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Evidence-Based Complementary and Alternative Medicine
Volume 2015 (2015), Article ID 309214, 6 pages
http://dx.doi.org/10.1155/2015/309214
Research Article

Purification and Characterization of Asparaginase from Phaseolus vulgaris Seeds

1Biochemistry Department, Faculty of Science, King Abdulaziz University, Jeddah, Saudi Arabia
2Biology Department, Faculty of Science, King Abdulaziz University, Jeddah, Saudi Arabia

Received 29 May 2015; Accepted 19 August 2015

Academic Editor: Roberto Miniero

Copyright © 2015 Saleh A. Mohamed et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

L-asparaginase from bacteria has been used in treatment of acute lymphoblastic leukemia. The aim of this study was to purify and characterize L-asparaginase from Phaseolus vulgaris seeds instead of microbial sources. L-asparaginase was purified to apparent homogeneity. The enzyme has molecular mass of 79 kDa. The purified asparaginase had very low activity toward a number of asparagine and glutamine analogues. L-asparaginase was free from glutaminase activity. Kinetic parameters, Km and Vmax of purified enzyme, were found to be 6.72 mM and 0.16 μM, respectively. The enzyme had optimum pH at 8.0. The enzyme showed high stability at alkaline pH (pH 7.5–9.0) when incubated for up to 24 h. L-asparaginase had the same temperature optimum and thermal stability at 37°C. K+ was able to greatly enhance the activity of asparaginase by 150% compared with other metals tested. In conclusion, L-asparaginase showed no glutaminase activity and good stability over a wide range of physiological conditions, and thus it could be used as a potential candidate for treatment of acute lymphoblastic leukemia.

1. Introduction

L-asparaginase (L-asparagine amidohydrolase E.C.3.5.1.1) is used in treatment of acute lymphoblastic leukemia and non-Hodgkin’s lymphoma [13]. The use of L-asparaginase in anticancer therapy is based on its ability to cleave L-asparagine, an amino acid essential for lymphoblasts’ growth, to ammonia and L-aspartic acid in serum and cerebrospinal fluid, since lymphoblasts are unable to produce endogenous L-asparagine which leads to death of these cells [4]. Most of the cancer cells are dependent on an exogenous source of this amino acid for survival. However, normal cells are able to synthesize L-asparagine and thus are less affected by its rapid depletion due to treatment with this enzyme. L-asparaginase can also be used to reduce the formation of acrylamide in fried and oven-cooked foods especially in potato chips [5, 6]. The formation of acrylamide was attributed to the reaction of free asparagine and reducing sugars [7]. The depletion of asparagine by asparaginase prevented acrylamide formation [7].

L-asparaginase is widely distributed among plants, animals, and microorganisms [8]. In plant, this enzyme was first detected in the developing seeds of Lupinus albus [9]. Asparaginase has also been purified from the testa of maturing seeds of L. polyphyllus [10]. Two forms of the enzyme have been identified. A K+-independent form is found in L. arboreus [11, 12] and L. polyphyllus [13] and a K+-dependent form is found in Pisum sativum and several other legume species, including other Lupinus species [14]. Work with antibodies to the K+-independent form from L. polyphyllus revealed no cross-reaction with either pea asparaginase or a number of varieties of Lupinus containing the K+-dependent enzyme, suggesting that the two forms of asparaginase are immunologically distinct [15].

Very little information has been reported about using of plant asparaginase in treatment of acute lymphoblastic leukemia [16]. Therefore, the main goal of this study was to purify and characterize L-asparaginase from Phaseolus vulgaris seeds free from L-glutaminase instead of L-asparaginase from microbial sources which is used as anticancer and caused side effects due to its immunological responses.

2. Material and Methods

2.1. Plant Materials

Mature seeds from Phaseolus vulgaris cv. Giza 6 were obtained from the Agricultural Research Centre, Cairo, Egypt.

2.2. Purification of Asparaginase
2.2.1. Crude Extract

The crude extract of asparaginase was prepared by homogenization of 50 g seeds from Phaseolus vulgaris cv. Giza 6 in 20 mM Tris-HCl buffer, pH 8.0 containing 10% glycerol, 50 mM KCl, 12.5 mM β-mercaptoethanol, and 1 mM PMSF. The homogenate was centrifuged at 10,000 ×g and the supernatant was designated as crude extract. The crude extract was concentrated by dialysis against solid sucrose.

2.2.2. DEAE-Sepharose Column

Concentrated crude extract was applied onto a DEAE-Sepharose column (15 × 1.6 cm i.d.) which was previously equilibrated with 20 mM Tris-HCl buffer, pH 8.0. The enzyme was eluted by different concentrations of KCl prepared in the same buffer at a flow rate of 60 mL/h and 3 mL fractions were collected. Three peaks of protein were eluted with asparaginase activity according to the elution order (asparaginases I, II, and III).

2.2.3. Sephacryl S-200

Asparaginase I with highest activity was applied onto a Sephacryl S-200 column (90 × 0.6 cm i.d.) which was previously equilibrated with the same buffer at a flow rate of 30 mL/h and 3 mL fractions were collected.

2.3. Asparaginase Assay

The activity of L-asparaginase was measured by modified method of Wriston [17]. The L-asparaginase catalyzes L-asparagine to L-aspartic acid and ammonia and the latter react with Nessler’s reagent to produce an orange colored product. The enzyme assay mixture consisted of 900 μL of freshly prepared L-asparagine (20 mM) in 50 mM Tris-HCl buffer (pH 8.0), 50 mM KCl, and 100 μL of crude extract of the enzyme. The reaction mixture was incubated at 37°C for 30 min and the reaction was stopped by adding 100 μL of 15% trichloroacetic acid. The reaction mixture was centrifuged at 10,000 ×g for 5 min at 4°C to remove the precipitates. The ammonia released in the supernatant was determined using colorimetric technique by adding 100 μL Nessler’s reagent into the sample containing 100 μL supernatant and 800 μL distilled water. The contents in the sample were vortexed and incubated at room temperature for 10 min and OD was measured at 425 nm. The ammonia produced in the reaction was determined based on the standard curve obtained with ammonium sulfate. One unit of L-asparaginase activity is defined as the amount of the enzyme that liberates 1 μmol of ammonia per min at 37°C.

2.4. Protein Determination

Protein was quantified by the method of Bradford [18] with bovine serum albumin as standard.

2.5. Molecular Weight Determination

The native molecular weight was determined by Sephacryl S-200. The column was calibrated with cytochrome C (12,400), carbonic anhydrase (29,000), bovine serum albumin (67,000), alcohol dehydrogenase (150,000), and β-amylase (200,000). Dextran blue (2,000,000) was used to determine the void volume (Vo). Subunit molecular weight was estimated by SDS-polyacrylamide gel electrophoresis [19]. SDS-denatured phosphorylase b (94,000), bovine serum albumin (67,000), ovalbumin (43,000), carbonic anhydrase (30,000), soybean trypsin inhibitor (20,000), and α-lactalbumin (14,200) were used for the calibration curve.

2.6. Characterization of Asparaginase
2.6.1. Substrate Specificity

Asparaginase activity was determined with some analogs of L-asparagine. The relative activity was expressed as the percentage ratio of the enzyme activity determined against different structure analogs of L-asparagine to enzyme activity with L-asparagine.

2.6.2. Kinetic Parameters

The values of Michaelis constants (Km) and maximum velocity (Vmax) were determined using L-asparagine as substrate in the range of 2–20 mM. Kinetic parameters were determined from Lineweaver-Burk plot.

2.6.3. Effect of pH

The optimum pH for the asparaginase activity was determined by assaying the activity at different pH values. The pH stability was tested by incubation of the enzyme at pH of 5.0–9.0 for 24 h at 4°C in the absence of substrate and residual activity was determined under the standard assay conditions.

2.6.4. Effect of Temperature

The optimum temperature for asparaginase activity was determined by assaying the enzyme at different temperatures. Heat stability was measured by incubating the enzyme alone at different temperatures for 1 h. After heat treatment, the enzyme solution was cooled and the residual activity was assayed after adding the substrates.

2.6.5. Metal Ion Effect

The effects of various metal ions on enzyme activity were determined by preincubating the enzyme alone with 10 mM metal ions for 15 min prior to adding the substrate. The activity which was assayed in the absence of metal ions was taken as 100%.

3. Results and Discussion

The results of purification steps of asparaginase from P. vulgaris are summarized in Table 1. The elution profile of the chromatography on DEAE-Sepharose column (Figure 1) showed three peaks of proteins with asparaginase activity. Peak one with the highest asparaginase activity was applied onto a Sephacryl S-200 column (Figure 2). L-asparaginase I was purified 21.7-fold with a specific activity 846 units/mg protein. The asparaginase I was proved to be pure after Sephacryl S-200 column as assessed by SDS-PAGE (Figure 3). The molecular weight of asparaginase I by Sephacryl S-200 and SDS-PAGE procedures yielded a value of 79 kDa as monomer subunit. This finding is in agreement with molecular weights for asparaginases from Vigna unguiculata (70 kDa) [20] and Lupinus polyphyllus (75 kDa) [15]. A medium molecular weight of 58 kDa was detected for asparaginase from pea leaves [21]. For bacterial asparaginases, the molecular weight ranged from 140 to 160 kDa with tetramer subunits [2225]. A very low molecular weight of 11.2 kDa was detected for Streptobacillus sp. KK2S4 asparaginase [26].

Table 1: Purification scheme of asparaginase from Phaseolus vulgaris cv. Giza 6 seeds.
Figure 1: A typical elution profile for the chromatography of asparaginase from P. vulgaris on DEAE-Sepharose column (15 × 1.6 cm i.d.) previously equilibrated with 20 mM Tris-HCl buffer, pH 8.0 at a flow rate of 60 mL/h and 3 mL fractions.
Figure 2: Gel filtration of asparaginase I from DEAE-Sepharose fraction on Sephacryl S-200 column (90 × 1.6 cm i.d.). The column was equilibrated with 20 mM Tris-HCl buffer, pH 8.0 at a flow rate of 30 mL/h and 3 mL fractions.
Figure 3: SDS-PAGE for homogeneity and molecular weight determination of asparaginase I from Phaseolus vulgaris. (1) Protein markers; (2) Sephacryl S-200 asparaginase I.

The substrate specificity of asparaginase I has been examined using a number of asparagine and glutamine analogues (Table 2). The activity with the L-asparagine was regarded as 100% activity. DL-asparagine exhibited 30% of enzyme activity, where DL-asparagine is composed of a 1 : 1 racemic mixture. D-asparagine, L-aspartic acid, and L-glutamic acid analogues had very low activity toward asparaginase I. No activity was detected in the presence of L-glutamine. Therefore, the asparaginase I from P. vulgaris is free from glutaminase. The contamination of asparaginase with glutaminase activity caused side effects during the course of anticancer therapy [27, 28]. The L. arboreus asparaginase hydrolyzed only L-asparagine and DL-aspartyl hydroxamate [12]. The V. unguiculata asparaginase was specific for L-asparagine, did not hydrolyze D-asparagine, and was not specific for L-glutamine [20].

Table 2: Relative activities of asparaginase I from P. vulgaris toward a number of asparagine and glutamine analogues at 20 mM concentration.

Kinetic parameters, Km and Vmax of purified enzyme, were found to be 6.72 mM asparagine and 0.16 μM ammonia/mL, respectively (Figure 4). Similar Km values of 6.6 and 7.0 mM were determined for asparaginases from L. arboreus and L. angustifolius, respectively [12]. Asparaginase from Lupinus seeds has high Km for asparagine (12.2 mM) [13]. Low Km (1.2 mM) was determined for asparaginase from V. unguiculata [20]. For bacteria, Km values for L-asparaginase from Escherichia coli and Erwinia carotovora were 3.5 and 7.14 mM, respectively [29, 30].

Figure 4: Lineweaver-Burk plot relating of asparaginase I from P. vulgaris velocities to different L-asparagine concentrations.

Asparaginase I exhibited pH optimum at 8.0 (Figure 5). Between pH 6.0 and 9.0, more than 50% of its activity was retained. Although maximum activity at physiological pH is one of the prerequisites of L-asparaginase for antitumor activity, the purified enzyme would be useful because 80% of the enzyme activity was retained at pH 7.5. The enzyme showed stability at alkaline pH (pH 7.5–9.0) as it retained 90% of its original activity when incubated up to 24 h (Figure 6). However, the pH optimum of L-asparaginases from several plants ranged from 8.0 to 8.5 [12, 20, 31]. Most of L-asparaginases from bacteria showed alkaline pH optima (8.0–10) [26, 30, 32, 33].

Figure 5: pH optimum of asparaginase I from P. vulgaris. The enzyme activity was measured at various pH’s using the standard assay method as previously described.
Figure 6: pH stability of asparaginase I from P. vulgaris at different pH after incubation for 24 h at 4°C.

Asparaginase I was found to have temperature optimum at 37°C (Figure 7). Similar temperature optimum of asparaginase from V. unguiculata (40°C) was reported [20]. This temperature was also similar to that reported for Pseudomonas aeruginosa and Pectobacterium carotovorum [32, 33]. The optimum activity of Streptobacillus sp. asparaginase was recorded at 35°C [26]. On the contrary, L-asparaginase from Chrombacteriaceae and Proteus vulgaris was observed at 20°C and 57°C, respectively [34, 35]. A nonlinear relation between asparaginase I and temperature stability was detected (Figure 8). The enzyme activity was stable up to 37°C after incubation for 1 h. Asparaginase from V. unguiculata was stable up to 40°C after incubation for 15 min [20]. Asparaginases from P. carotovorum and C. annuum retained their initial activity after incubation at 40°C and 45°C for 60 min, respectively [32, 33].

Figure 7: Temperature optimum of asparaginase I from P. vulgaris. The enzyme activity was measured at various temperatures using the standard assay method as previously described.
Figure 8: Thermal stability of asparaginase I from P. vulgaris. The reaction mixture was preincubated at various temperatures for 60 min prior to substrate addition, followed by cooling in an ice bath. The enzyme activity was measured using the standard assay method as previously described. Activity at zero time was taken as 100% activity.

The effect of different metal ions on asparaginase I was examined (Table 3). The metal ions were used at the concentration of 10 mM. K+ was able to greatly enhance the activity of asparaginase I by 150%. In plant, K+-independent and K+-dependent asparaginases had been identified [11, 14, 36]. K+ acted also as enhancer on P. carotovorum asparaginase [32]. Ca2+ slightly enhanced the activity by 110%, but Cu2+ slightly inhibited the activity of asparaginase I. In addition, Pb2+ and Hg2+ caused partially inhibitory effect on asparaginase I. However, V. unguiculata asparaginase was activated by Ni2+ and Co2+ and was inhibited by Mn2+, Zn2+, Ba2+, and Hg2+ [20]. EDTA as metal chelator agent caused partially inhibitory effect on asparaginase I. However, EDTA had no effect on P. carotovorum asparaginase [32].

Table 3: Effect of metal ions and EDTA at 10 mM concentration on asparaginase I activity.

4. Conclusions

The L-asparaginase I from P. vulgaris was purified in glutaminase-free form, which can reduce the possibility of side effects during the course of anticancer therapy. The enzyme showed good stability over a wide range of physiological conditions as pH and temperature. In the next step of our project, L-asparaginase I from P. vulgaris will be used as a potential candidate for treatment of acute lymphoblastic leukemia.

Conflict of Interests

The authors have no conflict of interests relevant to this paper to disclose.

Acknowledgments

This project was funded by the National Plan for Science, Technology and Innovation (MAARIFAH), King Abdulaziz City for Science and Technology, Saudi Arabia, award no. (11-BIO-1516-03). The authors also acknowledge with thanks Science and Technology Unit, King Abdulaziz University, for technical support.

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