Characterisation of photocrosslinked hydrogels
3.2.4.1 Morphological characterisation
The morphology of the internal structure of the hydrogels was investigated through
Scanning Electron Microscopy (SEM), using the Hitachi S3000N VPSEM system.
Alginate samples were produced using cylindrical moulds (8 mm diameter and 4 mm
high). After hydrogel formation, samples were extensively washed in distilled water,
frozen at -80°C and lyophilized. Samples were fixed on stubs using a double-sided
adhesive tape and sputter coated with platinum sputter-coating.
3.2.4.2 Mechanical characterisation
Compression tests were performed at constant strain rate using the Instron 3344
machine equipped with a 10-N load cell (Instron, Buckinghamshire, UK). Crosslinked
alginate hydrogel disks were prepared as described in Section (3.2.3) and maintained
in distilled water at 37ºC following the protocol described by Jeon (325). After 24
hours of incubation, swollen alginate-methacrylate hydrogel disks were measured
using callipers to determine both the diameter and thickness, and unconfined
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compression tests were performed on the hydrogel disks at room temperature, 0.5
mm/min of speed at a rate of 20% strain. Compressive modulus was determined from
the slope of stress versus strain plots and limited to the first 10% of strain as
recommended for cartilage applications (329).
3.2.4.3 Swelling and degradation characterisation
Alginate methacrylate hydrogel disks were frozen at -80 ºC, then, lyophilized and the
dry weights (Wi) were measured. Afterwards, the dried hydrogel samples were
immersed in distilled water (diH2O) and the same number of samples were also
immersed in Dulbecco’s Modified Eagle’s Medium - high glucose (DMEM) (Sigma-
UK) diluted with 10% FBS (Fetal Bovine Serum) (Thermofisher, UK) at pH 7 and
incubated at 37 ºC to reach an equilibrium swelling state. The distilled water and
DMEM were replaced every 1-2 days. Over the course of 3 weeks, samples were
removed from the DMEM/diH2O and the swollen hydrogel sample weights (Ws)
measured. The swelling ratio (Q) was calculated according to the following equation:
𝑄 =Ws
Wi (3.2)
where Wi is the dry weight and Ws is the weight of the swollen hydrogel sample. After
this, the swollen hydrogels were lyophilized and weighed again. The percentage of
mass loss was calculated as follows:
(Wi-Wd)/Wi x 100 (3.3)
where Wd is the weight after lyophilisation (N=3 for each time point).
Results and discussion
Alginate functionalization
The alginate modification with methacrylate anhydride was performed under standard
conditions, allowing the introduction of photo-reactive methacrylate groups into the
polymer backbone, as confirmed by 1HNMR analysis (Figures 3.3 to 3.5). Results
indicate the present of new characteristic peaks of methacrylate (MA) at 5.63 ppm and
6.09 ppm attributed to the methylene group in the vinyl bond, and a peak at 1.82 ppm
assigned to the methyl group, which are not present in the non-modified polymer,
showing that the polymers were successfully functionalized. Two different
functionalisation reaction times (8 and 24 hours) were also considered and the degree
of modification determined by dividing the relative integrations of methylene to
carbohydrate protons (330, 331). Results, presented in Table 3.1, show that the degree
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of modification increases by increasing the reaction time, reaching a maximum value
of 33 % at 24 hours.
Table 3.1: Effect of reaction time on the modification degree of alginate methacrylate.
Composition (% w/v) Reaction time (h) Degree of modification (%)
2% 8 21
2% 24 33
Figure 3.3: a) Non-functionalized alginate 1% w/v; b) Functionalized alginate 1% w/v
after 8 hours of reaction; c) Functionalized alginate 1% w/v after 24 hours of reaction.
The functionalization is confirmed by the presence of new peaks in the spectra at 5.63
ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82 ppm that
corresponds to the methyl group.
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Figure 3.4: a) Non-functionalized alginate 2% w/v, b) Functionalized alginate (2%
w/v) after 8 hours of reaction, c) Functionalized alginate 2% w/v after 24 hours of
reaction. The functionalization is confirmed by the presence of new peaks in the
spectra at 5.63 ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82
ppm that corresponds to the methyl group.
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Figure 3.5: a) Non-functionalized alginate 3% w/v; b) Functionalized alginate 2% w/v
after 8 hours of reaction; c) Functionalized alginate 2% w/v after 24 hours of reaction.
The functionalization is confirmed by the presence of new peaks in the spectra at 5.63
ppm and 6.09 ppm attributed to the methylene group and a peak at 1.82 ppm that
corresponds to the methyl group.
Rheological behaviour of pre-polymerised alginate methacrylate systems
Figures 3.6 to 3.9 show the stress versus shear rate behaviour of solutions containing
1, 2 and 3% w/v of alginate-methacrylate reacted for 8 and 24 hours. Key rheological
parameters are presented in Tables 3.2 and 3.3. A non-linear behaviour is observed for
all samples. Samples containing 2% w/v obtained after 24 hours of reaction show a
clear Bingham behaviour (332). Results also show a decrease of the equivalent
viscosity by increasing the alginate concentration for samples obtained after 24 hours
of reaction, while no trend was observed for samples obtained after 8 hours of reaction.
The flow behaviour is also closer to a Newtonian fluid for samples containing high
concentrations of alginate. Based on these results the system containing 2% w/v of
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alginate was selected as presents less variation of viscosity with the reaction time and
a clear shear-thinning behaviour being also less dependent with the reaction time
compared to the other systems.
Table 3.2: Rheological constants for solutions containing 15 mL of methacrylate
and different alginate concentrations, 24 h.
Composition (%w/v) Equivalent viscosity (Pa. s) Power law constant
1 4.36 ± 0.012 0.23
2 0.54 ± 0.014 0.68
3 0.16 ± 0.020 0.72
Table 3.3: Rheological constants for solutions containing 15 mL of methacrylate
and different alginate concentrations, 8h.
Composition (%w/v) Equivalent viscosity (Pa. s) Power law constant
1 0.09 ± 0.011 0.81
2 0.48 ± 0.012 0.48
3 0.08± 0.010 0.74
Figure 3.6: Stress versus shear rate profiles for alginate-methacrylate solutions
containing different alginate-methacrylate concentrations, reacted for 8 hours. a) 1%
w/v of alginate; b) 2% w/v of alginate; c) 3% w/v of alginate, and d) comparison of
all compositions.
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Figure 3.7: Stress versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 24 hours. a) 1% w/v of alginate, b) 2% w/v of
alginate, c) 3% w/v of alginate, and d) comparison of all compositions.
Figure 3.8: Viscosity versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 8 hours. a) 1% w/v; b) 2% w/v; c) 3% w/v d)
comparison of all compositions.
90
Figure 3.9: Viscosity versus shear rate for solutions containing different alginate-
methacrylate concentrations reacted for 24 hours. a) 1% w/v; b) 2% w/v; c) 3% w/v
d) comparison of all compositions.
Figure 3.10 and 3.11 show the variation of storage modulus (G'), loss modulus (G''),
complex modulus and tanδ as a function of frequency and strain for systems containing
2% w/v alginate-methacrylate concentrations and different reaction times. The results
show that both the storage and loss modulus are higher in samples obtained after high
functionalisation times. In both cases the complex modulus increases with frequency,
while the variation of G' and G'' with strain shows a shift point after which G'' becomes
higher than G'. This shift occurs at high frequencies for alginate samples obtained with
high functionalisation times.
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Figure 3.10: 2% wt. Alginate solution reacted for 8 hours. a) Storage and loss modulus
vs strain b) Storage and Loss modulus vs frequency; c) Complex modulus vs
frequency; d) tan δ vs frequency.
Figure 3.11: 2% wt. Alginate solution reacted for 24 hours. a) Storage and loss
modulus vs strain; b) Storage and Loss modulus vs frequency; c) Complex modulus
vs frequency; d) tan δ vs frequency.
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Rheological changes during the photopolymerization process
Based on the characterisation of the pre-polymerised samples only systems containing
2% w/v of alginate were considered for photopolymerization studies. The curing
kinetics was assessed by monitoring the variation of Gʹ and G" at room temperature
through a controlled frequency of 1Hz. Photo-rheology was used to characterise the
curing process (photopolymerization) of functionalised alginate polymers obtained
after 8 and 24 hours of reaction time, mixed with 0.5% w/v, 1% w/v and 1.5% w/v of
VA-086 photoinitiator.
As observed from Figures 3.12 and 3.13 by increasing the curing time Gʹ increases
becoming significantly higher than Gʺ showing the liquid to solid phase change of the
material. It is also possible to observe that by increasing the photoinitiator
concentration the gelation time, which corresponds to the time point where the Gʹ
curve crosses the Gʺ curve, decreases. It is also possible to observe that by increasing
the amount of photoinitiator Gʹ seems to tend to a plateau which corresponds to a
vitrification stage of the curing process (333, 334). The possible explanation for this
observation is that, for the layer thickness considered in this study (~100 µm), the
photoinitiator concentration is approaching a critical value. By increasing the
photoinitiator concentration above the critical values, the polymerization occurs very
fast at the polymer surface, reducing the light penetration and, consequently, the
overall polymerization reduces.
Figure 3.12: 2% wt. methacrylate alginate with different concentration of VA-086
photoinitiators functionalized for 8 hours a) 0.5% w/v of PI; b) 1% w/v of PI; c) 1.5%
w/v of PI; d) 0.05% w/v of PI.
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Figure 3.13: 2% wt. methacrylate alginate with different concentration of VA-086
photoinitiators functionalized for 8 hours a) 0.5% w/v of PI ; b) 1% w/v of PI; c) 1.5%
w/v of PI.
Viscoelastic properties of formed hydrogels
Hydrogel disks (4 mm of height and 8 mm of diameter) were produced using an acrylic
machined mould. Samples of 2 % w/v of alginate-methacrylate obtained after both 8
and 24 hours of reaction time containing different concentrations of photoinitiator
(0.5, 1 and 1.5% w/v) were polymerised during 8 minutes under a light intensity of 8
mW/cm2. Produced disks were then assessed and both Gʹ and G" measured at room
temperature through a controlled frequency of 1Hz as presented in Figures 3.14 and
3.15. In the case of alginate-methacrylate samples obtained after 8 hours of reaction
time it’s possible to observe that there is no significant change of both Gʹ and G" (the
storage modulus is always higher than the elastic modulus) with the increase in the
photoinitiator concentration. In the case of alginate-methacrylate samples obtained
after 24 hours of reaction time, results show that by increasing the photoinitiator
concentration Gʹ and G" increases. In this case, it is also possible to observe that the
difference between Gʹ and G" increases with the increase of photoinitiator
concentration, which is associated to the high crosslinked density.
The viscoelastic nature of the crosslinked disks is also observed from the Gʹ and G"
versus strain graphs. In this case, it is possible to observe for all samples that, till a
critical strain value, the storage modulus is higher than the loss modulus. After the
strain critical value, the loss modulus become more significant due to the break of the
crosslinked network. In the case of alginate-methacrylate samples obtained after 24
hours of reaction time, the storage modulus is always higher than the storage modulus
of alginate-methacrylate samples obtained after 8 hours of reaction time. This is due
to the high-crosslinking density of the alginate-methacrylate samples obtained after 24
hours of reaction time.
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Figure 3.14: 2% wt methacrylate alginate hydrogel with different concentration of
VA-086 functionalized for 8 hours a) 0.5% w/v of PI; b) 1% w/v of PI; C) 1.5% w/v
of PI.
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Figure 3.15: 2% wt methacrylate alginate with different concentration of VA-086
functionalized for 24 hours. a) 0.5% w/v of PI; b) 1% w/v of PI; C) 1.5% w/v of PI.
Internal morphology of alginate hydrogels
The internal structure of crosslinked alginate is presented in Figure 3.16. SEM images
were obtained for samples containing 2% w/v of alginate prepared during 8 and 24
hours of reaction time and 1% wt of photoinitiator. Results show that the reaction time
influences the hydrogel morphology, with high reaction times being associated to
structures presenting both small pore size and number of pores. In addition, results
seem to indicate that long reaction times generate structures with more closed pores.
Results also show associated porosity of 94.5% ± 0.75 (292.5 µm ± 10 pore size) and
90.8% ± 0.21(252.5 µm ± 20 pore size) for 8 and 24 h respectively.
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Figure 3.16: SEM images of crosslinked methacrylate-alginate hydrogel structures
obtained from alginate-methacrylate at different reaction times: 8 and 24 hours.
Mechanical characterisation
The mechanical performance of crosslinked alginate structures is presented in Figures
3.17 and 3.18. As observed, high compression moduli were obtained for crosslinked
disks produced with high functionalization times (13.16 kPa for 24 hours of reaction
time and 2.63 kPa for 8 hours of reaction time) and 0.5% w/v photoinitiator
concentration. These results can be explained by the high crosslinking density that
characterizes the structures obtained from alginate samples functionalized during long
reaction times and the corresponding internal morphology characterized by small size
and low number of pores. It also possible to observe that the mechanical properties
increase by increasing the photoinitiator concentration. For samples containing 1.5%
w/v of photoinitiator, compression moduli were obtained (75.4 kPa for 24 hours of
reaction time and 7.23 kPa for 8 hours of reaction time).
Figure 3.17: Compression tests for alginate methacrylate samples (8h) with different
photoinitiator concentrations a) 0.5% w/v; b) 1% w/v; and c) 1.5 % w/v.
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Figure 3.18: Compression tests for alginate methacrylate samples (24h) with different
photoinitiator concentrations a) 0.5% w/v; b) 1% w/v; and c) 1.5 % w/v.
Swelling and degradation kinetics
The swelling and degradation behaviour of crosslinked alginate hydrogel disks are
presented in Figure 3.19. Results show that samples absorb both DMEM and distilled
water until reaching a state of equilibrium. This state is accomplished when the
osmotic pressure from the swelling and the elasticity of the hydrogel network is equal.
It is also possible to observe that crosslinked samples prepared with alginate-
methacrylate obtained after 24 hours of functionalization present low swelling ratio,
which shows that the degree of crosslinking controls the swelling properties of the
hydrogel. In all samples, the equilibrium status was reached at day 3. Crosslinked
alginate structures based on functionalized alginate prepared during 24 hour of
reaction time swelled up to 155%, while alginate structures based on functionalized
alginate prepared during 8 hour of reaction time swelled up to 190 %. Moreover, it is
also possible to observe that the level of functionalization of the pre-polymerised
alginate not only determines the internal morphology of the crosslinked structures but
also the degradation process as shown in Figures 3.19b and d.
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Figure 3.19: Swelling and degradation rate for 2% wt. functionalized alginate (24 and
8) hours reaction time in a) distilled water b); degradation rate in distilled water; c)
DMEM; d) degradation rate in DMEM.
Conclusion
This Chapter describes the synthesis and characterisation of alginate systems for UV-
based bioprinting applications. The alginate was successfully functionalized in the
presence of methacrylate in order to introduce the necessary number of unsaturation
allowing its crosslinking upon photopolymerization. Two different functionalization
reaction times were considered and photocurable systems containing different
photoinitiator concentrations prepared. From the results it is possible to conclude that
high functionalization reaction times originates crosslinked structures with less
porosity, smaller pores and a larger number of closed pores, less swelling, higher
degradation properties and higher mechanical stiffness. By increasing photoinitiator
concentration it was possible to observe an increase of mechanical properties and
gelation time. Moreover, for high values of photoinitiator concentration the reaction
tends to reach verification.
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Chapter 4
Photocurable alginate
bioink development for
cartilage replacement
bioprinting†
† This Chapter based on the book Chapter: Hussein Mishbak, Enes Aslan, Glen Cooper, Paulo Bartolo,
“Photocurable alginate bioink development for cartilage replacement bioprinting”, Progress in Digital
and Physical Manufacturing. Lecture Notes in Mechanical Engineering, Springer. 2020. ISBN. 978-3-
030-29040-5
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Bioink design and assessment for tissue engineering replacement is a key topic of
research. This Chapter investigates suitable photocurable alginate bioink macromers
for bioprinting of 3D constructs for cartilage replacements. Alginate chemically
modified with methacrylate anhydride groups was assessed through different
techniques. 2% Alginate methacrylate (AlgMA) solutions containing different contents
of methacrylate at different reaction times were assessed. The methacrylate
functionalization and the degree of modification through various reaction times were
assessed through nuclear magnetic resonance (NMR), showing the ability to tune the
unsaturation degree by changing the reaction conditions. AlgMA synthesized using
different reaction times were also characterized by rheological analysis to investigate
the effect of reaction time on the rheological behavior. Results show that all Alginate
methacrylate samples exhibit a shear thinning behavior and the initial viscosity is
affected by the reaction time and methacrylate concentrations. These results indicate
that both the reaction conditions and methacrylate concentrations are of paramount
importance to control the extent methacrylation and rheological properties, which is
critical to design bioinks with appropriate properties of extrusion printing.
Biocompatibility and ecotoxicity were assessed through chondrocyte encapsulation.
Introduction
Articular cartilage is a non-vascularized tissue, covering the distal ends of the bones,
formed by a low density of cells called chondrocytes that maintain the structural and
functional integrity of the extracellular matrix (335-337). Cartilage is characterized by
a distinct zonal structure comprising, in descending order, the articular or superficial
surface, the middle (or transitional) zone, the deep zone, and the tidemark that
separates the non-calcified and calcified regions (181). However, it lacks inherent self-
repair capacity and hence the zonal structure and function are often irreversibly lost
following trauma and disease (338). As a result, cartilage defects are prone to develop
into osteoarthritis (OA), which is the predominant cartilage disease, characterized by
loss of cartilage, pain and debilitation (339). Despite the current therapeutic strategies
such microfracture, autologous chondrocyte implantation (ACI), matrix-assisted
autologous chondrocyte transplantation/implantation (MACT/MACI), autologous
matrix-induced chondrogenesis (AMIC), and osteochondral auto- and allografts (340,
341), articular cartilage repair is still a major clinical challenge. Tissue engineering
strategy emerged as a potential therapy through the fabrication of constructs
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mimicking the ECM structure of articular cartilage (342). Through this approach
different biocompatible and biodegradable materials with or without cells were
explored.
This Chapter focus on the use of photocurable alginate as a carrier of chondrocyte cells
for cartilage repair. Alginate material considered in this Chapter was previously
characterized in Chapter III and the rheological properties were further assessed in
order to guarantee good printability. Two different methacrylate concentration (15 and
25 mL for each gram of alginate) and two different reaction times (8 and 24 hrs) were
considered for each methacrylate concentration. Finally, cell-laden constructs were
produced, and cytotoxicity and cell proliferation tests performed.
Materials and methods
Synthesis of methacrylated alginate
Methacrylate alginate was prepared following a published protocol (343). In this
study, 2% wt of sodium alginate powder (W201502) was completely dissolved in
Dulbecco's Phosphate-Buffered Saline (DPBS) (Sigma-Aldrich, UK). Afterwards,
methacrylate anhydride (Sigma-Aldrich, UK) was added to alginate solution. The pH
of the solution was kept around 7-8.0 during the reaction time by adding 5M of NaOH.
After the chemical modification, the polymer solution was precipitated with 100%
ethanol, dried in an oven overnight at 40-50 Cº, then diluted with distilled water and
purified through dialysis for 6 days (SnakeSkin™ Dialysis Tubing, 3.5K MWCO-
Thermo fisher, UK). The solution was frozen at -80ºC and the polymer recovered by
lyophilization. Two different methacrylate concentration (15 and 25 mL for each gram
of alginate) were used and two different reaction times (8 and 24 hrs) were considered
for each methacrylate concentration. Crosslinked discs were produced by dissolving
the functionalized alginate (AlgMA) polymer in a 1% w/v photoinitiator solution (PI)
VA-086, 2,2'-Azobis[2-methyl-N-(2-hydroxyethyl) propionamide azo initiator (Wako
Pure Chemical Industries, USA). The photocurable material was then pipetting into a
custom-made cylindrical Teflon mould (diameter: 8 mm; height 4 mm).
Photopolymerization was conducted using a 365 nm UV light (Dymax 2000-EC,
Dymax, Germany) irradiating at 8 mW/cm2 for 8 min.
HNMR
1HNMR was used to characterize the chemical modification of alginate. Methacrylate
alginate solution was dissolved in deuterium oxide D2O and placed in an NMR tube.
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The 1HNMR spectra were recorded using the B400 Bruker Avance III 400 MHz
(Billerica, Massachusetts, USA) and the spectra acquired with 128 scans.
Rheological characterization
The rheological tests were carried out using the DHR2 TA Instrument (USA).
Rotational tests were considered, and all measurements were conducted at room
temperature.
Cell viability and proliferation
The cytotoxicity of the hydrogels was investigated through the encapsulation of
human chondrocyte cells (Cell Applications, USA) and a live/dead assessment
(Thermofisher Scientific, UK). Chondrocyte passage 4 were encapsulated at a density
of 0.75x106 cell/mL on sterilized hydrogel precursor solution. 160 µL of gel-cell
solution was pipetted into a 24-well custom mould and a UV radiation (365 nm of
wavelength emitted by a Dymax 2000-EC Lamp (Dymax 2000-EC, Dymax,
Germany) during 8 min with a light intensity of 8 mW/cm2. After 3 and 7 days the
cytotoxicity was analyzed by removing cell culture media, washing gently in DPBS
adding a live dead stain solution, and incubating for 30 min. The hydrogels were then
observed using a confocal fluorescence microscope (TCS-SP5, Leica, Germany). The
Alamar blue assay was also used to evaluate cell metabolism and proliferation after 1,
3, 5 and 7 days of culture.
Result and discussion
Chemical modification through 1HNMR
1HMNR results of non-functionalized and functionalized alginate are show in Figure
4.1. In the case of functionalized alginate results show the appearance of characteristic
peaks of methacrylate (MA) at 5.53 ppm and 6.10 ppm attributed to the methylene
group in vinyl bond, and a peak at 1.82 ppm associated to the methyl group. These
peaks are not presented in the nonmodified alginate (Figure 4.1a). The effect of
reaction time and methacrylate anhydride concentration on the degree of modification
(i.e., on the extent of methacrylation) determined by dividing the relative integrations
of methylene to carbohydrate protons (344), is shown in Table 4.1. In the case of 15
ml MA, Results show that the degree of modification increases by increasing the
reaction time, reaching a maximum value of 72.1% at 24 hours. However, by
increasing the methacrylate anhydride concentration up to 25 ml MA, the degree of
modification decreases, reaching 40.3% for 24h reaction time. We hypothesized that
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the reduction on the degree of modification can be a result of the unreacted
methacrylate, hydrolysis in aqueous conditions and elevated temperature (40ºC)
during the reaction as well as possible reactions between methacrylate groups during
dialysis, as previously reported (234). These results suggest that the modification
efficiency with methacrylic anhydride is significantly affected by the methacrylate
concentration.
Figure 4.1: 1H NMR spectra of a) unmodified alginate and; b) 2% wt methacrylate
alginate (15 mL MA) after 8 hrs of reaction; c) 2% wt methacrylated alginate (25 mL
MA) after 8 hrs of reaction; d) 2% wt methacrylate alginate (15 mL MA) after 24 hrs
of reaction.
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Table 4.1: Effect of reaction time on the degree of modification.
Composition (2 % w/v) Reaction time (hours) DoM (%)
AlgMA Low MA (15 ml) 8 55.9
AlgMA Low MA (15 ml) 24 72.1
AlgMA High MA (25 ml) 8 49.6
AlgMA High MA (25 ml) 24 40.35
Rheological characterization of alginate methacrylate
Figure 4.2 shows the variation of both the stress versus shear rate and the variation of
viscosity versus shear rate considering different reaction rates and methacrylate
concentration. Results show that all samples present a shear thinning behavior making
them suitable for printing. It is also possible to observe that by increasing the reaction
time the maximum stresses supported by the non-polymerised AlgMA increases. For
longer reaction times and high concentration of methacrylate mechanical properties
increases. Therefore, low methacrylate concentration (15 mL/g of alginate) will be
considered.
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Figure 4.2: Rheological characterization of 2 % wt methacrylate alginate samples. a)
Stress vs shear rate profile for samples functionalized for 8 hrs reaction time with
different methacrylate concentrations; b) Stress vs shear rate profile for samples
functionalized for 24 hrs reaction time with different methacrylate concentrations; c)
Viscoelastic behaviour low methacrylate concentration (15 mL); d) Viscoelastic
behaviour high methacrylate concentration (25 mL).
Cell viability assessment
Cell viability assessment was examined using a live/dead assay (Figures 4.3 a, b, c and
d). As observed for both the 3D cell laden constructs and 2D cell culture after 3 and 7
days of cell encapsulation, cell viability is higher than 85% with only few dead cells
being observed. The results demonstrate that the functionalized hydrogel presents low
cytotoxicity being a suitable bioink materials. The metabolic and proliferation of
human chondrocyte cells was also assessed using the Alamar blue assay (Figure 4.3e).
Results show that the encapsulated cells with AlgMA hydrogels present good
proliferation rate at day 1 and 3, while after day 5 cell proliferation starts to decrease.
This can be explained by the confined space available for cells due to the absence of
any degradable sites. Moreover, these results show that photocrosslinkable AlgMA
hydrogels are biocompatible and adequately support the encapsulated cells.
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Figure 4.3: Live/dead results at a) day 3, in AlgMA hydrogels; b) day 3, in the control;
c) day 7, in AlgMA hydrogels; d) day 7, in the control; and Alamar blue results e)
Fluorescence intensity as a function of time for different time point (1, 3, 5 and 7 days).
Note: in the live/dead results green corresponds to live cells and red to dead cells.
Conclusions
A bioink for cartilage applications is presented. Alginate was functionalized with
methacrylate groups and the effect of reaction time and methacrylation concentrations
on the degree of substitution and rheological properties were assessed through NMR
and rheological analysis, respectively. NMR data clearly show the ability to tailor the
methacrylation degree by changing the reaction time and methacrylate anhydride
concentration, enabling to tailor the properties of the bioink. Successful cell laden
constructs were produced, showing that the bioink is able to support cell proliferation
after 7 days of photopolymerization. No cytotoxicity emerging from both the alginate
and the photoinitiator was observed.
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Chapter 5
Photocrosslinkable gelatin
methacrylate (GelMA)
hydrogels: Towards 3D
cell culture and
bioprinting for cartilage
applications†
† This Chapter based on the paper: Hussein Mishbak, Glen Cooper, Paulo Bartolo, “Photocrosslinkable
Gelatin Methacrylate (GelMA) Hydrogels: towards 3D cell culture and bioprinting for cartilage
applications”, Journal of Applied Polymer Science, submitted.
108
Tissue engineering This Chapter investigates the use of gelatin methacrylate (GelMA)
as a potential photocurable bioink for cartilage applications. The methacrylate
functionalisation process is discussed, and the level of functionalisation investigated.
Photocurable constructs are produced using ultraviolet radiation (8 mW/cm2) and 8
min of irradiation time. The influence of the functionalisation time, polymer
concentration, degree of modification and viscoelastic behaviour on the mechanical
strength and cell viability is also discussed. Results show that the increase of polymer
concentration, photoinitiator concentration and reaction time increase the
mechanical properties. Moreover, compression results show acceptable values for
cartilage applications (up to 76 kPa). Rheology shows that the GelMA presents shear
thinning behaviour and proper crosslinking structure to support encapsulated cells
during the printing process. High cell viability (85-90%) is also observed.
Introduction
Osteoarthritis (OA) is a critical clinical irreversibly cartilage defect developed after
trauma or disease (175-178, 345, 346). Currently, OA is treated through a wide range
of therapies including chondrocyte implantation (347), bone marrow stimulation
(347), mosaicplasty (348), osteochondral implantation (349) and autologous and
allogeneic tissue transplantation (350). However, these therapies present several
limitations such as the formation of inferior fibrocartilage, donor site morbidity,
limited prevention of continued tissue degeneration and in some cases two surgeries
are required (351-353). Cell laden approaches have the potential to solve these
limitations. In this case additive manufacturing technologies are used to create the
constructs using bioinks made of suitable hydrogels and encapsulated cells. However,
the design of these bioinks is complex requiring complex mechanical-rheological-
degradation-and biological relationships to be addressed. Moreover, selected
hydrogels must present a structure resembling the structure of the native tissue and
good bio affinity to support cell encapsulation and sustain cell differentiation,
proliferation, cell-cell networks and extra-cellular matrix (ECM) formation (354).
Cell laden cartilage constructs can also be produced using both chondrocytes or
mesenchymal stem cells (MSCs) (355). Several crosslinking methods have been
explored to create cell laden constructs using different types of bioinks and successful
results were obtained for different types of tissues such as skin, (356, 357), bone (358),
cardiac (359), and liver (360) . Among these methods, photoinitiated crosslinking is
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particularly relevant as it is a relatively simple process, fast and can be performed
under physiological conditions (361). For cartilage, different photocrosslinkable
hydrogels were investigated (362, 363).
Among the different possible natural hydrogel materials, gelatin obtained from partial
hydrolysis of collagen and presenting arginyl-glycyl-aspartic acid (RGD) cell
adhesion motifs and matrix-metalloproteinase (MMP) degradation sites (356, 365), is
an ideal candidate for cartilage bioinks.
This Chapter investigates the use of gelatin as a potential photocurable bioink for
cartilage applications. The methacrylate functionalisation process is discussed, and the
level of functionalisation investigated. Photocurable constructs are produced using
ultraviolet radiation (8 mW/cm2) and 8 min of irradiation time. The influence of the
functionalisation time, polymer concentration, degree of modification and viscoelastic
behaviour on the mechanical strength and cell viability is also discussed.
Experimental
Synthesis of methacrylated gelatin
Photocrosslinkable gelatin was prepared through methacrylate functionalization
(Figure 5.1) following a protocol previously reported by Van den Bulcke et. al (366).
Briefly, powder of gelatin bovine skin type B (G9382) (Sigma-Aldrich, UK) was
dissolved at a concentration of 12.5% wt in Dulbecco's Phosphate Buffered Saline
DPBS (Sigma-Aldrich, UK) under a constant temperature of 50 °C. Then, 10% v/v
(10x molar excess) of methacrylate anhydride (MA) (Sigma-Aldrich, UK) was added
under vigorous stirring. The pH of the gelatin solution was kept around 7.4-8.0 during
the reaction period. Maintaining a higher pH during the reaction time is crucial to
enhance the reaction between the amine and hydroxyl groups, which lead to high
degree of modification. Different reaction times (2, 4 and 6 hrs) were considered.
Afterwards, the solution was diluted with of DPBS at 40 ºC, loaded at high
permeability dialysis tubes (12-14 kDa) (Spectra/Por 2, US) and purified against
distilled water for 7 days at 45 °C, changing water every day to remove the methacrylic
acid and other impurities. Finally, the pH of the final product was adjusted to 7~7.4
and frozen at -80 °C and the polymer recovered by lyophilization for 72 hours. The
final product (modified polymer) was frozen at -20 °C until further use.
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Figure 5.1: Schematic crosslinking mechanism of gelatin and methacrylate.
Photocurable hydrogel solutions
After gelatin functionalisation, 10 and 15% wt of gelatin methacrylate (GelMA)
concentrations were diluted with a photoinitiator solution (VA-086) (2,2'-Azobis[2-
methyl-N-(2-hydroxyethyl) propionamide azo initiator (Wako Pure Chemical
Industries, USA). Two different photoinitiator concentrations were considered (1 and
1.5% wt). Crosslinked discs were produced by pipetting the photocrosslinkable
GelMA solution in an acrylic mould with a diameter of 8 mm, and 4 mm of height,
then irradiated with a UV light source (365 nm wavelength) using a UV lamp model
Dymax 2000-EC (Dymax Europe GmbH, Wiesbaden, Germany). Light intensity at
the material surface was fixed at 8 mW/cm2 and the material was irradiated for 8
minutes.
HNMR characterization
The chemical structure of functionalized gelatin was assessed using the B400 Bruker
Avance III 400 MHz. 150 mg of GelMA was dissolved in 600 μL of deuterium oxide
(D2O) (Sigma-Aldrich, UK), and then transferred to NMR tubes (VWR, UK) and the
spectra acquired with 128 scans.
Rheological characterization
The rheological assessment of non-polymerised gelatin solutions were carryout using
the discovery hybrid rheometer system DHR2 (TA Instrument, USA). Samples were
placed between the test pad and cone geometry (40 mm dimeter) fixed at the rheometer
head. Two different tests (rotational and oscillation) were considered and performed
at room temperature Rotational tests were considered to evaluate viscosity and
material strength. It is assumed that the material flows by applying a stress being the
response measured alongside time. A controlled stress was applied, and the resulting
movement measured at constant frequency (1 Hz). Oscillation tests (amplitude and
frequency sweep tests) were considered to evaluate the viscoelastic behaviour of the
material and the dynamic modulus. During the frequency sweep samples were exposed
to small-deformation oscillations covering a range of frequencies (0.01-1000 Hz) to
assess short and long-time scale responses to deformations. While, during an
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amplitude sweep, the shear stress is varied, and the frequency is kept constant (1Hz).
The elastic or storage modulus (G') and the viscous or loss modulus (G") were
measured at room temperature. The viscoelastic behaviour was characterized by
measuring the energy stored (storage modulus, G') in the material during shearing and
the energy subsequently lost (loss modulus, G''). Shear strain was controlled by
varying the oscillation amplitude. For photocrosslinked hydrogels, the viscoelastic
properties were examined. Crosslinked hydrogels discs were placed between two
parallel plates and oscillatory tests were conducted using the DHR2 rheometer with a
20 mm diameter plate.
Scanning Electron Microscopy
The internal morphology of the hydrogel structure was observed using the Hitachi
S3000N VPSEM scanning electron microscopy system (Hitachi, Japan). Two
different hydrogel compositions were considered (10 and 15% wt of GelMA
concentrations), and both were irradiated at 8 mW/cm2 for 8 min. Gelatin methacrylate
hydrogels specimens were frozen at -80 °C for 3 days following lyophilization.
Finally, all samples were sputter-coated with gold by sputter-coating.
Mechanical characterization
Compression tests were conducted using the Instron 3344 machine (Instron, UK)
equipped with a 10-N load cell. Crosslinked gelatin hydrogel discs were prepared as
previously described and maintained in distilled water at 37 ºC. After 24 hrs of
incubation, swollen gelatin hydrogel discs were measured using callipers to determine
both the diameter and thickness. Unconfined compression tests were performed on
the hydrogel discs at room temperature and wet conditions, using a constant crosshead
speed of 0.5 mm/min, at a rate of 10% strain. Compressive young modulus was
determined from the slope of stress versus strain plots and limited to the first 10% of
strain as recommended for cartilage applications (329).
Swelling and degradation characterization
Crosslinked gelatin methacrylate hydrogel discs were frozen at -80 ºC, lyophilized and
then the dry weights (Wi) were measured. Then, dried hydrogel samples were
immersed in Dulbecco’s Modified Eagle’s Medium - high glucose (DMEM) (Sigma-
UK) diluted with 10% FBS (Fetal Bovine Serum) (Thermofisher, UK) at pH 7.4 and
incubated at 37 °C to reach an equilibrium swelling state. The DMEM was replaced
every 2 days. Over the course of 3 weeks, samples were removed from the DMEM
112
and the swollen hydrogel sample weights (Ws) measured. The swelling ratio (Q) was
calculated as follows:
Q=Ws/Wi (5.1)
After weighting the swollen hydrogels, the samples were freeze-dried and weighted
again to measure the weight after lyophilization (Wd). The percentage of mass loss
ratio was calculated according to the following equation:
((Wi-Wd)/Wi) *100 (5.2)
Measurements were performed in triplicate.
hADSCs Cell encapsulation
The gelatin methacrylate hydrogels (GelMA) were cytotoxically assessed, considering
both live dead and alamar blue assays. Human adipose-derived stem cells (hADSCs,
passage 4) (Stempro, Invitrogen, Waltham, MA, USA) were encapsulated with
hydrogel solution at 150000 cell/mL. 200 µL of the gel/cell (cell suspension) solution
was pipetted into custom-made cylindrical teflon moulds (diameter: 10 mm; height 4
mm), then exposed to 365 nm UV light, irradiating at 8 mW/cm2 for 8 min to cast the
encapsulated cell-hydrogel discs. Cell laden constructs were transferred into 24-well
plate and cell culture media (600 µl) was added until the hydrogel discs are fully
covered. The number of encapsulated cells was 30000 cell/well as recommended by
the well-plate manufacturer. The cytotoxicity was assessed at day 3, 7 and 19 by
removing cell culture media, washing gently in DPBS, and then live/dead stains
(Thermofisher Scientific, UK) were added. The Live/dead stain was prepared by
adding 5µl of the supplied calcein AM and 15µl of 2mM Ethidium homodimer (EthD-
1) stock solution to 10 mL of sterile, tissue culture-grade Dulbecco's phosphate-
buffered saline (DPBS), vortexing to ensure thorough mixing. Afterwards, 600 µl of
stain were added to each well to ensure that the hydrogel discs were fully covered.
Samples were kept in the incubator for 30 min prior to imaging. An inverted
fluorescence microscope (Leica DMI6000 B, Leica Microsystems, Wetzlar, Germany)
was used to obtain images of the hydrogel constructs. Images were processed and
analysed using ImageJ software. The Alamar blue assay was used to evaluate cell
bioactivity after 1, 3, 5 and 7 days of culture. For each time point, samples were
washed twice in DPBS and alamar blue solution 0.01% v/v (Sigma-Aldrich, UK) was
added to each well (600 µl of cell culture medium) and incubated for 4 hrs under
standard conditions (37 ºC, 5% of CO2 and 95% of humidity). After incubation, 150
113
µL of each sample solution was transferred to a 96-well plate and the fluorescence
intensity was measured at 540 nm excitation wavelength and 590 nm emission
wavelength with a spectrophotometer (Sunrise, Tecan, Männedorf, Zurich,
Switzerland). 2D cell culture was assessed as a control point. The experiments were
performed in triplicate (n=3).
Data analysis
All data are represented as mean ± standard deviation. Cell proliferation results were
subjected to one-way analysis of variance (one-way ANOVA) and post hoc Tukey’s
test using GraphPad Prism software version 8.0. Significance levels were set at p <
0.05.
Results and discussion
Characterization of gelatin and GelMA by HNMR
Figure 5.2a shows the resonance characteristic peaks of non-functionalized gelatin.
The following peaks were identified: methyl group of amino acids, valine, leucine and
isoleucine (Peak 1 at 0.5-0.7 ppm), methylene residues of threonine (Peak 2 at 0.9-1.1
ppm), alanine (Peak 3 at 1.1-1.3 ppm), lysine (Peak 4 at 1.2-1.4 ppm, and Peak 7 at
2.6-2.7 ppm), arginine (Peak 5 at 1.6-1.8 ppm, and Peak 8 at 2.8-3.0 ppm), methylene
resonances of aspartate (Peak 6 at 2.2-2.5 ppm), and proline (Peak 9 at 3.2-3.4 ppm).
These peaks are also present in the functionalized gelatin (Figures 5.2b and c). New
peaks at 1.6-2.19 ppm, 5.69 ppm and 5.93 ppm correspond to methylene protons
(H2C=C(CH3)) and confirm the successful functionalization with methacrylic
anhydride. After confirming the chemical functionalization of gelatin, the degree of
functionalization (DoF) was determined following the procedure previously described
by Billet et al (366), and the results are presented in Table 5.1. As observed the degree
of functionalization increases with the increase of the functionalization reaction time.
After 2 hours GelMA presents low levels of C=C bonds on the material backbone,
which will originate less dense crosslinked polymer networks upon irradiation, while
after 6 hours GelMA presents high levels of C=C bonds on the backbone, which will
originate more dense crosslinked networks. No significant increase on the degree of
functionalization was observed between 4 and 6 hours of reaction. Therefore, only
samples obtained after 2 and 6 hrs of functionalization were considered for further
analysis.
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Table 5.1: Effect of reaction time on the degree of functionalization.
Figure 5.2: 1H NMR spectra for non-functionalized and functionalized gelatin. (a)
Non-functionalized gelatin (b) GelMA functionalized for 2 hrs; c) GelMA
functionalized for 4 hrs; d) GelMA functionalized for 6 hrs.
Reaction time (hrs) Degree of functionalization (%)
2 40
4 52
6 54
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Rheological characterization
Prepolymer rheology
The stress versus shear rate and the variation of viscosity with shear rate for pre-
polymerised GelMA samples are shown in Figure 5.3. As observed, the materials
exhibit a shear-thinning behaviour. Results also show that the viscosity of the polymer
solution is dependent of the shear rate, decreasing by increasing the shear rate. This is
an important characteristic for 3D bioprinting applications as less pressure is required
during the printing process. It’s also possible to observe that the polymer concentration
has an impact on the maximum stress for a specific shear rate with high values being
obtained for long functionalization reaction times. Results show that for both GelMA
compositions viscosity decreases by increasing the functionalization time. For the
same functionalization time and different material compositions results show no
significant differences of viscosity for low shear rates, but for high shear rates, the
viscosity is significantly low in the case of high concentration of gelatin methacrylate
Figure 5.3: Rheological behaviour of 10 and 15% wt of GelMA samples considering
2 and 6 hrs of functionalization time. (a)10% wt of GelMA functionalized for 2 hrs;
(b) 10% wt of GelMA functionalized for 6 hrs; (c) 15% wt of GelMA functionalized
for 2 hrs; (d) 15% wt of GelMA functionalized for 6 hrs.
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Since the polymers exhibit a shear-thinning behaviour, a power law model can be used
to fit the experimental data:
τ = 𝜂γn (5.3)
where τ is the shear stress (Pa), γ is the shear rate (s-1), 𝜂 the consistency index or
equivalent viscosity (Pa. s) and n is the power law index (dimensionless).
Table 5.2 shows the values of the power law coefficients for the different materials. A
good approximation (R2 around 0.97) was obtained between the power law and the
experimental data.
Table 5.2: Power law coefficients for different reaction times and GelMA
concentration.
Polymer concentration - Reaction time (h) n value R2
10% wt - 2h 0.4978 0.9652
10% wt - 6h 0.5613 0.9834
15% wt - 2h 0.825 0.999
15% wt - 6h 0.5519 0.9868
Viscoelastic changes for pre-polymerised solutions were assessed using oscillation
tests (Figure 5.4).
For both concentrations, results show that both the storage and loss modulus are high
when the reaction time is long (6 hrs).
Results for GelMA samples functionalized during 2 hrs show that at low frequencies
the storage modulus is higher than the loss modulus. While for high frequencies, the
loss modulus increases and become higher than the storage modulus. For GelMA
samples functionalised during 6 hrs it is possible to observe that the loss modulus is
higher than the storage modulus for all frequencies.
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Figure 5.4: Oscillatory tests: storage and loss modulus of 10% wt GelMA for 2 and 6
hrs; (a) Amplitude sweep for 10 and 15% wt GelMA functionalized for 2hrs; (b)
Frequency sweep for 10 and 15% wt GelMA functionalized for 2hrs; (c) Amplitude
sweep for 10 and 15% wt GelMA functionalized for 6hrs (d) Frequency sweep for 10
and 15% wt GelMA functionalized for 6hrs.
Figures 5.5 and 5.6 show the variation of G' and G'' as a function of strain rate and
frequencies of crosslinked hydrogels. Amplitude sweep results show that for the two
different functionalisation times, G' is higher in the case of samples obtained from
solutions containing higher concentration of GelMA. For the same GelMA
concentration, G' also increases by increasing the functionalization time. The increase
of G' is associated with the increase in the crosslinking density. In all cases it is
possible to observe a critical strain rate value. Bellow this threshold strain, G' is higher
than G'', while above the threshold G'' becomes higher than G'. In the case of frequency
sweep, results show that the G' is always higher than G'' showing a dominant solid like
behaviour.
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Figure 5.5: Oscillatory results for GelMA hydrogel samples functionalized for 2 hrs
(a) Storage and loss modulus as a function of strain for 10 and 15% wt GelMA and
1% wt of PI; (b) Storage and loss modulus as a function of frequency for 10 and 15%
wt GelMA and 1% wt of PI; c) Storage and loss modulus as a function of strain for
10 and 15% wt GelMA and 1.5% wt of PI; d) Storage and loss modulus as a function
of frequency for 10 and 15% wt GelMA and 1.5% wt of PI.
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Figure 5.6: Oscillatory results for GelMA hydrogel samples functionalized for 6 hrs
(a) Storage and loss modulus as a function of strain for 10 and 15% wt GelMA and
1% wt of PI; (b) Storage and loss modulus as a function of frequency for 10 and 15%
wt GelMA and 1% wt of PI; c) Storage and loss modulus as a function of strain for
10 and 15% wt GelMA and 1.5% wt of PI; d) Storage and loss modulus as a function
of frequency for 10 and 15% wt GelMA and 1.5% wt of PI.
Morphological characterization
The internal pore size is crucial as it determines the internal free space to encapsulate
cells and to support cell growth and proliferation. In the case of cartilage bioinks for
3D bioprinting the references are chondrocytes cells and human adipose-derived stem
cells presenting around 20 m of diameter (367, 368). Figure 5.7 shows the internal
morphology of crosslinked GelMA hydrogels. Results show that crosslinked
structures obtained from solutions containing 10% wt of GelMA (2 and 6 hrs of
reaction time) and 1% wt of photoinitiator present pore sizes with 100 to 150 m of
dimeter (Figures 5.7 a and b). The increase of photoinitiator concentration reduces
both pore size and number of pores Figures 5.7c and d as it contributes to high
crosslinking density. Polymer solutions containing 15% wt of GelMA result in high
density crosslinked structures with small pores (23 to 25 m) (Figures 5.7e and f) or
almost no pores (Figures 5.7g and h). As observed the most suitable system for cell
120
encapsulation seems to be the one based on solutions containing 10% of GelMA and
1% wt of photoinitiator as it allows more free space to accommodate cell encapsulation
and proliferation. Therefore, this is the composition further considered.
Figure 5.7: Cross-section images of GelMA crosslinked structures considering
different GelMA concentrations, reaction times and PI concentration; (a) 10% of
GelMA, 2 hrs of functionalization time and 1% wt of PI; (b) 10% of GelMA, 6 hrs of
functionalization time and 1% wt of PI; (c) 10% of GelMA, 2 hrs of reaction time and
1.5% wt of PI; (d) 10% GelMA, 6 hrs of reaction time and 1.5% wt of PI; (e) 15% of
GelMA, 2 hrs of reaction time and 1% wt of PI; (f) 15% of GelMA, 6 hrs of reaction
time and 1% wt of PI; g) 15% of GelMA, 2 hrs of reaction time and 1.5% wt of PI; (h)
15% of GelMA, 6 hrs of reaction time and 1.5% wt of PI.
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Mechanical characterization
Compressive modulus of crosslinked GelMA discs were determined one day after
equilibrium swelling and the results are presented in Figure 5.8. As observed, high
compression modulus is obtained with high functionalisation times and high
photoinitiators concentrations. For the same functionalisation time and photoinitiator
concentration, compressive modulus increases by increasing the gelatin concentration.
These results can be explained by the high crosslinking density that characterises the
structures obtained from solutions containing high GelMA concentration,
functionalised during long reaction times and containing high concentration of
photoinitiators and the corresponding internal structure characterised by small size and
low numbers of pores.
Figure 5.8: Unconfined compression tests for gelatin methacrylate hydrogels samples
with different photoinitiator concentrations a) 10% wt GelMA functionalized for 2h
containing 1% wt of PI; (b) 10% wt GelMA functionalized for 2h containing 1.5% wt
of PI; (c) 10% wt GelMA functionalized for 6h containing 1% wt of PI; (d) 10% wt
GelMA functionalized for 6h containing 1.5% wt of PI.
Swelling and degradation characterization
The swelling and degradation behaviour of crosslinked GelMA disks are presented in
Figure 5.9. Results show that all samples absorb DMEM until reaching a state of
equilibrium. This state is accomplished when the osmotic pressure from the swelling
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and the elasticity of the hydrogel network is equal. In all samples, the equilibrium
status was reached at day three. It is also possible to observe that crosslinked samples
prepared with GelMA obtained after 6 hrs of functionalization present low swelling
ratio, which shows that the degree of crosslinking controls the swelling properties of
the hydrogel. Crosslinked GelMA structures based on GelMA prepared during 6 hours
of reaction time swelled up to 14%, while GelMA structures based on functionalized
gelatin prepared during 2 hour of reaction time swelled up to 20% (Figure 5.9a).
Moreover, it is also possible to observe that the level of functionalization of the pre-
polymerised gelatin not only determines the internal morphology of the crosslinked
structures but also the degradation process (Figure 5.9b). Results show that samples
produced using GelMA obtained considering high reaction times and solutions
containing high polymer concentration (15% wt) show lower degradation rates (20%
of mass loss for crosslinked GelMA obtained from gelatin functionalised during 6 hrs
and solutions containing 15% wt of GelMA, and 35% of mass loss for crosslinked
GelMA obtained from gelatine functionalized during 2 hrs and solutions containing
10% wt of gelatin).
Figure 5.9: Swelling and degradation profiles as a function of functionalization time
for different functionalized gelatin methacrylate systems; a) Swelling in DMEM ; b)
degradation rate in DMEM.
Cell viability and proliferation
The live/dead assay was used to investigate the potential toxicity of both GelMA
hydrogels, photoinitiator concentration and the effect of irradiation conditions on the
encapsulated cells. Results after 3, 7 and 19 days of cell-encapsulation are presented
in Figure 5.10. Results show that most of the hADSCs are alive (green) with few dead
cells (red) at day 3, indicating good biocompatibility for the produced materials. At
day 7, cells show an elongated cell morphology and a cell-cell networking can be
observed at day 19, which is more intensive in samples prepared with GelMA obtained
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at high functionalization times. This might be attributed to the higher functionalization
degree of GelMA obtained after 6 hrs of functionalization.
Cell proliferation was assessed using the alamar blue assay and the results are
presented in Figure 5.11, confirming the bioactivity of encapsulated hADSCs. At day
1, the 6 hrs GelMA hydrogel shows higher fluorescence intensity in comparison to the
2 hrs hydrogel group. However, this difference reduces after day 1. At day 5, both
GelMA groups shares similar fluorescence intensity and 2hrs GelMA hydrogel group
shows higher intensity at day 7. This might be attributed to the faster degradation of
2hrs hydrogel group which releases more cells attaching to the cell culture plate. These
results, which are aligned with the results presented in Figure 5.10c, shows that 6 hrs
hydrogel presents better cell affinity for a long cell culture time.
Figure 5.10: Live/dead images of adipose-derived mesenchymal stem cells
encapsulated in samples based on 10% wt GelMA dissolved at 1% wt of PI solution
and exposed to UV light (Light intensity of 8 mW/cm2) for 8 min a) After 3 days of
encapsulation; b) After 7 days of encapsulation; c) After 19 days of encapsulation.
Note: Green corresponds to live cells and red to dead cells.
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Figure 5.11: Alamar blue fluorescence intensity at different time points (1, 3, 5 and 7
days) considering samples functionalized at two different reaction times (2 and 6 hrs)
Conclusion
Photocrosslinkable hydrogels have shown great potential for cartilage repair, due to
their unique properties. GelMA systems were fully characterised in terms mechanical,
photopolymerization process, degradation, swelling and biological properties. Results
show the ability to tune these characteristics by controlling the functionalization
process. Moreover, the biological affinity between gelatin and cells were confirmed
being possible to observe that both material systems and processing conditions do not
induce any negative effect on cell survival. High cell attachment and proliferation was
observed. Results demonstrates the viability of using GelMA as a bioink for cartilage
applications.
Time (days)
0
20000
40000
60000
6h
Control
2h
D3D1 D5 D7
*
*
Flu
ore
sc
en
ce
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Chapter 6 Development and
characterisation of a
photocurable alginate-
gelatin for cartilage
applications†
† This Chapter based on the paper: Hussein Mishbak†, Cian Vyas†, Marie O'Brien, Glen Cooper, Paulo
Bartolo. “Development and characterisation of a photocurable alginate-gelatin for cartilage
applications”, Biomaterials Science and Engineering Journal, in preparation.
126
This Chapter focus on the design of three different photocrosslinkable hydrogels based
on alginate and gelatin for cartilage applications. The synthesis, morphological,
rheological, mechanical, and biological characterisation of AlgMA, GelMA, and
hybrid alginate-gelatin Alg-Gel(MA) methacrylate hydrogels are detailed. Results
show that the hybrid hydrogels display superior mechanical properties than the single
component hydrogels and present a more stable degradation behaviour. The hybrid
hydrogels also demonstrate high cell viability, improved cell adhesion, and increased
production of cartilage tissue markers such as collagen and glycosaminoglycan
GAGs. Both AlgMA and GelMA materials considered in this Chapter were
functionalized as described in Chapters III and V.
Introduction
Articular cartilage is a tissue which covers the ends of bones at joints and provides a
smooth and lubricated surface for articulation during movement and mechanical load
transmission (17, 369). The tissue has low metabolic activity and lacks a vasculature
thus disease or trauma can severely impact tissue functionality (369). Articular
cartilage heals poorly, typically forming fibrocartilage, and current therapies have
limited clinical efficacy in halting the degradation of the tissue which ultimately can
result in the requirement of a total joint replacement implant (370, 371). This has
motivated the development of tissue engineering strategies utilising biomaterials and
scaffolds to promote cartilage regeneration (85, 110, 372, 373). A promising class of
biomaterials are hydrogels, three-dimensional (3D) hydrated polymer networks, which
have properties that resemble the extracellular matrix (ECM) of biological tissues
(120, 374-377). Hydrogels have been investigated for tissue engineering applications
due to their biocompatibility, oxygen and nutrient permeability, and the ability to tailor
their properties (372, 378-381). Biodegradable and biocompatible synthetic and
natural based hydrogels have been explored to promote the repair and regeneration of
different tissues such as skin, nerve and cartilage (382-384).
Synthetic hydrogels have been widely investigated as a potential suitable biomaterial
for articular cartilage tissue engineering applications due to their ability to be
engineered to mimic the ECM and tailored to have similar properties in terms of
mechanical, morphological and biological properties (385-388). However, synthetic
hydrogels have limitations regarding their biocompatibility and biodegradability due
to the lack of inherent adhesion and degradation sites which requires the incorporation
127
of motifs such as the tripeptide Arg-Gly-Asp (RGD) sequences and matrix
metalloproteinases (389).
Alternatively, natural based hydrogels are attractive biomaterials due to their
biocompatibility and biodegradability and have been explored for cartilage tissue
engineering applications (390-393). Particular relevant are alginate and gelatin.
Alginate has been investigated due to its low cost, biocompatibility, hydrophilic
structure, stiff polymer backbone, ease of modification and processing (394, 395).
Alginate hydrogel based-scaffolds can be produced via ionic-crosslinking, phase
transition, free radical polymerisation, and click conjugation (396). Free radical
photopolymerization has gained tremendous attention due to the ease of use and rapid
gelation kinetics. Furthermore, photopolymerisation enables polymer solutions (pre-
polymerised monomers) containing cells or biomolecules to be printed using 3D
bioprinting technologies for the development of scaffolds or using in vivo minimally
invasive delivery technique (e.g. injection) with subsequently crosslinking through
light exposure (113, 383, 397). However, alginate has significant limitations which
limits its applicability as a single material for tissue engineering applications such as
the lack of cell binding motifs and slow gelation speed which affects gel uniformity
and strength (396). Alternatively, gelatin, obtained from the hydrolysis of collagen,
has been investigated due to its biocompatibility, biodegradability, promotion of cell
adhesion and proliferation (398, 399). The main advantages of gelatin are its
biocompatibility since it has high cell affinity and cell adhesion sites are abundant
(RGD peptides) and its ability to be degraded by native enzymatic processes (400,
401). However, gelatin has limitations such as poor mechanical properties (brittle) and
short biodegradation profile (401). Due to their limitations both alginate and gelatine
are not totally suitable for tissue engineering applications and for cartilage applications
in particular. However, the combination of both materials has the potential to
overcome their individual limitations.
This Chapter investigates the potential of using a hybrid AlgMA and GelMA
photocrosslinking hydrogel system for cartilage applications. The synthesis,
morphological, rheological, mechanical, and biological characterisation of AlgMA,
GelMA, and hybrid alginate-gelatin Alg-Gel(MA) methacrylate hydrogels are
detailed.
128
Materials and methods
Photocrosslinkable polymer preparation
Photocrosslinkable polymers were synthesised by reacting alginate and gelatin with
methacrylic anhydride to introduce methacrylate moieties into the polymer backbone
(326, 402, 403).
Alginate methacrylate preparation (AlgMA)
Alginate methacrylate AlgMA was prepared by dissolving sodium alginate (Sigma-
Aldrich, UK) at a concentration of 2% wt. in an aqueous solution containing
Dulbecco's phosphate buffered saline (DPBS) and dimethyl sulfoxide (DMSO),
(Sigma Aldrich, UK) at a ratio of 85:15. The dissolved solution was then mixed with
20% v/v methacrylic anhydride (MA) (Sigma Aldrich, UK) for 24 h, at room
temperature (RT), as previously described (404). The pH of the solution was
maintained between 7.4-8.0 by adding 5M NaOH (Sigma Aldrich, UK). After
chemical modification, the polymer solution was precipitated with 100% ethanol
(absolute ethanol ≥99.8%, AnalaR NORMAPUR®, WVR, UK), dried in an oven
overnight at 40-50°C, and purified through dialysis tubes (3.5 kDa) (Spectra/Por 2,
Fisher Scientific, USA) for 5 days. The solution was frozen at -80°C for 2 days and
the polymer recovered by lyophilisation for 3 days.
Similarly, GelMA was prepared by dissolving gelatin bovine skin type B (Sigma
Aldrich, UK) at a concentration of 12.5% wt. in DPBS at a temperature of 45°C. After
complete dissolution of gelatin a 10% v/v MA solution was added under vigorous
stirring. The pH was kept at 8 during the reaction time of 6 h. The solution was purified
through dialysis tubes (12-14 kDa) (Spectra/Por 2, Fisher Scientific, USA) for 5 days.
Then, the solution was frozen at -80ºC for 2 days and the polymer was recovered by
lyophilisation for 3 days.
Hydrogel formation
6.2.3.1 Photoinitiator solution preparation
Photoinitiator solution was prepared by dissolving the photoinitiator powder, 2,2'-
Azobis[2-methyl-N-(2-hydroxyethyl) propionamide azo initiator (VA-086) (Wako
Pure Chemical Industries, USA) in DPBS (Sigma-Aldrich, UK) at 40°C for 30 min,
to a final concentration of 1% wt. The PI concentration was previously investigated
for both alginate and gelatin single systems and the results presented in chapters III
and V.
129
6.2.3.2 Single hydrogel systems
The AlgMA and GelMA hydrogels are produced by dissolving 2% wt. and 10% wt.
respectively of the lyophilised polymer in the 1% wt. photoinitiator solution.
Crosslinked hydrogel discs were produced by pipetting the AlgMA and GelMA
solutions into custom-made cylindrical acrylic moulds (diameter: 8 mm, height: 4 mm)
and irradiated with ultraviolet (UV) light (365 nm wavelength) using a UV lamp
(Dymax 2000-EC, Dymax Europe GmbH, Germany). The light intensity at the
material surface was fixed at 8 mW/cm2 and samples were irradiated during 8 min.
The exposure conditions were selected using 365 nm and between 5–20 mW/cm2 for
2–20 min since these low UV light intensities have been reported to have a lower
impact on cell viability, proliferation and gene expression (405) (Figure 6.1).
Figure 6.1: Photocrosslinking mechanism to form a) AlgMA and b) GelMA hydrogels
using UV irradiation.
6.2.3.3 Hybrid hydrogel system
The hybrid hydrogel systems were synthesised by mixing 2% wt. AlgMA and 10%
wt. GelMA solutions at ratios of 75:25 AlgMA/GelMA, 50:50 AlgMA/GelMA, and
25:75 AlgMA/GelMA. These alginate-gelatin methacrylate hybrid hydrogels (Alg-
Gel(MA)) were crosslinked as previously described (Figure 6.2).
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Figure 6.2: Photocrosslinking of hybrid alginate-gelatin systems when exposed to UV
irradiation.
Structural conformation of the hybrid hydrogels
Proton nuclear magnetic resonance (NMR) spectroscopy (Bruker 400, Bruker
Corporation, USA) was used to assess the degree of methacrylate modification for all
three systems (AlgMA, GelMA, and Alg-Gel(MA)). Samples were prepared by
dissolving 150 mg of each polymer in 750 µl deuterium oxide (D2O) (Sigma Aldrich,
UK) and then transferred to NMR tubes (VWR, UK). The spectra were acquired at
400 MHz with 128 scans. The degree of methacrylation was calculated following the
procedure previously described by Billet et al (234).
Rheological characterisation
Rheological characterisation was used to determine the general flow behaviour and
viscoelastic characteristics of the functionalized pre- and polymerized hydrogels.
Rotational and oscillatory rheology (Discovery Hybrid Rheometer, TA Instruments,
USA) was considered. All samples (n=3) were measured at room temperature (RT).
Rotational tests were performed by loading the polymer samples using a cone and
plate geometry (60 mm diameter and 200 µm gap size), applying a torque to the top
plate exerts a rotational shear stress on the material to flow and the resulting shear rate
and movement are measured. The rotational speed depends on the viscosity computed
by means of stress and shear rate. By means of the flow curve it is possible to measure
the viscosity as a function of shear rate (0.01 – 1000 s-1).
The oscillatory tests were performed to measure the viscoelastic behaviour and the
stiffness of the specimens and dynamic moduli. Amplitude and frequency sweeps were
considered. A range of frequencies (0.01-100 Hz) was used to assess short and long-
time scale responses to deformations at a constant 20% strain, while the strain rate
varies during the amplitude sweep test, and the frequency was constant at 1 Hz. The
storage (G') and the loss (G") modulus were measured.
For photocrosslinked hydrogels, oscillatory tests were performed to evaluate the
hydrogel stiffness by subjecting the hydrogel to a shear stress. The hydrogel samples
131
were carefully placed onto the surface of the plate (20 mm in diameter) lowered to a
500 µm gap distance, shear stress was applied, and then, G' and G'' were measured as
a function of strain (0.1-500%).
Structure morphology and porosity
The hydrogel’s internal morphology was investigated using scanning electron
microscopy (SEM, S3000N, Hitachi, Japan). Cylindrical hydrogels samples (8 mm
diameter, 4 mm height) were frozen at -80°C for 2 days then lyophilised to recover the
dried hydrogel constructs. The samples were cut to obtain a cross-section and sputter
coated with gold prior to imaging.
Porosity is an important property of the hydrogel’s structure due to its influence on the
mechanical performance of the scaffold; fluid permeability; the supply of oxygen,
nutrients and removal of waste products; and the free volume provided for cells to
migrate and proliferate. The percentage of porosity of the hydrogels (n=3) was
calculated using a gravimetric method. Dry samples (n=3) were obtained by
lyophilisation and then the samples were placed in a desiccator under vacuum (VWR,
UK) for three days and the volume was determined by using a calliper. The porosity
was determined using the following equation:
𝑃𝑜𝑟𝑜𝑠𝑖𝑡𝑦 (%) = (1 − 𝑃ℎ𝑦𝑑𝑟𝑜𝑔𝑒𝑙
𝑃𝑚𝑎𝑡𝑒𝑟𝑖𝑎𝑙) × 100 (6.1)
where Phydrogel is the experimental density of the 3D hydrogel construct and Pmaterial is
the theoretical density of the polymer. The theoretical density for the hybrid systems
was calculated as follows:
𝑃𝑚𝑎𝑡𝑒𝑟𝑖𝑎𝑙 = 𝑋𝐴𝑙𝑔𝑀𝐴𝑃𝐴𝑙𝑔𝑀𝐴 + 𝑋𝐺𝑒𝑙𝑀𝐴 𝑃𝐺𝑒𝑙𝑀𝐴 (6.2)
where XAlgMA and XGelMA indicate the volume fractions and the densities of alginate, and
gelatin, PAlgMA and PGelMA, are 1.64 g/cm3 and 0.98 g/cm3, respectively.
The experimental apparent hydrogel density, Phydrogel, can be determined according to
the following equation:
𝑃ℎ𝑦𝑑𝑟𝑜𝑔𝑒𝑙 =𝑚𝑎𝑠𝑠
𝑣𝑜𝑙𝑢𝑚𝑒 (6.3)
where mass is the dry weight of the specimen and the volume is based on a
measurement of the dried sample.
The average pore size of the hydrogels was semi-quantified using ImageJ software
analysis of the SEM images through calculation of the Feret's diameter, which is an
approximation method to calculate the pore size dimeter (406).
132
Swelling and degradation kinetics of the hybrid hydrogels
The hydrogel discs were produced as previously mentioned in section (6.2.3) (n=3, at
each timepoint), frozen at -80°C for 2 days, and then lyophilised for 3 days to recover
dry hydrogel structures. After lyophilisation, the initial dry disc weights were
measured (Wi). The dry hydrogel samples were immersed in Dulbecco’s Modified
Eagle’s Medium (DMEM) (Sigma Aldrich, UK) supplemented with 10% fetal bovine
serum (FBS) (Thermofisher, UK) at pH 7, and incubated at 37°C to reach an
equilibrium swelling state. The swelling weights (Ws) were measured over the course
of 20 days and the DMEM was changed every two days.
The swelling ratio (Q) was calculated as follows:
𝑄 = 𝑊𝑠
𝑊𝑖 (6.4)
Where Wi is the initial dry weight and Ws is the swollen hydrogel sample weight.
For the degradation kinetics, the swollen hydrogels samples were frozen and
lyophilised at each timepoint and the dry weight (Wd) measured. The mass loss
percentage was calculated using the following equation:
𝑀𝑎𝑠𝑠 𝑙𝑜𝑠𝑠 (%) = (𝑊𝑖−𝑊𝑑
𝑊𝑖) × 100 (6.5)
Mechanical assessment
The mechanical behaviour of the crosslinked hydrogels was characterised through
unconfined compression testing using Instron 3344 single column system with a 10 N
load cell (Instron 3344, Instron, UK). Hydrogel discs (n=3) were prepared as
previously described using a custom-made cylindrical acrylic mould with a 1:1
dimension ratio (diameter 10 mm and height 10 mm) and incubated in DPBS at 37°C
for 24 h. The hydrogel discs were measured after 24 h to determine the diameter and
thickness, and unconfined compression tests were performed on the hydrogel discs at
RT. The compressive strain rate was fixed at 0.5 mm/min, and samples were loaded
up to a maximum strain of 20%. The compressive Young’s Modulus (E) was
calculated from the slope of the initial linear region of the stress-strain curve (elastic
deformation region) by calculating the tangent modulus from the curve fit equation at
20 % strain.
Biological assessment
The photocrosslinked hydrogels were biologically evaluated through the
encapsulation of human chondrocyte cells (Cell Applications, USA) and assessed for
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cell viability, proliferation, and ECM production. The AlgMA, GelMA, and Alg-
Gel(MA) 50:50 photocrosslinked hydrogels were selected for evaluation.
6.2.9.1 Cell culture and encapsulation
Human chondrocyte cells were cultured until passage four in a complete human
chondrocyte growth medium (Cell Applications, USA). Cells were harvested and
encapsulated at density of 0.6 x 106 cells/mL in the hydrogel solution. 160 µL of the
hydrogel/cell solution was pipetted into a custom-made cylindrical acrylic mould
(diameter 8 mm and height 4 mm) and exposed to UV light (wavelength 356 nm),
irradiated at 8 mW/cm2 for 8 min to cause gelation of the encapsulated hydrogel/cell
solution. Cell-laden hydrogels (n=3) were transferred into 24-well plates and cell
culture media added
6.2.9.2 Cell viability, proliferation, and metabolic activity
The cytotoxicity of the hydrogels was observed using a live/dead assay kit
(Thermofisher Scientific, UK). Cell viability was observed on day 3, 7 and 16 by
removing cell culture media, washing gently in DPBS, adding a 2 µM calcein-AM and
4 µM ethidium homodimer-1 solution, and incubating for 25 min. The hydrogels were
then observed using a confocal fluorescence microscope occupied with fluorescence
filter sets (A, I3 and N2.1) (TCS-SP5, Leica, Germany). Images were processed and
analysed using ImageJ software (n=3) (407).
Cell proliferation and metabolic activity was evaluated by using the resazurin (Alamar
blue) assay at day 1, 3, 5, 7 and 14 days of culture. At each time point, samples (n=3)
were washed twice in DPBS and 75 µL of Alamar blue solution 0.01% (wt. ) (Sigma-
Aldrich, UK) was added to each well in 750 µl of cell culture medium and incubated
for 4 h under standard conditions (37°C, 5% CO2, and 95% humidity). After
incubation, 150 µL of each sample solution was transferred to a 96-well plate and the
fluorescence intensity was measured at 540 nm excitation wavelength and 590 nm
emission wavelength with a plate reader (Infinite 200, Tecan, Männedorf, Zurich,
Switzerland). 2D tissue culture plastic (TCP) was assessed as a positive control for
both cell viability and proliferation.
Histological analysis
Histological analysis of the cell encapsulated hydrogels was investigated at day 14,
21, 28, and 35 to assess the amount of deposited ECM. Three histological stains were
used: Gomori trichrome, aggrecan immunohistochemistry, and safranin O.
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Gomori trichrome is used to quantify the total collagen secretion in the hydrogel as
collagen is a main structural component of cartilage representing more than 60% of its
dry weight (17). Gomori trichrome bind to the nuclei (dark purple) and collagen (green
or blue). Aggrecan immunohistochemistry is used to quantify the proteoglycan, which
represents more than 20% of the cartilage dry weight (408). Aggrecan, is specific
proteoglycan in cartilage tissue, and its crucial in a cartilage functioning (17, 409).
Safranin O used to identify the chondrocytes and the detection cartilage formation,
and it stains cell nuclei (dark red).
At each time-point, the crosslinked hydrogel systems were fixed with 10% (v/v)
formalin (Sigma Aldrich, UK) for 20 min at RT. After fixation the samples were
processed in a Tissue-Tek Vacuum Infiltration Processor (Bayer Diagnostics,
Newbury, UK). The processed tissue was embedded in Paraplast Plus paraffin medium
(Sigma Aldrich, UK) and sectioned at 5 µm before mounting on glass slides.
Gomori trichrome staining sections were de-waxed in xylene for 5 mins then hydrated
through descending grades of ethanol down to water. They were stained with Mayers
haematoxylin (Sigma Aldrich, UK) for 5 min, washed with water for 5 min and then
stained with Gomori (Sigma, UK) for 5 min. After rinsing with 0.2% acetic acid,
sections were blotted dry and dehydrated in ethanol before immersing in xylene and
finally cover-slipped.
Aggrecan immunohistochemistry staining sections were de-waxed in xylene for 5 min
then hydrated through descending grades of ethanol down to water. They were then
stained using Aggrecan (LSBio - LS-C359243) antibody on the Thermo Autostainer
480S Immunohistochemistry stainer. Briefly, antigen retrieval was performed using
citrate buffer pH 6. The primary antibody (Aggrecan, 1: 500) was added for 30 min
then the UltraVision™ Quanto Detection System HRP DAB (Thermo Scientific, UK)
was used. Sections were counterstained with Mayers Haematoxylin (Sigma Aldrich,
UK) then dehydrated in ethanol, immersed in xylene (Fisher Scientific, UK) and cover
slipped.
Safranin O staining sections were de-waxed in xylene for 5 min then hydrated through
descending grades of ethanol down to water. They were stained with Weigerts
haematoxylin (Fisher Scientific, UK) for 10 min, washed in water for 5 min and then
stained with 0.05% Fast Green (Sigma Aldrich, UK) for 5 min. After briefly rinsing
with 1% acetic sections were then stained with Safranin O (Sigma Aldrich, UK) for 5
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min, dehydrated in ethanol, immersed in xylene (Fisher Scientific, UK) and cover
slipped.
All sections were imaged on a Leica DM2700M microscope (Leica Biosystems, UK)
at x10 magnification and images were processed using ImageJ analysis software (407).
Glycosaminoglycan quantification
Glycosaminoglycan (GAGs) is a key marker of articular cartilage matrix production.
A dimethylmethylene blue (DMB) assay kit (Biocolor Ltd, UK) was used according
to the manufacturer’s instructions using a papain digestion method to quantify the
production of GAGs in the hydrogel samples (n=3, at each timepoint) and TCP control
at day 7, 14, 21, 28, and 35.
The papain extraction reagent was prepared by mixing 50 mL of prepared 0.2M
sodium phosphate buffer (pH 6.4) (Sigma Aldrich, UK) with 400 mg sodium acetate,
200 mg EDTA disodium salt, and 40 mg cysteine HCl (Sigma Aldrich, UK). Then, 5
mg of papain (Sigma, UK) was dissolved in 250 µL of deionised water before addition
to the extraction solution.
Cell culture media was removed from the samples (n=3), washed twice with DPBS,
and the samples digested for 3.5 h at 65°C by adding 1 mL of the papain digestion
solution to each well. After digestion, 50 µL of supernatant was added to 50 µL
deionised water, 1 mL DMB dye was added, and then mixed for 30 min on a
mechanical shaker. Samples were centrifuged at 12,000 rpm for 10 min and the
supernatants removed. The precipitated GAGs were dissociated by adding 0.5 mL
dissociation reagent, vortexed, and centrifuged at 12,000 rpm for 5 min.
The GAGs were measured by transferring the sample solution to a 96-well plate. A
microplate reader (Infinite 200, Tecan, Männedorf, Zurich, Switzerland) was used and
the absorbance measured at 656 nm.
Statistical analysis
The statistical analysis of cell proliferation, histology, and biochemical
characterisation (GAGs quantification and collagen content) were performed using
GraphPad Prism software version 8.0.1 (GraphPad Software, California, USA).
Significance levels were set at p < 0.05. Metabolic activity and proliferation were
subjected to one-way analysis of variance (one-way ANOVA) and post hoc Tukey’s
test.
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Results and discussion
Functionalisation confirmation and rheological characterisation
Methacrylate amino groups were successfully bonded to the alginate and gelatin
polymer backbones as confirmed by HNMR (Table 6.1 and Figure 6.3). Results show
that the reaction with methacrylate anhydride was successful and the polymers were
functionalized with methacrylate groups grafted onto the alginate and gelatin structure
(Figures 6.3 c and d). AlgMA shows methacrylation moieties at 6.2 ppm and 5.7 ppm,
corresponding to the protons on the alkene of the methacrylate, and at 1.7 ppm
corresponding to the methyl group on the methacrylate (CH3). GelMA shows new
peaks at 1.7-2.2 ppm, 5.69 ppm and 5.93 ppm corresponding to methylene protons
(H2C=C(CH3)), confirming the successful functionalisation with methacrylic
anhydride (Fig. 4d). The reaction between both polymers have resulted in the
appearance of new characteristic peaks of MA at 5.63 ppm and 6.09 ppm attributed to
the methylene group in the vinyl bond, and a peak at 1.82 ppm assigned to the methyl
group, which are not present in the non-modified polymers. The hybrid systems were
also successfully functionalized as shown in Figures 6.3 e, f, and g.
The degree of methacrylation was calculated and results are presented in Table 6.1.
The results show that all groups were reacted with methacrylic anhydride, and the
degree of carbon-carbon double bond substitution ranged between 55-79%. AlgMA
shows a high degree of methacrylation compared to other systems, which could be due
to using a high concentration of methacrylate anhydride (20%) reacted for long time
(24 h). GelMA shows the lowest substitution of methacrylate groups (55%). While in
the case of the hybrid systems, these values range between 65 and 71.5%.
Table 6.1: Degree of functionalization for all functionalized group polymers.
Sample (group) Degree of methacrylation
Alginate methacrylate(AlgMA) 79.0%
Gelatin methacrylate (GelMA) 55.0%
Hybrid IPN (Alg-Gel)MA 75:25 65.0%
Hybrid IPN (Alg-Gel)MA 50:50 71.5%
Hybrid IPN (Alg-Gel)MA 25:75 70.0%
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Figure 6.3: Representative 1H NMR spectra of a) non-modified alginate, b) non-
modified gelatin, c) AlgMA, d) GelMA, and the hybrid Alg-Gel(MA) systems e)
75:25, f) 50:50, and g) 25:75.
Rheological Characterization
The rheological behaviour of the polymers was investigated to determine their
viscoelastic properties which influences cell behaviour and their printability for the
development of a bioink. The viscoelastic behaviour of the polymers is directly related
to the molecular structure, percentage dilution, and functionalization processes. The
results show that all three systems (AlgMA, GelMA, and Alg-Gel(MA)) present shear-
thinning behaviour which is characterised by a decrease in the viscosity with the
increase of shear rate (Figure 6.4). This viscoelastic behaviour is important for
bioprinting cell laden constructs as the material will flow once a pressure is applied
and the lower pressure required to process the bioink through the printing nozzle will
improve cell viability (410). The cells also respond to the shear rate/time-dependent
138
properties of their substrates since viscoelastic polymers encourage cell aggregation
and promote ECM formation (286, 411, 412).
Figure 6.4: Viscosity vs share rate profiles of AlgMA, GelMA, and Alg-Gel(MA)
(25:75, 50:50, and 75:25) samples.
The measurement of the amplitude sweep dependence of the G' and G'' allows
quantification of the linear viscoelastic region (LVER) that determines the stability of
the polymer solution. The viscoelastic behaviour is observed to be independent of
stress or strain values by monitoring the moduli (G' and G'') versus strain curve and
the critical strain point when G' crosses G''. The results show that the polymer
specimens behave as a rigid body, when low deformation is applied to the polymer
samples, G' and G'' are constant (G' is higher than G'') and the sample structure is
undisturbed (Figure 6.5 a, c and e). At higher strain rates both G' and G'' decrease and
the structure of the polymer solution is disturbed. Once the critical strain point is
identified, G' crosses G'', the LVER ends and the polymer behaves as a fluid after this
point. The material behaves as a rigid body at low strain rates but flows as a viscous
fluid at high strain rates.
After identifying the critical strain point, where G' crosses G'', frequency sweep
measurements were performed to determine the material frequency dependence over
a range of oscillation frequencies (0.1-100 Hz). The results present the effect of
frequency on the G' and G'' for all hydrogel systems (Figure 6.5 b, d, and f). For all
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hydrogels, G' is higher than G'', showing that in all cases there is a prevalence of the
elastic behaviour in comparison to the viscous one, which can also allow for high print
fidelity after the printing process. It can also be seen that the G' and G'' is not effected
by increasing the frequency, showing a plateau behaviour. The results also show that
the AlgMA system presents lower elasticity (G') and viscous properties (G'') than
GelMA and consequently lower printability characteristics. The gelatin and hybrid
systems present higher mechanical properties with higher G’ in the LVER which is
also independent of strain to higher values with a shift in the G' and G'' crossing point
(Figure s 6.5 c and e).
Figure 6.5: Oscillatory results for pre-polymerized systems a) Storage and loss
modulus as a function of strain for AlgMA systems; b) Storage and loss modulus as a
function of frequency for AlgMA systems; c) Storage and loss modulus as a function
of strain for GelMA systems; d) Storage and loss modulus as a function of strain for
GelMA systems; e) Storage and loss modulus as a function of strain for hybrid
systems; f) Storage and loss modulus as a function of frequency for hybrid systems.
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Hydrogel rheological characterisation was performed on the photocrosslinked
hydrogel discs by means of oscillation rheology test. Amplitude sweep results (G' and
G'' plotted as a function of shear strain) show that all hydrogel systems have the same
trend of G' being higher than G'' at low strain rates. however, the hydrogel crosslinking
bonds begin to break at higher strain rates, when the G' crosses G'' and both decrease
(Figure 6.6). The hybrid systems have higher mechanical elastic properties (G')
compared to the single material only systems (AlgMA and GelMA). The hybrid
hydrogel containing equal percentage of each polymer (50:50 AlgMA-GelMA)
presents the highest mechanical properties among all hybrid systems and withstands
deformation at higher strains compared to other hydrogel systems, indicating
improved stability (413).
Figure 6.6: Oscillatory results for polymerized systems a) Storage and loss modulus
as a function of strain for AlgMA systems; b) Storage and loss modulus as a function
of frequency for AlgMA systems; c) Storage and loss modulus as a function of strain
for GelMA systems; d) Storage and loss modulus as a function of strain for GelMA
systems; e) Storage and loss modulus as a function of strain for hybrid systems; f)
Storage and loss modulus as a function of frequency for hybrid systems.
141
Structure morphology and porosity The hydrogels morphology was assessed using SEM (Figure 6.7). The
photocrosslinked hydrogel groups are characterised by a highly porous cellular
structure with an average pore size of ~250 µm for all systems. AlgMA has larger pore
size than GelMA, and different pore sizes were obtained for the hybrid systems as
shown in Table 6.2. This porous structure provides a route for nutrient supply, gas
exchange and metabolic activity as well as supporting and maintaining the phenotype
of the chondrocyte cells for articular cartilage applications. Accordingly, Mei Lien et
al. (414) reported that a pore size between 250-500 µm provides better ECM
production (62-64). All hydrogels provide highly porous structures (> 61%). The
AlgMA hydrogel have the highest porosity (90.8%) with an average pore size of 252.5
µm ± 20. The GelMA has the lowest porosity (61.0%) and an average pore size of
239.5 µm ± 30. The results show that the hybrid hydrogel samples present higher
porosity with higher amounts of AlgMA and that the porosity decreases by increasing
the incorporation of GelMA, which can be related to the inherent densities of the
biomaterials. These results are highly relevant for cartilage tissue engineering
applications since the highly porous structures produced, promote the secretion of
articular cartilage specific ECM and allows chondrocyte interactions and the creation
of a cell-cell network through the surrounding ECM.
Figure 6.7: Cross-section images of different hydrogel systems a) AlgMA, b)
GelMA, c) Alg-Gel(MA) 75:25, d) Alg-Gel(MA) 50:50, and e) Alg-Gel (MA) 25:75.
Scale bar: 200 µm.
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Table 6.2: Experimental density, porosity, and average pore size for the different
material systems
Sample Experimental
density (g/cm3) Porosity (%)
Average pore size
(µm)
AlgMA 0.149± 0.003 90.8%±0.21 252.5 ± 20
GelMA 0.382± 0.011 61.0%±1.16 239.5 ± 30
Alg-Gel(MA) 75:25 0.226± 0.001 84.5%±0.13 251 ± 24
Alg-Gel(MA) 50:50 0.263±0.001 79.9%±0.13 247 ± 30
Alg-Gel(MA) 25:75 0.340±0.005 70.2%±0.47 240 ± 15
Swelling and degradation kinetics and hydrogel
The swelling profile of all hydrogel groups is depicted in Figure 6.8. Results show that
the AlgMA hydrogel presents the highest swelling ratio, 50%, and GelMA hydrogels
present the lowest swelling, 18%. However, all hybrid systems show swelling ratios
ranging from 32%, 40%, and 17% for Alg-Gel(MA) 75:25, 50:50, and 25:75,
respectively. The swelling equilibrium was reached by day 3 for all hydrogels as
evidenced by a plateauing of the swelling curve. Moreover, results show that adding
AlgMA to the hybrid system improves the swelling ratio, indicating that the hydrogel
composition (ratio of biomaterials) controls the swelling properties.
The degradation profile of a hydrogel-based scaffold should match the development
and growth of new tissue with the ECM formation being able to maintain the
mechanical integrity of the structure (415). The degradation rates (percentage mass
loss) at day 22, for AlgMA was 23% , 27% for GelMA, and 17%, 20% and 47% for
the hybrid systems Alg-Gel(MA) 75:25, 50:50, and 25:75, respectively (Figure 6.8b).
However, these degradation rates can be tailored by increasing the crosslinking density
either by increasing the polymer solution/photoinitiator concentration and by
increasing the exposure time to the UV light source. The hydrogels containing gelatin
underwent higher degradation than alginate as gelatin undergoes faster rate of
hydrolytic degradation (416).
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Figure 6.8: Swelling and degradation profiles of all hydrogel groups. a) Swelling ratio
profile and b) degradation (mass loss profile).
Mechanical characterisation
The mechanical properties of the hydrogels were determined using unconfined
uniaxial compression testing (Figure 6.9). The hydrogel discs (cell-free constructs)
were measured on day 1 after incubation for 24 h at 37°C. The results show that
AlgMA and GelMA present an average compressive Young’s modulus of 28.1± 3.5
and 36.4± 6.0 kPa, respectively. The hybrid hydrogels exhibit an average of
compressive Young’s moduli 43.8 ± 3.1, 50.2 ± 4.4, and 66.2 ± 9.8 kPa for Alg-
Gel(MA) 25:75, 50:50, and 75:25 respectively. The Young’s modulus is highly
influenced by hydrogel composition, polymer concentration, photoinitiator
concentration, and exposure time as previously reported (417).
Figure 6.9: Mechanical properties of different photocrosslinked hydrogel, a) stress-
strain curve; b) Young modulus. Legend: A-alginate; G-gelatin; H-Hybrid system.
The mechanical compression test results are important to indicate the mechanical
stability of the hydrogels under potential physiological loading conditions. The
reported results within 20% strain are less than cartilage stiffness (400 to 600 kPa)
(418), however, it has been reported for other polymeric systems that similar
mechanical properties are appropriated to support the ECM formation and to maintain
144
chondrogenic differentiation (419-421). Moreover, the proposed hybrid system must
also be anchored to the subchondral bone using a stiffer polymeric material.
Hydrogel encapsulated chondrocyte viability and proliferation
The viability of the encapsulated cells in the hydrogel was assessed using a live/dead
assay (Figure 6.10). At day 3, AlgMA shows a few live cells and the encapsulated
chondrocytes are dying due to lack of cell binding motifs such as RGDs which are
present in fibronectin, collagen, and laminin to which mammalian cells can bind (422,
423). However, GelMA and the hybrid systems present high cell viability. At later
timepoints (day 7 and 16) the alginate viability improves potentially due to the binding
of proteins from the cell culture media and ECM formation of the surviving cells.
These results show that cell encapsulation conditions were suitable. The photoinitiator
concentration, UV wavelength (365 nm), light intensity (8 mW/cm2), and exposure
time (8 min) had limited cytotoxic effect on the cells. Preliminary evaluation was
performed to assess the cell morphology. In the case of alginate encapsulated
chondrocyte cells, the surviving cells retained a round morphology due to high
crosslinking density of alginate and lack of binding motifs. However, the encapsulated
cells in gelatin system have shown to exhibit phenotype drift, development of
hypertrophic chondrocytes which could be due to low crosslinking density. Cells
encapsulated in the hybrid system had a cell morphology with a more spherical shape
for the entire duration of the in vitro studies compared to the AlgMA, GelMA and 2D
TCP systems. The chondrocytes cultured on 2D TCP have an elongated shape and
fibroblastic morphology.
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Figure 6.10: Cell viability of human chondrocytes encapsulated in AlgMA, GelMA,
Alg-Gel(MA) 50:50, and seeded on a TCP control at day 3, 7, and 16. Scale bar: 200
µm.
Cell proliferation and metabolic activity in the hydrogels was assessed using the
Alamar blue assay at day 1, 3, 5 ,7 and 14 (Figure 6.11). The results show that the
cellular metabolic activity increases for all hydrogels up to day 3 before decreasing
with the AlgMA hydrogel exhibiting the largest decrease in metabolic activity. The
large decrease in AlgMA may be attributed to the lack of cell binding sites in alginate
thus poor viability, as previously shown, and the degradation of the hydrogel
146
preventing cell maintenance and proliferation. The GelMA and hybrid hydrogel show
higher cell metabolic activity up to day 14 compared to AlgMA, potentially due to the
presence of cell binding sites in gelatin allowing cell attachment. Furthermore, the
reduction and plateauing of chondrocyte metabolic activity after day 5 may be due to
the low metabolic and proliferative activity of chondrocytes when present in an
environment that mimics the native ECM environment of articular cartilage tissue.
Figure 6.11: Fluorescence intensity indicating the metabolic activity of human
Chondrocytes in AlgMA, GelMA, Alg-Gel (MA) 50:50 and TCP control at days 1, 3,
5, 7 and 14.
Histological assessment of hydrogel ECM formation
Histological evaluations were performed to visualise and semi-quantify the
cartilaginous specific ECM formation in the photocrosslinked hydrogels at day 14, 21,
28, and 35 (Figure 6.12). The Gomori trichrome staining results indicate that in all
experimental groups, most cells were positive, and collagen was produced, however,
the hybrid system presented higher collagen content (Figure 6.12 and 6.13). Semi-
quantitative analysis shows clear difference in the amount of collagen detected. The
amount of collagen in all hydrogels increased until day 21. At day 28 and 35, the
amounts of collagen started to decrease. A possible interpretation is due to the
degradation of the hydrogel, since at least a minimum of 20% of the hydrogel has
D1 D3 D5 D7 D14
0
2000
4000
6000
Time (days)
GelMA
Hybrid
AlgMA
Flu
ore
sc
en
ce
2D control
**
147
degraded by this timepoint. Thus, cells are migrating to attach to the TCP and amount
of collagen production is reduced and being removed during standard cell culture
procedures. This shows the importance of developing a hydrogel which maintains
structural stability long enough for sufficient ECM tissue formation to support the
cells.
The expression of aggrecan is investigated through immunohistological staining. The
results show that aggrecan was deposited within all the hydrogel systems. Aggrecan
was distributed throughout the hydrogels and was highest in the Alg-Gel(MA) hybrid
system at all timepoints whilst lowest in the AlgMA (Figure 6.12 and 6.13). The peak
aggrecan content is at day 28 before decreasing potentially due to the degradation of
the hydrogels.
The safranin-O staining is present in all hydrogels with the most proteoglycans
detected in the hybrid system with considerably stronger staining than AlgMA and
GelMA.
The histological staining and semi-quantification showed that the composition,
content, and distribution of the ECM varied among the hydrogels. The AlgMA had
the poorest capacity to support cartilage specific ECM formation, as shown by the
weak intensity of staining in the samples, due to the poor cell binding capacity The
GelMA and the hybrid hydrogel enabled the deposition of ECM by the encapsulated
chondrocytes and had the highest qualitative and semi-quantitative staining. This
indicates that the hybrid hydrogel is supportive of maintaining a chondrocyte
phenotype. The hybrid Alg-Gel(MA) is stiffer than the single component hydrogels
support the importance of stiffness as factor in hydrogel design as a stiffer hydrogel
system provides better chondrocyte stimulation to maintain chondrogenic phenotype
after encapsulation in 3D, these results align with Li et al. (424) demonstration of
different chondrocyte phenotypes based on the stiffness of a gelatin hydrogel.
148
(a) Gomori
Figure 6.12: Histological analysis. a) Gomori; b) Aggrecan; c) Safranin-O production
at days 14, 21, 28 and 35 in Alginate methacrylate hydrogels, Gelatin methacrylate
hydrogels and hybrid system (50:50 Alg-Gel)MA.
149
(b) Aggrecan
Figure 6.13 (Cont.): Histological analysis. a) Gomori; b) Aggrecan; c) Safranin-O
production at days 14, 21, 28 and 35 in Alginate methacrylate hydrogels, Gelatin
methacrylate hydrogels and hybrid system (50:50 Alg-Gel)MA.
150
(c) Safranin-O
Figure 6.14 (Cont.): Histological analysis. a) Gomori; b) Aggrecan; c) Safranin-O
production at days 14, 21, 28 and 35 in Alginate methacrylate hydrogels, Gelatin
methacrylate hydrogels and hybrid system (50:50 Alg-Gel)MA.
Figure 6.15: Semi-quantification of the relative area of histological staining of the
AlgMA, GelMA, and Alg-Gel(MA) hydrogels at day 14, 21, 28, and 35 for a) Gomori
trichrome and b) aggrecan.
151
GAGs quantification
GAGs are a major component of articular cartilage and an indicator of cartilage
formation. The secretion of GAGs was detected in the AlgMA, GelMA, and hybrid
Alg-Gel(MA) hydrogels at day 7, 14, 21, 28, and 35 (Figure 6.14). The results show a
clear difference in GAGs production in the three different hydrogel systems. The
AlgMA hydrogels show the lowest GAG production due to poor cell viability and cell
attachment. However, the GelMA and hybrid hydrogels produced larger quantities of
GAGs with the hybrid hydrogel having the largest production of GAGs by day 35.
The 2D TCP control produced similar amounts to the AlgMA hydrogel even though a
larger number of cells are present in the TCP control. This discrepancy can be
attributed to the elongated chondrocyte cell morphology present in 2D cell culture and
the dedifferentiation and phenotypic changes that occur as the chondrocytes proliferate
in 2D cell culture (425). GAGs are crucial ECM factors in cartilage tissue due to their
ability to strongly bind water, create osmotic pressure, and enable attachment of
proteins. The high quantity of GAGs produced in the hybrid system indicates that the
hydrogel can support the maintenance of the chondrocyte phenotype and secretion of
a cartilage specific marker.
Figure 6.16: Assessment of GAG secretion in the photocrosslinked AlgMA, GelMA,
and Alg-GelMA hydrogels at day 7, 14, 21, 28, and 35.
D7 D14 D21 D28 D35
0.0
0.5
1.0
1.5
2.0
Time (days)
Ab
so
rban
ce (
656 n
m)
Control
Hybrid
GelMA
AlgAM
✱✱
✱✱✱
✱✱✱✱
✱✱✱✱
✱✱✱✱
✱✱✱ ✱✱✱✱
✱✱✱✱
✱
✱✱
152
Conclusions
The AlgMA, GelMA, and hybrid Alg-Gel(MA) solutions and hydrogels were
extensively characterised aiming at understanding their suitability to be used as bioink
materials for cartilage applications. All polymers were successfully functionalised
with MA as observed by HNMR. Photopolymerisation was successfully used to
polymerised functionalized hydrogels. Porous structures with appropriate pore sizes
for cartilage applications were obtained. The hybrid system demonstrates that the
combination of both AlgMA and GelMA improves the viscoelastic behaviour of pre-
polymerised materials (improved printability) and mechanical properties of
polymerised hydrogels.
The hybrid system also presents high cell viability, proliferation, and production of
ECM proteins, and GAGs. The results show that the developed hybrid hydrogel is a
suitable bioink material for cartilage applications. It is able to support chondrocytes
proliferation, cell-cell interaction and ECM formation. Moreover, the properties of this
system can be easily tailored by changing the ration between AlgMA and GelMA.
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Chapter 7 Hybrid PCL/Hydrogel scaffold
fabrication and in-process plasma
treatment using PABS†
† This Chapter based on the paper: Fengiuan Liu, Hussein Mishbak, Paulo Bartolo, “Hybrid
polycaprolactone/hydrogel scaffold fabrication and in-process plasma treatment using PABS”,
International Journal of Bioprinting, 5(1): 174, 2019. http://dx/doi.org/10.18063/ijb.v5i1.174. A
preliminary version of this manuscript was also presented at the International Conference on Progress
in Additive Manufacturing (Singapore, 2018) and was awarded as the best paper.
154
The development of a new tissue engineering approach to enable the neocartilage
formation fully anchored to the underlying subchondral bone is critical for tissue
engineering. In Chapters III to VI, two different hydrogel materials (alginate and
gelatin) and a hybrid system based on both alginate and gelatin were characterised
and their potential for cartilage bioinks explored. These different polymeric systems
will enable to create a cartilage construct replicating the zonal structure of cartilage.
However, it is also important to guarantee a good interface between the subchondral
bone and the cell laden construct to guarantee the stable formation of neocartilage
tissue and to enable vertical integration. This interface must be created using both
hard and soft materials.
For bone tissue engineering scaffolds, a wide range of polymeric, ceramic and
polymer-ceramic materials have been investigated (426). Among these materials
polycaprolactone (PCL) has been one of the most popular material. However, due to
its hydrophobicity produced scaffolds are limited in terms of cell-seeding and
proliferation efficiency (427). Moreover, non-uniform cell distribution along the
scaffolds with limited cell attachment in the core region is a common problem. The
absence of commercially available additive manufacturing systems able to produce
multi-type-material and gradient scaffolds makes this problem difficult to address.
This Chapter investigates the use of a novel Plasma-Assisted Bio-extrusion System
(PABS), to produce multi-material scaffolds for the interface between the subchondral
bone and cartilage consisting in a synthetic biopolymer (PCL) and hybrid natural
hydrogel system (previously described in Chapter VII). The PABS system is also used
for the scaffold surface modification (N2 plasma modification).
Introduction
Tissue engineering is promising for organ replacement which minimizes the side
effects of organ transplantation (428, 429). Biomanufacturing is the major strategy of
tissue engineering aiming at the development of biological substitutes that restore,
maintain, or improve tissue function, and it requires the combined use of additive
manufacturing (AM), biocompatible and biodegradable materials, cells and
biomolecular signals (304).
The scaffolds-based strategies (Figure 7.1) for tissue engineering has been most
commonly used, depending strongly on materials and manufacturing processes. For
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materials, five types of biomaterials have been used: acellular tissue matrices,
synthetic polymers, natural polymers, ceramics and polymer/ceramic composites
(430-434).The most commonly used biomaterial for producing scaffolds are synthetic
polymers, such as polycaprolactone (PCL). Polymeric scaffolds play a pivotal role in
tissue engineering through cell seeding, proliferation, and new tissue formation in
three dimensions, showing great promise in the research of engineering a variety of
tissues. Moreover, Scaffolds made from collagen are being rapidly replaced with
ultraporous scaffolds from biodegradable polymers.
Figure 7.1: scaffold-based approach for tissue engineering.
Biodegradable polymers are attractive candidates for scaffolding materials because
they degrade as the new tissues are formed, eventually leaving nothing foreign to the
body. The major challenges in scaffold manufacturing lies in the design and
fabrication of customizable biodegradable constructs with properties that promote cell
adhesion and cell porosity, along with sufficient mechanical properties that match the
host tissue, with predictable degradation rate and biocompatibility (435, 436).
For the fabrication methods, AM techniques have been commonly applied in scaffold
fabrication due to the superior ability in controlling pore size, pore shape and pore
distribution, and thus creating interconnected porous structures (304, 437).When
combined with clinical imaging data, these fabrication techniques can be used to
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produce constructs that are customized to the shape of the defect or injury (438). In
terms of tissue and organ manufacturing, the additive nature ensures minimal waste of
scarce and expensive building material, namely cells, growth factors and biomaterials
(439-441). Among the AM techniques, Material Extrusion has been mostly applied in
the bioengineering field due to the flexibility in material selection based on the use of
pneumatic (442, 443), piston (444) and screw-assisted (445-447) extrusion systems
enabling a wider range of materials to be applied. Some processes operate at room
temperature, thus allowing for cell encapsulation and biomolecule incorporation
without significantly affecting viability. However, cell-seeding and proliferation
efficiency is currently a big challenge due to the following limitations (448-451):
• Most AM techniques are limited to single-material fabrication, which is difficult
to provide appropriate environment for cells due to the inadequate chemical,
physical and biological cues provided during AM processes.
• Additionally, non-uniform cell distribution, especially rare cell adhesion in the
core region of scaffolds, is often caused by the tortuosity of the constructs.
• Moreover, the synthetic biopolymers, most commonly used, are hydrophobic, and
the cell colonization.
Different strategies have been explored to solve the above problems. Multi-material
have been developed and utilized to produce multiple-material scaffolds (442, 452).
However, most of these systems can only form one type of biomaterials, either soft
hydrogels containing cells or bio-signals in the scale of KPa, or rigid biopolymers and
composites in the scale of MPa, which fails in the mimicry of natural tissues.
Additionally, Additionally, low temperature plasma modification is capable of
improving the hydrophilicity of biopolymers by inducing certain functional groups on
the surface to change the chemistry, wettability and energy without altering the bulk
properties (453, 454). However, most plasma treatment can be conducted after
scaffolds printed and the penetration depth is limited, which results in non-uniform
cell distribution along the scaffold.
A novel plasma-assisted bioprinting system (PABS) has been developed in the
University of Manchester, allowing processing soft-hard biomaterial integration and
plasma surface modification layer by layer during the fabrication process in the same
chamber. This paper utilized the plasma-assisted bioextrusion system (PABS) to
produce PCL/Hydrogel hybrid scaffolds and plasma fully treated scaffolds. The
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hydrogel is assesssed with the preparation procees, functionalizaiton process and
rhology properteis, while the PCL fully treated scaffolds are both morphlogically and
bilogically assessed.
Materials and Methods
Polycaprolactone (PCL)
PCL (CAPATM6500, Mw = 50,000 g/mol), purchased from Perstorp (Cheshire, UK)
in the form of 3 mm pellets, was used to produce the scaffolds. PCL is an easy-to-
process semi-crystalline polymer with a density of 1.1 g/cm3, a melting temperature
between 58-60 °C, and a glass transition temperature of - 60 °C.
Hybrid hydrogel) methacrylate anhydride (Alg-Gel)MA preparation
Hybrid hydrogel system platform were considered in this paper. hydrogel which made
of mixing alginate methacrylate and gelatin methacrylate at 50:50% v/v.
Functionalization process for both polymer (alginate and gelatin) is necessary to
introduce the carbon-carbon double bond into the polymer chains that eventually
convert the polymer into photopolymerized polymer. According to published
protocols (455), alginate was functionalized with methacrylate groups with minor
modifications to be photopolymerized. The 2% wt powder alginate (Sigma-Aldrich,
UK) was dissolved in Dulbecco's Phosphate Buffered Saline (DPBS) (Sigma-Aldrich,
UK), and then mixed with methacrylate anhydride (MA) (Sigma-Aldrich, UK) at 23%
v/v of alginate solution under vigorous stirring. The pH of the solution was kept around
7.4 during the reaction time by the addition of 5M NaOH. The reaction time was 24
hours. After the chemical modification, the polymer solution was precipitated with
cold ethanol, dried in an oven overnight at 45 °C and purified through dialysis for 6
days. The solution was then frozen at -80 ºC and recovered by lyophilization.
Gelatin was functionalized by dissolving gelatin bovine skin type B (Sigma-Aldrich,
UK) at a concentration of 12.5%, in Dulbecco's Phosphate Buffered Saline (DPBS)
(Sigma-Aldrich, UK) at a temperature of 45ºC. After gelatin dissolution, MA (10x
molar excess) was added under vigorous. The pH of the solution was kept around 7.0-
8.0 during the reaction. The reaction time was 6 hours. The solution was purified
through dialysis for 7 days, frozen at -80C° and the polymer recovered by
lyophilization.
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Plasma-assisted Bioextrusion System set up
Scaffolds were produces using a hybrid additive manufacturing system called PABS,
being developed at University of Manchester. PABS (Figure 7.2 a) comprises two
main units, a multi-extrusion unit and a three-inlet plasma modification unit (Figure
7.2b). The multi-extrusion unit consists of two pressure-assisted extruders and one
screw-assisted extruder, allowing operating a range of biomaterials, such as synthetic
biopolymers, hydrogels and biopolymer/ceramic composites. The extrusion unit has
four movements: one rotational movement (C1) for selecting the required extrusion
heads, a second rotational movement (C2) for driving and controlling the screw
rotational speed of the screw-assisted extruder, and two linear movements (X and Y)
in the X-Y plane. All these four movements are controlled by stepper motors and CNC
drives. The build platform moves in the z-direction and constitutes the sixth
controllable axis. The build platform was fabricated using 7076 aluminium plate (250
mm x 200 mm x 7.5 mm) and is attached to the z-axis rail guide with an L-shape
support underneath.
The plasma modification unit is mounted on the X-Y platform which is co-planar with
the extrusion platform. Both platforms share common cylindrical guide rails in the X-
direction. The Y-direction movement (V axis) for the plasma modification unit is
independently driven by a stepper motor parallel to the Y axis of the extrusion unit. A
quartz capillary (outside diameter of 7 mm; inner diameter r of 5 mm; length of 70
mm) with three gas inlets serves as the reaction jet. A tungsten rod (inner diameter of
2 mm) and one copper film (10 mm of width) wrapped around the quartz tube serve
as the high-voltage and ground electrodes, respectively. The electrode is connected to
a high-voltage DC power supply (applied voltage of 10 kV; frequency of 50 kHz). The
plasma is generated from the top central electrode, expanding to the surrounding air
inside and outside the nozzle.
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Figure 7.2: a) Set-up of plasma-assisted bio-extrusion system; b) system diagram:
multi-extrusion system, plasma modification system and control system.
The control system consists of a motion control system, temperature control system
and gas supply control system. The motion control system utilizes a Geo Brick LV
motion controller (Delta Tau Data Systems, Inc) to manipulate all motors. The built-
in software allows for complete machine logic control, including G code execution.
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The temperature control system consists of four digital temperature controllers (P.I.D.
Omron E5CN), which are used to precisely control the temperature in the extruder
heating chamber with polyimide thermos-foil heating elements (Omega
Online/Kapton Heaters), and thermocouples (Omega). The gas supply control system
includes an air compressor which works as the main gas supply, regulators and gauges
(SMC, UK), which enables pressure on/off control and manually adjustment. Power
supply (230V ac, PHOENIX CONTACT) offers 24v output voltage and 40A current
for all the control system. Safety considerations were taken into account regarding the
electrical parts, including fuses, main circuit breakers (MCBs), main filter, push
buttons and estops (all supplied by OneCall Electronics Company, UK), and circuits.
The control software was developed in MATLAB as previously reported, and G code
files was generated containing all the instructions for the fabrication process (456).
This configuration enables multi-material dispensing and plasma modification in a
sequential mode. The system is able to achieve a maximum linear velocity of 20 mm/s
and resolution of 0.05 mm.
Scaffolds printing strategies
Scaffolds with a cross-section of 10x10 mm and a height of 3 mm were fabricated
using the single laydown pattern of 0/90°.and a filament distance of 1 mm with pore
size of 1 mm (slice thickness of 0.5 mm; heating temperature of 90°C; extrusion screw
rotational speed of 15 rpm; and nozzle tip size of 0.5 mm.). The strategies for printing
hybrid scaffolds and plasma treated scaffolds are as follows (Figure 7.3):
• Hybrid PCL/hydrogel scaffolds fabrication (Figure 7.3a): After the scaffold being
printed with screw-assisted extruder, the extruder selection unit rotated with 120°,
and then the hydrogel solution was printed in the pores using the pressure-assisted
extruder.
• Full layer treated scaffolds fabrication (Figure 7.3b): The N2 plasma modification
was performed after one-layer PCL was deposited, and the process was repeated
until the last layer of PCL was complete. The treatment was conducted at a
pressure of 0.689 bar and a flow rate of 5 L/mm. The deposition speed of the
plasma jet was 3 mm/s and each layer was subjected to the plasma treatment for
one minute. The distance from the bottom of the jet to the surface of the PCL
filaments was 10 mm.
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Figure 7.3: a) Sequence of operations to fabricate hybrid PCL/hydrogel scaffolds; b)
Sequence of operations to fabricate full-layer plasma treated scaffolds.
Nuclear Magnetic Resonance characterisation
Hybrid hydrogel were characterized by means of 1HNMR to confirm the
functionalization process. The chemical structure of functionalized hybrid hydrogel
system was assessed through Nuclear Magnetic Resonance Spectroscopy (1HNMR),
using the B400 (Bruker Avance III, USA) 400 MHz. Polymeric materials were
dissolved in Deuterium oxide (D2O), transferred to NMR tubes and the spectra
acquired with 128 scans.
Rheological characterisation
To assessing the mechanical properties of the hybrid hydrogel quantitatively, a
deformation rheology tests are performed on polymeric hydrogels discs. The
rheological analyses were carried out using the DHR2 Rheometer (TA Instrument,
USA). Small amplitude oscillatory shear measurements tests were considered, the
shear storage modulus, G′, loss modulus, G″ were quantified. It is assumed that the
material flows by applying a stress being the response measured. A controlled stress
was applied, and the resulting movement measured. Small strain oscillations have
been used to measure viscoelastic properties without destroying the sample structure
the oscillatory test provides a mechanical spectrum for the material.
Morphology Characterization
Scanning electron microscopy (SEM) was used to assess the morphology and surface
characteristic of printed scaffolds. The scaffolds were gold/palladium coated using a
Q150T turbo-pumped sputter coater (Quorum technologies, UK) and imaged at 10 kV
(Hitachi S3000N, Japan). These images were then analysed using ImageJ software.
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Wettability measurement
Water Contact Angle (WCA) measurements on the flat surfaces of untreated and
plasma-treated PCL scaffolds were carried out with a commercial KSV CAM 200
system (KSV Instruments, Finland). The system is equipped with a CCD video camera
and a micrometric liquid dispenser to drop 2 µL of distilled water on the surface of the
scaffold. The measurements of the contact angles are automatically calculated with
the instrument software.
Biological tests
In vitro biological assessments were conducted with human adipose-derived stem cells
(hADSCs) (STEMPRO, Invitrogen, Waltham, MA, USA). Before cell seeding,
scaffolds were sterilized by soaking in 70% ethanol for 2 hours. After sterilization,
samples were rinsed twice in phosphate buffered saline (PBS) (Gibco, ThermoFisher
Scientific, Waltham, MA, USA), transferred to 24-well plates and air-dried for 24
hours at room temperature 50,000 cells were seeded on each sample, including
plasma-treated and untreated scaffolds.
Cell viability/proliferation behavior and the percentage of cells attached to the
scaffolds (cell-seeding efficiency) were assessed through Alamar Blue assay (also
termed the Resazurin assay, reagents from Sigma-Aldrich, UK). Cell
viability/proliferation was measured at 1, 3, 7 and 14 days after cell seeding. For each
measurement, cell-seeded scaffolds were transferred to a new 24-well plate and 0.7 ml
of Alamar Blue solution was added to each well, the plate was incubated for 4 hours
under standard condition (37 ºC, 5% CO2 and 95% humidity). After incubation, 150
µL of each sample solution was transferred to a 96-well plate and the fluorescence
intensity measured at 540 nm excitation wavelength and 590 nm emission wavelength
with a spectrophotometer (Sunrise, Tecan, Männedorf, Zurich, Switzerland).
Cell attachment and distribution are assessed using laser confocal microscopy, with
cell nuclei stained. At day one of cell culture and after 14 days, scaffolds were removed
from 24-well cell culture plate, rinsed twice in phosphate-buffered saline (PBS)
(Gibco, ThermoFisher Scientific, Waltham, MA, USA), fixed with 10% neutral
buffered formalin (Sigma-Aldrich, Dorset, UK) for 30 minutes at room temperature
After fixation, samples were rinsed twice with PBS for the removal of formalin, then
permeabilised with 0.1 % Triton-X100 (Sigma-Aldrich, Dorset, UK) in PBS at room
temperature for 10 minutes, rinse twice for the removal of Triton-X100. Cell nuclei
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were stained blue by soaking scaffolds in a PBS solution containing 4′,6-Diamidine-
2′-phenylindole dihydrochloride (DAPI) (Sigma-Aldrich, Dorset, UK) at the
manufacturer recommended concentration. Samples were left in the staining solution
for 10 min prior to removal, rinsed twice thoroughly with PBS. Confocal images were
obtained using a 3D rendering mode on a Leica TCS SP5 (Leica, Milton Keynes, UK)
confocal microscope, and cell colonization was quantified using a standard z-stack
method. All images were taken at the centre area of the scaffolds and the experiments
were performed three times in triplicate.
Data analysis
All data are represented as mean ± standard deviation. Biological results were
subjected to one-way analysis of variance (one-way ANOVA) and post hoc Tukey’s
test using GraphPad Prism software. Significance levels were set at p < 0.05.
Results
Hybrid Scaffold Fabrication
The hybrid scaffold, consisting of PCL and hydrogel solution, was successfully
fabricated using PABS. Figure 7.4a shows the image of the hybrid scaffold, where the
porous structures hold the hydrogel solution without any deformation. The position of
the deposited hydrogel was precisely controlled.
Full-layer treated PCL scaffold
Figure 7.4b shows that the printed full-layer N2 plasma treated scaffolds has a well-
bonded interconnected structure with uniform pore distribution and pore size in the
range of ~500 µm (Figure 7.4c). The N2 plasma treatment was conducted at a pressure
of 0.689 bar and a flow rate of 5 L/mm. The deposition speed of the plasma jet was 3
mm/s and each layer was subjected to the plasma treatment for one minute. The
distance from the bottom of the jet to the surface of the PCL filaments was 10 mm.
Figure 7.4d presents the filament surface after N2 plasma modification, where lines in
the direction of plasma movement can be observed making the surface roughness
increased.
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Figure 7.4: (a) Hybrid polycaprolactone (PCL)/hydrogel scaffold; (b) Scanning
electron microscopy (SEM) image of top view of PCL/hydrogel scaffold; (c) SEM
image of side view of PCL/ hydrogel scaffold; (d) photo of a full-layer N2 plasma-
treated PCL scaffold; (E) SEM image of top view of full-layer N2 plasma treated PCL
scaffold; (f) SEM image of filament surface of full-layer N2 plasma-treated PCL
scaffold.
Wettability assessment of full-layer plasma modified scaffold
WCA measurements were performed on untreated and fully treated plasma PCL
scaffold surfaces to determine the effect of plasma modification on the surface
wettability. Table 7.1 highlights the WCA results at different time points after the
droplet was dropped on the surface of the scaffolds. The results show that in the case
of an untreated PCL scaffold, there are no significant changes in the WCA values with
time with values varying between 83.2±2.0° and 80.9±2.7°. For treated scaffolds, the
WCA value, at 0 s, was lower (63.0±3.1°), leading to a fully wetting value of 26.7±0.9
° at 0.5 s. At 3 s, the droplet was fully absorbed.
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Figure 7.5: a) Temporal variation of fluorescence intensity of cell-seeded PCL
scaffolds with and without N2 plasma treatment; b) Confocal microscope images of
untreated and full-layer treated of cell seeded scaffolds, 1 day and 14 days after cell
culture. Scale bar 250 µm.
Table 7.1: Temporal variation of water contact angles for treated and untreated
scaffolds.
Time PCL scaffolds N2 plasma fully treated
0s 83.2±2.0 ° 63.0±3.1 °
0.5s 82.9±1.2 ° 26.7±0.9 °
3s 80.9±2.7 ° Fully absorbed
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Biological assessment of full-layer plasma modified scaffold
The adhesion and proliferation of hADSCs cells on plasma full-layer modified PCL
scaffolds was studied and compared with untreated ones. The biological
characterization was assessed using Alamar Blue Assay. The fluorescence intensity of
cell seeded scaffolds measured at four different culture time points (Day 1, 3, 7 and
14) is shown in Figure 7.5a. Higher fluorescence intensity corresponds to more
metabolically active cells. As observed, cell proliferation increases with time in all
types of scaffolds, suggesting that they are suitable structures for cell attachment and
proliferation. However, a fast proliferation rate is observed in the case of plasma
treated scaffolds. The different performance is statistically significant after day 3.
Confocal microscopy images (Figure 7.5b) present the cell attachment and distribution
after cell seeding (day 1) and proliferation (day 14). It can be observed that plasma
treated scaffolds presented higher numbers of cells than untreated scaffolds.
Additionally, it is also possible to observe that plasma surface treated scaffolds
presented best cell attachment and dispersion.
Discussion
The printed hybrid PCL scaffolds filled with hydrogel present the printability of
PBAS, enabling the soft-hard material integration. The photo and SEM images of the
whole printed structure indicate that the plasma modification process does not affect
the physical appearance of the structure and potentially no effect on the mechanical
performances (457). Moreover, SEM image of the filament surface confirms the
increased surface roughness is due to the etching process (458), which results in the
stripping off the topmost layer of the polymer filament. From this study, the increase
surface roughness is also resulted from the linear scratches attributed to the gas flow
by the plasma jetting directly after the PCL deposition when the material is still in the
molten status. As the printed material is not totally cooled down, when the plasma
modification occurs, the gas flow effect is stronger, significantly influencing the
surface topography. Moreover, the increase of surface roughness is beneficial for cell
colonization in the scaffolds (459).
The wettability results reveal that the hydrophilicity of the surface is dramatically
improved due to the ionisable groups introduced on the surface by the N2 plasma,
which enhances the hydrogel bonding with water. Compared with the results published
in (454,460), the absorption speed is dramatically increased, due to chemical
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heterogeneity on the surface of each layer because of the plasma modification layer
upon layer. However, the effect of plasma modification can last within a certain period
of time depending on the density of chemical regents deposited on the surface, and the
effect also decreases with time since the structural rearrangement of polymer chains
resulting in the decreased surface energy (461).
In addition, it is important to control hydrogels printability window (injection,
deposition and extrusion) during printing process to mimic the native organ structures.
To achieve precise printable properties, hydrogels have been designed to achieve
adjustable viscoelastic behaviour, and the SEM images confirm the liquid-like-gel
structure before printing and quick gelation kinetics to produce structure with good
fidelity. Hybrid hydrogel system presents an adjustable viscoelastic behaviour that
could be changed/ tailored with temperature, shear thinning and polymer
concentrations. The rheological assessment result confirms that the hybrid hydrogel
system has clear linear viscoelastic region (LVE) which characterize by both storage
moduli G′ and loss moduli G″ are independent of shear strain and the system is solid-
like-gel (G′ ≫ G″). These characteristics make it easy to inject hybrid hydrogel
system (Alg-Gel)MA.
Consistent with the other studies (462, 463), a significant increase in the biological
behavior is observed after plasma modification. Since the hydrophilicity has been
improved with the plasma modification process, the environment is changed to be
more suitable for cell colonization and proliferation. Also, with the full-layer plasma
modification capability, the plasma active species can reach the walls of the pores on
each layer of the scaffold, leading to the uniform cell distribution along the scaffold.
This will enable higher rate of tissue formation in the clinical research.
Conclusions
This paper presents a novel additive manufacturing system comprising a multi-
material printing unit and a plasma jet unit. To assess the system, hybrid PCL/hydrogel
scaffolds and full-layer plasma treated PCL scaffolds were produced. The effect of
plasma treatment on PCL samples was examined. WCA results confirmed that the
hydrophilic character of the PCL samples increased due to the nitrogen groups
introduced by the plasma jetting on the scaffold filaments. It was also possible to
observe that the plasma treatment positively influences cell attachment and
proliferation. Applications that may benefit from this technology include hybrid tissue,
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which has compositional variations depending on the region or organ-like structure
that require continuous vascular network to facilitate nutrient diffusion.
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Chapter 8
Conclusions and future
work
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Conclusions
Cartilage is an avascular tissue with limited regenerative capabilities. Its structure, role
and main diseases and clinical therapies were detailed in Chapter II (research objective
1). Despite different treatments have been proposed and being clinically used they still
present several limitations such as high cost, poor clinical outcomes, and limited
temporal efficacy. In order to address these limitations cartilage tissue engineering
approaches based on the use of biocompatible and biodegradable materials and
additive manufacturing technologies to produce scaffolds for cartilage repair or cell
laden constructs based on the use of bioinks have been proposed. The scaffold-based
approach is based on the use of 3D structures that will provide the substrate for cell
adhesion, proliferation and differentiation. In this approach scaffolds can be used as
acellular structures and implanted into the defect, recruiting cells from the surrounding
tissue; or seeded with cells and pre-cultured in a bioreactor prior implantation. The
success of this approach has been limited and the scaffolds being proposed so far are
not able to recapitulate the zonal structure of cartilage. Cell laden constructs seems to
be the ideal strategy not only because it allows to print a cartilage-like construct
encapsulating relevant cartilage cells and materials with a structure similar to cartilage
but also because it allows the development of future in situ printing approaches.
Bioprinting approaches to produce cell laden constructs for cartilage repair have been
proposed. However, few limitations still exist related to materials (e.g. tailoring
viscoelasticity), printing process (e.g. shear stresses and shape fidelity) and risk of
contamination during the bioprinting process. The development of novel constructs
for cartilage applications is critical and requires the:
• Design of suitable materials, able to be printed and presenting suitable
mechanical, swelling, degradability and morphology and able to sustain cell
growth and ECM formation;
• Design of a multi-layer construct able to replicate the zonal structure of
cartilage;
• Selection of the best additive manufacturing technique (e.g. crosslink
mechanism).
As discussed in Chapter 2, natural-based hydrogels are ideal candidates for cartilage
applications and photocrosslinking reactions a suitable method to produce cell laden
constructs. However, only two photocurable hydrogels are commercially available
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(ChonDuxTM and GelrinC). This an area that requires more research not only in terms
of design the hydrogels (e.g. level of C=C in the pre-polymer chain) but also on
investigating the effect of the curing process on both printability and cell survival.
However, this is not a simple task as high levels of C=C bonds increase the
crosslinking density, improving mechanical properties and shape fidelity during the
fabrication process but decreases biocompatibility as the free space available to
support cell growth is reduced. Similarly, high levels of photoinitiator increase the
curing kinetics and crosslinking density but might also induces some toxicity. Light
intensity and irradiation time must also be optimised in order to avoid any negative
effects on cells. Some of these correlations were investigated in this research work and
the results presented in Chapters III to VI.
Based on the aims and research objectives presented in Chapter I, the main novelty
of this research is the development of a novel multi-material cell laden construct
for cartilage based on two different polymer materials (alginate and gelatin) and
a hybrid system based on the combination of both alginate and gelatin. Single type
materials are considered for both the superficial zone and the deeper region of
cartilage, while the hybrid system is considered for the transitional zone. Both alginate
and gelatin have been explored before for different tissue engineering applications but
their combination to create a zonal construct such the one proposed by this
dissertation was never investigated before. Each material was investigated in detail
as a single material and the results presented in Chapters III and IV for alginate and
Chapter V for gelatin. Each material was successfully functionalized with
methacrylate anhydride as observed through NMR and it was possible to control the
functionalization process by changing the polymer concentration, methacrylate
anhydride concentration and reaction time (research objective 2). Key conclusions
emerging from this part of the work are:
• By increasing the polymer concentration, keeping the reaction time and the
methacrylate anhydride concentration constant, the degree of modification
(level of unsaturation) decreases;
• By increasing the methacrylate anhydride concentration, keeping polymer
concentration and reaction time constant, the degree of modification
decreases;
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• By increasing the reaction time, keeping both methacrylate anhydride and
polymer concentration constant, the degree of modification increases.
The effect of the functionalization process on the rheological, printability, mechanical,
morphological, swelling and degradation properties was also investigated for both
materials (Chapters III and V) (research objective 3). Results show that is possible to
tailor the properties of each single material and the main conclusions are:
• The increase of the degree of modification increases the crosslinking density,
printability and mechanical properties;
• The increase of the degree of modification decreases the swelling properties
and slow down the degradation process;
• The increase of the degree of modification produces structures with high
number of pores with small pore sizes.
Based on the results presented in Chapters III to V the following single material
systems were considered (research objective 3):
• AlgMA (2% wt of alginate and 20% v/v of methacrylate anhydride)
functionalized during 24 h and dissolved in a solution containing 1% wt of
photoinitiator;
• GelMA (12.5% wt of gelatin and 10% v/v of methacrylate anhydride)
functionalized during 6 h and dissolved in a solution containing 1% wt of
photoinitiator;
These systems were used to encapsulate mesenchymal stem cells (Chapter V) and
human chondrocytes (Chapter IV) and cell laden constructs were produced using a
UV lamp (8 mW/cm2 of light intensity) and 8 min of irradiation time (research
objective 3). Results show that:
• All material showed no toxicity effects;
• All materials were able to support cell growth. However, fast cell
proliferation was observed for GelMA, which can be attributed to the
presence of specific cell adhesion motifs as discussed in Chapter V.
Chapter VI investigates hybrid systems obtained through the combination of different
ratios between alginate and gelatin. These materials were investigated before and after
photopolymerisation and the effect of material composition in terms of rheological,
mechanical, swelling, degradation properties and biological properties was
investigated (research objective 4). Results show that:
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• AlgMA and GelMA hybrid systems are able to support cell growth and ECM
formation;
• The addition of AlgMA increases the mechanical properties, swelling
characteristics and slow down the degradation process;
• The levels of collagen, aggrecan and GAGs formation were significantly
higher in the hybrid systems in comparison to the single material systems.
Moreover, GelMA presents higher levels of ECM formation in comparison to
AlgMA.
Finally, Chapter VII investigates the use of a scaffold produced with a novel additive
manufacturing system and comprising two main materials (PCL and hybrid
alginate/gelatin system). This construct was investigated aiming to define a proper
vertical integration between the subchondral bone and cartilage (research objective 5).
Due to hydrophobic the nature of PCL (a material commonly used for bone tissue
engineering scaffolds) plasma treatment was used. Results showed that it was not only
possible to create a construct using these two different polymeric systems but also that
the plasma treatment positively influenced cell attachment and proliferation.
Future works
This thesis discusses the use of hydrogel-based constructs scaffolds for tissue
engineering produced for cartilage replacements through additive manufacturing. An
extensive in vitro work was conducted to design and assess the materials and the 3D
produced scaffolds. Despite the contributions to the current knowledge provided by
this research work, it was possible also to open new research questions that will be
addressed in the future. Moreover, additional work should be conducted to complete
the current research. Planned activities include:
(1) A zonal construct containing layers of alginate, gelatin and alginate/gelatin will be
produce encapsulating chondrocytes but also stem cells and growth factors. The
construct will be characterized in terms of overall mechanical properties, adhesion
between layers and the ability to sustain cell adhesion, proliferation and
differentiation. The zonal construct will be produced using the materials
investigated in these research work;
(2) Investigate new functionalization methods for both alginate and gelatin by
introducing C=C on the hydroxyl (e.g. oxidation, sulfation and copolymerization)
174
and carboxyl (esterification and amidation) groups in order to improve both
mechanical, rheological, biological and degradability characteristics;
(3) Investigate the effect of light intensity, irradiation time and photoinitiator
concentration on the different properties of the printed constructs;
(4) The lubrication properties of cartilage, particularly the upper zone of cartilage, is
an important property not considered in this research. The coefficient of friction,
under both dynamic and static loading conditions, of the different materials as a
function of functionalization and processing conditions will be assessed;
(5) Cartilage is an avascular tissue and as a consequence chondrogenesis improves
under hypoxia conditions. The effect of the functionalization process and printing
conditions in terms of oxygen permeability will be investigated allowing to design
constructs creating a more suitable biological environment;
(6) In order to have a deeper understanding on the interactions between the hydrogel
and cells, additional protein and gene expression tests will be conducted. This will
include the quantification of the transcription factor SOX-6 and SOX-9, Collagen
II, and cartilage oligomeric protein (COMP) of chondrocytes after long periods of
culture;
(7) Free radical polymerization was used in this research. This is a chain-growth
reaction allowing the spatiotemporal control of the polymeric network but
producing heterogeneous networks. In the future, other chemistries such as
photoclick reactions (step-growth mechanism) will be explored to allow fast and
more efficient reactions with minimal network defects;
(8) Scaffolds will be also characterized in vivo. Initially, constructs will be
subcutaneously implanted into the flanks of nude mice to investigate swelling,
degradability and neocartilage formation. Later, more detailed studies will be
performed considering osteochondral defects created in rabbits.
175
References 1. Altman R, Asch E, Bloch D, Bole G, Borenstein D, Brandt K, et al.
Development of criteria for the classification and reporting of osteoarthritis:
classification of osteoarthritis of the knee. Arthritis & Rheumatism: Official Journal
of the American College of Rheumatology. 1986;29(8):1039-49.
2. Mauck RL, Soltz MA, Wang CC, Wong DD, Chao P-HG, Valhmu WB, et al.
Functional tissue engineering of articular cartilage through dynamic loading of
chondrocyte-seeded agarose gels. Journal of biomechanical engineering.
2000;122(3):252-60.
3. Hutmacher DW. Scaffolds in tissue engineering bone and cartilage. The
biomaterials: Silver jubilee compendium: Elsevier; 2000, 175-89.
4. Coburn J, Gibson M, Bandalini PA, Laird C, Mao H-Q, Moroni L, et al.
Biomimetics of the extracellular matrix: an integrated three-dimensional fiber-
hydrogel composite for cartilage tissue engineering. Smart structures and systems.
2011;7(3):213.
5. Gater R, Njoroge W, Owida H, Yang Y. Scaffolds mimicking the native
structure of tissues. Handbook of Tissue Engineering Scaffolds: Volume One:
Elsevier; 2019, 51-71.
6. De Bari C, Roelofs AJ. Stem cell-based therapeutic strategies for cartilage
defects and osteoarthritis. Current opinion in pharmacology. 2018;40:74-80.
7. Cheng A, Schwartz Z, Kahn A, Li X, Shao Z, Sun M, et al. Advances in porous
scaffold Design for Bone and Cartilage Tissue Engineering and regeneration. Tissue
Engineering Part B: Reviews. 2019;25(1):14-29.
8. Javaid M, Haleem A. Current status and challenges of Additive manufacturing
in orthopaedics: an overview. Journal of clinical orthopaedics and trauma.
2019;10(2):380-6.
9. Ngo TD, Kashani A, Imbalzano G, Nguyen KT, Hui D. Additive
manufacturing (3D printing): A review of materials, methods, applications and
challenges. Composites Part B: Engineering. 2018;143:172-96.
10. Li J, Illeperuma WRK, Suo Z, Vlassak JJ. Hybrid Hydrogels with Extremely
High Stiffness and Toughness. ACS Macro Letters. 2014;3(6):520-3.
11. Palmese LL, Thapa RK, Sullivan MO, Kiick KL. Hybrid hydrogels for
biomedical applications. Current Opinion in Chemical Engineering. 2019;24:143-57.
176
12. Madry H, van Dijk CN, Mueller-Gerbl M. The basic science of the subchondral
bone. Knee Surgery, Sports Traumatology, Arthroscopy. 2010;18(4):419-33.
13. Lin Z, Willers C, Xu J, Zheng MH. The Chondrocyte: Biology and Clinical
Application. Tissue Engineering. 2006;2(7):1971-84.
14. Duarte Campos DF, Drescher W, Rath B, Tingart M, Fischer H. Supporting
Biomaterials for Articular Cartilage Repair. Cartilage. 2012;3(3):205-21.
15. Mankin HJ. The response of articular cartilage to mechanical injury. JBJS.
1982;64(3):460-6.
16. Szafranski JD, Grodzinsky AJ, Burger E, Gaschen V, Hung HH, Hunziker EB.
Chondrocyte mechanotransduction: effects of compression on deformation of
intracellular organelles and relevance to cellular biosynthesis. Osteoarthritis and
cartilage. 2004;12(12):937-46.
17. Sophia Fox AJ, Bedi A, Rodeo SA. The basic science of articular cartilage:
structure, composition, and function. Sports health. 2009;1(6):461-8.
18. Camarero-Espinosa S, Rothen-Rutishauser B, Foster EJ, Weder C. Articular
cartilage: From formation to tissue engineering. Biomaterials Science. 2016;4(5):734-
67.
19. Science H, Zealand N, Poole Ca, Science H, Zealand N. Articular cartilage
chondrons: form, function and failure. Journal of Anatomy. 1997;191(1997):1-13.
20. Huey DJ, Hu JC, Athanasiou KA. Unlike Bone, Cartilage Regeneration
Remains Elusive. Science. 2012;338(6109):917-21.
21. Malda J, Groll J, van Weeren PR. Rethinking articular cartilage regeneration
based on a 250-year-old statement. Nature Reviews Rheumatology. 2019;15:571–72.
22. Benjamin M, Evans EJ. Fibrocartilage. Journal of anatomy. 1990;171:
PMC1257123.
23. Bhosale AM, Richardson JB. Articular cartilage: structure, injuries and review
of management. British medical bulletin. 2008;87(1):77-95.
24. Poole AR, Kojima T, Yasuda T, Mwale F, Kobayashi M, Laverty S.
Composition and structure of articular cartilage: a template for tissue repair. Clinical
Orthopaedics and Related Research®. 2001;391:S26-S33.
25. Eyre D. Articular cartilage and changes in Arthritis: Collagen of articular
cartilage. Arthritis Research & Therapy. 2001;4(1):30-35.
26. Basser PJ, Schneiderman R, Bank RA, Wachtel E, Maroudas A. Mechanical
Properties of the Collagen Network in Human Articular Cartilage as Measured by
177
Osmotic Stress Technique. Archives of Biochemistry and Biophysics.
1998;351(2):207-19.
27. Cancedda R. Cartilage and bone extracellular matrix. Current pharmaceutical
design. 2009;15(12):1334-48.
28. Lipshitz H, Glimcher MJ. In vitro wear of articular cartilage. The Journal of
bone and joint surgery American volume. 1975;57(4):527-34.
29. Temenoff JS, Mikos AG. Review: Tissue engineering for regeneration of
articular cartilage. Biomaterials. 2000;21(5):431-40.
30. Roughley PJ. The structure and function of cartilage proteoglycans. European
Cells and Materials. 2006;12(9):92-101.
31. Eyre DR, Wu JJ. Collagen of fibrocartilage: a distinctive molecular phenotype
in bovine meniscus. FEBS Letters. 1983;158(2):265-70.
32. Marlovits S, Hombauer M, Truppe M, Vècsei V, Schlegel W. Changes in the
ratio of type-I and type-II collagen expression during monolayer culture of human
chondrocytes. The Journal of Bone and Joint Surgery British volume. 2004;86-
B(2):286-95.
33. Schnabel M, Marlovits S, Eckhoff G, Fichtel I, Gotzen L, Vecsei V, et al.
Dedifferentiation-associated changes in morphology and gene expression in primary
human articular chondrocytes in cell culture. Osteoarthritis and cartilage.
2002;10(1):62-70.
34. Changoor A, Nelea M, Méthot S, Tran-Khanh N, Chevrier A, Restrepo A, et
al. Structural characteristics of the collagen network in human normal, degraded and
repair articular cartilages observed in polarized light and scanning electron
microscopies. Osteoarthritis and cartilage. 2011;19(12):1458-68.
35. Thambyah A, Broom N. On how degeneration influences load-bearing in the
cartilage bone system: a microstructural and micromechanical study. Osteoarthritis
and cartilage. 2007;15(12):1410-23.
36. Karl K. Matrix loading: Assembly of extracellular matrix collagen fibrils
during embryogenesis. Birth Defects Research Part C: Embryo Today: Reviews.
2004;72(1):1-11.
37. Lindahl A. From gristle to chondrocyte transplantation: treatment of cartilage
injuries. Philosophical Transactions of the Royal Society B: Biological Sciences.
2015;370(1680): 20140369.
178
38. Maroudas A, Muir H, Wingham J. The correlation of fixed negative charge
with glycosaminoglycan content of human articular cartilage. Biochimica et
Biophysica Acta (BBA) - General Subjects. 1969;177(3):492-500.
39. Lorenzo P, Bayliss MT, Heinegårdt D. A novel cartilage protein (CILP)
present in the mid-zone of human articular cartilage increases with age. Journal of
Biological Chemistry. 1998;273(36):23463-8.
40. Perrimon N, Bernfield M, editors. Cellular functions of proteoglycans—an
overview. Seminars in Cell & Developmental Biology. 2001;12(2):65-7.
41. Venn M, Maroudas A. Chemical composition and swelling of normal and
osteoarthrotic femoral head cartilage. I. Chemical composition. Annals of the
Rheumatic Diseases. 1977;36(2):121-9.
42. Holopainen JT, Brama PAJ, Halmesmaki E, Harjula T, Tuukkanen J, van
Weeren PR, et al. Changes in subchondral bone mineral density and collagen matrix
organization in growing horses. Bone. 2008;43(6):1108-14.
43. Castaneda S, Roman-Blas JA, Largo R, Herrero-Beaumont G, Castañeda S,
Roman-Blas JA, et al. Subchondral bone as a key target for osteoarthritis treatment.
Biochem Pharmacol. 2012;83(3):315-23.
44. Makris EA, Gomoll AH, Malizos KN, Hu JC, Athanasiou KA. Repair and
tissue engineering techniques for articular cartilage. Nature Reviews Rheumatology.
2015;11:21-34.
45. Schinagl RM, Gurskis D, Chen AC, Sah RL. Depth‐dependent confined
compression modulus of full‐thickness bovine articular cartilage. Journal of
Orthopaedic Research. 1997;15(4):499-506.
46. M SR, Donnell G, C CA, L SR. Depth‐dependent confined compression
modulus of full‐thickness bovine articular cartilage. Journal of Orthopaedic
Research.15(4):499-506.
47. Nguyen LH, Kudva AK, Saxena NS, Roy K. Engineering articular cartilage
with spatially-varying matrix composition and mechanical properties from a single
stem cell population using a multi-layered hydrogel. Biomaterials. 2011;32(29):6946-
52.
48. Kumar P, Oka M, Toguchida J, Kobayashi M, Uchida E, Nakamura T, et al.
Role of uppermost superficial surface layer of articular cartilage in the lubrication
mechanism of joints. Journal of Anatomy. 2001;199(3):241-50.
179
49. Gudas R, Gudaitė A, Mickevičius T, Masiulis N, Simonaitytė R, Čekanauskas
E, et al. Comparison of Osteochondral Autologous Transplantation, Microfracture, or
Debridement Techniques in Articular Cartilage Lesions Associated With Anterior
Cruciate Ligament Injury: A Prospective Study With a 3-Year Follow-up.
Arthroscopy. 2013;29(1):89-97.
50. Goyal D, Keyhani S, Lee EH, Hui JHP. Evidence-Based Status of
Microfracture Technique: A Systematic Review of Level I and II Studies.
Arthroscopy. 2013;29(9):1579-88.
51. Steadman JR, Briggs KK, Rodrigo JJ, Kocher MS, Gill TJ, Rodkey WG.
Outcomes of microfracture for traumatic chondral defects of the knee: Average 11-
year follow-up. Arthroscopy. 2003;19(5):477-84.
52. Kreuz PC, Steinwachs MR, Erggelet C, Krause SJ, Konrad G, Uhl M, et al.
Results after microfracture of full-thickness chondral defects in different
compartments in the knee. Osteoarthritis and cartilage. 2006;14(11):1119-25.
53. Dorotka R, Windberger U, Macfelda K, Bindreiter U, Toma C, Nehrer S.
Repair of articular cartilage defects treated by microfracture and a three-dimensional
collagen matrix. Biomaterials. 2005;26(17):3617-29.
54. Nukavarapu SP, Dorcemus DL. Osteochondral tissue engineering: Current
strategies and challenges. Biotechnology Advances. 2013;31(5):706-21.
55. Yousefi AM, Hoque ME, Prasad RG, Uth N. Current strategies in multiphasic
scaffold design for osteochondral tissue engineering: a review. Journal of biomedical
materials research Part A. 2015;103(7):2460-81.
56. Peterson L, Minas T, Brittberg M, Nilsson A, Sjögren-Jansson E, Lindahl A.
Two- to 9-Year Outcome After Autologous Chondrocyte Transplantation of the Knee.
Clinical Orthopaedics and Related Research (1976-2007). 2000;374.
57. Gomoll AH, Probst C, Farr J, Cole BJ, Minas T. Use of a Type I/III Bilayer
Collagen Membrane Decreases Reoperation Rates for Symptomatic Hypertrophy after
Autologous Chondrocyte Implantation. The American Journal of Sports Medicine.
2009;37(Suppl 1):20S-23S
58. Darling EM, Athanasiou KA. Rapid phenotypic changes in passaged articular
chondrocyte subpopulations. Journal of Orthopaedic Research. 2005;23(2):425-32.
59. Martinez I, Elvenes J, Olsen R, Bertheussen K, Johansen O. Redifferentiation
of in vitro expanded adult articular chondrocytes by combining the hanging-drop
180
cultivation method with hypoxic environment. Cell transplantation. 2008;17(8):987-
96.
60. Caron MMJ, Emans PJ, Coolsen MME, Voss L, Surtel DAM, Cremers A, et
al. Redifferentiation of dedifferentiated human articular chondrocytes: comparison of
2D and 3D cultures. Osteoarthritis and cartilage. 2012;20(10):1170-8.
61. Demange M, Gomoll AH. The use of osteochondral allografts in the
management of cartilage defects. Current Reviews in Musculoskeletal Medicine.
2012;5(3):229-35.
62. Krych AJ, Harnly HW, Rodeo SA, Williams RJIII. Activity Levels Are Higher
After Osteochondral Autograft Transfer Mosaicplasty Than After Microfracture for
Articular Cartilage Defects of the Knee: A Retrospective Comparative Study. JBJS.
2012;94(11):971-8.
63. Gudas R, Kalesinskas RJ, Kimtys V, Stankevicius E, Toliusis V, Bernotavicius
G, et al. A Prospective Randomized Clinical Study of Mosaic Osteochondral
Autologous Transplantation Versus Microfracture for the Treatment of Osteochondral
Defects in the Knee Joint in Young Athletes. Arthroscopy. 2005;21(9):1066-75.
64. Bentley G, Biant LC, Vijayan S, Macmull S, Skinner JA, Carrington RWJ.
Minimum ten-year results of a prospective randomised study of autologous
chondrocyte implantation versus mosaicplasty for symptomatic articular cartilage
lesions of the knee. The Journal of Bone and Joint Surgery British volume. 2012;94-
B(4):504-9.
65. Lee WYW, Wang B. Cartilage repair by mesenchymal stem cells: Clinical trial
update and perspectives. Journal of Orthopaedic Translation. 2017;9:76-88.
66. Jeon OH, Kim C, Laberge R-M, Demaria M, Rathod S, Vasserot AP, et al.
Local clearance of senescent cells attenuates the development of post-traumatic
osteoarthritis and creates a pro-regenerative environment. Nature Medicine.
2017;23(6):775-81.
67. Outerbridge RE. the Etiology of Chondromalacia Patellae. Bone & Joint
Journal. 1961;43-B(4):752-7.
68. Huang BJ, Hu JC, Athanasiou KA. Cell-based tissue engineering strategies
used in the clinical repair of articular cartilage. Biomaterials. 2016;98:1-22.
69. Steadman JR, Rodkey WG, Rodrigo JJ. Microfracture: Surgical Technique and
Rehabilitation to Treat Chondral Defects. Clinical Orthopaedics and Related
Research®. 2001;(391 Suppl):S362-9.
181
70. Steadman JR, Rodkey WG, Singleton SB, Briggs KK. Microfracture technique
forfull-thickness chondral defects: Technique and clinical results. Operative
Techniques in Orthopaedics. 1997;7(4):300-4.
71. Spahn G, Kahl E, Mückley T, Hofmann GO, Klinger HM. Arthroscopic knee
chondroplasty using a bipolar radiofrequency-based device compared to mechanical
shaver: results of a prospective, randomized, controlled study. Knee Surgery, Sports
Traumatology, Arthroscopy. 2008;16(6):565-73.
72. Bae DK, Yoon KH, Song SJ. Cartilage Healing After Microfracture in
Osteoarthritic Knees. Arthroscopy. 2006;22(4):367-74.
73. Azizeh‐Mitra Y, Enamul HM, V PRGS, Nicholas U. Current strategies in
multiphasic scaffold design for osteochondral tissue engineering: A review. Journal of
Biomedical Materials Research Part A. 2014;103(7):2460-81.
74. McCarthy JC, Noble PC, Schuck MR, Wright J, Lee J. The role of labral
lesions to development of early degenerative hip disease. Clinical Orthopaedics and
Related Research®. 2001;393:25-37.
75. Felson DT, Lawrence RC, Dieppe PA, Hirsch R, Helmick CG, Jordan JM, et
al. Osteoarthritis: new insights. Part 1: the disease and its risk factors. Annals of
internal medicine. 2000;133(8):635-46.
76. Alford JW, Cole BJ. Cartilage restoration, part 2: techniques, outcomes, and
future directions. The American journal of sports medicine. 2005;33(3):443-60.
77. Drobnič M, Radosavljevič D, Cör A, Brittberg M, Stražar K. Debridement of
cartilage lesions before autologous chondrocyte implantation by open or
transarthroscopic techniques. The Journal of Bone and Joint Surgery British volume.
2010;92-B(4):602-8.
78. Mirza MZ, Swenson RD, Lynch SA. Knee cartilage defect: marrow
stimulating techniques. Current Reviews in Musculoskeletal Medicine.
2015;8(4):451-6.
79. Wang L, Lazebnik M, Detamore MS. Hyaline cartilage cells outperform
mandibular condylar cartilage cells in a TMJ fibrocartilage tissue engineering
application. Osteoarthritis and cartilage. 2009;17(3):346-53.
80. Knutsen G, Engebretsen L, Ludvigsen TC, Drogset JO, Grøntvedt T, Solheim
E, et al. Autologous Chondrocyte Implantation Compared with Microfracture in the
Knee: A Randomized Trial. JBJS. 2004;86(3):455-64.
182
81. Peterson L, Minas T, Brittberg M, Lindahl A. Treatment of osteochondritis
dissecans of the knee with autologous chondrocyte transplantation: results at two to
ten years. JBJS. 2003;85(Suppl_2):17-24.
82. Bachmeier CJM, March LM, Cross MJ, Lapsley HM, Tribe KL, Courtenay
BG, et al. A comparison of outcomes in osteoarthritis patients undergoing total hip
and knee replacement surgery. Osteoarthritis and cartilage. 2001;9(2):137-46.
83. Sibanda N, Copley LP, Lewsey JD, Borroff M, Gregg P, MacGregor AJ, et al.
Revision rates after primary hip and knee replacement in England between 2003 and
2006. PLoS medicine. 2008;5(9):1398-1408.
84. Park YB, Ha CW, Rhim JH, Lee HJ. Stem cell therapy for articular cartilage
repair: review of the entity of cell populations used and the result of the clinical
application of each entity. The American journal of sports medicine.
2018;46(10):2540-52.
85. Kwon H, Brown WE, Lee CA, Wang D, Paschos N, Hu JC, et al. Surgical and
tissue engineering strategies for articular cartilage and meniscus repair. Nature
Reviews Rheumatology. 2019;15(9):550-70.
86. Balakrishnan B, Banerjee R. Biopolymer-Based Hydrogels for Cartilage
Tissue Engineering. Chemical Reviews. 2011;111(8):4453-74.
87. Gobbi A, Nehrer S, Neubauer M, Herman K. Tissue Engineering for
the Cartilage Repair of the Ankle. In: Canata GL, d'Hooghe P, Hunt KJ, Kerkhoffs
GMMJ, Longo UG, editors. Sports Injuries of the Foot and Ankle: A Focus on
Advanced Surgical Techniques. Berlin, Heidelberg: Springer Berlin Heidelberg; 2019,
119-24.
88. Fuentes-Mera L, Camacho A, Engel E, Pérez-Silos V, Lara-Arias J, Marino-
Martínez I, et al. Therapeutic Potential of Articular Cartilage Regeneration using
Tissue Engineering Based on Multiphase Designs. Cartilage Tissue Engineering and
Regeneration Techniques: IntechOpen; 2019.
89. Li L, Yu F, Zheng L, Wang R, Yan W, Wang Z, et al. Natural hydrogels for
cartilage regeneration: Modification, preparation and application. Journal of
orthopaedic translation. 2019;17:26-41.
90. Sánchez-Téllez AD, Téllez-Jurado L, Rodríguez-Lorenzo ML. Hydrogels for
Cartilage Regeneration, from Polysaccharides to Hybrids. Polymers. 2017;9(12): 671.
183
91. Tchobanian A, Van Oosterwyck H, Fardim P. Polysaccharides for tissue
engineering: Current landscape and future prospects. Carbohydrate Polymers.
2019;205:601-25.
92. Rodríguez Vázquez M, Vega-Ruiz B, Ramos-Zúñiga R, Saldaña-Koppel DA,
Quiñones Olvera LFJBri. Chitosan and its potential use as a scaffold for tissue
engineering in regenerative medicine. 2015;2015: 821279.
93. Raghunath J, Salacinski HJ, Sales KM, Butler PE, Seifalian AMJCoib.
Advancing cartilage tissue engineering: the application of stem cell technology.
2005;16(5):503-9.
94. Hacker MC, Krieghoff J, Mikos AG. Synthetic polymers. Principles of
regenerative medicine: Elsevier; 2019. p. 559-90.
95. Coenen AMJ, Bernaerts KV, Harings JAW, Jockenhoevel S, Ghazanfari S.
Elastic materials for tissue engineering applications: Natural, synthetic, and hybrid
polymers. Acta Biomaterialia. 2018;79:60-82.
96. Badylak SF, Freytes DO, Gilbert TW. Extracellular matrix as a biological
scaffold material: Structure and function. Acta Biomaterialia. 2009;5(1):1-13.
97. Beachley V, Ma G, Papadimitriou C, Gibson M, Corvelli M, Elisseeff
JJJoBMRPA. Extracellular matrix particle–glycosaminoglycan composite hydrogels
for regenerative medicine applications. 2018;106(1):147-59.
98. Liu X, Meng H, Guo Q, Sun B, Zhang K, Yu W, et al. Tissue-derived scaffolds
and cells for articular cartilage tissue engineering: characteristics, applications and
progress. 2018;372(1):13-22.
99. Kim YS, Majid M, Melchiorri AJ, Mikos AG. Applications of decellularized
extracellular matrix in bone and cartilage tissue engineering. Bioengineering &
translational medicine. 2018;4(1):83-95.
100. Kim YS, Majid M, Melchiorri AJ, Mikos AGJB, medicine t. Applications of
decellularized extracellular matrix in bone and cartilage tissue engineering.
2019;4(1):83-95.
101. Benders KEM, Weeren PRv, Badylak SF, Saris DBF, Dhert WJA, Malda J.
Extracellular matrix scaffolds for cartilage and bone regeneration. Trends in
Biotechnology. 2013;31(3):169-76.
102. Kim YS, Majid M, Melchiorri AJ, Mikos AG. Applications of decellularized
extracellular matrix in bone and cartilage tissue engineering. 2019;4(1):83-95.
184
103. Benders KE, Terpstra ML, Levato R, Malda JJJ. Fabrication of Decellularized
Cartilage-derived Matrix Scaffolds. 2019(143):e58656.
104. Iop L, Dal Sasso E, Menabò R, Di Lisa F, Gerosa G. The Rapidly Evolving
Concept of Whole Heart Engineering. Stem cells international. 2017;2017:8920940.
105. Badylak SF, Freytes DO, Gilbert TWJAb. Extracellular matrix as a biological
scaffold material: structure and function. 2009;5(1):1-13.
106. Schwarz S, Koerber L, Elsaesser AF, Goldberg-Bockhorn E, Seitz AM,
Durselen L, et al. Decellularized cartilage matrix as a novel biomatrix for cartilage
tissue-engineering applications. Tissue engineering Part A. 2012;18(21-22):2195-209.
107. Melchels FPW, Domingos MAN, Klein TJ, Malda J, Bartolo PJ, Hutmacher
DW. Additive manufacturing of tissues and organs. Progress in Polymer Science.
2012;37(8):1079-104.
108. Derakhshanfar S, Mbeleck R, Xu K, Zhang X, Zhong W, Xing M. 3D
bioprinting for biomedical devices and tissue engineering: A review of recent trends
and advances. Bioactive Materials. 2018;3(2):144-56.
109. Wu Y, Kennedy P, Bonazza N, Yu Y, Dhawan A, Ozbolat I. Three-
Dimensional Bioprinting of Articular Cartilage: A Systematic Review. CARTILAGE.
2018:1947603518809410.
110. Vyas C, Poologasundarampillai G, Hoyland J, Bartolo P. 3D printing of
biocomposites for osteochondral tissue engineering. In: Ambrosio L, editor.
Biomedical Composites (Second Edition): Woodhead Publishing; 2017: 261-302.
111. Lim KS, Levato R, Costa PF, Castilho MD, Alcala-Orozco CR, van
Dorenmalen KMA, et al. Bio-resin for high resolution lithography-based
biofabrication of complex cell-laden constructs. Biofabrication. 2018;10(3):034101.
112. Bernal PN, Delrot P, Loterie D, Li Y, Malda J, Moser C, et al. Volumetric
Bioprinting of Complex Living-Tissue Constructs within Seconds. Advanced
Materials. 2019;0(0):1904209.
113. Pereira RF, Bártolo PJ. 3D bioprinting of photocrosslinkable hydrogel
constructs. Journal of Applied Polymer Science. 2015;132(48): 42458.
114. Hospodiuk M, Dey M, Sosnoski D, Ozbolat IT. The bioink: A comprehensive
review on bioprintable materials. Biotechnology Advances. 2017;35(2):217-39.
115. Gungor-Ozkerim PS, Inci I, Zhang YS, Khademhosseini A, Dokmeci MR.
Bioinks for 3D bioprinting: an overview. Biomaterials Science. 2018;6(5):915-46.
185
116. Paxton N, Smolan W, Böck T, Melchels F, Groll J, Jungst T. Proposal to assess
printability of bioinks for extrusion-based bioprinting and evaluation of rheological
properties governing bioprintability. Biofabrication. 2017;9(4):044107.
117. Hu W, Wang Z, Xiao Y, Zhang S, Wang J. Advances in crosslinking strategies
of biomedical hydrogels. Biomaterials Science. 2019;7(3):843-55.
118. Gao T, Gillispie GJ, Copus JS, Pr AK, Seol YJ, Atala A, et al. Optimization of
gelatin–alginate composite bioink printability using rheological parameters: a
systematic approach. Biofabrication. 2018;10(3):034106.
119. Ribeiro A, Blokzijl MM, Levato R, Visser CW, Castilho M, Hennink WE, et
al. Assessing bioink shape fidelity to aid material development in 3D bioprinting.
Biofabrication. 2017;10(1):14102.
120. Malda J, Visser J, Melchels FP, Jüngst T, Hennink WE, Dhert WJA, et al. 25th
anniversary article: Engineering hydrogels for biofabrication. Advanced Materials.
2013;25(36):5011-28.
121. Bertassoni LE, Cardoso JC, Manoharan V, Cristino AL, Bhise NS, Araujo
WA, et al. Direct-write bioprinting of cell-laden methacrylated gelatin hydrogels.
Biofabrication. 2014;6(2):024105.
122. Nair K, Gandhi M, Khalil S, Yan KC, Marcolongo M, Barbee K, et al.
Characterization of cell viability during bioprinting processes. Biotechnology Journal.
2009;4(8):1168-77.
123. Murphy SV, Atala A. 3D bioprinting of tissues and organs. Nature
Biotechnology. 2014;32:773-85.
124. He Y, Yang F, Zhao H, Gao Q, Xia B, Fu J. Research on the printability of
hydrogels in 3D bioprinting. Scientific Reports. 2016;6:29977.
125. Zou X, Kui X, Zhang R, Zhang Y, Wang X, Wu Q, et al. Viscoelasticity and
Structures in Chemically and Physically Dual-Cross-Linked Hydrogels: Insights from
Rheology and Proton Multiple-Quantum NMR Spectroscopy. Macromolecules.
2017;50(23):9340-52.
126. Chimene D, Lennox KK, Kaunas RR, Gaharwar AKJAoBE. Advanced
Bioinks for 3D Printing: A Materials Science Perspective. 2016;44(6):2090-102.
127. Kwon H, Brown WE, Lee CA, Wang D, Paschos N, Hu JC, et al. Surgical and
tissue engineering strategies for articular cartilage and meniscus repair. Nature
reviews Rheumatology. 2019;15(9):550-70.
186
128. Kwon H, Paschos NK, Hu JC, Athanasiou K. Articular cartilage tissue
engineering: the role of signaling molecules. Cellular and molecular life sciences.
2016;73(6):1173-94.
129. Fortier LA, Barker JU, Strauss EJ, McCarrel TM, Cole BJ. The role of growth
factors in cartilage repair. Clinical Orthopaedics and Related Research®.
2011;469(10):2706-15.
130. Koons GL, Mikos AG. Progress in three-dimensional printing with growth
factors. Journal of controlled release. 2019;295:50-9.
131. Demoor M, Ollitrault D, Gomez-Leduc T, Bouyoucef M, Hervieu M, Fabre H,
et al. Cartilage tissue engineering: molecular control of chondrocyte differentiation for
proper cartilage matrix reconstruction. Biochimica et Biophysica Acta (BBA)-General
Subjects. 2014;1840(8):2414-40.
132. Danišovič Ľ, Varga I, Polák Š. Growth factors and chondrogenic
differentiation of mesenchymal stem cells. Tissue and Cell. 2012;44(2):69-73.
133. Fortier LA, Barker JU, Strauss EJ, McCarrel TM, Cole BJ. The role of growth
factors in cartilage repair. Clinical orthopaedics and related research.
2011;469(10):2706-15.
134. Ahn J, Kim SA, Kim KW, Oh JH, Kim SJ. Optimization of TGF-β1-
transduced chondrocytes for cartilage regeneration in a 3D printed knee joint model.
PLoS One. 2019;14(5):e0217601.
135. Diao H, Wang J, Shen C, Xia S, Guo T, Dong L, et al. Improved cartilage
regeneration utilizing mesenchymal stem cells in TGF-beta1 gene-activated scaffolds.
Tissue engineering Part A. 2009;15(9):2687-98.
136. Wei FY, Lee JK, Wei L, Qu F, Zhang JZ. Correlation of insulin-like growth
factor 1 and osteoarthritic cartilage degradation: a spontaneous osteoarthritis in
guinea-pig. European Review for Medical and Pharmacological Sciences.
2017;21(20):4493-500.
137. Moncada-Saucedo NK, Marino-Martinez IA, Lara-Arias J, Romero-Diaz VJ,
Camacho A, Valdes-Franco JA, et al. A Bioactive Cartilage Graft of IGF1-Transduced
Adipose Mesenchymal Stem Cells Embedded in an Alginate/Bovine Cartilage Matrix
Tridimensional Scaffold. Stem Cells Int. 2019;2019:9792369.
138. Ertan AB, Yılgor P, Bayyurt B, Çalıkoğlu AC, Kaspar Ç, Kök FN, et al. Effect
of double growth factor release on cartilage tissue engineering. 2013;7(2):149-60.
187
139. Zykwinska A, Marquis M, Godin M, Marchand L, Sinquin C, Garnier C, et al.
Microcarriers Based on Glycosaminoglycan-Like Marine Exopolysaccharide for
TGF-beta1 Long-Term Protection. Marine drugs. 2019;17(1):E65.
140. Moncada-Saucedo NK, Marino-Martínez IA, Lara-Arias J, Romero-Díaz VJ,
Camacho A, Valdés-Franco J, et al. A Bioactive Cartilage Graft of IGF1-Transduced
Adipose Mesenchymal Stem Cells Embedded in an Alginate/Bovine Cartilage Matrix
Tridimensional Scaffold. 2019 2019:9792369,.
141. Fahy N, Alini M, Stoddart MJ. Mechanical stimulation of mesenchymal stem
cells: Implications for cartilage tissue engineering. Journal of Orthopaedic Research.
2018;36(1):52-63.
142. Grad S, Eglin D, Alini M, Stoddart MJ. Physical stimulation of chondrogenic
cells in vitro: a review. Clinical orthopaedics and related research. 2011;469(10):2764-
72.
143. Athanasiou KA, Responte DJ, Brown WE, Hu JC. Harnessing Biomechanics
to Develop Cartilage Regeneration Strategies. Journal of Biomechanical Engineering.
2015;137(2):020901.
144. Salinas EY, Hu JC, Athanasiou K. A Guide for Using Mechanical Stimulation
to Enhance Tissue-Engineered Articular Cartilage Properties. Tissue Engineering Part
B: Reviews. 2018;24(5):345-58.
145. Panadero JA, Lanceros-Mendez S, Ribelles JLG. Differentiation of
mesenchymal stem cells for cartilage tissue engineering: Individual and synergetic
effects of three-dimensional environment and mechanical loading. Acta Biomaterialia.
2016;33:1-12.
146. Osborne AC, Lamb KJ, Lewthwaite JC, Dowthwaite GP, Pitsillides AA.
Short-term rigid and flaccid paralyses diminish growth of embryonic chick limbs and
abrogate joint cavity formation but differentially preserve pre-cavitated joints. J
Musculoskelet Neuronal Interact. 2002;2(5):448-56.
147. Roddy KA, Prendergast PJ, Murphy P. Mechanical influences on
morphogenesis of the knee joint revealed through morphological, molecular and
computational analysis of immobilised embryos. PloS one. 2011;6(2):e17526-e.
148. Fang J, Hall BK. Differential expression of neural cell adhesion molecule
(NCAM) during osteogenesis and secondary chondrogenesis in the embryonic chick.
Int J Dev Biol. 1995;39(3):519-28.
188
149. Zhao J, Griffin M, Cai J, Li S, Bulter PEM, Kalaskar DM. Bioreactors for
tissue engineering: An update. Biochemical Engineering Journal. 2016;109:268-81.
150. Li K, Zhang C, Qiu L, Gao L, Zhang X. Advances in Application of
Mechanical Stimuli in Bioreactors for Cartilage Tissue Engineering. Tissue
Engineering Part B: Reviews. 2017;23(4):399-411.
151. Nigel M, Sandip H, Wasim SK. The Role of Bioreactors in Cartilage Tissue
Engineering. Current Stem Cell Research & Therapy. 2012;7(4):287-92.
152. Meinert C, Schrobback K, Hutmacher DW, Klein TJ. A novel bioreactor
system for biaxial mechanical loading enhances the properties of tissue-engineered
human cartilage. Scientific Reports. 2017;7(1):16997.
153. Schatti O, Grad S, Goldhahn J, Salzmann G, Li Z, Alini M, et al. A
combination of shear and dynamic compression leads to mechanically induced
chondrogenesis of human mesenchymal stem cells. Eur Cell Mater. 2011;22:214-25.
154. Vainieri ML, Wahl D, Alini M, van Osch GJVM, Grad S. Mechanically
stimulated osteochondral organ culture for evaluation of biomaterials in cartilage
repair studies. Acta Biomaterialia. 2018;81:256-66.
155. Lee JK, Huwe LW, Paschos N, Aryaei A, Gegg CA, Hu JC, et al. Tension
stimulation drives tissue formation in scaffold-free systems. Nature Materials.
2017;16(8):864-73.
156. Langer R, Vacanti JP. Tissue engineering. Science. 1993;260(5110):920-926.
157. Stevens MMJNn. Toxicology: Testing in the third dimension. 2009;4(6):342-
3.
158. Place ES, George JH, Williams CK, Stevens MMJCsr. Synthetic polymer
scaffolds for tissue engineering. 2009;38(4):1139-51.
159. Jell G, Swain R, Stevens MM. Raman spectroscopy: a tool for tissue
engineering. Emerging Raman Applications and Techniques in Biomedical and
Pharmaceutical Fields: Springer; 2010:419-37.
160. Place ES, Evans ND, Stevens MM. Complexity in biomaterials for tissue
engineering. Nature Materials. 2009;8: 457-70.
161. Verissimo AR, Nakayama KJDP, Biofabrication. Scaffold-Free
Biofabrication. 2018:431-50.
162. DuRaine GD, Brown WE, Hu JC, Athanasiou KAJAobe. Emergence of
scaffold-free approaches for tissue engineering musculoskeletal cartilages.
2015;43(3):543-54.
189
163. Huey DJ, Hu JC, Athanasiou KAJS. Unlike bone, cartilage regeneration
remains elusive. 2012;338(6109):917-21.
164. Jung Y, Ji H, Chen Z, Fai Chan H, Atchison L, Klitzman B, et al. Scaffold-
free, Human Mesenchymal Stem Cell-Based Tissue Engineered Blood Vessels.
Scientific reports. 2015;5:15116.
165. Ovsianikov A, Khademhosseini A, Mironov V. The Synergy of Scaffold-
Based and Scaffold-Free Tissue Engineering Strategies. Trends in Biotechnology.
2018;36(4):348-57.
166. DeForest CA, Anseth KS. Advances in bioactive hydrogels to probe and direct
cell fate. Annu Rev Chem Biomol Eng. 2012;3:421-44.
167. Lutolf MP. Biomaterials: Spotlight on hydrogels. Nat Mater. 2009;8(6):451-3.
168. Camci-Unal G, Annabi N, Dokmeci MR, Liao R, Khademhosseini A.
Hydrogels for cardiac tissue engineering. Npg Asia Materials. 2014;6:e99.
169. Hoffman AS. Hydrogels for biomedical applications. Advanced Drug Delivery
Reviews. 2002;54(1):3-12.
170. Lim HL, Hwang Y, Kar M, Varghese S. Smart hydrogels as functional
biomimetic systems. Biomaterials Science. 2014;2(5):603-18.
171. Lutolf MP, Lauer-Fields JL, Schmoekel HG, Metters AT, Weber FE, Fields
GB, et al. Synthetic matrix metalloproteinase-sensitive hydrogels for the conduction
of tissue regeneration: Engineering cell-invasion characteristics. 2003;100(9):5413-8.
172. Pereira RF, Bártolo PJ. 3D Photo-Fabrication for Tissue Engineering and Drug
Delivery. Engineering. 2015;1(1):90-112.
173. Kim IL, Mauck RL, Burdick JAJB. Hydrogel design for cartilage tissue
engineering: a case study with hyaluronic acid. 2011;32(34):8771-82.
174. van Weeren PR. General anatomy and physiology of joints. Joint disease in
the horse: Elsevier; 2016, 1-24.
175. Perera J, Gikas P, Bentley G. The present state of treatments for articular
cartilage defects in the knee. 2012;94(6):381-7.
176. Armiento A, Stoddart M, Alini M, Eglin DJAb. Biomaterials for articular
cartilage tissue engineering: Learning from biology. 2018;65:1-20.
177. Duarte Campos DF, Drescher W, Rath B, Tingart M, Fischer HJC. Supporting
biomaterials for articular cartilage repair. 2012;3(3):205-21.
190
178. Jones KJ, Sheppard WL, Arshi A, Hinckel BB, Sherman SLJC. Articular
cartilage lesion characteristic reporting Is highly variable in clinical outcomes studies
of the knee. 2018:1947603518756464.
179. Nukavarapu SP, Dorcemus DL. Osteochondral tissue engineering: current
strategies and challenges. Biotechnol Adv. 2013;31(5):706-21.
180. Huang GP, Molina A, Tran N, Collins G, Arinzeh TL. Investigating cellulose
derived glycosaminoglycan mimetic scaffolds for cartilage tissue engineering
applications. 2018;12(1):e592-e603.
181. Guo T, Lembong J, Zhang LG, Fisher J. Three-dimensional printing articular
cartilage: recapitulating the complexity of native tissue. 2017;23(3):225-36.
182. Lories RJ, Luyten FP. The bone-cartilage unit in osteoarthritis. Nature reviews
Rheumatology. 2011;7(1):43-9.
183. Temenoff JS, Mikos AG. Review: tissue engineering for regeneration of
articular cartilage. Biomaterials. 2000;21(5):431-40.
184. Izadifar Z, Chen X, Kulyk W. Strategic design and fabrication of engineered
scaffolds for articular cartilage repair. Journal of functional biomaterials.
2012;3(4):799-838.
185. Camarero-Espinosa S, Rothen-Rutishauser B, Foster EJ, Weder C. Articular
cartilage: from formation to tissue engineering. Biomater Sci. 2016;4(5):734-67.
186. Zhang L, Hu J, Athanasiou KA. The role of tissue engineering in articular
cartilage repair and regeneration. Crit Rev Biomed Eng. 2009;37(1-2):1-57.
187. Mollon B, Kandel R, Chahal J, Theodoropoulos J. The clinical status of
cartilage tissue regeneration in humans. Osteoarthritis and cartilage.
2013;21(12):1824-33.
188. Hunziker EB. Articular cartilage repair: basic science and clinical progress. A
review of the current status and prospects. Osteoarthritis and cartilage.
2002;10(6):432-63.
189. Lin Z, Willers C, Xu J, Zheng MH. The chondrocyte: biology and clinical
application. Tissue Eng. 2006;12(7):1971-84.
190. Kjellen L, Lindahl U. Proteoglycans: structures and interactions. Annu Rev
Biochem. 1991;60:443-75.
191. Sugawara E, Nikaido H. Properties of AdeABC and AdeIJK efflux systems of
Acinetobacter baumannii compared with those of the AcrAB-TolC system of
Escherichia coli. Antimicrob Agents Chemother. 2014;58(12):7250-7.
191
192. Abusara Z, Von Kossel M, Herzog W. In Vivo Dynamic Deformation of
Articular Cartilage in Intact Joints Loaded by Controlled Muscular Contractions.
PLoS One. 2016;11(1):e0147547.
193. Lusse S, Claassen H, Gehrke T, Hassenpflug J, Schunke M, Heller M, et al.
Evaluation of water content by spatially resolved transverse relaxation times of human
articular cartilage. Magn Reson Imaging. 2000;18(4):423-30.
194. Buckwalter JA, Mankin HJ. Articular cartilage: tissue design and chondrocyte-
matrix interactions. Instr Course Lect. 1998;47:477-86.
195. Weiss C. The Physiologoy and Pathology of Hyaluronic Acid in Joints. Upsala
Journal of Medical Sciences. 1977;82(2):95-6.
196. Schmidt TA, Gastelum NS, Nguyen QT, Schumacher BL, Sah RL. Boundary
lubrication of articular cartilage: role of synovial fluid constituents. Arthritis and
rheumatism. 2007;56(3):882-91.
197. Li Y, Wei X, Zhou J, Wei L. The age-related changes in cartilage and
osteoarthritis. BioMed research international. 2013;2013:916530.
198. Chung C, Burdick JA. Engineering cartilage tissue. Adv Drug Deliv Rev.
2008;60(2):243-62.
199. Correa D, Lietman SA. Articular cartilage repair: Current needs, methods and
research directions. Semin Cell Dev Biol. 2017;62:67-77.
200. International Cartilage Regeneration and Joint Preservation Society (ICRS).
Other Cartilaginous Parts of the Body 2019, April 24 [Available from:
https://cartilage.org/patient/about-cartilage/welcome-to-our-joint/other-cartilaginous-
parts-of-the-body/.
201. Swieszkowski W, Tuan BH, Kurzydlowski KJ, Hutmacher DW. Repair and
regeneration of osteochondral defects in the articular joints. Biomol Eng.
2007;24(5):489-95.
202. Redman SN, Oldfield SF, Archer CW. Current strategies for articular cartilage
repair. European cells & materials. 2005;9:23-32.
203. Liu Y, Zhou G, Cao Y. Recent Progress in Cartilage Tissue Engineering—Our
Experience and Future Directions. Engineering. 2017;3(1):28-35.
204. Kalamegam G, Memic A, Budd E, Abbas M, Mobasheri A. A Comprehensive
Review of Stem Cells for Cartilage Regeneration in Osteoarthritis. Advances in
experimental medicine and biology. 2018;1089:23-36.
192
205. Loebel C, Burdick JA. Engineering Stem and Stromal Cell Therapies for
Musculoskeletal Tissue Repair. Cell Stem Cell. 2018;22(3):325-39.
206. Maia FR, Carvalho MR, Oliveira JM, Reis RL. Tissue Engineering Strategies
for Osteochondral Repair. Advances in experimental medicine and biology.
2018;1059:353-71.
207. Abbas M, Alkaff M, Jilani A, Alsehli H, Damiati L, Kotb M, et al.
Combination of Mesenchymal Stem Cells, Cartilage Pellet and Bioscaffold Supported
Cartilage Regeneration of a Full Thickness Articular Surface Defect in Rabbits.
Journal of Tissue Engineering and Regenerative Medicine.2018;15(5):661-71.
208. Omidian H, Park K. Hydrogels. In: Siepmann J, Siegel RA, Rathbone MJ,
editors. Fundamentals and Applications of Controlled Release Drug Delivery. Boston,
MA: Springer US; 2012. p. 75-105.
209. Barbetta A, Barigelli E, Dentini M. Porous alginate hydrogels: synthetic
methods for tailoring the porous texture. Biomacromolecules. 2009;10(8):2328-37.
210. Lee JH, Khang G, Lee JW, Lee HB. Interaction of Different Types of Cells on
Polymer Surfaces with Wettability Gradient. Journal of colloid and interface science.
1998;205(2):323-30.
211. Utech S. A review of hydrogel-based composites for biomedical applications:
enhancement of hydrogel properties by addition of rigid inorganic fillers. Journal of
materials science. 2016;51(1):271-310.
212. Billiet T, Vandenhaute M, Schelfhout J, Van Vlierberghe S, Dubruel P. A
review of trends and limitations in hydrogel-rapid prototyping for tissue engineering.
Biomaterials. 2012;33(26):6020-41.
213. Straccia MC, Romano I, Oliva A, Santagata G, Laurienzo P. Crosslinker
effects on functional properties of alginate/N-succinylchitosan based hydrogels.
Carbohydr Polym. 2014;108:321-30.
214. Liu M, Zeng X, Ma C, Yi H, Ali Z, Mou X, et al. Injectable hydrogels for
cartilage and bone tissue engineering. Bone research. 2017;5:17014.
215. Wang QG, Hughes N, Cartmell SH, Kuiper NJ. The composition of hydrogels
for cartilage tissue engineering can influence glycosaminoglycan profile. European
cells & materials. 2010;19:86-95.
216. Malda J, Visser J, Melchels FP, Jungst T, Hennink WE, Dhert WJ, et al. 25th
anniversary article: Engineering hydrogels for biofabrication. Advanced materials
(Deerfield Beach, Fla). 2013;25(36):5011-28.
193
217. Markstedt K, Mantas A, Tournier I, Martinez Avila H, Hagg D, Gatenholm P.
3D Bioprinting Human Chondrocytes with Nanocellulose-Alginate Bioink for
Cartilage Tissue Engineering Applications. Biomacromolecules. 2015;16(5):1489-96.
218. Mauck RL, Soltz MA, Wang CC, Wong DD, Chao PH, Valhmu WB, et al.
Functional tissue engineering of articular cartilage through dynamic loading of
chondrocyte-seeded agarose gels. Journal of biomechanical engineering.
2000;122(3):252-60.
219. Ponticiello MS, Schinagl RM, Kadiyala S, Barry FP. Gelatin-based resorbable
sponge as a carrier matrix for human mesenchymal stem cells in cartilage regeneration
therapy. Journal of biomedical materials research. 2000;52(2):246-55.
220. Yang K, Sun J, Wei D, Yuan L, Yang J, Guo L, et al. Photo-crosslinked mono-
component type II collagen hydrogel as a matrix to induce chondrogenic
differentiation of bone marrow mesenchymal stem cells. Journal of Materials
Chemistry B. 2017;5(44):8707-18.
221. Ibusuki S, Papadopoulos A, Ranka MP, Halbesma GJ, Randolph MA,
Redmond RW, et al. Engineering cartilage in a photochemically crosslinked collagen
gel. The journal of knee surgery. 2009;22(1):72-81.
222. Omobono MA, Zhao X, Furlong MA, Kwon CH, Gill TJ, Randolph MA, et al.
Enhancing the stiffness of collagen hydrogels for delivery of encapsulated
chondrocytes to articular lesions for cartilage regeneration. Journal of Biomedical
Materials Research Part A. 2015;103(4):1332-8.
223. Tan H, Chu CR, Payne KA, Marra KG. Injectable in situ forming
biodegradable chitosan-hyaluronic acid based hydrogels for cartilage tissue
engineering. Biomaterials. 2009;30(13):2499-506.
224. Suh JK, Matthew HW. Application of chitosan-based polysaccharide
biomaterials in cartilage tissue engineering: a review. Biomaterials.
2000;21(24):2589-98.
225. Kim IL, Mauck RL, Burdick JA. Hydrogel design for cartilage tissue
engineering: a case study with hyaluronic acid. Biomaterials. 2011;32(34):8771-82.
226. Fu S, Thacker A, Sperger DM, Boni RL, Buckner IS, Velankar S, et al.
Relevance of rheological properties of sodium alginate in solution to calcium alginate
gel properties. AAPS PharmSciTech. 2011;12(2):453-60.
194
227. Stagnaro P, Schizzi I, Utzeri R, Marsano E, Castellano M. Alginate-
polymethacrylate hybrid hydrogels for potential osteochondral tissue regeneration.
Carbohydr Polym. 2018;185:56-62.
228. Rouillard AD, Berglund CM, Lee JY, Polacheck WJ, Tsui Y, Bonassar LJ, et
al. Methods for photocrosslinking alginate hydrogel scaffolds with high cell viability.
Tissue Eng Part C Methods. 2011;17(2):173-9.
229. Paepe ID, Declercq H, Cornelissen M, Schacht E. Novel hydrogels based on
methacrylate-modified agarose. 2002;51(10):867-70.
230. Tripathi A, Kumar A. Multi-featured macroporous agarose-alginate cryogel:
synthesis and characterization for bioengineering applications. Macromolecular
bioscience. 2011;11(1):22-35.
231. Lin H, Cheng AW, Alexander PG, Beck AM, Tuan RS. Cartilage Tissue
Engineering Application of Injectable Gelatin Hydrogel with In Situ Visible-Light-
Activated Gelation Capability in Both Air and Aqueous Solution. 2014;20(17-
18):2402-11.
232. Zhao X, Lang Q, Yildirimer L, Lin ZY, Cui W, Annabi N, et al.
Photocrosslinkable Gelatin Hydrogel for Epidermal Tissue Engineering. Adv Healthc
Mater. 2016;5(1):108-18.
233. Skardal A, Zhang J, McCoard L, Xu X, Oottamasathien S, Prestwich GD.
Photocrosslinkable hyaluronan-gelatin hydrogels for two-step bioprinting. Tissue
engineering Part A. 2010;16(8):2675-85.
234. Billiet T, Van Gasse B, Gevaert E, Cornelissen M, Martins JC, Dubruel P.
Quantitative contrasts in the photopolymerization of acrylamide and methacrylamide-
functionalized gelatin hydrogel building blocks. Macromolecular bioscience.
2013;13(11):1531-45.
235. Li X, Chen S, Li J, Wang X, Zhang J, Kawazoe N, et al. 3D Culture of
Chondrocytes in Gelatin Hydrogels with Different Stiffness. Polymers. 2016;8(8):269.
236. Zhou Y, Liang K, Zhao S, Zhang C, Li J, Yang H, et al. Photopolymerized
maleilated chitosan/methacrylated silk fibroin micro/nanocomposite hydrogels as
potential scaffolds for cartilage tissue engineering. International Journal of Biological
Macromolecules. 2018;108:383-90.
237. Cho IS, Cho MO, Li Z, Nurunnabi M, Park SY, Kang S-W, et al. Synthesis
and characterization of a new photo-crosslinkable glycol chitosan thermogel for
biomedical applications. Carbohydrate Polymers. 2016;144:59-67.
195
238. Jukes JM, Aa LJvd, Hiemstra C, Veen Tv, Dijkstra PJ, Zhong Z, et al. A Newly
Developed Chemically Crosslinked Dextran–Poly(Ethylene Glycol) Hydrogel for
Cartilage Tissue Engineering. 2010;16(2):565-73.
239. Szafulera K, Wach RA, Olejnik AK, Rosiak JM, Ulański P. Radiation
synthesis of biocompatible hydrogels of dextran methacrylate. Radiation Physics and
Chemistry. 2018;142:115-20.
240. Chen G, Kawazoe N, Ito Y. Photo-Crosslinkable Hydrogels for Tissue
Engineering Applications. In: Ito Y, editor. Photochemistry for Biomedical
Applications: From Device Fabrication to Diagnosis and Therapy. Singapore:
Springer Singapore; 2018, 277-300.
241. Oliveira JT, Martins L, Picciochi R, Malafaya PB, Sousa RA, Neves NM, et
al. Gellan gum: a new biomaterial for cartilage tissue engineering applications. Journal
of biomedical materials research Part A. 2010;93(3):852-63.
242. Sun W, Xue B, Li Y, Qin M, Wu J, Lu K, et al. Polymer-Supramolecular
Polymer Double-Network Hydrogel. 2016;26(48):9044-52.
243. Seol YJ, Park JY, Jeong W, Kim TH, Kim SY, Cho DW. Development of
hybrid scaffolds using ceramic and hydrogel for articular cartilage tissue regeneration.
Journal of biomedical materials research Part A. 2015;103(4):1404-13.
244. Mintz BR, Cooper JA, Jr. Hybrid hyaluronic acid hydrogel/poly(varepsilon-
caprolactone) scaffold provides mechanically favorable platform for cartilage tissue
engineering studies. Journal of biomedical materials research Part A.
2014;102(9):2918-26.
245. Formica FA, Ozturk E, Hess SC, Stark WJ, Maniura-Weber K, Rottmar M, et
al. A Bioinspired Ultraporous Nanofiber-Hydrogel Mimic of the Cartilage
Extracellular Matrix. Adv Healthc Mater. 2016;5(24):3129-38.
246. Naseri N, Deepa B, Mathew AP, Oksman K, Girandon L. Nanocellulose-
Based Interpenetrating Polymer Network (IPN) Hydrogels for Cartilage Applications.
Biomacromolecules. 2016;17(11):3714-23.
247. Zhang X, Kim GJ, Kang MG, Lee JK, Seo JW, Do JT, et al. Marine
Biomaterial-Based Bioinks for Generating 3D Printed Tissue Constructs.
2018;16(12): E484.
248. Chimene D, Peak CW, Gentry JL, Carrow JK, Cross LM, Mondragon E, et al.
Nanoengineered ionic–covalent entanglement (NICE) bioinks for 3D bioprinting.
2018;10(12):9957-68.
196
249. Lorson T, Jaksch S, Lubtow MM, Jungst T, Groll Jr, Luhmann T, et al. A
thermogelling supramolecular hydrogel with sponge-like morphology as a
cytocompatible bioink. 2017;18(7):2161-71.
250. O’Connell CD, Di Bella C, Thompson F, Augustine C, Beirne S, Cornock R,
et al. Development of the Biopen: a handheld device for surgical printing of adipose
stem cells at a chondral wound site. Biofabrication. 2016;8(1):015019.
251. Onofrillo C, Duchi S, O’Connell CD, Blanchard R, O’Connor AJ, Scott M, et
al. Biofabrication of human articular cartilage: a path towards the development of a
clinical treatment. Biofabrication. 2018;10(4):045006.
252. Bidarra SJ, Barrias CC, Granja PL. Injectable alginate hydrogels for cell
delivery in tissue engineering. Acta Biomaterialia. 2014;10(4):1646-62.
253. Pan X, Tasdelen MA, Laun J, Junkers T, Yagci Y, Matyjaszewski K.
Photomediated controlled radical polymerization. Progress in Polymer Science.
2016;62:73-125.
254. Hennink WE, van Nostrum CF. Novel crosslinking methods to design
hydrogels. Advanced drug delivery reviews. 2002;54(1):13-36.
255. Rastogi RP, Richa, Kumar A, Tyagi MB, Sinha RP. Molecular Mechanisms of
Ultraviolet Radiation-Induced DNA Damage and Repair. Journal of Nucleic Acids.
2010;2010:592980.
256. Cadet J, Sage E, Douki T. Ultraviolet radiation-mediated damage to cellular
DNA. Mutation Research/Fundamental and Molecular Mechanisms of Mutagenesis.
2005;571(1):3-17.
257. Ravanat J-L, Douki T, Cadet J. Direct and indirect effects of UV radiation on
DNA and its components. Journal of Photochemistry and Photobiology B: Biology.
2001;63(1):88-102.
258. Wood JPM, Lascaratos G, Bron AJ, Osborne NN. The influence of visible light
exposure on cultured RGC-5 cells. Molecular vision. 2007;14:334-44.
259. Maverakis E, Miyamura Y, Bowen MP, Correa G, Ono Y, Goodarzi H. Light,
including ultraviolet. Journal of autoimmunity. 2010;34(3):J247-J57.
260. Tsihlis ND, Murar J, Kapadia MR, Ahanchi SS, Oustwani CS, Saavedra JE, et
al. Isopropylamine NONOate (IPA/NO) moderates neointimal hyperplasia following
vascular injury. Journal of vascular surgery. 2010;51(5):1248-59.
197
261. Roberts JJ, Bryant SJ. Comparison of photopolymerizable thiol-ene PEG and
acrylate-based PEG hydrogels for cartilage development. Biomaterials.
2013;34(38):9969-79.
262. Tanaka F, Edwards SF. Viscoelastic properties of physically crosslinked
networks: Part 1. Non-linear stationary viscoelasticity. Journal of Non-Newtonian
Fluid Mechanics. 1992;43(2):247-71.
263. Zhao L, Mitomo H, Yosh F. Synthesis of pH-Sensitive and Biodegradable CM-
Cellulose/Chitosan Polyampholytic Hydrogels with Electron Beam Irradiation.
2008;23(4):319-33.
264. Eslahi N, Abdorahim M, Simchi AJB. Smart polymeric hydrogels for cartilage
tissue engineering: a review on the chemistry and biological functions.
2016;17(11):3441-63.
265. Moncada-Saucedo NK, Marino-Martínez IA, Lara-Arias J, Romero-Díaz VJ,
Camacho A, et al. A Bioactive Cartilage Graft of IGF1-Transduced Adipose
Mesenchymal Stem Cells Embedded in an Alginate/Bovine Cartilage Matrix
Tridimensional Scaffold. Stem Cells International. 2019;2019:9792369.
266. Miyazaki T, Takeda Y, Akane S, Itou T, Hoshiko A, En KJP. Role of boric
acid for a poly (vinyl alcohol) film as a cross-linking agent: Melting behaviors of the
films with boric acid. 2010;51(23):5539-49.
267. Ullah F, Othman MBH, Javed F, Ahmad Z, Akil H, C E. Classification,
processing and application of hydrogels: A review. 2015;57:414-33.
268. Pereira RF, Bártolo PJJE. 3D photo-fabrication for tissue engineering and drug
delivery. 2015;1(1):090-112.
269. Jivan F, Fabela N, Davis Z, Alge DLJJoMCB. Orthogonal click reactions
enable the synthesis of ECM-mimetic PEG hydrogels without multi-arm precursors.
2018;6(30):4929-36.
270. Shih H, Lin C-CJB. Cross-linking and degradation of step-growth hydrogels
formed by thiol–ene photoclick chemistry. 2012;13(7):2003-12.
271. Yu I-M, Hughson FMJAroc, biology d. Tethering factors as organizers of
intracellular vesicular traffic. 2010;26:137-56.
272. Wang LS, Du C, Toh WS, Wan AC, Gao SJ, Kurisawa MJB. Modulation of
chondrocyte functions and stiffness-dependent cartilage repair using an injectable
enzymatically crosslinked hydrogel with tunable mechanical properties.
2014;35(7):2207-17.
198
273. Bian L, Hou C, Tous E, Rai R, Mauck RL, Burdick JAJB. The influence of
hyaluronic acid hydrogel crosslinking density and macromolecular diffusivity on
human MSC chondrogenesis and hypertrophy. 2013;34(2):413-21.
274. Chung C, Mesa J, Randolph MA, Yaremchuk M, Burdick JA. Influence of gel
properties on neocartilage formation by auricular chondrocytes photoencapsulated in
hyaluronic acid networks. Journal of biomedical materials research Part A.
2006;77(3):518-25.
275. Neumann AJ, Quinn T, Bryant SJ. Nondestructive evaluation of a new
hydrolytically degradable and photo-clickable PEG hydrogel for cartilage tissue
engineering. Acta Biomater. 2016;39:1-11.
276. Ingavle GC, Gehrke SH, Detamore MS. The bioactivity of agarose-PEGDA
interpenetrating network hydrogels with covalently immobilized RGD peptides and
physically entrapped aggrecan. Biomaterials. 2014;35(11):3558-70.
277. Skaalure SC, Dimson SO, Pennington AM, Bryant SJ. Semi-interpenetrating
networks of hyaluronic acid in degradable PEG hydrogels for cartilage tissue
engineering. Acta Biomater. 2014;10(8):3409-20.
278. Rodell CB, Dusaj NN, Highley CB, Burdick JA. Injectable and
Cytocompatible Tough Double-Network Hydrogels through Tandem Supramolecular
and Covalent Crosslinking. Advanced materials (Deerfield Beach, Fla).
2016;28(38):8419-24.
279. Jung H, Park JS, Yeom J, Selvapalam N, Park KM, Oh K, et al. 3D tissue
engineered supramolecular hydrogels for controlled chondrogenesis of human
mesenchymal stem cells. Biomacromolecules. 2014;15(3):707-14.
280. Wei K, Zhu M, Sun Y, Xu J, Feng Q, Lin S, et al. Robust Biopolymeric
Supramolecular “Host−Guest Macromer” Hydrogels Reinforced by in Situ Formed
Multivalent Nanoclusters for Cartilage Regeneration. Macromolecules.
2016;49(3):866-75.
281. Guo Y, Yuan T, Xiao Z, Tang P, Xiao Y, Fan Y, et al. Hydrogels of
collagen/chondroitin sulfate/hyaluronan interpenetrating polymer network for
cartilage tissue engineering. Journal of materials science Materials in medicine.
2012;23(9):2267-79.
282. Wang T, Lai JH, Yang F. Effects of Hydrogel Stiffness and Extracellular
Compositions on Modulating Cartilage Regeneration by Mixed Populations of Stem
Cells and Chondrocytes In Vivo. Tissue engineering Part A. 2016;22(23-24):1348-56.
199
283. Bryant SJ, Anseth KS. Hydrogel properties influence ECM production by
chondrocytes photoencapsulated in poly(ethylene glycol) hydrogels. Journal of
biomedical materials research. 2002;59(1):63-72.
284. Chaudhuri O, Gu L, Klumpers D, Darnell M, Bencherif SA, Weaver JC, et al.
Hydrogels with tunable stress relaxation regulate stem cell fate and activity. Nature
Materials 2016;15(3):326-34.
285. Darnell M, Young S, Gu L, Shah N, Lippens E, Weaver J, et al. Substrate
Stress-Relaxation Regulates Scaffold Remodeling and Bone Formation In Vivo.
Advanced healthcare materials. 2017;6(1),1601185.
286. Lee HP, Gu L, Mooney DJ, Levenston ME, Chaudhuri O. Mechanical
confinement regulates cartilage matrix formation by chondrocytes. Nat Mater.
2017;16(12):1243-51.
287. Richardson BM, Wilcox DG, Randolph MA, Anseth KS. Hydrazone covalent
adaptable networks modulate extracellular matrix deposition for cartilage tissue
engineering. Acta Biomater. 2019;83:71-82.
288. Neves SC, Pereira RF, Araújo M, Barrias CC. 4 Bioengineered peptide-
functionalized hydrogels for tissue regeneration and repair. Peptides and Proteins as
Biomaterials for Tissue Regeneration and Repair 2018, 101-25.
289. Pereira RF, Sousa A, Barrias CC, Bártolo PJ, Granja PL. A single-component
hydrogel bioink for bioprinting of bioengineered 3D constructs for dermal tissue
engineering. Materials Horizons. 2018;5(6):1100-11.
290. Lee HJ, Yu C, Chansakul T, Hwang NS, Varghese S, Yu SM, et al. Enhanced
chondrogenesis of mesenchymal stem cells in collagen mimetic peptide-mediated
microenvironment. Tissue engineering Part A. 2008;14(11):1843-51.
291. Salinas CN, Anseth KS. Decorin moieties tethered into PEG networks induce
chondrogenesis of human mesenchymal stem cells. Journal of biomedical materials
research Part A. 2009;90(2):456-64.
292. Connelly JT, Garcia AJ, Levenston ME. Inhibition of in vitro chondrogenesis
in RGD-modified three-dimensional alginate gels. Biomaterials. 2007;28(6):1071-83.
293. Villanueva I, Weigel CA, Bryant SJ. Cell-matrix interactions and dynamic
mechanical loading influence chondrocyte gene expression and bioactivity in PEG-
RGD hydrogels. Acta Biomater. 2009;5(8):2832-46.
200
294. Pereira RF, Barrias CC, Bartolo PJ, Granja PL. Cell-instructive pectin
hydrogels crosslinked via thiol-norbornene photo-click chemistry for skin tissue
engineering. Acta Biomateriala. 2018;66:282-93.
295. Parmar PA, Chow LW, St-Pierre JP, Horejs CM, Peng YY, Werkmeister JA,
et al. Collagen-mimetic peptide-modifiable hydrogels for articular cartilage
regeneration. Biomaterials. 2015;54:213-25.
296. Bonnans C, Chou J, Werb Z. Remodelling the extracellular matrix in
development and disease. Nature reviews Molecular cell biology. 2014;15(12):786-
801.
297. Schultz GS, Wysocki A. Interactions between extracellular matrix and growth
factors in wound healing. Wound repair and regeneration : official publication of the
Wound Healing Society [and] the European Tissue Repair Society. 2009;17(2):153-
62.
298. Sridhar BV, Doyle NR, Randolph MA, Anseth KS. Covalently tethered TGF‐
β1 with encapsulated chondrocytes in a PEG hydrogel system enhances extracellular
matrix production. Journal of biomedical materials research Part A.
2014;102(12):4464-72.
299. Feng Q, Lin S, Zhang K, Dong C, Wu T, Huang H, et al. Sulfated hyaluronic
acid hydrogels with retarded degradation and enhanced growth factor retention
promote hMSC chondrogenesis and articular cartilage integrity with reduced
hypertrophy. Acta Biomater. 2017;53:329-42.
300. Bian L, Zhai DY, Tous E, Rai R, Mauck RL, Burdick JA. Enhanced MSC
chondrogenesis following delivery of TGF-beta3 from alginate microspheres within
hyaluronic acid hydrogels in vitro and in vivo. Biomaterials. 2011;32(27):6425-34.
301. Sridhar BV, Brock JL, Silver JS, Leight JL, Randolph MA, Anseth KS.
Development of a cellularly degradable PEG hydrogel to promote articular cartilage
extracellular matrix deposition. Advanced healthcare materials. 2015;4(5):702-13.
302. Pereira RF, Bártolo PJ. 3D bioprinting of photocrosslinkable hydrogel
constructs. 2015;132(48).
303. Zhou D, Ito YJSCC. Visible light-curable polymers for biomedical
applications. 2014;57(4):510-21.
304. Vyas C, Pereira R, Huang B, Liu F, Wang W, Bartolo P. Engineering the
vasculature with additive manufacturing. Current Opinion in Biomedical Engineering.
2017;2:1-13.
201
305. Wang W, Caetano G, Ambler WS, Blaker JJ, Frade MA, Mandal P, et al.
Enhancing the Hydrophilicity and Cell Attachment of 3D Printed PCL/Graphene
Scaffolds for Bone Tissue Engineering. Materials (Basel, Switzerland).
2016;9(12):992-1002.
306. Nicodemus GD, Bryant SJ. Cell encapsulation in biodegradable hydrogels for
tissue engineering applications. Tissue engineering Part B, Reviews. 2008;14(2):149-
65.
307. You F, Eames BF, Chen X. Application of Extrusion-Based Hydrogel
Bioprinting for Cartilage Tissue Engineering. International journal of molecular
sciences. 2017;18(7),E1597.
308. Highley CB, Rodell CB, Burdick JA. Direct 3D Printing of Shear-Thinning
Hydrogels into Self-Healing Hydrogels. 2015;27(34):5075-9.
309. Pawar AA, Saada G, Cooperstein I, Larush L, Jackman JA, Tabaei SR, et al.
High-performance 3D printing of hydrogels by water-dispersible photoinitiator
nanoparticles. 2016;2(4):e1501381.
310. Banerjee A, Arha M, Choudhary S, Ashton RS, Bhatia SR, Schaffer DV, et al.
The influence of hydrogel modulus on the proliferation and differentiation of
encapsulated neural stem cells. 2009;30(27):4695-9.
311. Song S-J, Choi J, Park Y-D, Hong S, Lee JJ, Ahn CB, et al. Sodium Alginate
Hydrogel-Based Bioprinting Using a Novel Multinozzle Bioprinting System.
2011;35(11):1132-6.
312. Pereira R, Tojeira A, Vaz DC, Mendes A, Bártolo P. Preparation and
Characterization of Films Based on Alginate and Aloe Vera. International Journal of
Polymer Analysis and Characterization. 2011;16(7):449-64.
313. Pereira R, Carvalho A, Vaz DC, Gil MH, Mendes A, Bártolo P. Development
of novel alginate based hydrogel films for wound healing applications. International
Journal of Biological Macromolecules. 2013;52:221-30.
314. Pawar SN, Edgar KJ. Alginate derivatization: A review of chemistry,
properties and applications. Biomaterials. 2012;33(11):3279-305.
315. Hermansson E, Schuster E, Lindgren L, Altskär A, Ström A. Impact of solvent
quality on the network strength and structure of alginate gels. Carbohydrate Polymers.
2016;144:289-96.
202
316. Daemi H, Barikani M. Synthesis and characterization of calcium alginate
nanoparticles, sodium homopolymannuronate salt and its calcium nanoparticles.
Scientia Iranica. 2012;19(6):2023-8.
317. Ouwerx C, Velings N, Mestdagh MM, Axelos MAV. Physico-chemical
properties and rheology of alginate gel beads formed with various divalent cations.
Polymer Gels and Networks. 1998;6(5):393-408.
318. Stagnaro P, Schizzi I, Utzeri R, Marsano E, Castellano M. Alginate-
polymethacrylate hybrid hydrogels for potential osteochondral tissue regeneration.
Carbohydrate Polymers. 2018;185:56-62.
319. Yang X, Lu Z, Wu H, Li W, Zheng L, Zhao J. Collagen-alginate as bioink for
three-dimensional (3D) cell printing based cartilage tissue engineering. Materials
Science and Engineering: C. 2018;83:195-201.
320. Müller M, Öztürk E, Arlov Ø, Gatenholm P, Zenobi-Wong MJAoBE. Alginate
Sulfate–Nanocellulose Bioinks for Cartilage Bioprinting Applications.
2017;45(1):210-23.
321. Axpe E, Oyen MJIjoms. Applications of alginate-based bioinks in 3D
bioprinting. 2016;17(12):E1976.
322. Szekalska M, Puci, et al. Alginate: Current Use and Future Perspectives in
Pharmaceutical and Biomedical Applications. International Journal of Polymer
Science. 2016;2016: 7697031.
323. Augst AD, Kong HJ, Mooney DJ. Alginate Hydrogels as Biomaterials.
2006;6(8):623-33.
324. Spadari C, Lopes LB, Ishida K. Potential Use of Alginate-Based Carriers As
Antifungal Delivery System. Frontiers in microbiology. 2017;8:97.
325. Jeon O, Bouhadir KH, Mansour JM, Alsberg EJB. Photocrosslinked alginate
hydrogels with tunable biodegradation rates and mechanical properties.
2009;30(14):2724-34.
326. Benton JA, DeForest CA, Vivekanandan V, Anseth KS. Photocrosslinking of
gelatin macromers to synthesize porous hydrogels that promote valvular interstitial
cell function. Tissue engineering Part A. 2009;15(11):3221-30.
327. Sudhakar CK, Upadhyay N, Jain A, Verma A, Narayana Charyulu R, Jain S.
Chapter 5 - Hydrogels—Promising Candidates for Tissue Engineering. In: Thomas S,
Grohens Y, Ninan N, editors. Nanotechnology Applications for Tissue Engineering.
Oxford: William Andrew Publishing; 2015, 77-94.
203
328. Lee JH, Khang G, Lee JW, Lee HB. Interaction of Different Types of Cells on
Polymer Surfaces with Wettability Gradient. Journal of Colloid and Interface Science.
1998;205(2):323-30.
329. Smeriglio P, Lai JH, Yang F, Bhutani N. 3D Hydrogel Scaffolds for Articular
Chondrocyte Culture and Cartilage Generation. Journal of visualized experiments :
JoVE. 2015(104):53085.
330. Moral Çiğdem K, Doğan Ö, Sanin Faika D. Comparison of chemical
fractionation method and 1H-NMR spectroscopy in measuring the monomer block
distribution of algal alginates. Journal of Polymer Engineering2013, 2012-0066.
331. Smeds KA, Pfister-Serres A, Miki D, Dastgheib K, Inoue M, Hatchell DL, et
al. Photocrosslinkable polysaccharides for in situ hydrogel formation.
2001;55(2):254-5.
332. Lam C, Jefferis SA. Interpretation of viscometer test results for polymer
support fluids. Tunneling and Underground Construction2014, 439-49.
333. Bartolo P, Lenz EJCa. Computer simulation of stereolithographic curing
reactions: phenomenological versus mechanistic approaches. 2006;55(1):221-5.
334. Matias JM, Bartolo PJ, Pontes AV. Modeling and simulation of
photofabrication processes using unsaturated polyester resins. 2009;114(6):3673-85.
335. Buckwalter JA, Mankin HJ. Articular cartilage: degeneration and
osteoarthritis, repair, regeneration, and transplantation. Instr Course Lect.
1998;47:487-504.
336. Simon TM, Jackson DWJSm, review a. Articular cartilage: injury pathways
and treatment options. 2018;26(1):31-9.
337. Flik KR, Verma N, Cole BJ, Bach BR. Articular Cartilage. In: Williams RJ,
editor. Cartilage Repair Strategies. Totowa, NJ: Humana Press; 2007, 1-12.
338. Nukavarapu SP, Dorcemus DLJBa. Osteochondral tissue engineering: current
strategies and challenges. 2013;31(5):706-21.
339. Buckwalter JJCO, Research R. Articular cartilage injuries. 2002;402:21-37.
340. Swieszkowski W, Tuan BHS, Kurzydlowski KJ, Hutmacher DWJBe. Repair
and regeneration of osteochondral defects in the articular joints. 2007;24(5):489-95.
341. Redman S, Oldfield S, Archer CJECM. Current strategies for articular
cartilage repair. 2005;9(23-32):23-32.
204
342. Fragonas E, Valente M, Pozzi-Mucelli M, Toffanin R, Rizzo R, Silvestri F, et
al. Articular cartilage repair in rabbits by using suspensions of allogenic chondrocytes
in alginate. Biomaterials. 2000;21(8):795-801.
343. Jeon O, Bouhadir KH, Mansour JM, Alsberg E. Photocrosslinked alginate
hydrogels with tunable biodegradation rates and mechanical properties. Biomaterials.
2009;30(14):2724-34.
344. Smeds KA, Grinstaff MW. Photocrosslinkable polysaccharides for in situ
hydrogel formation. 2001;54(1):115-21.
345. Buckwalter JA, Mankin HJ. Articular cartilage: degeneration and
osteoarthritis, repair, regeneration, and transplantation. Instructional course lectures.
1998;47:487-504.
346. Vinatier C, Guicheux J. Cartilage tissue engineering: From biomaterials and
stem cells to osteoarthritis treatments. Annals of Physical and Rehabilitation
Medicine. 2016;59(3):139-44.
347. Brittberg M, Lindahl A, Nilsson A, Ohlsson C, Isaksson O, Peterson L.
Treatment of deep cartilage defects in the knee with autologous chondrocyte
transplantation. New england journal of medicine. 1994;331(14):889-95.
348. Krych A, Harnly H, Rodeo S, Williams III R. Activity levels are higher after
osteochondral autograft transfer mosaicplasty than after microfracture for articular
cartilage defects of the knee: a retrospective comparative study. Journal of Bone and
Joint Surgery. 2012;94(11):971-8.
349. Sessa A, Perdisa F, Di Martino A, Zaffagnini S, Filardo G. Cell-Free
Biomimetic Osteochondral Scaffold: Implantation Technique. JBJS Essential Surgical
Techniques. 2019;9(3):e27.
350. Horas U, Pelinkovic D, Herr G, Aigner T, Schnettler R. Autologous
chondrocyte implantation and osteochondral cylinder transplantation in cartilage
repair of the knee joint: a prospective, comparative trial. Journal of Bone and Joint
Surgery. 2003;85(2):185-92.
351. Andriolo L, Merli G, Filardo G, Marcacci M, Kon E. Failure of Autologous
Chondrocyte Implantation. Sports Medicine and Arthroscopy Review. 2017;25(1):10-
8.
352. Albrecht C, Reuter CA, Stelzeneder D, Zak L, Tichy B, Nurnberger S, et al.
Matrix Production Affects MRI Outcomes After Matrix-Associated Autologous
Chondrocyte Transplantation in the Knee. Am J Sports Med. 2017;45(10):2238-46.
205
353. Andriolo L, Reale D, Di Martino A, Zaffagnini S, Vannini F, Ferruzzi A, et al.
High Rate of Failure After Matrix-Assisted Autologous Chondrocyte Transplantation
in Osteoarthritic Knees at 15 Years of Follow-up. American Journal of Sports
Medicine. 2019:363546519855029.
354. Choi SM, Lee K, Ryu SB, Park YJ, Hwang YG, Baek D, et al. Enhanced
articular cartilage regeneration with SIRT1-activated MSCs using gelatin-based
hydrogel. Cell Death Dis. 2018;9(9):866-78.
355. Jo CH, Lee YG, Shin WH, Kim H, Chai JW, Jeong EC, et al. Intra-articular
injection of mesenchymal stem cells for the treatment of osteoarthritis of the knee: a
proof-of-concept clinical trial. Stem cells (Dayton, Ohio). 2014;32(5):1254-66.
356. Bashari M, Abdelhai MH, Abbas S, Eibaid A, Xu X, Jin ZJUs. Effect of
ultrasound and high hydrostatic pressure (US/HHP) on the degradation of dextran
catalyzed by dextranase. 2014;21(1):76-83.
357. Abbadessa A, Blokzijl MM, Mouser VHM, Marica P, Malda J, Hennink WE,
et al. Photo-Cross-Linked Laminarin-Based Hydrogels for Biomedical Applications.
Carbohydrate Polymers. 2016;11(5):1-15.
358. Zhai X, Ruan C, Ma Y, Cheng D, Wu M, Liu W, et al. 3D‐Bioprinted
Osteoblast‐Laden Nanocomposite Hydrogel Constructs with Induced
Microenvironments Promote Cell Viability, Differentiation, and Osteogenesis both In
Vitro and In Vivo. Advanced Science. 2018;5(3):1700550.
359. Nachlas AL, Li S, Jha R, Singh M, Xu C, Davis ME. Human iPSC-derived
mesenchymal stem cells matured into valve interstitial-like cells using PEGDA
hydrogels. Acta biomaterialia. 2018;71: 235-46.
360. Hao Y, Lin CC. Degradable thiol‐acrylate hydrogels as tunable matrices for
three‐dimensional hepatic culture. Journal of biomedical materials research Part A.
2014;102(11):3813-27.
361. Pepelanova I, Kruppa K, Scheper T, Lavrentieva A. Gelatin-Methacryloyl
(GelMA) hydrogels with defined degree of functionalization as a versatile toolkit for
3D cell culture and extrusion bioprinting. Bioengineering. 2018;5(3), E55.
362. Levett PA, Melchels FPW, Schrobback K, Hutmacher DW, Malda J, Klein TJ.
A biomimetic extracellular matrix for cartilage tissue engineering centered on
photocurable gelatin, hyaluronic acid and chondroitin sulfate. Acta Biomaterialia.
2014;10(1):214-23.
206
363. Lin H, Cheng AW, Alexander PG, Beck AM, Tuan RS. Cartilage Tissue
Engineering Application of Injectable Gelatin Hydrogel with In Situ Visible-Light-
Activated Gelation Capability in Both Air and Aqueous Solution. Tissue Engineering
Part A. 2014;20(17-18):2402-11.
364. Wei D, Xiao W, Sun J, Zhong M, Guo L, Fan H, et al. A biocompatible
hydrogel with improved stiffness and hydrophilicity for modular tissue engineering
assembly. Journal of Materials Chemistry B. 2015;3(14):2753-63.
365. Lien S-M, Li W-T, Huang T-JJMS, C E. Genipin-crosslinked gelatin scaffolds
for articular cartilage tissue engineering with a novel crosslinking method.
2008;28(1):36-43.
366. Van Den Bulcke aI, Bogdanov B, De Rooze N, Schacht EH, Cornelissen M,
Berghmans H. Structural and rheological properties of methacrylamide modified
gelatin hydrogels. Biomacromolecules. 2000;1(1):31-8.
367. Freitas Jr RA. Nanomedicine, Vol. IIA: Biocompatibility: Karger Publishers;
2003.
368. Becker WM, Kleinsmith LJ, Hardin J, Bertoni GP. The world of the cell:
Benjamin/Cummings Publishing Company; 2003.
369. Iwamoto M, Ohta Y, Larmour C, Enomoto-Iwamoto M. Toward regeneration
of articular cartilage. Birth Defects Res C Embryo Today. 2013;99(3):192-202.
370. Caldwell KL, Wang J. Cell-based articular cartilage repair: the link between
development and regeneration. Osteoarthritis and cartilage. 2015;23(3):351-62.
371. Huey DJ, Hu JC, Athanasiou KA. Unlike Bone, Cartilage Regeneration
Remains Elusive. Science. 2012;338(6109):917-21.
372. Armiento AR, Stoddart MJ, Alini M, Eglin D. Biomaterials for articular
cartilage tissue engineering: Learning from biology. Acta Biomater. 2018;65:1-20.
373. Makris EA, Gomoll AH, Malizos KN, Hu JC, Athanasiou KA. Repair and
tissue engineering techniques for articular cartilage. Nature Reviews Rheumatology.
2014;11:21.
374. Zhang Y, Yu J, Ren K, Zuo J, Ding J, Chen X. Thermosensitive Hydrogels as
Scaffolds for Cartilage Tissue Engineering. Biomacromolecules. 2019;20(4):1478-92.
375. Xia H, Zhao D, Zhu H, Hua Y, Xiao K, Xu Y, et al. Lyophilized Scaffolds
Fabricated from 3D-Printed Photocurable Natural Hydrogel for Cartilage
Regeneration. ACS Applied Materials & Interfaces. 2018;10(37):31704-15.
207
376. Chai Q, Jiao Y, Yu X. Hydrogels for Biomedical Applications: Their
Characteristics and the Mechanisms behind Them. Gels. 2017;3(1):6-20.
377. Sun W, Xue B, Li Y, Qin M, Wu J, Lu K, et al. Polymer‐Supramolecular
Polymer Double‐Network Hydrogel. Advanced Functional Materials.
2016;26(48):9044-52.
378. Feksa LR, Troian EA, Muller CD, Viegas F, Machado AB, Rech VC.
Hydrogels for biomedical applications. Nanostructures for the Engineering of Cells,
Tissues and Organs: Elsevier; 2018. p. 403-38.
379. Cheng A, Schwartz Z, Kahn A, Li X, Shao Z, Sun M, et al. Advances in Porous
Scaffold Design for Bone and Cartilage Tissue Engineering and Regeneration. Tissue
Eng Part B Rev. 2019;25(1):14-29.
380. Tormos C, Madihally S. Chitosan for cardiac tissue engineering and
regeneration. Chitosan Based Biomaterials Volume 2: Elsevier; 2017. p. 115-43.
381. Visser J, Melchels FPW, Jeon JE, van Bussel EM, Kimpton LS, Byrne HM, et
al. Reinforcement of hydrogels using three-dimensionally printed microfibres. Nature
Communications. 2015;6:6933.
382. Zhang X, Zhang W, Yang M. Application of Hydrogels in Cartilage Tissue
Engineering. Curr Stem Cell Res Ther. 2018;13(7):497-516.
383. Li J, Chen G, Xu X, Abdou P, Jiang Q, Shi D, et al. Advances of injectable
hydrogel-based scaffolds for cartilage regeneration. Regen Biomater. 2019;6(3):129-
40.
384. Chuang EY, Chiang CW, Wong PC, Chen CH. Hydrogels for the Application
of Articular Cartilage Tissue Engineering: A Review of Hydrogels. Advances in
Materials Science and Engineering. 2018;2018:1-13.
385. Eslahi N, Abdorahim M, Simchi A. Smart Polymeric Hydrogels for Cartilage
Tissue Engineering: A Review on the Chemistry and Biological Functions.
Biomacromolecules. 2016;17(11):3441-63.
386. Sharma B, Fermanian S, Gibson M, Unterman S, Herzka DA, Cascio B, et al.
Human cartilage repair with a photoreactive adhesive-hydrogel composite. Sci Transl
Med. 2013;5(167):167ra6.
387. El Sayed K, Marzahn U, John T, Hoyer M, Zreiqat H, Witthuhn A, et al. PGA-
associated heterotopic chondrocyte cocultures: implications of nasoseptal and
auricular chondrocytes in articular cartilage repair. J Tissue Eng Regen Med.
2013;7(1):61-72.
208
388. Hung KC, Tseng CS, Hsu SH. Synthesis and 3D printing of biodegradable
polyurethane elastomer by a water-based process for cartilage tissue engineering
applications. Advanced Healthcare Materials. 2014;3(10):1578-87.
389. Yan S, Wang T, Feng L, Zhu J, Zhang K, Chen X, et al. Injectable in situ self-
cross-linking hydrogels based on poly(L-glutamic acid) and alginate for cartilage
tissue engineering. Biomacromolecules. 2014;15(12):4495-508.
390. Malafaya PB, Silva GA, Reis RL. Natural-origin polymers as carriers and
scaffolds for biomolecules and cell delivery in tissue engineering applications.
Advanced Drug Delivery Reviews. 2007;59(4-5):207-33.
391. Li L, Yu F, Zheng L, Wang R, Yan W, Wang Z, et al. Natural hydrogels for
cartilage regeneration: Modification, preparation and application. Journal of
orthopaedic translation. 2019;17:26-41.
392. Jabbari E. Challenges for Natural Hydrogels in Tissue Engineering. Gels.
2019;5(2):30.
393. Puppi D, Chiellini F, Piras A, Chiellini E. Polymeric materials for bone and
cartilage repair. Progress in polymer Science. 2010;35(4):403-40.
394. Klontzas ME, Drissi H, Mantalaris A. The Use of Alginate Hydrogels for the
Culture of Mesenchymal Stem Cells (MSCs): In Vitro and In Vivo Paradigms.
Alginates: IntechOpen; 2019.
395. Ruvinov E, Re'em TT, Witte F, Cohen S. Articular cartilage regeneration using
acellular bioactive affinity-binding alginate hydrogel: A 6-month study in a mini-pig
model of osteochondral defects. Journal of orthopaedic translation. 2019;16:40-52.
396. Sun J, Tan H. Alginate-Based Biomaterials for Regenerative Medicine
Applications. Materials (Basel). 2013;6(4):1285-309.
397. Singh YP, Moses JC, Bhardwaj N, Mandal BB. Injectable hydrogels: a new
paradigm for osteochondral tissue engineering. Journal of Materials Chemistry B.
2018;6(35):5499-529.
398. Jaipan P, Nguyen A, Narayan RJ. Gelatin-based hydrogels for biomedical
applications. MRS Communications. 2017;7(3):416-26.
399. Zhang Z, Ortiz O, Goyal R, Kohn J. Biodegradable Polymers. In: Lanza R,
Langer R, Vacanti J, editors. Principles of Tissue Engineering. Boston: Academic
Press; 2014, 441-73.
209
400. Li X, Zhang J, Kawazoe N, Chen G. Fabrication of Highly Crosslinked Gelatin
Hydrogel and Its Influence on Chondrocyte Proliferation and Phenotype. Polymers
(Basel). 2017;9(8):309-22.
401. Van Vlierberghe S, Graulus GJ, Keshari Samal S, Van Nieuwenhove I,
Dubruel P. Porous hydrogel biomedical foam scaffolds for tissue repair. In: Netti PA,
editor. Biomedical Foams for Tissue Engineering Applications: Woodhead
Publishing; 2014, 335-90.
402. Gentile P, Ghione C, Ferreira AM, Crawford A, Hatton PV. Alginate-based
hydrogels functionalised at the nanoscale using layer-by-layer assembly for potential
cartilage repair. Biomater Sci. 2017;5(9):1922-31.
403. Donaldson AR, Tanase CE, Awuah D, Vasanthi Bathrinarayanan P, Hall L,
Nikkhah M, et al. Photocrosslinkable Gelatin Hydrogels Modulate the Production of
the Major Pro-inflammatory Cytokine, TNF-alpha, by Human Mononuclear Cells.
Front Bioeng Biotechnol. 2018;6(116):116-27.
404. H. H M, Cooper G, Bartolo PJDS. Development and Characterisation of a
Photocurable Alginate Bioink for 3D Bioprinting. International Journal of Bioprinting.
2019;5(2):12-26.
405. Wong DY, Ranganath T, Kasko AM. Low-Dose, Long-Wave UV Light Does
Not Affect Gene Expression of Human Mesenchymal Stem Cells. PLoS One.
2015;10(9):e0139307.
406. Haeri M, Haeri M. ImageJ plugin for analysis of porous scaffolds used in tissue
engineering. Journal of Open Research Software. 2015;3(1), e1.
407. Schindelin J, Arganda-Carreras I, Frise E, Kaynig V, Longair M, Pietzsch T,
et al. Fiji: an open-source platform for biological-image analysis. Nat Methods.
2012;9(7):676-82.
408. Lohmander S. Proteoglycans of joint cartilage: Structure, function, turnover
and role as markers of joint disease. Baillière's Clinical Rheumatology. 1988;2(1):37-
62.
409. Kiani C, Chen L, Wu YJ, Yee AJ, Yang BB. Structure and function of
aggrecan. Cell research. 2002;12(1):19-32.
410. Lepowsky E, Muradoglu M, Tasoglu S. Towards preserving post-printing cell
viability and improving the resolution: Past, present, and future of 3D bioprinting
theory. Bioprinting. 2018;11:e00034.
210
411. Cacopardo L, Guazzelli N, Nossa R, Mattei G, Ahluwalia A. Engineering
hydrogel viscoelasticity. J Mech Behav Biomed Mater. 2019;89:162-7.
412. Roy N, Saha N, Kitano T, Saha P, editors. Importance of viscoelastic property
measurement of a new hydrogel for health care. AIP Conference Proceedings; 2009:
AIP.
413. Cuomo F, Cofelice M, Lopez F. Rheological Characterization of Hydrogels
from Alginate-Based Nanodispersion. Polymers (Basel). 2019;11(2):259-70.
414. Lien SM, Ko LY, Huang TJ. Effect of pore size on ECM secretion and cell
growth in gelatin scaffold for articular cartilage tissue engineering. Acta Biomater.
2009;5(2):670-9.
415. Aigner J, Tegeler J, Hutzler P, Campoccia D, Pavesio A, Hammer C, et al.
Cartilage tissue engineering with novel nonwoven structured biomaterial based on
hyaluronic acid benzyl ester. J Biomed Mater Res. 1998;42(2):172-81.
416. Tondera C, Hauser S, Krüger-Genge A, Jung F, Neffe AT, Lendlein A, et al.
Gelatin-based Hydrogel Degradation and Tissue Interaction in vivo: Insights from
Multimodal Preclinical Imaging in Immunocompetent Nude Mice. Theranostics.
2016;6(12):2114-28.
417. Yan X, Yang J, Chen F, Zhu L, Tang Z, Qin G, et al. Mechanical properties of
gelatin/polyacrylamide/graphene oxide nanocomposite double-network hydrogels.
Composites Science and Technology. 2018;163:81-8.
418. Bian L, Guvendiren M, Mauck RL, Burdick JA. Hydrogels that mimic
developmentally relevant matrix and N-cadherin interactions enhance MSC
chondrogenesis. Proceedings of the National Academy of Sciences.
2013;110(25):10117-22.
419. Assmann A, Vegh A, Ghasemi-Rad M, Bagherifard S, Cheng G, Sani ES, et
al. A highly adhesive and naturally derived sealant. Biomaterials. 2017;140:115-27.
420. Brown GCJ, Lim KS, Farrugia BL, Hooper GJ, Woodfield TBF. Covalent
Incorporation of Heparin Improves Chondrogenesis in Photocurable Gelatin-
Methacryloyl Hydrogels. Macromolecular bioscience. 2017;17(12), 1700158.
421. Alsberg E, Jeon O, Kim T. Hydrogels with dynamically adjustable mechanical
properties. 2019; Patent No. US20190054207.
422. Lee KY, Mooney DJ. Alginate: properties and biomedical applications. Prog
Polym Sci. 2012;37(1):106-26.
211
423. Bidarra SJ, Barrias CC. 3D Culture of Mesenchymal Stem Cells in Alginate
Hydrogels. Methods in molecular biology (Clifton, NJ). 2019;2002:165-80.
424. Li X, Chen S, Li J, Wang X, Zhang J, Kawazoe N, et al. 3D Culture of
Chondrocytes in Gelatin Hydrogels with Different Stiffness. Polymers (Basel).
2016;8(8):269-84.
425. Caron MM, Emans PJ, Coolsen MM, Voss L, Surtel DA, Cremers A, et al.
Redifferentiation of dedifferentiated human articular chondrocytes: comparison of 2D
and 3D cultures. Osteoarthritis and cartilage. 2012;20(10):1170-8.
426. Ma H, Feng C, Chang J, Wu C. 3D-printed bioceramic scaffolds: From bone
tissue engineering to tumor therapy. Acta biomaterialia. 2018;79:37-59.
427. Wu Q, Debnath D. Interaction of Graphene and Polycaprolactone at Atomic
Level. 2019.
428. Pereira RF, Sousa A, Barrias CC, Bayat A, Granja PL, Bártolo PJ. Advances
in bioprinted cell-laden hydrogels for skin tissue engineering. Biomanufacturing
Reviews. 2017;2(1):1-26.
429. Melchels FP, Domingos MA, Klein TJ, Malda J, Bartolo PJ, Hutmacher DW.
Additive manufacturing of tissues and organs. Progress in Polymer Science.
2012;37(8):1079-104.
430. Rahman S, Carter P, Bhattarai N. Aloe vera for tissue engineering applications.
Journal of functional biomaterials. 2017;8(1):6-25.
431. Maldonado MA, Bonham AJ. Conductive Gel Polymers as an Extracellular
Matrix Mimic and Cell Vehicle for Cardiac Tissue Engineering. The FASEB Journal.
2017;31(1_supplement): 925.1-925.1.
432. Black CR, Goriainov V, Gibbs D, Kanczler J, Tare RS, Oreffo RO. Bone tissue
engineering. Current molecular biology reports. 2015;1(3):132-40.
433. Asghari F, Samiei M, Adibkia K, Akbarzadeh A, Davaran S. Biodegradable
and biocompatible polymers for tissue engineering application: a review. Artificial
cells, nanomedicine, and biotechnology. 2017;45(2):185-92.
434. Trombetta R, Inzana JA, Schwarz EM, Kates SL, Awad HA. 3D printing of
calcium phosphate ceramics for bone tissue engineering and drug delivery. Annals of
biomedical engineering. 2017;45(1):23-44.
435. Vacanti JP, Langer R. Tissue engineering: the design and fabrication of living
replacement devices for surgical reconstruction and transplantation. The lancet.
1999;354:S32-S4.
212
436. Mohanty AK, Misra Ma, Hinrichsen G. Biofibres, biodegradable polymers and
biocomposites: An overview. Macromolecular materials and Engineering.
2000;276(1):1-24.
437. Kumar A, Mandal S, Barui S, Vasireddi R, Gbureck U, Gelinsky M, et al. Low
temperature additive manufacturing of three dimensional scaffolds for bone-tissue
engineering applications: Processing related challenges and property assessment.
Materials Science and Engineering: R: Reports. 2016;103:1-39.
438. Forrestal DP, Klein TJ, Woodruff MA. Challenges in engineering large
customized bone constructs. Biotechnology and bioengineering. 2017;114(6):1129-
39.
439. Bártolo P, Chua C, Almeida H, Chou S, Lim A. Biomanufacturing for tissue
engineering: present and future trends. Virtual and Physical Prototyping.
2009;4(4):203-16.
440. Bártolo PJ, Domingos M, Patrício T, Cometa S, Mironov V. Biofabrication
strategies for tissue engineering. Advances on Modeling in Tissue Engineering:
Springer; 2011, 137-76.
441. Bartolo P, Kruth J-P, Silva J, Levy G, Malshe A, Rajurkar K, et al. Biomedical
production of implants by additive electro-chemical and physical processes. CIRP
Annals-Manufacturing Technology. 2012;61(2):635-55.
442. Rutz AL, Hyland KE, Jakus AE, Burghardt WR, Shah RN. A multimaterial
bioink method for 3D printing tunable, cell‐compatible hydrogels. Advanced
Materials. 2015;27(9):1607-14.
443. Jakus AE, Shah RN. Multi and mixed 3 D‐printing of graphene‐hydroxyapatite
hybrid materials for complex tissue engineering. Journal of Biomedical Materials
Research Part A. 2017;105(1):274-83.
444. Hoque ME, Chuan YL, Pashby I. Extrusion based rapid prototyping technique:
an advanced platform for tissue engineering scaffold fabrication. Biopolymers.
2012;97(2):83-93.
445. Bellini A. Fused deposition of ceramics: a comprehensive experimental,
analytical and computational study of material behavior, fabrication process and
equipment design. PhD thesis, Drexel University, 2002.
446. Almeida H, Bartolo P, Mota C, Mateus A, Ferreira N, Domingos M. Processo
e equipamento de fabrico rápido por bioextrusão. Portuguese Patent Application.
2010;104247.
213
447. Zhang LG, Fisher JP, Leong K. 3D bioprinting and nanotechnology in tissue
engineering and regenerative medicine: Academic Press; 2015.
448. Giannitelli S, Mozetic P, Trombetta M, Rainer A. Combined additive
manufacturing approaches in tissue engineering. Acta biomaterialia. 2015;24:1-11.
449. Sobral JM, Caridade SG, Sousa RA, Mano JF, Reis RL. Three-dimensional
plotted scaffolds with controlled pore size gradients: effect of scaffold geometry on
mechanical performance and cell seeding efficiency. Acta biomaterialia.
2011;7(3):1009-18.
450. Oh SH, Lee JH. Hydrophilization of synthetic biodegradable polymer
scaffolds for improved cell/tissue compatibility. Biomedical materials.
2013;8(1):014101.
451. Yang J, Wan Y, Yang J, Bei J, Wang S. Plasma‐treated, collagen‐anchored
polylactone: Its cell affinity evaluation under shear or shear‐free conditions. Journal
of Biomedical Materials Research Part A: An Official Journal of The Society for
Biomaterials, The Japanese Society for Biomaterials, and The Australian Society for
Biomaterials and the Korean Society for Biomaterials. 2003;67(4):1139-47.
452. Ozbolat IT, Chen H, Yu Y. Development of ‘Multi-arm Bioprinter’for hybrid
biofabrication of tissue engineering constructs. Robotics and Computer-Integrated
Manufacturing. 2014;30(3):295-304.
453. Intranuovo F, Gristina R, Brun F, Mohammadi S, Ceccone G, Sardella E, et al.
Plasma Modification of PCL Porous Scaffolds Fabricated by Solvent‐
Casting/Particulate‐Leaching for Tissue Engineering. Plasma Processes and Polymers.
2014;11(2):184-95.
454. Intranuovo F, Gristina R, Fracassi L, Lacitignola L, Crovace A, Favia P.
Plasma processing of scaffolds for tissue engineering and regenerative medicine.
Plasma Chemistry and Plasma Processing. 2016;36(1):269-80.
455. Jeon O, Bouhadir KH, Mansour JM, Alsberg E. Photocrosslinked alginate
hydrogels with tunable biodegradation rates and mechanical properties. Biomaterials.
2009;30(14):2724-34.
456. Liu F, Hinduja S, Bartolo P. User interface tool for a novel plasma-assisted
bio-additive extrusion system. Rapid prototyping. 2018:24(2);368–378.
457. Park K, Ju YM, Son JS, Ahn K-D, Han DK. Surface modification of
biodegradable electrospun nanofiber scaffolds and their interaction with fibroblasts.
Journal of Biomaterials Science, Polymer Edition. 2007;18(4):369-82.
214
458. Thakur S, Neogi S. Tailoring the Adhesion of Polymers using Plasma for
Biomedical Applications: A Critical Review. Reviews of Adhesion and Adhesives.
2015;3(1):53-97.
459. Gross M, Zhao X, Mascarenhas V, Wen Z. Effects of the surface physico-
chemical properties and the surface textures on the initial colonization and the attached
growth in algal biofilm. Biotechnology for biofuels. 2016;9(1):38-51.
460. Hashimoto M, Hossain S, Masumura S. Effect of aging on plasma membrane
fluidity of rat aortic endothelial cells. Experimental gerontology. 1999;34(5):687-98.
461. Wavhal DS, Fisher ER. Hydrophilic modification of polyethersulfone
membranes by low temperature plasma-induced graft polymerization. Journal of
Membrane Science. 2002;209(1):255-69.
462. Pappa AM, Karagkiozaki V, Krol S, Kassavetis S, Konstantinou D, Pitsalidis
C, et al. Oxygen-plasma-modified biomimetic nanofibrous scaffolds for enhanced
compatibility of cardiovascular implants. Beilstein journal of nanotechnology.
2015;6:254-62.
463. Sousa I, Mendes A, Pereira RF, Bártolo PJ. Collagen surface modified poly (ε-
caprolactone) scaffolds with improved hydrophilicity and cell adhesion properties.
Materials Letters. 2014;134:263-7.