Molecular characterization of two trypsinogens in the orange-spotted grouper, Epinephelus coioides,...
Transcript of Molecular characterization of two trypsinogens in the orange-spotted grouper, Epinephelus coioides,...
Molecular characterization of two trypsinogensin the orange-spotted grouper, Epinephelus coioides,and their expression in tissues during early development
Chun-Hung Liu • Ya-Huei Chen • Ya-Li Shiu
Received: 7 November 2011 / Accepted: 5 July 2012 / Published online: 17 July 2012
� Springer Science+Business Media B.V. 2012
Abstract In this study, we cloned two trypsinogens
of the orange-spotted grouper, Epinephelus coioides,
and analyzed their structure, expression, and activity.
Full-length trypsinogen complementary (c)DNAs,
named T1 and T2, were 900 and 875 nucleotides,
and translated 242 and 244 deduced amino acid
peptides, respectively. Both trypsinogens contained
highly conserved residues essential for serine protease
catalytic and conformational maintenance. Results
from isoelectric and phylogenetic analyses suggested
that both trypsinogens were grouped into trypsinogen
group I. Both trypsinogens had similar expression
patterns of negative relationship with body weight;
expression was first detected at 1 day post-hatching
(DPH) and exhibited steady-state expression during
early development at 1–25 DPH. Both expression and
activity levels significantly increased after 30 DPH
due to metamorphosis. Grouper larval development is
very slow with insignificant changes in total length
and body weight before 8 DPH. The contribution of
live food to an increase in the trypsin activity profile
may explain their importance in food digestion and
survival of larvae during early larval development.
Keywords Orange-spotted grouper � Trypsinogen �Trypsin activity � Digestion � Larval development
Introduction
Trypsin is an endopeptidase belonging to the serine
protease family (Rawlings and Barrett 1994). It plays a
key role in the digestive capacity of fish larvae and
other animals. Trypsins are characterized by a cata-
lytic triad composed of three essential amino acid
residues of His-75, Asp-102, and Asp-189 in the
S1-binding pocket, which confers specificity to cleav-
age at the peptide bond on the carboxyl side of basic
L-amino acids such as arginine and lysine residues
(Graf et al. 1988), and Tyr-172 participates in
substrate specificity (Hedstrom et al. 1994). Trypsin
is synthesized as a preproenzyme that is processed to
the proenzyme of trypsinogen (Mithofer et al. 1998).
The N-terminal activation peptide of trypsinogen is
removed by specific cleavage between a Lys or an Arg
residue and an Ile residue to convert it into its active
form, trypsin (Light and Janska 1989). In addition, the
Ile residue at the amino-terminal end bends inward and
makes several internal contacts when forming the
catalytically active trypsin (Bolognesi et al. 1982). In
turn, the resulting trypsins themselves activate all
other pancreatic digestive zymogens including more
trypsinogens (Chen et al. 2003).
Several isoforms of trypsin were described in both
mammals and fish (Manchado et al. 2008). On the
C.-H. Liu (&) � Y.-H. Chen � Y.-L. Shiu
Department of Aquaculture, National Pingtung University
of Science and Technology, Pingtung 91201,
Taiwan, ROC
e-mail: [email protected]
123
Fish Physiol Biochem (2013) 39:201–214
DOI 10.1007/s10695-012-9691-4
basis of their amino acid sequence identities and to a
lesser degree, their charges at physiologic pH, they are
classified into three groups: I, II, and III. Most
vertebrates possess at least one trypsinogen gene from
groups I and II. However, group III has so far only
been found in teleosts (Manchado et al. 2008). The
isoforms of trypsin have different expression patterns
in teleosts during their life cycle and in different
tissues indicating functional differences (Murray et al.
2004; Manchado et al. 2008).
Digestive enzymes affect the digestive capacity and
set physiologic limits on the growth rate and feed
conversion ratio (Perez-Casanova et al. 2006). Trypsin
activity in the pyloric cecum was shown to be
positively involved in the growth rate of Atlantic
cod, Gadus morhua (Lemieux et al. 1999), and
Atlantic salmon, Salmo salar (Rungruangsak-Torris-
sen et al. 2006). However, a contrary finding about
trypsin activity with the growth status of orange-
spotted grouper, Epinephelus coioides, was found in
our previous study (Liu et al. 2012). The different
expression patterns of trypsin are considered to be
species specific, and other proteases, like pepsin, play
more important roles in regulating growth of grouper
through protein digestion (Liu et al. 2012). However,
trypsin plays important roles in digestive function
during the early larval stage. The study of trypsin
activity and other digestive enzymes during early
development of the digestive system in marine fish is a
valuable tool to better understand the digestive
physiology of larvae, since they can be used as
indicators of the nutritional status (Eusebio et al. 2004;
Fujii et al. 2007).
In this study, two complete trypsinogen cDNAs
from orange-spotted grouper were isolated, and a
phylogenetic analysis revealed the presence of two
distinct groups. In addition, the expression and
enzymatic activity of each isoform were analyzed
during early development.
Materials and methods
Experimental rearing and sampling
Orange-spotted grouper, E. coioides (at 3 cm in total
length), were reared for 5 months and sampled from a
farm of the Department of Aquaculture, National
Pingtung University of Science and Technology,
Taiwan. Fish were reared in a cement tank
(6 9 2 9 1.5 m) with 10 tons of saltwater at 15 %salinity and continuous aeration through an air stone.
The temperature, pH, and dissolved oxygen (DO) were
maintained in ranges of 27–29 �C, 7.5–8.0, and
5.6–6.1 mg/l, respectively. Fish were fed a commer-
cial diet at a ratio of 5 % of their body weight once
daily.
For the analysis of trypsinogen expression during
larval development, grouper larvae were reared.
Orange-spotted grouper-fertilized eggs were a kind
gift from a private fish farm in Pingtung County,
Taiwan. Eggs were placed in fiberglass-reinforced
plastic (FRP) tanks with 500 L of 30 % saltwater and
continuous aeration. Grouper larvae hatched in about
24 h after fertilization at a temperature of 27 �C. After
hatching, larvae were transferred with water into two
cement tanks (6 9 2 9 1.5 m) with 10 metric tons of
30 % saltwater and continuous aeration. In addition,
larval stock in a smaller cement tank (1.8 9 1.3 9
1 m) with 2 metric tons of 30 % saltwater and
continuous aeration was used as the unfed treatment.
The water temperature, pH, and DO were maintained
in ranges of 27–29 �C, 7.7–7.9, and 5.3–6.0 mg/l,
respectively, during the experiment. The stock density
was 5000 larvae per metric ton of water. During larval
breeding, the water was not changed. Two days after
hatching, larvae were fed oyster trochophores three
times per day for 5 days. Rotifers screened through a
200-mesh phytoplankton net were fed to larvae four
times per day from 6 to 10 days post-hatching (DPH).
Thereafter, rotifers that passed through a 150-mesh
phytoplankton net were fed to larvae four times per day
until 22 DPH. After 17 DPH, copepods were also used
as live food to gradually replace the rotifers, and only
copepods were used for larval feeding four times per
day after 22 DPH until more than 95 % of the fish had
undergone metamorphosis (the pelvic fins and dorsal
fin completely shortened) (at 35 DPH). Fish were then
fed ad libitum with shrimp paste for 5 days followed by
semi-moist feed, mixed with shrimp paste and com-
mercial feed powder at a ratio of 8:2 (Table 1).
Grouper were randomly sampled from the rearing
tank using a hand net. Before sampling, fish were not
fed for 2 days in order to empty the gut and facilitate
dissection. For trypsinogen cDNA cloning, total RNA
isolated from the pyloric cecum of juvenile
(35.6 ± 3.6 g) fish was used. Fish with an average
weight of 118.5 ± 1.27 g were used for expression
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analysis of the two trypsinogens (T1 and T2) in
different tissues, including the esophagus, stomach,
pyloric cecum, anterior intestine, middle intestine,
hind intestine, eyes, liver, gills, skin, heart, head
kidney, mid-kidney, hind kidney, spleen, brain, dorsal
muscles, and blood by a reverse-transcription poly-
merase chain reaction (RT-PCR). In addition, tissues
with abundant trypsinogen expression, including the
pyloric cecum, anterior intestine, middle intestine,
hind intestine, and spleen were used for a real-time
PCR analysis. To analyze the relationship between
size and expression of the two trypsinogen genes by a
real-time PCR, the pyloric cecum, anterior intestine,
middle intestine, and hind intestine were dissected
from grouper at a size range of 26.35–179.1 g. In order
to investigate the beginning of trypsinogen transcrip-
tion in the life cycle, an RT-PCR was performed.
Thirty fertilized eggs, 10 living larvae from the
feeding treatment at 0, 2, 4, 6, and 12 h, and 1, 2, 3,
and 4 DPH, and 10 living larvae from unfed treatment
at 2 and 3 DPH were sampled to analyze trypsinogen
expression by an RT-PCR. Samples consisting of 30
eggs or 10 larvae from each sampling were pooled.
Trypsinogen expression and trypsin activity assays
during larval development were also carried out.
Twenty larvae were pooled for each replicate at 1, 2, 3,
and 4 DPH, five larvae were pooled for each replicate
at 8 DPH, three larvae were pooled for each replicate
at 12 and 16 DPH, and one larva was used for each
replicate at 20, 25, 30, 35, 40, 45, and 50 DPH. Each
sampling consisted of six replicates. Larvae were
individually collected; the body weight and total
length were measured; then larvae were washed with
DEPC water, frozen in liquid nitrogen, and stored at
-80 �C. At 1–25 DPH, whole larvae were used for the
analysis. The digestive tract of a larva was sampled for
analysis at 30–50 DPH. Oyster trochophores were also
prepared for the analysis of trypsin activity.
Cloning of trypsinogens and phylogenetic analysis
Total RNA was extracted from the pyloric cecum of
fish and further purified using ULTRASPECTM RNA
and Total RNA Isolation Reagent (Biotecx, Houston,
TX, USA) following the manufacturer’s instructions.
First-strand cDNA synthesis in RT was accomplished
using Super-Script II RNase H- reverse transcriptase
(Promega, Madison, WI, USA) to transcribe poly (A)?
RNA with oligo-d(T)18 as the primer. Reaction
conditions recommended by the manufacturer were
followed.
Full-length trypsinogen cDNA of grouper was
obtained by an RT-PCR, and 30 and 50 rapid ampli-
fication of cDNA (RACE) methods. Degenerate
primers were designed based on the highly conserved
teleost amino acid sequence of trypsinogen in Gen-
Bank and another database (Benson et al. 1994) and
using the ClustalW program (http://align.genome.jp/).
The degenerate primer pair of CTF1 and CTR1
(Table 2) was used to amplify partial grouper tryp-
sinogen cDNA fragments. The PCR was carried out in
a 50-ll reaction volume containing 10 ng of cDNA,
1 9 ProTaq buffer (Protech, Taipei, Taiwan), 2.5 U of
Pro Taq Plus DNA polymerase (Protech), 0.25 mM of
dNTPs, and 0.25 lM of each primer. PCRs were
performed as follows: 30 cycles of denaturation at
94 �C for 1 min, annealing at 50 �C for 1 min, and
elongation at 72 �C for 2 min, followed by a 10-min
extension at 72 �C and cooling to 4 �C.
Total RNAs from the grouper pyloric cecum were
also used for the 50 and 30 RACE. The RACE cDNA
template was synthesized using the ExactSTARTTM
Eukaryotic mRNA 50-& 30-RACE Kit (cat no.
ES80910, Epicentre, Madison, WI, USA) according
to the manufacturer’s protocol and amplified by a PCR
with PRIMER 1 and PRIMER 2 supplied by the kit.
For trypsinogen 1 (T1), the 50 and 30 ends were
amplified by nested PCRs with PRIMER 1 and specific
primers (T15RACER1 and T15RACER2), and PRI-
MER 2 and specific primers (T13-GTA-F1 and T13-
GTA-F2), respectively. For trypsinogen 2 (T2),
50and 30 ends were amplified by nested PCRs with
PRIMER 1 and specific primers (T25RACER1 and
T25RACER2), and PRIMER 2 and specific primers
(T2GT3-1F and T2GT3-2F), respectively (Table 2).
Table 1 Feeding schedule for grouper larval rearing
Day post-hatching Feeding schedule
2 ? 7 Oyster trochophores 3 times per day
6 ? 10 Rotifer screened through 200 mesh
net 4 times per day
11 ? 22 Rotifer screened through 150 mesh
net 4 times per day
17 ? 35 Copepods 4 times per day
35 ? 40 Shrimp paste (Litopenaeus vannamei)
41 ? 50 Semi-moist feed (mixed with shrimp
paste and feed powder at a ratio of 8:2)
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The PCR was performed in 50-ll reactions as
described above and under the following cycling
conditions: 30 cycles of denaturation at 94 �C for
1 min, annealing at 50 �C for 1 min, and elongation at
72 �C for 2 min, followed by a 10-min extension at
72 �C and cooling to 4 �C.
The PCR fragments were subjected to electropho-
resis on a 1.5 % agarose gel for length difference, and
all PCR-amplified cDNA fragments were cloned into
the PCRII TOPO vector of the TOPO TA cloning
system (Invitrogen) and transferred into Escherichia
coli cells according to the manufacturer’s protocol.
Recombinant bacteria were identified by blue/white
screening and confirmed by a PCR. Plasmids contain-
ing the insert were purified using the Wizard� Plus
Miniprep DNA Purification System (Promega) and
used as a template for DNA sequencing.
A nucleotide sequence analysis was performed
using the dideoxynucleotide chain termination method
(Sanger et al. 1977) on a DNA sequencer (Model
373A, Applied Biosystems, Lincoln, NE, USA).
Plasmid DNA at 1 lg was used for sequencing with
a Dye Terminator Cycle Sequencing Kit (Applied
Biosystems) and was subjected to electrophoresis on
6 % denaturing gels. Clones were sequenced with the
M13 forward and reverse primers. Trypsinogen gene
sequences were analyzed and compared using the
BLASTX and BLASTP search programs (http://blast.
genome.ad.jp) with a GenBank database search.
Multiple sequence alignments of grouper trypsinogen
genes were created using the ClustalW program
(http://align.genome.jp/).
Phylogenetic trees were constructed on the basis of
the proportion of amino acid differences (p-distances)
by the neighbor-joining (NJ) method (Saitou and Nei
1987) using MEGA 4 software (Kumar et al. 1993).
For phylogenetic tree construction, indels were
removed from multiple alignments. The reliability of
the tree obtained was assessed by bootstrapping using
1000 bootstrap replications (Felsenstein 1985).
Gene expression
For expression of the two trypsinogen genes in
different tissues and expression of two trypsinogen
and trypsin activity during early development by an
RT-PCR, 3 lg of total RNA from each tissue was
transcribed with oligo (dT). Specific primer pairs,
TI-F1/TI-R1 and TII-F1/TII-R2, were, respectively,
used for T1 and T2 fragment amplification, and the
primer pair, ActinF/ActinR, was used to amplify the
b-actin fragment as the internal control. The PCR
conditions were the same as those described above
except the respective annealing temperatures for T1,
T2, and b-actin were 49, 56, and 50 �C.
For the real-time PCR analysis, a SYBR green I
real-time PCR assay for transcription of the relative
grouper trypsinogens was carried out using an ABI
PRISM 7900 Sequence Detection System (Applied
Biosystems) according to the method described by Liu
et al. (2007a). The accuracy and reproducibility of the
real-time PCR assays were determined by running
standard curves. The amplification efficiency was
obtained from given slopes of the standard curve:
Eslop = 10(-1/slope) - 1. The slopes of T1, T2, and
b-actin were -3.2153, -3.3133, and -3.2186, which
Table 2 Primers used for full-length trypsinogen cDNA
cloning, and gene RT-PCR and real-time PCR
Primers Sequence (50 ? 30)
CTF1 AAGATYGTCGGAGGSTATGAGTG
CTR1 CCGTARCCCCAGGACACMACACC
T13-GTA-F1 CCTACCCTGGCATGATCACTG
T13-GTA-F2 TCGTGTGCAACGGTGAGCTTC
T15RACER1 GTGGAGCTCATGGTGTTG
T15RACER2 AGAGCCTCCACAGAAGTG
T2GT3-1F GCCACCCTCAACCAGTAC
T2GT3-2F ATTGACTACACCATGTTCTG
T25RACER1 GTGGAGCTCATGGTGTTG
T25RACER2 AGAGCCTCCACAGAAGTG
PRIMER2 TAGACTTAGAAATTAATACGACTC
ACTATAGGCGCGCCACCG
PRIMER1 TCATACACATACGATTTAGGTGACACTA
TAGAGCGGCCGCCTGCAGGAAA
Q-TIF4 CTGCCTCTTCAACGACTG
Q-TIR4 AGATGTAGGACTTTATTGACTCA
Q-TIIF2 CTATTAACTCCACATCCAACCT
Q-TIIR2 TGATTCCAGCAAAGACAAGA
TI-F1 CCTGGCATGATCACCAATG
TI-R1 GAACATGCTCGTTCAGATC
TII-F1 GGAGGCTCTCTGATCTCCAGC
TII-R1 TGTCATTGTCCAGGTTGCGGC
Q-actinF CTATTAACTCCACATCCAACCT
Q-actinR TGATTCCAGCAAAGACAAGA
ActinF TAGGTGGTCTCGTGGATGCC
ActinR GAGACCTTCAACACCCCCGC
204 Fish Physiol Biochem (2013) 39:201–214
123
correlated with respective amplification efficiencies of
104.7, 100.4, and 104.5 % (Fig. 1). All of them were
within the acceptable efficiency of 100 ± 10 %.
The respective primer pairs used for T1, T2, and
b-actin (internal control) for amplification were
Q-TIF4/-TIR4, Q-TIIF2/Q-TIIR2, and Q-actinF/Q-
actinR (Table 2). Amplifications were performed in a
96-well plate in a 25 ll reaction volume containing
12.5 ll of 29 SYBR Green Master Mix (PE Applied
Biosystems), 2.5 ll each of the forward and reverse
primers (10 mM), 1 ll of template (1 lg cDNA), and
9 ll of DEPC water. The thermal profile for the SYBR
green real-time PCR was 50 �C for 2 min and 95 �C
for 10 min followed by 40 cycles of 95 �C for 15 s and
60 �C for 1 min. Each sample was analyzed in
duplicate. Distilled water replaced the template as
the negative control. Relative mRNA expression of
target genes to the reference gene was calculated using
the 2-DDCt method (Livak and Schmittgen 2001). To
analyze trypsinogen expression during larval devel-
opment, relative expression of T1 and T2 from whole
larvae at 1–25 DPH and digestive tracts from larvae at
30–50 DPH was separately analyzed using the 2-DDCt
method. To calculate relative expression levels of T1
(A)
(C)
(B)
Y = 0.3214X - 3.2153
R2 = 0.99720
1
2
3
4
5
6
7
Ct
Lo
g (
dilu
tio
ns)
(D)
Y = 0.3326X - 3.3133
R2 = 0.99370
1
2
3
4
5
6
7
Ct
Lo
g (
dilu
tio
ns)
(E)
Y = 0.3251X - 3.2186
R2 = 0.99710
1
2
3
4
5
6
7
10 12 14 16 18 20 22 24 26 28 30
10 12 14 16 18 20 22 24 26 28 30
10 12 14 16 18 20 22 24 26 28 30
Ct
Lo
g (
dilu
tio
ns)
(F)
Fig. 1 Amplification efficiency determination via a standard
curve analysis. Amplification profiles for T1 (a), T2 (b), and b-
actin (c) generated by six quantities of cDNA, ranging from 4 to
0.00004 lg in tenfold decrements. T1 (d), T2 (e), and b-actin
(f) standard curves were generated by plotting the cycle
threshold value against the log of concentration
Fish Physiol Biochem (2013) 39:201–214 205
123
and T2, data were calibrated to whole larvae and
digestive tracts at 1 and 30 DPH, respectively.
Trypsin activity assay
The method for the trypsin activity assay was modified
from Liu et al. (2007b) using BAEE as a substrate.
Samples were individually homogenized in 250 ll of
50 mM Tris–HCl buffer (pH 8.0), and the homogenate
was centrifuged at 10,0009g for 30 min at 4 �C.
Supernatants were used to measure trypsin activity as
a crude enzyme solution. An enzyme solution at an
appropriate dilution (20 ll) was mixed with 0.6 ml of
0.5 mM BAEE in 50 mM Tris–HCl buffer (pH 8.0)
and 10 mM CaCl2, and then the increment in absor-
bance at 1 and 3 min was detected at 253 nm. One unit
of activity was defined as the amount causing an
increase of 1 in the absorbance at 253 nm per minute.
Statistical analysis
Experimental data were statistically analyzed by one-
way analysis of variance (ANOVA), and a multiple-
comparisons (Tukey’s) test was conducted to examine
significant differences among treatments using the
SAS computer software (SAS Institute, Cary, NC,
USA). Statistically significant differences required
p \ 0.05. A linear regression was used from Microsoft
Excel (Microsoft, Redmond, WA, USA) to study the
relationship between trypsinogen expression levels of
T1 and T2 and body weight.
Results
Molecular characterization of two grouper
trypsinogens
A 900-bp cDNA of T1 contained a 50-untranslated
region (UTR) of 14 bp, an open reading frame (ORF)
of 726 bp, and a 30-UTR of 160 bp with a stop codon
(TAA), a consensus polyadenylation signal
(AATAAA) 19 bp upstream from the poly A tail,
and a poly A tail of 27 bp. T2 with a full-length
sequence of 875 bp consisted of a 50-UTR of 24 bp, an
ORF of 732 bp, and a 30-UTR of 119 bp containing a
stop codon (TAA), a consensus polyadenylation signal
(AATAAA) 12 bp upstream from the poly A tail, and
a poly A tail of 20 bp. The T1 and T2 sequences were
deposited in GenBank under respective accession nos.
JN848593 and JN848594.
T1 and T2 appeared to contain all of the structural
features of eukaryotic mRNA transcripts. The nucle-
otide sequences of T1 and T2 were predicted to encode
the preproprotein of 242 and 244 amino acids (aa),
respectively, starting from the first methionine
(Fig. 2). As with all known trypsins, those of grouper
were also assumed to be synthesized as preproenzymes
Grouper T1 MKSLIFVLLIGAAFAT--EDDKIVGGYECTPHSQPHQVSLNSGYHFCGGSLVNENWVVSA Grouper T2 MKYFILLALFAAAYAAPIEDDKIVGGYECRKNSVAYQVSLNSGYHFCGGSLISSTWVVSA
Grouper T1 AHCYKSRVEVRLGEHNLRVTEGKEQFIRSSRVIRHPEYSSYNIDNDIMLIKLSEPATLNQ Grouper T2 AHCYKSRIQVRLGEHNIAVNEGTEQFINSARVIRHPSYNSRNLDNDIMLIKLSEPATLNQ
+Grouper T1 YVQPVALPTSCAPAGTMCTVSGWGNTMSSTADKNKLQCLDIPILSFEDCDNSYPGMITDA Grouper T2 YVQPVALPTSCAPAGTMCKVSGWGNTMSSTADSNRLQCLDIPILSDEDCERSYPGIIDYT
+Grouper T1 MFCAGYLEGGKDSCQGDSGGPVVCNGELQGVVSWGYGCAEKDHPGVYAKVCLFNDWLERT Grouper T2 MFCAGYLEGGKDSCQGDSGGPVVCNGELQGVVSWGYGCAEKDHPGVYSKVCVQTDWLLET L1 S1 S1 L2 S1
Grouper T1 MAKY Grouper T2 MASY
Fig. 2 Alignment of deduced amino acid sequences of the two
grouper trypsinogens. Identical residues are indicated by dots.
The T1 and T2 signal peptides are underlined. Vertical arrowsfrom the amino-terminus indicate the activation peptide
cleavage site. Residues forming the catalytic triad (His, Asp,
and Ser) are indicated by dots. Cysteine residues are marked
with stars. Two trypsin determinant residues are marked with
plus signs. Two surface loops (L1 and L2) and residues in the S1
binding pocket are, respectively, double-underlined and boxed.
Dashed lines indicate sequences that match the peptide
sequences of a purified trypsin from the pyloric cecum of
grouper in our previous study (Liu et al. 2012)
206 Fish Physiol Biochem (2013) 39:201–214
123
that contain an amino-terminal signal peptide followed
by a short activation peptide. The deduced amino acid
sequences of both grouper trypsinogens had a hydro-
phobic signal sequence of 15 residues as predicted by
SignalP. The trypsinogen activation peptides were 4
and 6 aa long in T1 and T2, respectively. The catalytic
triads of His-61, Asp-104, and Ser-198 in T1, and of
His-63, Asp-106, and Ser-200 in T2 were conserved in
both grouper trypsinogens. Also conserved in both
grouper trypsinogens were Asp-190 in T1 and Aps-192
in T2 at the bottom of the substrate-binding pocket,
Gly-213 and Gly 223 in T1, and Gly-215 and Gly 225
in T2 lining the sides of the binding pocket, Tyr-171 in
T1 and Tyr-173 in T2 involved in trypsin substrate
specificity, and 12 cysteine residues responsible for the
formation of six disulfide bonds. Two surface loops, L1
and L2, supporting the substrate-binding pocket were
both preserved in the two grouper trypsinogens. In
addition, the consensus repeat 196GDSGG200 in T1 and198GDSGG202 in T2, and a diagnostic repeat residue of
a serine protease around the active Ser site were found
in both trypsinogens.
The grouper T1 aa sequence demonstrated a
distribution of charged residues very similar to that
of grouper T2 (80.74 % identity). The calculated
molecular masses of T1 and T2 were 26.46 and
26.58 kDa, with respective estimated pI values of 5.20
and 5.06. The composition revealed a 47-aa substitu-
tion in total. The grand average hydropathicity indices
of T1 and T2, calculated using the hydropathicity scale
given by Kyte and Doolittle (1982), were estimated to
be -0.177 and -0.100, respectively. Based on the
results of pI and hydrophobicity, both grouper tryp-
sinogens appeared to be anionic.
A phylogenetic tree constructed by the NJ method
from a multiple sequence alignment of grouper
trypsinogens, and a range of other teleost counterparts
belonging to groups I, II, and III is shown in Fig. 3.
Both grouper trypsinogens were phylogenetically
related to group I of teleost anionic trypsinogens.
Tissue expression
Tissue expression of the two grouper trypsinogens as
analyzed by an RT-PCR is shown in Fig. 4. T1 was
abundantly expressed in the pyloric cecum, all intes-
tinal tissues, and spleen, but only slightly expressed in
other tested tissues except the stomach and blood. T2
was expressed in the digestive tract, including the
esophagus, stomach, pyloric cecum, anterior intestine,
middle intestine, hind intestine, and spleen.
From the RT-PCR results, both grouper trypsino-
gens were mainly synthesized in tissues of the pyloric
cecum, anterior intestine, middle intestine, hind
intestine, and spleen. Expression levels of the two
trypsinogens in these tissues were analyzed by a real-
time PCR. Among all tested tissues, relative expres-
sion of T1 in the pyloric cecum and anterior intestine
was significantly higher compared with those of other
selected tissues. Relative expression of T1 in the
pyloric cecum and anterior intestine was 165.0 ±
25.2-fold and 110.9 ± 44.8-fold higher, respectively,
than T1 expression in the spleen (Fig. 5a). T2 had a
similar expression profile to T1. Nevertheless, even if
T2 showed higher expression levels in the pyloric
cecum and anterior intestine, it did not significantly
differ from those of the middle intestine and hind
intestine. Relative expression of T2 in the pyloric
cecum and anterior intestine were, respectively,
1469.0 ± 298.4-fold and 1639.0 ± 198.9-fold higher
compared with the expression of T2 in the spleen
(Fig. 5b).
Relationship of T1 and T2 expression
with body weight
Relationship between the expression of the two
trypsinogen genes and grouper body weight are shown
in Fig. 6. Fish within a size range of 26.35–179.1 g
had increased DCt values of T1 and T2 in all tissues,
including the pyloric cecum, anterior intestine, middle
intestine, and hind intestine with an increase in body
weight. As the copy number of the target gene and Ct
values were inversely related, a sample containing a
higher number of copies of the target gene had a lower
Ct value than that of a sample with a lower number of
copies of the same target. Therefore, expression of T1
and T2 in the pyloric cecum, anterior intestine, middle
intestine, and hind intestine decreased with increased
body weight. However, the expression of trypsinogen
exhibited individual differences resulting in insignif-
icant differences among fish of different sizes.
Expression of the two trypsinogens during early
grouper development
Grouper larvae showed slow development before 8
DPH. Thereafter, exponential growths in total length
Fish Physiol Biochem (2013) 39:201–214 207
123
and body weight were found in larvae from 12 DPH
until the end of the study at 50 DPH (Fig. 7).
Expression analyses of the two trypsinogens during
early development of grouper by an RT-PCR are
shown in Fig. 8. No amplified fragment of grouper
trypsinogens by the RT-PCR was detected in fertilized
eggs or larvae before 12 h post-hatching. T2 tran-
scription was first detected in larvae at 1 DPH.
Although T1 transcription was not detected at 1
DPH by the RT-PCR, it was detected at 1 DPH by the
more sensitive method of a real-time PCR (Fig. 9).
T1 mRNA detected by the real-time PCR is
shown in Fig. 9a. A steady-state transcript level of
T1 was found in larvae during 1–25 DPH. Increased
expression of T1 was quantified in larvae at 35–50
DPH compared with larvae at 30 DPH (Fig. 9a). T2
showed a gene expression profile similar to that of
T1 with a constant steady-state expression during
1–25 DPH. T2 showed a sharp increase in expression
after 45 DPH (Fig. 9b). The expression of b-actin did
not significantly differ in larvae at 1–25 and 35–50
DPH.
Gro
up
I G
rou
p II
G
rou
p II
I
Fig. 3 Phylogenic
relationship among full-
length amino acid sequences
of trypsinogens from a wide
range of teleosts using the
neighbor-joining (NJ)
method. Taxon names are
shown as common names of
the species plus their
corresponding GenBank
accession numbers. The
scale for the branch length is
shown below the tree.
Sequences of grouper
trypsinogens are shown as
orange-spotted grouper T1
and T2
208 Fish Physiol Biochem (2013) 39:201–214
123
An interesting variation in trypsin activity was
observed during grouper larval development. Rela-
tively high trypsin activity was detected in larvae with
a yolk sac at 1 DPH, and then trypsin activity
significantly decreased at the end of the yolk sac
absorption phase at 2 DPH (Fig. 10). Trypsin activity
in larvae fed oyster trochophores (2–5 DPH) sharply
increased from 0.38 ± 0.06 U/mg at 2 DPH to
1.53 ± 0.37 U/mg at 4 DPH and then decreased
significantly to 0.14 ± 0.01 U/mg in larvae fed SS-
type rotifers at 8 DPH. After 8 DPH, trypsin activity
did not significantly change in larvae until 25 DPH. In
the metamorphosis phase, trypsin activity significantly
increased after 40 DPH.
Discussion
Trypsin plays an important role in protein digestion
and growth of marine fish larvae (Cahu and Zambon-
ino-Infante 1994; Moyano et al. 1996; Fujii et al. 2007;
Manchado et al. 2008). In this work, two full-length
trypsinogen isoforms were cloned and identified in the
pyloric cecum of orange-spotted grouper. Nucleotide
sequences of the coding regions of T1 and T2 shared
70.74 % nucleotide sequence identity, whereas the
amino acid sequence identity of the encoded proteins
was 80.74 %. In our previous study, a trypsin was
purified from the pyloric cecum of E. coioides (Liu
et al. 2012) in which two fragments of the peptide
sequence were identified (LGEHNI and NLDN-
DIML), and it was suggested that the purified trypsin
was T2 when aligned with grouper T1 and T2
sequences. Both of them had completely conserved
catalytic triad residues of His, Asp, and Ser (His-61,
Asp-104, and Ser-198 in T1, and His-63, Asp-106, and
Ser-200 in T2). The amino acids generating the S1
substrate-binding pocket were of a typical trypsin
nature in both grouper sequences with Asp (Asp-190
in T1 and Aps-192 in T2) at the bottom and two Gly
residues (Gly-213 and Gly 223 in T1, and Gly-215 and
Gly 225 in T2) lining the sides of the pocket. The
consensus repeat, GDSGG, around the active site, Ser,
is usually diagnostic of a serine protease (Krem et al.
1999), which was also well conserved in both grouper
trypsinogens (196GDSGG200 in T1 and 198GDSGG202
in T2). The Tyr residue (Tyr-171 of T1 and Tyr-173 of
T2) was shown to be a key residue in determining
substrate specificity of trypsins (Hedstrom et al. 1994),
Fig. 4 Expression of grouper trypsinogens, T1 (a) and T2 (b),
and b-actin (c) in the esophagus (lane 1), stomach (lane 2),
pyloric cecum (lane 3), anterior intestine (lane 4), middle
intestine (lane 5), hind intestine (lane 6), eye (lane 7), liver (lane8), gills (lane 9), skin (lane 10), heart (lane 11), head kidney
(lane 12), mid-kidney (lane 13), hind kidney (lane 14), spleen
(lane 15), brain (lane 16), dorsal muscle (lane 17), and blood
(lane 18) as analyzed by RT-PCR. M: 100-bp DNA ladder
marker
020406080
100120140160180200
Pyloricceca
Anteriorintestine
Middleintestine
Hindintestine
Spleen
Rel
ativ
e ex
pre
ssio
n
(A)a
bbb
a
0200400600800
100012001400160018002000
Pyloricceca
Anteriorintestine
Middleintestine
Hindintestine
Spleen
Tissues
Rel
ativ
e ex
pre
ssio
n
(B)a
ab
a
ab
b
Fig. 5 Relative expression of T1 (a) and T2 (b) in different
tissues of grouper. Data (mean ± SE) with different letters
among different tissues significantly differed (p \ 0.05)
Fish Physiol Biochem (2013) 39:201–214 209
123
and the two loops supporting the substrate-binding
pocket (Hedstrom et al. 1992) were also conserved in
grouper trypsins as in other trypsins. In addition, two
surface loops supporting the substrate-binding pocket
and 12 cysteine residues generating six disulfide
bridges were highly conserved in both grouper tryp-
sins, which suggests that both paralogous genes are
functional.
Trypsin is activated after its secretion into the gut
via the removal of a short, highly charged activation
peptide by enterokinase, which prevents trypsinogen
from being accidentally activated within the pancreas
(Gudmundsdottir et al. 1993; Manchado et al. 2008).
Different trypsinogen genes were identified in teleos-
tean fishes (Gudmundsdottir et al. 1993; Liu et al.
2007b; Manchado et al. 2008; Ruan et al. 2010). The
Y = 0.0261X - 15.26 (R2 = 0.1892)-22-20-18-16-14-12-10
-8-6-4-2
0 20 40 60 80 100 120 140 160 180 200
ΔC
T
(E)
Y = 0.0138X - 7.2498 (R2 = 0.1304)-10
-9
-8
-7
-6
-5
-4
-3
-2
0 20 40 60 80 100 120 140 160 180 200Δ
CT
(F)
Y = 0.0173X - 7.8329 (R2 = 0.1793)-12
-10
-8
-6
-4
-2
0
0 20 40 60 80 100 120 140 160 180 200
ΔC
T(G)
Y = 0.0229X - 4.6275 (R2 = 0.2532)-7-6-5-4-3-2-1012
0 20 40 60 80 100 120 140 160 180 200
Body weight (g)
ΔC
T
(H)
Y = 0.0255X - 1.4617 (R2 = 0.1721)
-8
-6
-4
-2
0
2
4
6
8
0 20 40 60 80 100 120 140 160 180 200
ΔC
T(A)
Y = 0.0168X + 5.8241 (R2 = 0.1128)0
2
4
6
8
10
12
0 20 40 60 80 100 120 140 160 180 200
ΔC
T
(B)
Y = 0.0233X + 5.7639 (R2 = 0.2177 )0
2
4
6
8
10
12
14
0 20 40 60 80 100 120 140 160 180 200
ΔC
T
(C)
Y = 0.0356X + 7.0735 (R2 = 0.2064)02468
101214161820
0 20 40 60 80 100 120 140 160 180 200
Body weight (g)
ΔC
T
(D)
Fig. 6 Analysis of relationship of body weight with T1 and T2 expression in the pyloric cecum (a or e), anterior intestine (b or f),middle intestine (c and g), and hind intestine (d or h)
210 Fish Physiol Biochem (2013) 39:201–214
123
enzyme cleaves the activation peptide in the presence
of two acidic residues at P2 and P3 and an alkaline
residue, Lys or Arg, at P1 (Chen et al. 2003). The
activation peptide usually possesses three or four
acidic resides, Asp and Glu in groups I and II of many
teleostean fish, whereas most mammalian trypsino-
gens have four continuously arranged Asp residues
before Lys-P1 (Chen et al. 2003). This seems to be the
case for grouper T1 and T2 with three acidic residues
preceding Lys-P1, which differs from the characters of
group III trypsinogen by activation peptides possess-
ing an Arg at P1 and a deletion or a substitution of Asp
at P2 (Chen et al. 2003). In addition, both grouper
trypsinogens appeared to be anionic. This is similar to
group I trypsins that are usually, but not always,
anionic at physiologic pH, whereas group II trypsins
are usually, but not always, cationic at physiologic pH,
and group III trypsins represent a rapidly evolving
group of extremely psychrophilic enzymes (Roach
et al. 1997; Roach 2002). Those data are in agreement
with the phylogenetic analysis demonstrating that both
T1 and T2 of the grouper belong to group I
trypsinogens.
The RT-PCR analysis demonstrated that trypsino-
gen was synthesized in almost all selected tissues.
Similar results of wide expression of trypsinogens in
different tissues were also found in other fishes (Braun
et al. 1990; Lilleeng et al. 2007). Different expression
in multiple tissues may involve different functions,
0
0.5
1.0
1.5
2.0
2.5
3.0
3.5
4.0
4.5
0 5 10 15 20 25 30 35 40 45 50
Day post hatching
Tota
l len
gth
(cm
)
0.0
0.2
0.4
0.6
0.8
1.0
1.2
Total length
Body weight
Fig. 7 Mean body weight and total length of orange-spotted
grouper larvae during the experiment
Fig. 8 RT-PCR detection of T1 (a), T2 (b), and b-actin (c) gene
expression at different life stages of the egg (lane 1), and larvae
of 0 (lane 2), 2 (lane 3), 4 (lane 4), 6 (lane 5), and 12 h (lane 6),
and 1 (lane 7), 2 (fed larvae, lane 8; unfed larvae, lane 9), 3 (fed
larvae, lane 10; unfed larvae, lane 11), and 4 (lane 12) days post-
hatching. Lane M: 100-bp ladder DNA marker
05
10152025303540455055
0 5 10 15 20 25 30 35 40 45 50
Rel
ativ
e ex
pre
ssio
n Whole larva
Digestive tract only
xaa
y
y
y
y
aaa
aa a a
(A)
y
05
10152025303540455055
Day post hatchingR
elat
ive
exp
ress
ion
(B) Digestive tract only
Whole larva
x x
y
y
z
aaaaaaaaa
0 5 10 15 20 25 30 35 40 45 50
Fig. 9 Relative expression of T1 (a) and T2 (b) during grouper
larval development quantified by an SYBR Green real-time RT-
PCR. Data (mean ± S.E.) with different letters during 1–25 or
30–50 DPH (x, y) significantly differed (p \ 0.05)
0.0
0.4
0.8
1.2
1.6
2.0
2.4
0 5 10 15 20 25 30 35 40 45 50
Day post hatching
Tryp
sin
act
ivit
y (U
/mg
) Whole larva Digestive tract only
yy
xxxcdcd
ddd
c
b
b
a
Fig. 10 Enzymatic activity of trypsin during grouper larval
development. Data (mean ± S.E.) with different letters (a, b, c,
d) during 1–25 day post-hatching (DPH) and (x, y) during 30–50
DPH significantly differed (p \ 0.05)
Fish Physiol Biochem (2013) 39:201–214 211
123
such as involvement in ionic regulation in nephrons
(Nesterov et al. 2008). However, the expression of T2
was only detected in digestion-related tissues of the
esophagus, stomach, pyloric cecum, anterior intestine,
middle intestine, hind intestine, and spleen, while T1
was widely expressed in almost all sampled tissues.
Therefore, it is thought that T2 might play a more
relevant role in the digestive function of proteins. On
the other hand, the pancreas is dispersed in the
intestinal mesentery of fish (Ostaszewska et al. 2006).
Both trypsinogen genes detected in intestinal samples
may be (at least partially) pancreatic. It is considered
that in situ hybridization could be used to determine
whether there is indeed pancreatic tissue and pancre-
atic expression.
Trypsin activity was reported to be positively
correlated with the fish growth rate in previous studies
of Atlantic cod, G. morhua (Lemieux et al. 1999), and
Atlantic salmon, S. salar (Rungruangsak-Torrissen
et al. 2006). It was also used as an indicator to evaluate
the nutritional condition and is considered to be the
main proteolytic enzyme of marine fish larvae that
lack a morphological stomach (Govoni et al. 1986;
Moyano et al. 1996; Gawlicka et al. 2000; Eusebio
et al. 2004; Darias et al. 2007; Fujii et al. 2007).
However, a different result in our previous study
showed that trypsin activity in the pyloric cecum of
E. coioides was not positively related to the fish body
weight (Liu et al. 2012), which is in agreement with
the results of the relationship between trypsinogen
mRNA expression and fish body weight in the present
study. The different expression patterns of trypsin in
grouper could be caused by zymogen activation in
ingested food rather than direct digestion of food
(Oozeki and Bailey 1995), and other proteinases, such
as pepsin (Feng et al. 2008), play more important roles
than trypsin in protein digestion in the growing
grouper.
A low survival rate and slow growth during larval
development of E. coioides are major problems
encountered by fish farms culturing grouper (Pierre
et al. 2008). In this study, early larval stages had a very
small size, and larval development presented insig-
nificant increments in body weight and total length
before 8 DPH; therefore, the larval period is very long.
With the production of grouper larvae in this study,
7.68 and 10.73 % survival rates were found with the
two feeding treatments which are higher than the
average survival rates of grouper breeding in practice.
In the period of 2–30 DPH, grouper undergo the
process of mouth-opening, followed by metamorpho-
sis, which are two critical stages with high mortality,
induced by some unknown factors, such as disease or
food. Expression and activity of trypsin in Lutjanus
guttatus were detected at hatching at very low levels
and concomitantly increased with larval development
(Galaviz et al. 2012), which agreed with other findings
in previous studies (Oozeki and Bailey 1995; Moyano
et al. 1996; Murray et al. 2006; Alvarez-Gonzalez
et al. 2010). In this study, trypsin activity was detected
in larvae before the first feeding consistent with the
result shown by Zambonino-Infante and Cahu (1994),
who reported enzymatic activities of trypsin and other
digestive enzymes in Dicentrarchus labrax at 4 DPH,
while the first feeding occurred at 6 DPH. This
suggests that enzyme activity is derived from genet-
ically preprogrammed expression and not by the first
exogenous feeding (Lazo et al. 2000; Zambonion-
Infante and Cahu 2001). The opening of the mouth
began at 2–3 DPH, in grouper larvae at 2–3 mm.
Trypsin activity of larvae increased after feeding with
oyster trochophores, but expression of T1 and T2 was
low. The increased trypsin activity may be considered
to be due to the secretion of pancreatic enzymes in the
intestinal lumen during the first 3 weeks of larval life
(Zambonino-Infante and Cahu 2001). In addition, a
relatively higher trypsin activity of 3.14 ± 0.30 U/mg
was detected in oyster trochophores compared with
trypsin activity in larvae, which may be involved in
activating other pancreatic digestive zymogens
including trypsinogens (Chen et al. 2003), leading to
the increase in trypsin activity after the first feeding. In
L. guttatus larvae, the peak of trypsin expression
preceded that of specific activity and generally
coincided with changes in the food supply. According
to profiles of trypsin activity and trypsinogen expres-
sion, the pancreas was fully functional after 25 DPH
since the maximum trypsinogen expression occurred
at 25 DPH, and maximum levels of trypsin activity
occurred at 35 DPH (Galaviz et al. 2012). An increase
in trypsinogen expression preceding that of trypsin
activity was also found in grouper larvae. Expression
of T1 and T2, respectively, increased after 35 and 40
DPH, whereas increased trypsin activity was found
after 40 DPH. Larvae of E. coioides after 30 DPH
underwent metamorphosis with a developing stomach
and pyloric cecum (Eusebio et al. 2004), and changes
in the structure of the digestive system seemed to
212 Fish Physiol Biochem (2013) 39:201–214
123
result in significant increases in trypsin activity and
trypsinogen expression.
In conclusion, two trypsinogens were cloned from
E. coioides. The phylogenetic analysis classified them
as group I trypsinogens. T2 is considered to play a
more relevant role in digestive function since it was
only found in digestive tissues. Larvae are able to
synthesize trypsinogen at 1 DPH before the first
feeding, and the increased trypsin activity after the
first feeding may be required to digest food. Increased
trypsinogen expression and trypsin activity after 30
DPH were mostly related to metamorphosis with a
developing stomach and pyloric cecum.
Acknowledgments This research was supported by a grant
from the National Science Council (NSC99-2313-B-020-005-
MY3), Taiwan. The authors thank Sian-Ru Fu and Jhih-Syuan
Chen who assisted with carrying out this project.
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