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� Review of literature
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Chapter 2 Review of literature
2.1 Historical perspectives of enzymes
Enzymes occur in every living cell, hence in all microorganisms. Enzymes are biocatalysts
produced by living cells to bring about specific biochemical reactions generally forming
parts of the metabolic processes of the cells. Enzymes are highly specific in their action on
substrates and often many different enzymes are required to bring concerted action, the
sequence of metabolic reactions performed by the living cell. Almost all enzymes which
have been purified are protein in nature, and may or may not possess a non protein
prosthetic group for their biological activity. The practical application and industrial use of
enzymes to accomplish certain reactions apart from the cell, dates back many centuries and
practiced long before the nature or function of enzymes was understood. Use of barley
malt for starch conversion in brewing and treatment of hides in leather making are
examples of ancient use of enzymes. It was not until nearly the turn of this century that the
causative agents or enzymes responsible for bringing about such biochemical reactions
became known. Then crude preparations of enzymes from certain animal tissues such as
pancreas and stomach mucosa, or from plant tissues such as papaya fruit, were prepared
which found technical applications in the textile, leather, brewing, and other industries.
Once the favorable results of employing such enzyme preparations were established, a
search began for better properties (stability and activity against alkaline, acidic, high
temperature, metal ions, surfactants, protease resistant, etc), less expensive and more
readily available sources of such enzymes. It was found that certain microorganisms
produce enzymes similar in action to the amylases of malt and pancreas, or to the proteases
of the pancreas and papaya fruit. This led to the development of processes for producing
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such microbial enzymes on a commercial scale. Great diversity exists in microbial enzyme
production, each single strain of a organism produces a large number of enzymes such as
hydrolases, oxido/reducatases, transferases, isomerases, lyases and ligases, which are
metabolic in nature. But the absolute and relative amounts of the various individual
enzymes produced will vary depending on cellular need and it differs markedly between
species and even between strains of the same species. Hence, it is customary to select
microbial strains for commercial production of specific enzymes that have the capacity for
producing highest amounts of the particular enzymes with properties desired.
The roots of modem enzymology may be traced back to the last century when scientists
such as Payen and Pesoz, showed that an alcohol precipitate of malt extract contained a
thermolabile substance which converted starch into fermentable sugars. The enzyme
responsible was proved to be diastase because of its ability to yield soluble dextrins from
insoluble starch granules. The existence of several additional enzymes including pepsin,
polyphenol oxidase, peroxidase and invertase was recognized by the mid-nineteenth
century. The first enzyme preparation to be patented for industrial use was termed Taka-
Diastase, an amylolytic preparation produced by A. oryzae when grown on rice. The patent
was granted to Dr. Takamine, a Japanese immigrant to the U.S in 1884 (Miles Inc. 1988).
Microbial biotechnology of enzymes production has substantially made an impact on
healthcare, production and processing of food, basic molecular studies, genetic
engineering, agriculture and forestry, environmental protection, and biotransformation of
chemical compounds. Among the major new technologies that have appeared since 1970s,
microorganisms for biotechnological enzymes production perhaps attracted the most
attention. Microbes proved capable of generating enormous wealth and influencing every
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significant sector of the economy. In a conservative estimate, microbial enzymes represent
almost 90% of the total market. Industrial enzymes are currently manufactured by three
major suppliers, Novozymes A/S (headquartered in Denmark), Genencor International Inc.
(headquartered in the US), recently acquired by Danisco A/S (headquartered in Denmark)
and DSM N.V. (headquartered in the Netherlands). Industrial uses of enzymes have
increased greatly during the past few years. Prospects are excellent for continuing
increased usage of presently available enzymes in different applications.
Enzymes have several distinct advantages for use in industrial processes:
1. They are of natural origin and are nontoxic.
2. They have great specificity of action; hence can bring about reactions not otherwise
easily carried out.
3. They work best under mild conditions of moderate temperature and near neutral pH,
thus not requiring drastic conditions of high temperature, high pressure, high
acidity/alkaline, which necessitate special expensive equipment.
4. They act rapidly at relatively low concentrations, and the rate of reaction can be
readily controlled by adjusting temperature, pH, and amount of enzyme employed.
5. They are easily inactivated when reaction completed as far as desired.
Because of these inherent advantages, many industries are keenly interested in
adapting enzymatic methods to the requirements of their processes. Examples of some
applications under intensive investigation of different sectors include biofuel, food
processing, textile, leather, pulp and paper, fruit juice and beverages etc,. Nowadays
advances in extremophilic microbiology, isolation, identification and industrial
exploitation of extremophiles i.e. microbes adapted to exist and grow at extreme
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environments, are getting considerable attention. Eventhough such extremophiles are
difficult to grow under laboratory conditions, their genes can be cloned into suitable
mesophilic hosts as illustrated by the cloning of thermophilic enzyme genes from archaea
and bacteria, and psychrophilic enzyme genes into mesophilic expression host systems
(Feller et al. 1998; Bertoldo and Antranikian 2002; Viikari 2007). In fact, the advances in
molecular genetics and genetic engineering in the last few decades have made possible to
clone and express virtually any gene in a suitable microbial host, so that now enzymes
from other microorganisms and also from higher organisms can be produced in convenient
representative microbial hosts like bacteria (Escherichia coli), yeasts (Pichia pastorius)
and fungi (A.niger) (Glick and Pasternak 2003). This fact has contributed significantly to
limitless application of enzymes that can be produced by microbial fermentation and also
to increase the productivity of the fermentation and the quality of the enzyme product. It
was estimated that about 50% of the industrial enzymes (on a mass basis) were produced
from genetically engineered organisms (Hodgson 1994). This proportion might have
increased significantly in the last decade because of the advances in recombinant DNA
technology and protein engineering and also because of the increasing production of
speciality enzymes for the pharmaceutical and fine-chemicals industries (Dannert and
Arnold 1999; Schulein 2000; McCoy 2001; Rasor and Voss 2001; Thomas et al. 2002).
2.2 Cellulose source materials and their derivatives
Industrial sustainability aims to achieve sustainable production and processing within the
context of ecological and social sustainability (Miyamoto 1997). Compared to
conventional production, sustainable processes and production systems should be more
profitable because they require less energy, result in less emissions of greenhouse gases
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and other pollutants, enable greater and more efficient use of renewable resources and to
lessen dependence on nonrenewable resources. Lignocellulosic biomass is the major
sustainable resource, comprising around half of the plant matter produced by
photosynthesis and representing the most abundant renewable organic matter.
Lignocellulosic residues from wood, grass, agricultural and forestry wastes and municipal
solid wastes are particularly abundant in nature and have a potential for bioconversion and
the production on global scale of these sources are given in table 2.1. They constitute a
renewable resource from which many useful biological and chemical products can be
derived (Zosel 1994; Berkel 2000; Gavrilescu 2004; Gavrilescu and Nicu 2004). Industry
is truly sustainable only when it is economically viable, environmentally compatible, and
socially responsible (OECD 1998; UNEP 1999). Lignocellulosic biomass consists of three
types of polymers, cellulose, hemicellulose and lignin that are strongly intermeshed and
chemically bonded by non-covalent forces and by covalent cross linkages. The major
component is cellulose, followed by hemicellulose and lignin. The composition and
proportions of these compounds vary between plants and chemical composition of some of
lignocellulosic residues are given in table 2.2 (McKendry 2002; Malherbe and Cloete
2002; John et al. 2006, Prassad et al. 2007; Carmen 2009). Only a small amount of the
cellulose, hemicellulose and lignin produced as by-products in agriculture or forestry is
used, the rest being considered waste.
Many microorganisms are capable of degrading and utilizing cellulose and
hemicelluloses as carbon and energy sources. However, a much smaller group of
filamentous fungi has evolved with the ability to break down lignin, the most recalcitrant
component of plant cell walls. These are known as white-rot fungi, which possess the
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unique ability of efficiently degrading lignin to CO2. Accumulation of lignocellulose in
large quantities in places where agricultural residues present a disposal problem results not
only in deterioration of the environment but also in loss of potentially valuable material
that can be used in paper manufacture, biomass fuel production, composting, human and
animal feed among others (Pandey et al. 2000).
Table 2.1 Lignocellulosic residues generated from different agricultural sources
Source: Carmen 2009
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Table 2.2 Composition of some lignocellulosic materials
Lignocellulosic
residues
Lignin (%) Hemicellulose
(%)
Cellulose (%) Ash (%)
Hardwood stems 18–25 24–40 40–55 NA
Softwood stems 25–35 25–35 45–50 NA
Nut shells 30–40 25–30 25–30 NA
Corn cobs 15 35 45 1.36
Paper 0–15 0 85–99 1.1–3.9
Rice straw 18 24 32.1 NA
Cotton seed hairs 0 5–20 80–95 NA
Newspaper 18–30 25–40 40–55 8.8–1.8
Waste paper from
chemical pulps 5–10 10–20 60–70 NA
Switch grass 12.0 31.4 45 NA
Grasses (average
values for grasses) 10–30 25–50 25–40 1.5
Sugarcane bagasse 19–24 27–32 32–44 4.5–9
Wheat straw 16–21 26–32 29–35 NA
Barley straw 14–15 24–29 31–34 5–7
Oat straw 16–19 27–38 31–37 6–8
Rye straw 16–19 27–30 33–35 2–5
Bamboo 21–31 15–26 26–43 1.7–5
Bast fiber Kenaf 15–19 22–23 31–39 2–5
Bast fiber Jute 21–26 18–21 45–53 0.5–2
Leaf Fiber Abaca
(Manila) 8.8 17.3 60.8 1.1
Leaf Fiber Sisal
(agave) 7–9 21–24 43–56 0.6–1.1
Leaf Fiber Henequen 13.1 4–8 77.6 0.6–1
Banana waste 14 14.8 13.2 11.4
NA = Not available. Source: Carmen 2009
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2.3 Cellulose chemistry
Cellulose is the end product of photosynthesis in terrestrial environments, and the most
abundant renewable bioresource produced in the biosphere (~100 billion dry tonns/year)
(Jarvis 2003; Zhang and Lynd 2004). Cellulose is an organic compound with the formula
(C6H10O5)n, a polysaccharide consisting of a linear chain of several hundred to over ten
thousand β(1→4) linked D-glucose units. Payen (1795 - 1871) was a French chemist
known for discovering the carbohydrate cellulose. Although it took many decades after the
identification of cellulose, it was later shown to be a long chain polymer with repeating
units of D-glucose, a simple sugar. In the cellulose chain, the glucose units are in 6-
membered rings, called pyranoses. They are joined by single oxygen atoms (acetal
linkages) between the C-1 of one pyranose ring and the C-4 of the next ring. Since a
molecule of water is lost when an alcohol and a hemiacetal react to form an acetal, the
glucose units in the cellulose polymer are referred to as anhydroglucose units (Fig. 2.1 A &
B).
2.4 Enzymatic hydrolysis of cellulose
The physical heterogeneity of cellulosic substrates together with the complexity of
cellulase system produced by different microorganisms have led to the development of
several assay procedures for the measurement of cellulase activities. All existing
cellulolytic enzymes activity assays can be divided into three types: (1) the accumulation
of products after hydrolysis, (2) the reduction in substrate quantity, and (3) the change in
the physical properties of substrates. The considerable difference in the nature of substrates
used, variation in assay procedures adopted for measuring different cellulase components,
and the synergistic action of cellulase components have made the comparison of results
among laboratories difficult. Therefore, in 1984, the IUPAC
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Fig. 2.1 A. Schematic structures of cellulose chains. B. The structure of cellulose
showing the chains held together by hydrogen bonds.
Sources of links A. http://www.doitpoms.ac.uk/tlplib/wood/figures/cellulose.png
B. http://chempolymerproject.wikispaces.com/Cellulose-D-TPNR
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Commission on Biotechnology published standard assay procedures for measuring
cellulase activities (Ghosh 1984). Some of these recommendations have been readily
accepted, but many of these procedures are quite restricted and not satisfactory for
understanding the mechanism of action and substrate specificities of cellulases in detail.
Consequently, Wood and Bhat (1988) reviewed the cellulase assays used by laboratories
working on fungal cellulases. The majority of assays involve the accumulation of
hydrolysis products, i.e. quantification of reducing sugars, and chromophores. The most
common reducing sugar assays include the dinitrosalicyclic acid (DNS) method (Miller
1959; Ghosh 1984) and the Nelson-Somogyi method (Nelson 1944; Somogyi 1952). The
traditional protocols for quantification of cellulolytic enzymes, substrates and assay are
given in table 2.3. The synergistic action of cellulolytic enzymes on cellulose degradation
was shown in figure 2.2.
2.5 Sources of cellulases
Microbial cellulases are the most economic and available sources to meet the
industrial scale, because microorganisms can grow on an inexpensive media such as
agriculture and food industries by-products. Certain microbial sources that are studied for
cellulase production are listed in table 2.4.
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Table 2.3 Substrates and assay procedures for mesuring cellulolytic enzymes activity.
Enzyme Substrate Assay
Endo-β-1,4-D-glucanase
(endoglucanase, CM-
cellulase, endocellulase)
Carboxymethyl cellulose
Hydroxyethylcellulose
Release of reducing sugars (Miller
1959).
Decrease in viscosity (Wood and Bhat
1988; Tolan and Foody 1999).
Exo- 1,4-13-D-glucanase
(exocellulase or Avicelase or
FPase)
Filter paper
Avicel
Hydrocellulose
Dyed Avicel
Release of reducing sugars (Miller
1959)
-do-
-do-
Release of dyed cellobiose (Nummi et
al. 1981; Wood and Bhat 1988 )
β-D-Glucosidase or
Cellobiase
Cellobiose
p-Nitrophenyl- β -D-
glucopyranoside
Release of glucose and Release of o- or
p-nitrophenol (Wood and Bhat1988).
Fig. 2.2 Cellulose hydrolysis by a cellulase system (Winkelmann 1992).
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Table 2.4 Certain microbial sources for cellulolytic enzymes production.
Organism Enzyme Reference
I. Bacteria
Acidothermus cellulolyticus Endoglucanase Ding (2006), Himmel et al. (1994),
Sakon et al. (1996)
Alkalophilic Streptomyces Cellulase,
Endoglucanase,
Nakai et al. (1988), Damude et al.
(1993)
Anaerocellum thermophilum Endoglucanase Zverlov et al. (1998)
Bacillus sp. KSM-S237 Endoglucanase Hakamada et al. (1997)
Caldocellulosiruptor
saccharolyticus
Endoglucanase
Exoglucanase
Bergquist et al. (1999), Te’o et al.
(1995)
Caldocellum saccharolyticum Endoglucanase Te’o et al. (1995)
Cellulomonas flavigena β-D-glucosidases Gaspar et al. (2007)
Clostridium stercorarium Endoglucanase
Exoglucanase
Bronnenmeier and Staudenbauer
(1990), Bronnenmeier et al. (1991),
Clostridium thermocellum Endoglucanase Fauth et al. (1991),
Romaniec et al. (1992)
Lactobacillus plantarum β-D-glucosidase Sestelo et al. (2004)
Pseudomonas fluorescens Cellulase Yamane et al. (1970)
Pyrococcus furiosus Cellulase Voorhorst et al. (1999)
Rhodothermus marinus Endoglucanase Hreggvidsson et al. (1996)
Sulfolobus solfataricus Cellulase Moracci et al. (2001)
II. Fungi
Aspergillus aculeatus Cellulase Murao et al. (1988)
Aspergillus glaucus XC9 Cellulase
(endoglucanase)
Chang et al. (2006)
Aspergillus nidulans β-D-glucosidases Kwon et al. (1992)
Aspergillus nidulans β-D-glucosidases Bagga et al. (1990)
Aspergillus niger Cellulase Okada (1988)
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Aspergillus niger B-glucosidase Johanssona and Reczey (1998
Aspergillus oryzae β-D-glucosidases Zhang et al. (2007)
Aspergillus sojae β-D-glucosidases Kimura et al. (1999)
Chaetomium thermophilum Endoglucanase Li et al. (2003)
Cladosporium sp. Endoglucanase
Exoglucanase
Abrha and Gashe (1992)
Humicola insolen,
Humicola grisea
Cellulase
Cellulase
Hayashida et al. (1988)
Melanocarpus albomyces Endoglucanase Oinonen et al. (1996)
Metschnikowia pulcherrima β-D-glucosidase Pombo et al. (2008)
Mucor circinelloides Endoglucanase Nakamura et al. (2001)
Penicillium pinophilurn Cellulase Wood et al. (1989),
Wood and McCrae (1986)
Rhizopus oryzae Endoglucanase
β-D-glucosidase
Murashima et al. (2002)
Thermoascus aurantiacus Cellulase,
β-D-glucosidase
Hong et al. (2007)
Trichoderma reesei Cellulase Bhikhabhai et al. (1984)
Trichoderma viride Cellulase Voragen et al. (1988)
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2.6 Application of cellulases
Cellulose biodegradation by cellulolytic microorganisms represents a major carbon flow
from fixed carbon sinks to atmospheric CO2 (Falkowski et al. 2000; Melillo et al. 2002;
Berner 2003) is very important in several agricultural and waste treatment processes
(Russell and Rychlik 2001; vanWyk 2001; Hamer 2003; Angenent et al. 2004; Haight
2005), and could be widely used to produce sustainable biobased products and bioenergy
to replace depleting fossil fuels (Lynd 1996; Mielenz 2001; Galbe and Zacchi 2002; Lynd
et al. 2002; Wyman 1994; 1999; 2003; Angenent et al. 2004; Kamm and Kamm 2004;
Demain et al. 2005; Reddy and Yang 2005). Commercial production of cellulase enzymes
by submerged culture fermentation began in the early 1970s, with cellulase made by
Trichoderma sold for use in research and pilot studies. The mid-1980s saw the first large
industrial uses of cellulase for stonewashing denim and as an additive for animal feeds.
This was accompanied by the introduction of commercial cellulases made by fungi of the
genera Aspergillus, Penicillium, and most importantly Humicola, introduced by Novo in
1986 (Nielsen 1995).
Cellulosic wastes have great potential as a feedstock for producing fuels and
chemicals. Cellulose is a renewable resource that is inexpensive, widely available and
present in ample quantities. Large amounts of waste cellulose products are generated by
commercial and agricultural processes. Concerns about diminishing resources, and the
excessive production of greenhouse gases continue to motivate the search for alternatives
to fossil fuel. The present challenge is to substantially increase the production and use of
biofuels for the transport sector. In order to reach the future goals of substituting fossil
based fuels, it will be necessary to promote the transition towards second generation
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biofuels. The hydrolysis of lignocelluloses to fermentable sugars remains the greatest
challenge in the development of economical plant biomass feedstock for the biorefinery
industry (Brown 2003). These can be produced from a wider range of feedstock, including
lignocellulosic raw materials. Biomass resources can be broadly categorised as agricultural
or forestry-based, including secondary sources derived from agro- and wood industries,
waste sources and municipal solid wastes. Fuels from lignocellulosic biomass have a
higher potential to reduce greenhouse gas emissions, and hence are an important means to
fulfil the CO2 emission targets, as compared with first generation biofuels. Lignocellulosic
raw materials comprise an abundant source of carbohydrates (cellulose and hemicellulose)
for a variety of biofuels, including bioethanol. The conversion technologies of
lignocellulosic raw materials are, however, more complex and need novel enzyme systems
and advanced fermentation technologies. The rate-limiting step in the conversion of
cellulose to fuels is hydrolysis, especially the initial attack on the highly ordered cellulose
structure. In spite of recent achievements, further developments are still needed to improve
the overall economy of the lignocellulose-to-ethanol process. These novel conversion
techniques would also be applicable for the production of other sugar platform-based
chemicals, the schematic representation of biological conversion of lignocellulosic material
to value added products is shown in fig. 2.3.
2.6.1 Textile industry
The textile industry is one of the first to benefit from targeted use of biotechnology. The
introduction of cellulases in the 1980s truly revolutionized denim garment processing
(Stewart 1996; Kumar and Yoon 1997). Denim finishing with cellulases emerged in the
1980s, radically changed the conventional process by reducing the need for pumice stones,
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and created the largest market segment for enzyme technology in textiles (Schafer et al.
2007). Enzymes are applied during the preparation, dyeing, and finishing (“wet process”)
stages of textile production, during which the fibers are exposed to water for depilling,
softening and denim abrasion of cellulose (Fig. 2.4). Biopolishing is a treatment in which
cellulase is used to remove small fuzz and fibrils from the surface of the fabric. This
versatile treatment can be carried out as a separate step or in combination with other
enzymatic preparation processes on cellulose-containing (cotton, viscose rayon, lyocell)
yarns, fabrics and garments to reduce the pilling (or fibrillation) tendency of the fabric and
provide a softer feel. Frequently, improvements in dye uptake are also observed. Enzyme
inactivation is needed after treatment with cellulase to stop the hydrolysis before damage
occurs. Typical inactivation is carried out by raising the liquid pH to 10 with sodium
carbonate and heating at 80 ◦C for 10 min (Kumar and Harden 1999).
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Fig. 2.4 Enzyme treatments in denim process: amylase desized (left),
cellulase abrasion (center), and laccase/mediator decolorization (right).
(Roland and Sell 2007)
Fig. 2.3 Schematic representation of biological conversion of
lignocellulosic materials to value added products. (Jorgensen et al. 2007)
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2.6.2 Laundry detergents
The use of cellulase in household laundry detergent originated in 1993 with the
introduction of Humicola endoglucanase. Cellulase in laundry detergent removes the hairs,
known as pills that occur on cotton clothes after repeated wearing and machine washing.
The cellulase removes the existing pills, and conditions the surface of new or unpilled
clothes. The result is an appearance that more closely resembles a new garment in
sharpness of color and smoothness of appearance. The use of cellulase can eliminate the
need for cationic fabric softeners, which have disposal and cost problems (Eriksen 1996).
Several types of cellulases are used in laundry detergents. Cellulases can both boost
cleaning performance and provide fabric care benefits (Kirk et al. 2004; Gormsen et al.
1998).
2.6.3 Pulp and paper industry
Over the last two decades the application of enzymes in the pulp and paper industry has
increased dramatically. The cellulase mainly acts by strengthening, refining, deinking and
drainage improvement of pulp. To name a few, lipase for pitch control, esterase for stickies
removal and pectinases for charge control (Schafer et al. 2007). Historically, cellulases
were perceived as having negative impact on paper strength and yield. However,
remarkable improvement in dry tensile and tear strength of bleached kraft pulps in paper
preparation were observed after the treatment by a few selected cellulases (Lonsky and
Negri 2003).
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2.6.4 Fruit juice and beverage processing
Cellulase enzymes break down cellulose and beta-glucan associated with the cell walls,
thereby decreasing the viscosity of the mash and increasing the ease of the juice recovery.
The conversion of cellulose and beta-glucans into soluble sugar provides another increase
in the overall juice solids yield. The enzyme treatment can also increase the clarity of the
juice by solubilizing small particles. The enzyme treatment can enhance the flavor of the
juice by increasing the extractability of flavor compounds in the mash. Where disposal of
the solid residue is costly, cellulase helps to decrease waste disposal costs. Another
concern in using cellulase in beverages, particularly beer and wine, is the possibility of
changes in flavor. Although increasing flavor extractability is often desirable, many beer
and wine brand names maintain a constant flavor that is undesirable to change. Most
cellulase used in the juice industry is Trichoderma cellulase,because of the typically low
pH present in the mash. Cellulase from Aspergillus niger is also used (Tolan and Foody
1999).
2.6.5 Alcohol production
Ethanol from cellulose represents an enormous opportunity to make a transportation fuel
that is an alternative to gasoline (Lynd 1996; Mielenz 2001; Lynd et al. 2002; Galbe and
Zacchi 2002; Wyman 2003; Angenent et al. 2004; Kamm and Kamm 2004; Demain et al.
2005; Reddy and Yang 2005). Development of such a fuel is motivated by 1) an increased
cleanliness of automobile exhaust with decreased levels of carbon monoxide and nitrous
oxides 2) a need for a fuel that does not contribute to an increase in the greenhouse effect,
3) the desire to decrease the dependence on imported petroleum, and 4) the possibility of
creating wealth in regions where cellulose is a prevalent natural resource. Cellulose is
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converted to ethanol by making glucose and then fermenting the glucose to ethanol using
yeast (Tolan and Foody 1999).
2.7 Aspergillus sp. as source of enzymes
The species of the genus Aspergillus most abundant and widely distributed microfungi in
decomposing organic material of soil, water, air, stored seeds, food, etc. The Aspergillus
was first identified by Micheli (1729). The genus Aspergillus consists of more than 180
officially recognized species, and comprises a particularly important group of filamentous
ascomycete species. Although it includes the major pathogen of humans. ex. Aspergillus
fumigatus (Brookman and Denning 2000; Latge 1999) and industrially and
environmentally useful members for degradation of plant polysaccharides (deVries et al.
2000; deVries 2003). Aspergillus species are also important for the large-scale production
of both homologous and heterologous enzymes (Fawole and Odunfa 2003; Wang et al.
2003). The biochemical and physiological methods are important in the systematics of
Aspergillus species, besides morphological properties that are commonly used for initial
identification (Christensen et al. 2000; Klich 2002; Asan 2004). The typical outline
microscopic morphology of Aspergillus sp. is shown in fig. 2.5.
2.7.1 Aspergillus flavus – a source for enzymes of biotechnological applications
Aspergillus, having inherent property of high capacity for secreting extracellular enzymes
and organic acids, played an important role in commercial production of industrially
valuable enzymes and other products (vanKuyk et al. 2000; Nutan et al. 2002; Kumar et
al. 2004). Its genes and genomes are being extensively investigated in an effort to
understand the associated cellular mechanisms and to expand these applications
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(Aleksenko et al. 2001; Mabey et al. 2004; Hombergh et al. 1997). Ojumu et al. (2003)
attempted cellulase (FPase) production in submerged fermentation by A. flavus L. NSPR
101 fermented using sawdust, bagasse and corncob. Long et al. (1997) isolated A. flavus
and used for mycelium bound lipase to modify the triglyceride structure of vegetables oils.
Awe and Akinyanu (1997) reported amylase production by A. flavus and A. niger using
cassava peels. Rosfarizan et al. (1998) exploited A. flavus for direct fermentation of
gelatinised sago starch to kojic acid. Rosfarizan, and Ariff, (2006) A. flavus used for kojic
acid fermentation using sucrose as a carbon source.
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Fig. 2.5 Out line microscopic morphology of Aspergillus sp.
Source:http://www.mould.ph/aspergillus
mould.htm
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Naganagouda et al., (2009) reported the isolation and identification of mannanase-
producing A. flavus and A.niger. They studied the mannanase production using cheaper
sources and partially characterized the enzyme. Mariana et al. (2008) screened nine
thermophilic fungi for production of protease in solid and submerged cultivation media
and the tested fungi were Thermoascus aurantiacus, Thermomyces lanuginosus,
T.lanuginosus, A. flavus, Aspergillus sp Aspergillus sp Aspergillus sp Rhizomucor
pusillus and Rhizomucor sp. Banga and Tripathi (2009) reported the isolation and
identification of a novel heparinase producing fungal culture A. flavus (MTCC-8654), and
its production and purification. Khoo et al. (1994) studied the purification and
characterization of the α-amylase produced by A. flavus grown on raw low-grade tapioca
starch as a fermentation substrate.
2.8 Exploitation of microbial sources for production of cellulolytic
enzymes
The cellulolytic enzymes have attracted considerable attention in recent years due to their
great biotechnological and industrial potential. Conversions of food industries and
agriculture wastes to valuable sugars are the great uses of cellulase enzymes (Bothast and
Saha 1997). Enzymatic treatment of cellulosic materials to produce carbohydrates, that can
be used as source for alcohol fermentation, or for production of industrial chemicals and
beverages.
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2.8.1 Submerged fermentation
Submerged fermentation involves the growth of a microorganism as a suspension in liquid
medium, in which various nutrients are either dissolved or suspended as particulate solids
in many cases of commercial media (Frost and Moss 1987). Filamentous fungi are
preferred for commercially important enzyme productions, because the level of enzymes
produced by these cultures is higher than those obtained from yeast and bacteria (Bakri et
al. 2003). A. niger and T. viride are important and safe organisms for industrial use and
they are good producers of cellulases (Berka et al..1992; Oxenboll 1994). Commercial
production of cellulase enzymes by submerged culture fermentation began in the early
1970s with cellulase made by Trichoderma sold for use in research and pilot studies.
Almost all commercial cellulases produced by submerged fermentation are made by the
fungi Trichoderma, Aspergillus, and Penicillium (Tolan and Foody 1999).
The cellulase producing microorganisms are abundantly present but the main
objective remains selection of promising strains that can produce the acceptable yield to
meet the industrial requirements. There is a very huge demand to improve the stability of
the enzymes to meet the requirements set by specific applications, especially with respect
to temperature and pH. Synthesis of enzymes depends on the type of nutrients available to
the organism and besides an adequate carbon source, other nutrients may be equally
important to the composition of the medium. Besides the carbon source, it has been
suggested that the nitrogen source can also control cellulolytic enzymes production. The
induction of cellulolytic enzymes requires substrates having β-1,4 glycoside bond, include
cellulose, CMC, cellobiose, filter paper etc. The past fifty years have witnessed remarkable
progress in (a) isolation of microorganisms producing cellulases; (b) improving the
32
enzyme productivity by medium engineering by submerged and solid state fermentation (c)
purifying and characterizing the cellulase components; (d) understanding the mechanism
of cellulose degradation; (e) cloning and expression of cellulase genes; and (h)
demonstrating the industrial potential of cellulases. Optimization of the medium for
cellulase production by selecting the best nutritional and environmental conditions is
important to increase the produced cellulase yield (Gomes et al. 2000). Optimized culture
conditions for cellulolytic enzymes production by certain microorganisms are given in the
table 2.5. The typical unit operations involved in screening, selection, optimization of
fermentation cultural conditions for submerged fermentation and solid state fermentation
are shown in fig. 2.6.
Table 2.5 Optimized cultural conditions for certain cellulolytic enzymes production by submerged fermentation
Si.No Microorganism Cellulolytic enzyme
Optimum conditions Medium
Referance Temperature
(oC)
pH Carbon source
(s)
Nitrogen
source (s)
1 Mucor
circinelloides
(NRRL 26519),
Endoglucanase,
Cellobiohydrolase,
and β-D-glucosidase)
30 5
Lactose,
Cellobiose, or
Sigmacell 50
Corn steep
liquor Badal 2004
2. Aspergillus niger
β-D-glucosidase 30 5.5-6
Glucose
Malt extract
Johansson and
Reczey 1998
3. Aspergillus niger
VKMF-2092
β-D-glucosidase 29 4.5-5.5 NA
NaNO2,
(NH4)2SO4
NH4 NO2
Urea
Kerns et al. 1987
4. Trichoderma
reesei Rut C 30
Filter paperase
β-D-glucosidase 30 6.0
Cellulose
powder
Dry yeast
Szengyel 2000
5. Aspergillus niger
NCIM 1207
Endoglucanase
β-D-glucosidase 28 3-5.5
Cellulose
powder
(NH4)2SO4N
H4H2PO4 and
corn-steep
liquor
Gokhale 1991
6 Aspergillus niger
(CBS 55464),
Aspergillus
niger (420)
Aspergillus oryzae
(CBS 12559)
β-D-glucosidase 30 NA
Quercetin, rutin,
Cellobiose
Glucose
(NH4)2HPO4
(NH4)2SO4
Gunata and Vallier
1999
7 Aspergillus
nidulans β-D-glucosidase 37 NA
Glucose
NA Lee et al. 1996
8 Lactobacillus
plantarum USC1
β-D-glucosidase 30 NA Glucose
NA Sestelo et al. 2004
34
9 Aspergillus
nidulans
Endoglucanase,
Cellobiohydrolase,
and β-D-glucosidase)
37 NA
Sugarcane
bagasse
NA Bagga 1990
10 Aspergillus
terreus
Endoglucanase,
Cellobiohydrolase,
and β-D-glucosidase)
40 5.2
Cellulose
powder,
wheat bran
Urea,
(NH4)2SO4 Bastawde 1992
11 Trichoderma
reesei Rut C-30
(Mutant strains)
Endoglucanase,
Cellobiohydrolase,
and β-D-glucosidase)
28 5.5 Lactose Yeast cream Jun et al. 2009
NA – Not available
Fig. 2.6 Schematic representation of traditional fermentation unit process for microbial enzyme
production and characterization
Selection of sites rich
with cellulose getting
microbial degradation
36
2.8.2. Soild state fermentation
Solid state fermentation (SSF) is generally defined as the growth of the microorganism on solid
material in the absence or near absence of free flowing water. Microbial enzymes are produced
mainly by submerged fermentation under tightly controlled environmental conditions (Rose
1980; Chahal 1985; Lonsane et al.. 1992; Singh et al. 2008). However, SSF also has good
potential for the production of enzymes, especially those from filamentous organisms that are
particularly suited for surface growth (Raimbault 1998; Pandey et al. 1999). The high cost of
microbial enzyme production and low yields are the major problems for industrial application.
Therefore, investigations on the ability of the cellulose and hemicelluloses hydrolyzing microbial
strains to utilize inexpensive substrates have been carried. Much work has been directed to
develop hyper producing microbial strains while also focusing on improvement of the
fermentation processes (Esterbauer et al. 1991; Haltrich et al. 1996).
Microbial enzymes, particularly those related to lignocellulose degradation, are produced
by SSF (Duenas et al. 1995; Pandey et al.. 2000; Kanga et al. 2004). Other hydrolases like
amylases (Bogar et al. 2002), proteases (George et al.. 1997) and phytase (Bogar et al. 2003;
Vohra and Satyanarayana 2003; Roopesh et al. 2006) are also produced by SSF. Thus SSF holds
tremendous potential for the production of enzymes, as this process has low capital investment,
superior productivity, less energy requirements and low effluent generation (Chahal 1985;
Nigam and Singh 1994). SSF compares favorably with submerged fermentation in terms of
energy requirements, volumetric productivity and product recovery; it represents a good option
when production costs should be reduced as is the case of the microbial enrichment of
agricultural residues or the production of bulk inexpensive enzymes (Illanes et al. 1992; Pandey
et al. 2000).
37
The cellulolytic enzymes are inducible enzymes, and that cellulose is the best inducer. In
SSF for cellulase production, cellulosic materials act as either the carbon source or the inducer.
The recent studies SSF process for cellulolytic enzyme production have explored a variety of
substrates varying from agro- residues to wastes of industries such as sugarcane bagasse, wheat
bran, rice bran, maize bran, gram bran, wheat straw, rice straw, rice husk, soyhull, sago hampas,
grapevine trimmings dust, saw dust, corncobs, coconut coir pith, banana waste, tea waste,
cassava waste, palm oil mill waste, sugar beet pulp, sweet sorghum pulp, apple pomace, peanut
meal, rapeseed cake, coconut oil cake, mustard oil cake, cassava flour, wheat flour, corn flour,
steamed rice, steam pre-treated willow, starch, etc (Pandey et al. 2000). The natural resources
such as wheat bran, rice hull, corn straw, corncob, fruit peels and seeds and effluents from paper
industry have increased as a result of industrialization, becoming a problem regarding space for
disposal and environmental pollution. However, the above residues represent alternative source
for the microbial growth aiming the production of biomass or enzymes (daSilva et al. 2005). The
wastes such as saw dust and wood chippings have a huge potential for cellulases and
hemicellulases production. In order to ensure viable commercialization of enzyme production via
SSF system, a cheap system with hyper enzyme producers has been established (Mitchell et al.
2006). Certain microbial sources of cellulolytic enzymes production using various
agricultural/industrial residues by SSF are given in table 2.6. If SSF used to produce cellulase,
the following advantages and disadvantages may be noted (Cen and Xia 1999):
1. The raw materials required to produce cellulase are cheap and abundant. Natural cellulosic
materials such as plant stems and corn cobs can be used as carbon source. The composition of
the medium is simple and of low cost. Because of the high capability of cellulosic materials to
buffer the pH value, it is not necessary to add additional expensive buffer solution.
38
3 There is no stirrer in most types of solid-state fermentor and the requirements for water and
aeration are less than that in submerged fermentation. Therefore, the energy consumption is
low and there is no waste water produced in the process.
4 In solid-state fermentation, the productivity per unit reactor volume is high and the solid
cellulase koji can be directly applied to hydrolyze cellulosic materials.
5 The equipment in the solid-state fermentation process is relatively simple and the capital
investment is low. However, new types of fermentors for large scale cellulase production
need to be developed.
6 The process is generally labor intensive and hard to control. The reproducibility is relatively
poor with batch-to-batch difference. In addition, more care is needed in order to prevent
contamination.
The composition of a fermentation medium influences the supply of nutrients and metabolism
of cells, therefore, the productivity of a fermentation process also depends on the culture medium
used. Of the major culture medium nutrients, carbon and nitrogen sources generally play a
dominant role in fermentation productivity. Traditional method for determining optimal
conditions in fermentation processes is ‘one variable at a time’ i.e. varying one parameter while
keeping others at a constant level (Adinaryana et al. 2003). This is a time consuming, laborious
and cost ineffective method, in addition, does not include interaction effects among variables.
Because of the large number of quantitative and qualitative variables involved in a bioprocess,
methods of statistical experimental design are used in many studies for optimizing fermentation
media. To reduce the experimental workload, simple batch cultures in a parallel approach are
carried out in shake flasks. Optimization using factorial design and response surface method can
overcome such drawbacks. Factorial design technique has been successfully used to optimize
and to evaluate the effects of process parameters in the production of enzymes and other
metabolites (Cordova 1998; Muralidhar 2001). To obtain a suitable medium for enzyme
39
production in SSF, a series of statistically designed studies were conducted to investigate the
effect of various cultural conditions and media components. The optimization process firstly
identify the significant factor preferably nutrients (carbon sources, nitrogen sources and essential
elements) for enzyme production. The basic research goal when studying industrial applications
is reduction of the enzyme production cost by optimization of the cultivation medium and
conditions. The statistical analysis offers many tools for optimizing medium components. The
response surface methodology (RSM) is probably the most extensively used statistical
optimization method. RSM can be used to determine the optimal production conditions and
ranges of controllable variables as well as to generate a polynomial equation. RSM can also be
used to estimate the relationships between controllable variables and observed results. Recently,
statistical designs for the optimization have been successfully employed, demonstrating that
these statistical methods are powerful and useful tools (Dey et al. 2001; Park et al. 2002; Wejse
et al. 2003; Chandrika and Fereidoon 2005; Chen et al. 2005). The significant factor optimized
by varying one factor at a time while keeping the others constant, then focus on the most
important factors and then focus on the critical subset of cultural conditions and media
components, finally a RSM was derived to optimize the critical components and maximize the
enzyme production. RSM was proved to be a powerful tool in optimizing the fermentation
process. In general, the procedure applied can be subdivided into four steps: identification of the
most important medium components, identification of the variable range, search for the optimum
value of the variables and experimental verification of the optimum (Botz 2000). Certain
previous reports of statistical optimization of microbial fermentations such as production of
glucoamylase by a thermophilic mold Thermomucor indicae-seudaticae (Kumar and
Satyanarayana 2004), γ- polyglutamic acid production by Bacillus subtilis ZJU-7 (Shi et al.
2006), increase in xylanase production by Aspergillus niger XY-1 (Xing et al. 2008) and ethanol
from sugarcane bagasse (Sasikumar and Viruthagiri 2008).
40
Table 2.6 Cellulolytic enzymes production by certain microbial sources grown on substrates
by SSF
Si.No Microorganism Substrate Referance
1 Penicillium echinulatum
Sugarcane bagasse,
Wheat bran Camassola and Dillon. 2007
2. Trichoderma harzianum Wheat straw and bran Deschamps et al. 1985
3. Penicillium decumbens Wheat straw and
Wheat bran Moet et al. 2004
4. T. reesei LM-UC 4 and
Aspergillus phoenicis
Sugarcane bagasse Correa and
Tengerdy 1997
5 Thermoascus aurantiacus Dry wheat straw Kalogeris et al. 2003
6. Myceliophthora sp.
Rice straw, wheat straw
Wheat bran, bagasse and
Corn cob
Badhan et al. 2007
7. A. niger
Wheat straw and wheat
bran
Jecu 2000
8. A. ustus
Rice straw and wheat
bran
Shamala and Sreekantiah
1986
9 Aspergillus niger
Sugarcane bagasse
Correa et al. 1999
10 Aspergillus niger KK2, Rice straw and wheat
bran Kang et al. 2004
11 Aspergillus ellipticus and
Aspergillus fumigatus
Sugarcane bagasse, dry
wheat straw, wheat bran,
rice bran and groundnut
shell
Gupta and Madamwar 1997
12
Trichoderma reesei LM-
UC4
Aspergillus phoenicis
QM329
Sugarcane bagasse Correa and Tengerdey 1997
41
2.9 Purification of cellulolytic enzymes
To study the biochemical and physical properties of enzymes, it is necessary to purify and
concentrate the preparation. The level of downstream processing to which any enzyme or other
protein to be subjected is largely dependent on the intended application of the finished product
(Bruton 1983; Wheelwright 1987). Generally the optimized conditions of physical and medium
compostion are used for enzyme production. Purification to desired level of enzymes normally
involves several steps and they are chosen according to its intended use. Enzymes application in
pharmaceutical, clinical diagnostic and basic molecular biological sectors requires high-purity
grade enzymes, where as concentrated and partially purified enzymes used for industrial
biotechnological conversions of lignocellulosic materials to biofuels, text tile, paper and pulp,
fruit juice clarification, and detergents need concentrated highly active enzyme. Thus, it is
significant to develop economic processes for their purification to obtain concentrated enzymes
with maximum activity (Headon 1994).
Microbial enzymes to be exploited as reagents in any field, be it analytical or industrial, it
must first be concentrated and purified to a degree that removes any other enzyme capable of
catalysing undesirable side-reactions. This may or may not mean purification to homogeneity.
Traditionally the purification of cellulase from fermentation media has been done in several
steps, which include centrifugation of the culture, and selective concentration of the supernatant,
usually by selective precipitation of the enzyme by ammonium sulphate or organic solvents such
as ethanol in the cold. Then the crude enzyme is subjected to various preparative
chromatographic techniques to meet desired level of purity. The traditional purification steps
reported for microbial cellulolytic enzymes are given in the table 2.7.
42
Table 2.7 Schemes used for purification of cellulolytic enzymes
Si.no Organism
(Enzyme)
Purification
scheme
Final
purification
fold
Reference
1 Cellulomonas flavigena
(β-D-glucosidase)
• wild-type
• Mutant PN-120
Crude extract
Q Sepharose anion
exchange column
Bio Gel P60 column
Bio Gel P100 column
28.85
15.63
Gaspar et al., 2007
2
Mucor circinelloide
(endoglucanase)
Culture supernatant
Ethanol precipitation
CM Bio-Gel A
Bio-Gel A-0.5m
408
Badal 2004
3
Candida sake
(β-D-Glucosidase)
Culture supernatant
Sephacryl S-300
Chromatography
Q-Sepharose
Chromatography
35.5
Gueguen et
al.2001
4
Aspergillus niger
(β-D-Glucosidase)
Culture supernatant
Ammonium sulphate
precipitation
Sephadex G-75 fraction
6.0
Peshin et al. 1999
5.
Aspergillus nidulans
(Endoglucanase/
Exo gluconase/
β-D-Glucosidase)
Culture supernatant
Ammonium sulphate
precipitation
NA
Bagga et al. (1990)
43
Sephadex G-200
DEAE Sephadex A-50
6.
A. nidulans
(β-D-Glucosidase)
Ultrafiltration
Non denaturing
polyacrylamide slab gel
Ion exchange
chromatography
NA
Kwon et al. 1992
7.
Aspergillus niger No. 5.1
(β-D-Glucosidase)
Culture supernatant
Ammonium sulphate
precipitation
Chitopearl-DEAE
Sephadex G-100
NA
Xie et al. 2004
8
Aspergillus sojae
(β-D-Glucosidase)
Culture supernatant
Sephacryl S-200 HR
Q-Sepharose HP
G-l
G-2
G-2 purification
Sephacryl S-300 HR
Methyl HIC
Bio gel HPT
NA
Kimura, et al.
1999
NA – Not available
44
2.10. Properties of cellulases
Looking into the depth of microbial diversity, there is always a chance of finding microorganism
producing novel enzyme with improved properties for commercialization. Microbial enzymes
show great diversity in relation to their properties and biological activities. As there is growing
demand of cellulase application on different industrial sectors, it is necessary to identify and
standardize the novel features of cellulolytic enzymes. The cellulase system from the fungal
strain contains all three enzyme activities needed to produce glucose from cellulose and has great
potential to be used in enzymic saccharification of various lignocellulosic substrates. The use of
these cellulolytic enzymes as agents in bioconversion of plant residues or other wastes to
valuable products (such as fuel alcohols) has been the subject of intense study in recent years. At
present there is considerable interest for cellulolytic enzymes with highest activity and stability
against temperature, pH, cationic metals and resistance against feedback inhibition.
The concentrated and purified enzyme is necessary to evaluate the biochemical properties
of enzymes such as SDS-PAGE analysis to know the homogeneity and molecular mass of the
selected enzyme, optimum physiological conditions for activity, temperature and pH stability,
and kinetic parameters to know the Km and Vmax . The biological activity of cellulolytic enzyme
complex is of great importance, as revealed by studies carried out on hydrolysis of cellulosic
substrates. Such processes, if they are to be economically feasible, will require stable enzymes
able to retain their activities during prolonged reactions and recycling and in the presence of high
concentrations of end-products. The reported cellulolytic enzymes of bacterial and fungal
sources and their biochemical properties are summarized in table 2.8.
Table 2.8 Optimum bio-chemical properties of certain extracellular cellulase components from microbial sources
S.
No Organism
Cellulolytic
enzyme
Molecular mass
(kDa)
Optimum assay
conditions
Kinetic
parameters Referance
Tempera
ture (oC)
pH Km
(mM)
Vmax
(U)
Bacterial source
1. Cellulomonas flavigena β-D-glucosidase 210 37-40 6 114 90.1 Gaspar et al. 2007
2. Lactobacillus
plantarum β-D-glucosidase 40 45 5.0 1.82 4.89 Sestelo et al. 2004
3. Streptomyces
albaduncus
Endoglucanase
Exoglucanase
β-D-glucosidase
-
-
-
50
6
6
6.5
40
92
1.7
0.606
33.33
0.109
Harchand and Singh
1997
Fungal source
4. A.niger USDB 0827
A. niger USDB 0828
β-D-glucosidase
β-D-glucosidase -
65
65
4.6
4.6
0.75
0.89
3067
3629 Hoh et al. 1992
5. Aspergillus aculeatus Endoglucanase
25
38
66
68
50
65
70
60
4.5
4.0
5.0
2.5
- - Murao et al. 1988
6. Aspergillus niger Endoglucanase 31 - 4 - - Okada 1988
7. Aspergillus niger No.
5.1 β-D-glucosidase 67.5 60 6 5.34 2.57 Xie et al. 2004
8. Aspergillus ornatus β-D-glucosidase - 60 4.6 0.76 - Yeoh et al. 1986
9. Coriolus versicolor Endoglucanase 29.5 55 5 - - Idogaki and
Kitamoto 1992
10. Dichomitus squalens
Endoglucanase I
Endoglucanase II
Endoglucanase III
42
56
47
55-60
55-60
55-60
4.8-5.0
4.8
4.6-4.8
Rouau and Foglietti
1985
46
11. Humicola insolen
Humicola grisea
Endoglucanase
Endoglucanase I
Endoglucanase II
57
63
58
50
50
50
5
5
5
- -
Hayashida et al.
1988
12. Metschnikowia
pulcherrima β-D-glucosidase 49 50 4.2 1.5 0.8 Pombo et al. 2008
13. Mucor circinelloides Endoglucanase 27 55 4-6 - - Saha 2004
14. Rhizopus oryzae Endoglucanase I
Endoglucanase II
41
61
55
55
5-6
5-6 - -
Murashima et al.
2002
15. Thermoascus
aurantiacus
Endoglucanase 34 7.-80 4.0-4.4 - -
Parry et al., 2002
16. Thermoascus
aurantiacus β-D-glucosidase - 70 5 - - Hong et al. 2007
17. Trichoderma koningii
Endoglucanase I
Endoglucanase II
Endoglucanase III
Endoglucanase IV
13
31
48
48
- - - - Wood and McCrac
1978
18. Trichoderma reesei
Endoglucanase I
Endoglucanase II
Endoglucanase III
Endoglucanase IV
Endoglucanase V
20
43
48
55
56
- - - - Bhikhabhai et al.
1984
19. Trichoderma viridae QM
9414
Endoglucanase I
Endoglucanase II
Endoglucanase III
Endoglucanase IV
Endoglucanase V
23.5
45
50
52
57
5.5
4.0
5.1
4.5
4.5
- - Voragen et al. 1988
‘-’ Not available
47
2.11 Immobilization of cellulase
The use of microbial enzymes in industrial applications has been limited by several factors,
mainly the high cost of the enzymes production, their instability, and availability in small
amounts. Also the enzymes are soluble in aqueous media and it is difficult and expensive to
recover them at the end of catalytic process. This restricts the use of soluble enzymes to batch
operations. Over the last few decades, intense research in the area of enzyme technology has
provided many approaches to overcome these limitations to facilitate their practical applications.
Among them, the newer technological developments in the field of immobilized biocatalysts can
offer the possibility of a wider and more economical exploitation of biocatalysts in industry,
waste treatment, medicine, and in the development of biosensor (Souze 1980). Immobilization of
biocatalysts helps in their economic reuse and in the development of continuous bioprocesses.
The variety of chemical transformations catalyzed by enzymes has made these catalysts a prime
target of exploitation by the emerging biotech industries.
In general, the term immobilization refers to the act of the limiting movement or
restricting movement to a confined space (Qung et al. 2004). Immobilization of biocatalysts
helps in their economic reuse and in the development of continuous bioprocesses. Biocatalysts
can be immobilized either using the isolated enzymes or the whole cells. Several methods that
have been used to immobilize the cells/enzymes, include cross linking, physical adsorption, ionic
binding, metal binding, covalent binding and entrapment methods. All of these experimental
biocatalyst immobilization systems normally fall into one of three categories: 1. Biocatlyst
entrapment in polymer gels or porous supports. 2. Adhesion on micro carrier surface and 3.
Capture behind membrane (encapsulation). Sometimes the distinction between these different
categories may not be very clear, depending on the particular immobilization system employed.
However, every method has its advantages and drawbacks. The major components of an
48
immobilized biocatalyst include enzyme, matrix and mode of interaction of the enzyme with the
carrier. A large number of enzymes have been immobilized on inorganic carriers like porous
glass (Adamich et al. 1978), ceramics (Dale and White 1979), carbon (Cho and Bailey 1978) and
sand (Puls et al. 1977) by different techniques. The most extensively studied immobilization
method is the entrapment of microbial cells/enzymes in polymer matrices. The matrices used are
agar, alginate, carrageenan, cellulose and its derivatives, collagen, gelatin, epoxy resin, photo
cross-linkable resins, polyacrylamide, polyester, polystyrene and polyurethane. Among the
above matrices, entrapment of cells/enzymes in alginate gel is popular because of the
requirement for mild conditions and the simplicity of the used procedure. Several reports on
employing alginate gel are available (Kierstan and Bucke 1977).
Enzymes such as cellulases and amylases are currently used by several industries to
hydrolyze cellulose or starch to products such as dextrins, syrups, and sugars. Such reactions
represent the key first step toward the production of a variety of useful chemicals and sweeteners
and are also useful in the pulp and paper industry for fiber modification. Enzymatic hydrolysis of
cellulosics, the most abundant renewable resource on earth, offers an attractive alternative, if the
process can be made economically competitive. Several previous studies have considered the
advantages of immobilized enzymes with soluble substrates, and a few studies have also
investigated the properties of immobilized enzymes with insoluble substrates. The performance
of cellulase and amylase immobilized on siliceous supports was evaluated with respect to
immobilization conditions and thermal stability (Bradley et al. 2004). Enzyme immobilization
has been reported to improve the thermal stability of enzymes and may also affect binding of
substrates and inhibitors to the enzyme, thereby affecting the Michaelis constant and enzyme
inhibition (Wiseman 1994, Lim and Macdonald 2003). Sadhukhan et al. (1993) observed that
immobilization of amylase onto Sepharose, alginate beads, and polyacrylamide gels could
49
increase the optimum reaction temperature to about 70°C, compared with about 60°C for the
soluble form. Natural cellulases from most fungal sources are limited in their overall activity by
low amounts of β-glucosidase (Klyosov 1986) and by cellobiose inhibition of cellobiohydrolase
(Sundstrom et al.1981). Although advantageous to the growth of the fungus, these characteristics
are inconvenient for the industrial use of cellulase in cellulose processing. Improved cellulose
hydrolysis and increased glucose yield can be achieved under laboratory or industrial conditions
by combining additional β-glucosidase with fungal cellulases (Sundstrom et al. 1981). However,
β-glucosidase is an expensive enzyme to produce and, if used in a soluble form that cannot be
recycled, is not cost effective for industrial use. The coimmobilization of cellulase and β-
glucosidase and resulted in the improved kinetic properties of the enzyme system and the
improved glucose yield as compared to cellulase function alone (Chakrabarti and Storey 1989). It
is therefore conceivable that the use of immobilized enzyme or cells may offer a solution
towards a reduction in the cost of cellulase production.