Journal of Biosciences and Medicines, 2014, 2, 54-62
Published Online June 2014 in SciRes. http://www.scirp.org/journal/jbm
http://dx.doi.org/10.4236/jbm.2014.24009
How to cite this paper: Kantharaju, S. and Siddalinga Murthy, K.R. (2014) Characterization of Esterases of Tamarindus indi-
ca Seeds. Journal of Biosciences and Medicines, 2, 54-62. http://dx.doi.org/10.4236/jbm.2014.24009
Characterization of Esterases of Tamarindus
indica See ds
S. Kantharaju, K. R. Siddalinga Murthy
Department of Biochemistry, Central College Campus, Bangalore University, Bangalore, Karnataka, India
Received February 2014
Abstract
Germinating seeds of Tamarindus indica synthesizes various enzymes which are required for
the degradation of seed reserves such as xyloglucans, fatty acid esters and proteins. Among
these, esterases, belonging to a group of hydrolytic enzymes catalyze the hydrolysis of various
types of esters. They play an important role in cell expansion as well as detoxification of xeno-
biotics and many agrochemicals and insecticides. The esterases are extracted from the germi-
nating tamarind seeds using 50 mM phosphate buffer, pH 7. The Km with α-naphthyl acetate as
the substrate is 19.23 µM and the enzymes are optimally active at pH 7.0 to 7.5 and are stable
between pH 5.0 to 9.0. The optimum temperature of esterase activity of tamarind seed is be-
tween 37˚C - 50˚C and is stable up to 40˚C. The activity d ecl ined by 30% at 60˚C and about 90% at
70˚C. Highest esterase activity and specific activity are observed on the 21st day of germination.
The polyacrylamide gel electrophoresis (PAGE) indicated the presence of nine isozymes of este-
rases. Band numbers 1, 5 and 6 are the major esterolytic bands present throughout the germi-
nation period while band numbers 2 & 3 are minor bands present only during the latter period
of the germination. Based on substrate and inhibitor specificity in conjunction with electropho-
resis, the esterases 1 to 8 have been classified as carboxylesterases sensitive to organophos-
phate inhibitor (OP) and PCMB (p-chloromercuribenzoate) while esterase 9 is classified as car-
boxylesterase sensitive to OP. These esterases are unaffected by carbamate inhibitor, eserine
sulphate.
Keywords
Tamarindus indica, Ge rminat ion, Esterase, α-Nap h th ylac et at e, p-C hlor omercu ribenzo ate,
Eserine Sulphate, Dichlorv os
1. Introduction
Esterases are an important group of hydrolytic enzymes, catalyzing the hydrolysis of various endogenous and
exogenous short chain carboxyl esters. They are widely distributed in nature and occur in multiple molecular
forms and exhibit broad substrate specificity [1]. Esterases play an important role in the metabolism and detox-
ification of agrochemicals. In particular, carboxylesterases play an important role in agrochemical efficacy and
detoxification by interacting with two major classes of agrochemicals, organophospate (OP) insecticides and

S. Kantharaju, K. R. Siddalinga Murthy
55
pyrethroids [2]-[4]. The variability in esterase levels and relative isozyme abundance contributes to the selective
toxicity of ester-containing insecticides in a range of organisms, from fish to insects and mammals. In animals,
OP and carbamate insecticides exhibit their toxicity by irreversibly inhibiting acetylcholinesterase causing the
disruption of the nerve impulse transmission due to the buildup of the neurotransmitter acetylcholine. In plants,
esterases acts as an insecticide sink and protect insect acetylcholinesterases from OP/carbamate mediated toxic-
ity. The present investigation was carried out to study the variation in esterase activity during the germination of
tamarind seeds and characterize the esterases.
2. Materials and Method
2.1. Materials
BSA, gl yci ne , tris, phosphoric acid, hydrochloric acid, glycerol, methanol, acetic acid, bromophenol blue, acetic
acid, sodium dihydrogen phosphate, disodium hydrogen phosphate, α-naphthyl acetate, diazo blue B, Fast Blue
RR, acrylaminde, methylene bisacrylamide are of analytical grade obtained from Sisco Research Laboratories
Pvt. Ltd., India.
The seeds of Tamarindus indica are collected using random sampling technique (RST) from local areas of
Bangalore district, Karnataka State, India, during February to May. After dehulling the seeds, immature and
damaged seeds are removed and the mature seeds washed under tap water, dried and stored under refrigeration
in plastic containers until further use. From this bulk population sample, subsamples are obtained.
2.2. Methods
2.2.1. Germination Studies
Healthy Tamarind seeds (one hundred) are soaked in cold 50% H2SO4 for 60 mins and then washed thoroughly
with distilled water and dispensed into the soil (1:1 ratio of acid washed sand and cocco peat). The seeds are
germinated and the endosperms are collected every alternate day starting from 1st day till 25th d ay.
2.2.2. Extraction of Ester ase
A 10% extract of the endosperm (at an interval of every 24 hours during germination) are prepared in 0.05 M
phosphate buffer pH 7.0, by blending in a mixer for 5 mins and centrifuged at 10,000 rpm for 15 mins at 4˚C.
The resulting supernatant was used for the analysis of esterases and proteins.
2.2.3. Enzyme Assay
Esterase activity using α-naphthylacetate (a stock solution of 0.03 M α-naphthyl acetate in acetone was prepared
and diluted 100 times in 0.033 M phosphate buffer, pH 7.0, just before assay) as a substrate was determined [5]
[6] 1.0 ml of suitably diluted enzyme extract was added to 5.0 ml of the substrate and incubated for exactly 15
mins at 25˚C. The reaction is stopped by the addition of 1.0 ml of DBLS reagent (5% SDS and 1% diazo blue B
mixed in the ratio 5: 2, just before use). One unit of enzyme activity is defined as the amount of enzyme that re-
leases one µmol of α-naphthol per min at pH 7.0 and 25˚C.
2.2.4. Protein Estimation
Protein was quantitatively estimated using bovine serum albumin (BSA) as standard [7].
2.3. Kinetic Parameters
2.3.1. Effect of Ti me
Effect of time on the crude enzyme extract (15 day endosperm extract) from the seeds of tamarind is carried out
by incubating with α-naphthyl acetate for different time intervals and assayed as described above.
2.3.2. Effect of Substrate Concentration
The endosperm extract is assayed for esterase by incubating with different concentration of the substrate,
α-naphthyl acetate for 15 mins as described above. Km and Vmax for esterase is determined by construction of
LB-plot.

S. Kantharaju, K. R. Siddalinga Murthy
56
2.3.3. pH Optima
The endosperm extract is assayed, using α-naphthyl acetate in 50 mM buffers of different pH (acetate buffer pH
4.0, 4.5, 5.0 and 5.5, phosphate buffer pH 6.0, 6.5, 7.0 and 7.5, Tris-HCl buffer pH 8.0, 8.5 and 9.0 and carbo-
nate buffer pH 9.5, 10.0, 10.5 and 11.0) as described above.
2.3.4. pH Stability
The endosperm extract is pre-incubated with 50 mM buffers of different pH (acetate buffer pH 4.0, 4.5, 5.0 and
5.5, phosphate buffer pH 6.0, 6.5, 7.0 and 7.5, Tris-HCl buffer pH 8.0, 8.5 and 9.0, carbonate buffer pH 9.5, 10.0,
10.5 and 11.0) for 2 hrs at 4˚C. A known aliquots from the pre–incubated samples were removed and assayed as
described above at an optimum pH of 7.0.
2.3.5. Temperature Optima
The optimum temperature is determined by assaying the endosperm extract at different temperatures, such as,
5˚C, 10˚C, 17˚C, 22˚C, 27˚C, 32˚C, 37˚C, 42˚C, 47˚C, 52˚C, 60˚C, 70˚C and 80˚C using α-naphthyl acetate as
the substrate, for 15 mins.
2.3.6. Temperature Stability
The endosperm extract is pre-incubated at different temperatures, such as, 5˚C, 10˚C, 17˚C, 22˚C, 27˚C, 32˚C,
37˚C, 42˚C, 47˚C, 52˚C, 60˚C, 70˚C and 80˚C for 30 mins, rapidly cooled to 0˚C and assayed using α-naphthyl
acetate at 25˚C, as described above.
2.3.7. Polyacrylamide Gel Electrophoresis (PAG E)
Polyacrylamide gel electrophoresis (PAGE) was performed essentially [8] [9] at pH 8.9. A discontinuous vertic-
al slab gel system (8 cm × 8 cm) containing 10% separating gel and 4.5% spacer gel was used. An aliquot of the
enzyme extract suitably diluted with 40% glycerol solution containing bromophenol blue was carefully layered
into the wells and subjected to electrophoresis for 2 hrs at 10˚C maintaining a current of 20 mA.
2.3.8. Staining for Esterase Activity
Esterase activities on polyacrylamide gels are detected by the method of Hunter and Markert [10]. The electro-
phoresed gels were placed in 100 ml of 0.1 M sodium phosphate buffer, pH 7.0, containing 40 mg Fast Blue RR
salt and 20 mg α-naphthyl acetate in 1 ml acetone, for 15 minutes at 37˚C. The gels are stored in 7% acetic acid.
2.3.9. Inhibition Studies
Inhibition studies are carried out employing colorimetric method. Suitably diluted enzyme extract (0.5 ml) is
pre-incubated with 0.5 ml of different concentrations (1 × 10–3 to 1 × 10–10 M) of organophosphate (dicholrvos),
carbamates (eserine sulphate) and sulphydryl (PCMB) inhibitors for 30 mins at 27˚C. The residual esterase ac-
tivity is then assayed using 5.0 ml of α-naphthyl acetate as described above.
2.3.10. Inhibition Studies Employing PAGE
The effect of different inhibitors (dichlorvos, eserine sulphate and PCMB) on the esterases separated after elec-
trophoresis is studied by pre-incubating the gels in different inhibitor solutions (1 × 10–5 M) for 30 mins, fol-
lowed by thorough washing of the gels with 0.05 M phosphate buffer, pH 7.0 and staining for esterase activity
as described above.
3. Result
Preliminary experiments are carried out to determine the standard conditions for the assay of esterases from the
tamarind seed extract. The esterase activity of the crude enzyme extract is linear up to 50 µg protein (Figure 1)
and 50 mins (Figure 2). Km is a measure of the affinity of an enzyme for a particular substrate. The Km value
of esterase extract with α-naphthyl acetate as substrate is found be 19.23 µM (Figure 3 and Figure 4). The pH
optima of plant esterases usually lie in the range of 4 to 9. The pH optima of tamarind seed esterase is 7.0 to 7.5
(Figure 5) and is stable between pH 5.0 to 9.0 (Fig u r e 6). The optimum temperature of esterase activity of ta-
marind seed is between 37˚C - 50˚C (Figur e 7) and is stable up to 40˚C. The activity declined by 30% at 60˚C
and about 90% at 70˚C (Fi g u re 8).

S. Kantharaju, K. R. Siddalinga Murthy
57
Figure 1 . Effect of protein concentration on esterase activity.
Figure 2. Time curve for esterase.
Figure 3. Effect of substrate concentration on esterase activity.
The tamarind seeds are germinated for 25 days and the changes in total esterase activity, specific activity and
protein are followed every alternate day (F igure 9). Analysis of the total esterase activity pattern during germi-
nation of the endosperm showed highest activity on 5th day, 11th to 15th day and 21st day of germination and
lowest activity on 7th and 9th day and 17th and 19th day. They exhibited a constant cyclic increase and decrease of
total activity during the germination period. The specific activity was maximum on 21st day of germination and
exhibited a cyclic increase and decrease of specific activity during the germination period similar to total activi-
ty. However, the specific activity constantly increased during the whole germination period reaching a maxi-

S. Kantharaju, K. R. Siddalinga Murthy
58
Figure 4. Km & Vmax of esterase.
Figure 5. Effect of pH on esterase activity.
Figure 6. pH stability of esterase.
Figure 7. Effect of temperature on esterase activity.

S. Kantharaju, K. R. Siddalinga Murthy
59
Figure 8. Temperature stability of esterase.
Figure 9. Germination profile of esterase.
mum on 21st day. The total protein of the endosperm is maximum on 1st and 5th day of germination and exhibited
a cyclic increase and decrease during the germination period similar to total esterase activity. However, in con-
trast to the specific activity which continuously increased during the germination period, the protein conti-
nuously decreased during the germination period reaching a minimum on 19th day. The effect of continuous de-
crease in protein and a constant increase and decrease in total esterase activity resulted in a continuous increase
in specific activity during the germination period.
Electrophoretic analysis of the esterase activity during the germination from 1st to 25th day is shown in Fig ure
10. Totally nine isozymes were separated by PAGE. The bands were numbered consecutively from the anodic
end of the gel. Band number 1, 4, 5, 6 and 9 are present on all the days while band numbers 2 & 3 were minor
bands present only during the latter period of the germination. Band numbers 1, 5 and 6 were the major estero-
lytic bands present throughout the germination period.
Highe st esterase activity and specific activity and very low protein content were present in the endosperms on
21st day of germination. Hence, 21-day-old germinated endosperms were used to characterize the esterases. The
plots of pI (inhibitor concentration) versus percent inhibition of the esterases with dichlorvos, PCMB and esi-
rene sulphate is presented in Figure 11. Single sigmoidal curves are obtained with both the organophosphate
and PCMB, while eserine sulphate did not affect the activity of esterases. Dichlorvos completely inhibited the
esterases activity at pI 5, while with PCMB only 50% activity is inhibited. The I50 of dichlorvos and PCMB are
in the range of pI 6 to 7 and pI 5, respectively.
The results of inhibition studies in conjunction with electrophoresis are shown in F igure 12. The esterolytic
bands 1 to 8 are completely inhibited by OP inhibitor PCMBs, while band 9 is inhibited only by OP inhibitor.
However, all the bands are resistant to carbamate inhibitor, eserine sulphate.

S. Kantharaju, K. R. Siddalinga Murthy
60
Figure 10. Electrophoretic pattern of esterase during germination of tamarind seeds.
Figure 11. Effect of Inhibitors on esterase activity.
Figure 12. PAGE of effect of Inhibitors on esterase activity.
4. Discussion
The esterases have been extracted from plants using various buffer systems and phosphate buffer, pH 7, is found
to be ideal for the extraction [11]. During the germination of seeds, there is continuous synthesis and/or degra-
dation of specific enzymes and structural proteins. The appearance of new or increased enzyme activity results
from either the de novo synthesis of the enzyme molecule or the activation of a pre-existing enzyme precursor.
Non-specific esterases represent a large, diverse and complex group of major hydrolytic enzymes and posses
the property of overlapping substrate specificity, hydrolysing both endogenous and exogenous esters of widely
differing structures leading to problems of identification and classification [12] [13]. Generally esterases have
been classified into three types based on their interactions with inhibitors [14]. Carboxylesterases are inhibited

S. Kantharaju, K. R. Siddalinga Murthy
61
by OP while cholinesterases are inhibited by both OP and carbamate inhibitors. However, arylesterases are not
inhibited by OP but hydrolyze OP while acetylesterases are not inhibited by OP or do not hydrolyze OP.
A subsequent elaboration of the Aldridge and Reiner [14] scheme has been used to classify esterase isozymes
detected after native PAGE and stained with various artificial ester substrates, in conjunction with organophos-
phate (OP), sulfhydryl, and the carbamate inhibitors [15]-[17]. Based on the above studies, the esterases from
the tamarind seeds have been classified as carboxylesterases and carboxylesterases sensitive to sulphydryl inhi-
bitors. Similarly on the basis of above criteria, two purified Mucuna pruriens seed esterases (MEIII and ME-IV)
separated by PAGE were stained with 1-naphthyl acetate in conjunction with OPs, carbamates and sulphydryl
inhibitors and the esterases were classified as carboxylesterases. Similar observations were noticed in case of
insect carboxylesterases [18] [19].
Acknowledgements
We acknowledge University Grant Commission, New Delhi, for providing Fellowship and DOS in Biochemistry,
Bangalore University, Bangalore for offering facilities to carry out the research work.
References
[1] Jung, Y.J., Lee, J.K., Sung, C.G., Oh, T.K. and Kima, H.K. (2003) Nonionic Detergent Induced Activation of an Este-
rase from Bacillus megaterium 20-1. Journal of Molecular Catalysis B: Enzymatic, 26 , 223-229.
http://dx.doi.org/10.1016/j.molcatb.2003.06.006
[2] Potter, P.M. and Wadkins, R.M. (2006) Carboxylesterases: Detoxifying Enzymes and Targets for Drug Therapy. Cur-
rent Medicinal Chemistry, 13, 1045-1054. http://dx.doi.org/10.2174/092986706776360969
[3] Abernathy, C.O. and Casi da, J.E. (1973) Pyrethroid Insecticides: Esterase Cleavage in Relation to Selective Toxicity.
Science, 179 , 1235-1236. http://dx.doi.org/10.1126/science.179.4079.1235
[4] Wheelock, C.E., Miller, J.L., Miller, M.G., Shan, G., Gee, S.J. and Hammo ck, B.D. (2004) Development of Toxicity
Identification Evaluation (TIE) Procedures for Pyrethroid Detection Using Esterase Activity. Environmental Toxicolo-
gy and Chemistry, 23, 2699-2708 . http://dx.doi.org/10.1897/03-544
[5] Gomori, G. (1953) Human Esterases. Journal of Laboratory and Clinical Medicine, 42, 445-453.
[6] Van Asperen, K. (1962) A Study of House Fly Esterase by Means of a Sensitive Colorimetric Method. Journal of In-
sect Physiology, 8, 401-416. http://dx.doi.org/10.1016/0022-1910(62 )90 074 -4
[7] Lowry, O.H., Rosebrough, N.J., Farr, A.L. and Randall, R.J. (1951) Protein Measurements with the Folin Phenol Rea-
gent. Journal of Bio logical Chemistry, 193, 265-275.
[8] Davis, B.J. (1964) Disc Electrop horesis-II Method and Application to Human Serum Proteins. Annals of the New York
Academy of Sciences, 121, 404-427. http://dx.doi.org/10.1111/j.1749-6632.1964.tb14213.x
[9] Ornstein, L. (1964) Disc Electrophoresis. I. Background and Theory. Annals of the New York Academy of Sciences,
121, 321-349. http://dx.doi.org/10.1111/j.1749-6632.1964.tb14207.x
[10] Hunter, R.L. and Markert, C.L. (1957) Histochemical Demonstration of Isozymes Separated by Zone Electrophoresis
in Starch Gels. S cience, 125 , 1294-12 95. http://dx.doi.org/10.1126/science.125.3261.1294-a
[11] Subramani, T., Manjunath, K.C., Siddalinga Murthy, K.R. and Ramachandra Swamy, N. (2012) Esterase Activity from
the Germinated Jatropha curcas Seeds in Different Extraction Buffers. International Journal of Science and Nature
(IJSN), 3, 170-172.
[12] Dixo n, M. and Webb , E.C. (1979) In Enzymes. Academic Press, London, 207-215.
[13] Walker, C.H. and Mackness, M.I. (1983) Esterases: Problems of Identification and Classification. Biochemical Phar-
macology, 32, 3265-3326. http:// dx.d oi .or g/1 0.10 16/ 0006 -2952(83)90349-0
[14] Aldridge, W.N. and Reiner, E. (1972) In Enzyme Inhibitors as Substrates . North Holland, Amsterdam.
[15] Hol mes, R.S. and Masters, C.J. (1967) The Developmental Multiplicity and Isoenzyme Status of Cavian Esterases. Bi-
ochimica et Biophysica Acta, 132, 379 -399. http://dx.doi.org/10.1016/0005-2744(67)90157-X
[16] Coates , P.M., Mestriner, M.A. and Hopkins on, D.A. (1975) A Preliminary Genetic Interpretation of the Esterase Iso-
zymes of Human Tissues. Annals of Human Genetics, 39,1-20. http://dx.doi.org/10.1111/j.1469-1809.1975.tb00103.x
[17] Heal y, M.J., Dumancic, M.M. and Oakeshott, J.G. (1991) Biochemical and Physisological Studies of Soluble Esterases
from Drosophila melanogaster. Biochemical Genetics, 29, 365-388. http://dx.doi.org/10.1007/BF00554144
[18] Sreerama, L. and Veerabhadrappa, P.S. (1991) Purification and Properties of Carboxylesterases from the Midgut of the
Termite Odentotermes horni. Insect Biochemistry, 21 , 833-84 4. http: // dx. doi .or g/1 0.10 16/ 0020 -1790(91)90090-2

S. Kantharaju, K. R. Siddalinga Murthy
62
[19] Siddalinga Murthy, K.R. and Veerabhadrappa, P.S. (1996 ) Purification, Characterization and Properties of Carbox-
ylesterase from the Midgut of the Silkworm, Bombyx mori L. Insect Biochemistry and Molecular Biology, 26, 287-296.
http://dx.doi.org/10.1016/0965-1748(95)00091-7