Lipases (triacylglycerol acylhydrolases EC.184.108.40.206) catalyse the hydrolysis of long-chain triacylglycerols by acting at the oil-water interface. They also catalyse the reverse reactions of esterification, transesterification and interesterification in non-aqueous environments. Formation of aggregate super substrates such as an emulsion, results in a drastic increase in lipase activity upon comparison to monomeric substrates. This is known as the phenomenon of interfacial activation (1). The lid that covers the active site might be displaced during interfacial activation, hence allowing access to the active site. When a hydrophobic surface such as an oil droplet is present, the lid gets displaced and the enzyme turns into an ‘open’ form. This permits the hydrophobic inner face and the hydrophobic residues that surround the active site to interact with the substrate (2).
The need for interfacial activation poses some practical constraints when immobilized lipases existing within a porous structure are applied in the industrial context. The enzyme molecules are inaccessible to any external interface and hence cannot undergo interfacial activation. Immobilizing the enzyme by adsorption onto hydrophobic supports could serve as a simple alternative to circumvent this problem (3). The hydrophobic supports resemble the surface of the enzyme’s natural substrate and hence the enzyme binds to them with high affinity. When the procedure is carried out under conditions of low ionic strength, other water soluble proteins are excluded and the process becomes highly selective for the lipases (4). Hydrophobic areas surrounding the active site and located in the internal face of the lid are involved in this adsorption process. This fixes the enzyme in its open conformation and enables good enzyme activity regardless of whether the interface required for its activation is present or not.
Lipase immobilized in this manner could be productively exploited for a wide range of applications, and in the present study, it was used for biodiesel production. Alternatives to fossil fuels, biodiesel derived from vegetable oils is gaining prominence. Replacing the chemical catalysts used in biodiesel production with biocatalysts shall further enhance the environmental acceptability of the process and lipases could play a prominent role in this sector. They catalyse the transesterification of triacylglycerol with short chain alcohols and immobilization of the enzyme is especially advantageous as it enhances stability and permits reusability (5). The enzyme used in this study was the purified lipase derived from Bacillus sp. that was previously isolated in our lab from oil contaminated site.
2. Materials and Methods
p-Nitrophenyl palmitate and Diaion HP-20 beads were purchased from Sigma-Aldrich, USA. All other chemicals used were of analytical grade and obtained from standard sources in India.
2.2. Source of Lipase
This study was performed with the bacterial strain Bacillus sp. PS35 (Accession No. KJ020927) that was previously isolated in our lab from soil sample exposed to poultry slaughterhouse effluent. Its genomic DNA library was constructed in pUC18 and E. coli DH5a cells were transformed with the ligated products. Clone 4 which showed good lipase activity was sequenced. The deduced nucleotide sequence of the lipase gene was submitted to Genbank (Accession No. KM225297). The recombinant enzyme (designated as C-4 lipase) was purified 19.41-fold from E. coli culture and its molecular weight was determined to be around 29 kDa.
2.3. Lipase Immobilization
C-4 lipase was immobilized by cross-linking of the enzyme molecules with gluteraldehyde and adsorption onto Diaion HP-20 beads, comprising of a hydrophobic Sty-Dvb resin (6). The hydrophobicity of the resin can impede penetration of water into its pores. Hence, the beads (1g) were suspended in 100 mL of the organic solvent acetonitrile for 1 h, followed by addition of an equal amount of water and left for another 1 h, both processes being carried out under mild agitation of 30 rpm. The beads were washed with 4 volumes of water.
One half of the washed beads were treated with 2.5% gluteraldehyde for 1 h. They were washed 3 times with distilled water to remove residual gluteraldehyde. 5 mL of purified C-4 lipase was added to the beads, with and without gluteraldehyde treatment, and left on shaker (60 rpm) for 90 min. The samples were centrifuged at 1000 ×g for 5 min. The supernatant was tested for unbound protein and enzyme activity. HP-20 beads were washed thrice in 50 mM phosphate buffer, pH 7 and used for the experiments. The immobilized enzymes were referred to as Sty-Dvb (non-cross-linked) and Sty-Dvb-Glu (cross-linked).
Lipase activity was quantified using spectrophotometric assay with p-NPP as the substrate (7). The absorbance was measured at 410 nm, against an enzyme-free blank. Molar extinction coefficient of 0.0146 mM-1cm-1 was used. One unit of lipase activity was defined as mM of p-Nitrophenol released per minute under the assay conditions. All activity assays were performed in triplicate and the values given represent the mean. Protein content was measured using Folin’s phenol reagent (8).
2.4. Characterization of the Immobilized Lipase
The efficiency of the immobilization process was evaluated by determining the enzyme activity, specific activity, protein loading, and activity yield.
2.5. Stability Studies
After incubating the lipase preparations under various conditions for 1 h, activity assays were performed using phosphate buffer pH 7, under standard conditions of 30°C incubation temperature and 15 min incubation time. The free enzyme was used as such for the assay and the immobilized lipase was separated by filtration, air dried and then used. The results were expressed as relative activities, taking the activity of the unincubated enzyme sample to be 100%
2.6. pH and Temperature Stability
For testing the pH stability, the enzymes were incubated in buffers of pH 3.0-10.0. Citrate, phosphate and Tris-HCl buffers (100 mM) were used for the acidic, neutral and alkaline ranges, respectively. The thermal stability was determined through activity assays performed after incubating the enzyme preparations at 30-80ºC.
2.7. Organic Solvent Stability
The organic solvent stability of the free and immobilized forms of the enzyme was assessed by incubating them in 10% (v/v) ethanol, methanol, isopropanol, n-hexane, toluene, and chloroform followed by checking of the residual activity.
2.8. Storage Stability and Reusability
The stability of the free and immobilized enzymes stored in phosphate buffer pH 7.0, at 4°C was tested over a month’s period and any activity loss occurring during this period was documented by taking the freshly obtained enzyme as control. The reusability of the immobilized enzyme was evaluated by repeatedly using the enzyme for p-NPP hydrolysis. After each use, the enzyme beads were washed thrice in phosphate buffer, pH 7.0.
2.9. Kinetic Constants
Initial reaction velocity was measured by varying the substrate concentration at constant enzyme concentration and used for determining the Michaelis-Menten kinetics. The concentration of the p-NPP substrate was varied from 3.0 to 24.0 mM. The slope and y-axis intercept on the Lineweaver–Burk plot of 1/S versus 1/V were used for calculating the Km and Vmaxvalues, respectively.
2.10. Biodiesel Production Using the Immobilized C-4 Lipase
Palm oil was used for methanolysis and the reaction was performed in screw cap bottles. The immobilized enzyme was reacted with methanol and oil that were added in a molar ratio of 4:1. The reaction mixture consisted of 100 beads of the immobilized enzyme, palm oil 9.63 g, methanol 0.37 g, and distilled water 0.5 g. It was incubated for 96 h at a temperature of 40ºC, in an incubator-shaker set at 90 rpm.
2.11. Optimization of Process Parameters
The reaction conditions were modified in order to assess their effects on methanolysis efficiency. Firstly, the methanol additions were performed in a phased manner (single, two and three step additions), occurring at 0, 36 and 72 h of reaction, amounting to a total of 4 molar equivalents of palm oil. This measure was aimed at avoiding enzyme inactivation by the high methanol content. Subsequently, the molar ratio of methanol and oil was varied (1:4, 1:5 and 1:6) and the ratio for optimal FAME synthesis was determined. The effect of water activity on the reaction was also studied by varying the water content from 0 to 20%. The incubation temperature of the reaction mixture was later varied (40ºC, 45ºC and 50ºC) and its effect on FAME production was assessed.
2.12. Gas Chromatography Analysis
Samples were withdrawn from the reaction mixture at regular time intervals and centrifuged at 12,000 ×g for 5 min. The upper oil layer was withdrawn and analysed using a gas chromatographic system (Shimadzu, Japan). Methyl ester (ME) content and glycerides content (mono, di and triglycerides) were estimated. A DB-5 capillary column (0.25 mm × 15 m, Agilent, India) of fused silica type and flame ionization detector (FID) (split/splitless injection system with auto-sampler) were used. Hydrogen was used as carrier gas (average linear velocity 30 mL/min). The injector and detector temperatures were maintained at 245 and 320ºC, respectively. The column temperature was initially set at 150ºC for 1 min, then increased to 300ºC at the rate of 10ºC per min and maintained at that temperature for 10 min. The result for the FAME content was expressed as a mass fraction in percent using methyl heptadecanoate (C17) as the internal standard.
3.1. Lipase immobilization and Characterization
The Sty-Dvb-Glu lipase exhibited an activity of 15.48 U/g of support and a specific activity of 1.09 U/mg of protein. Higher protein loading of 74.12% onto the resin was also achieved after enzyme cross-linking, as against a loading rate of 56.32% without cross-linking. Cross-linking also resulted in a better activity yield of 79.48%.
3.2. Stability Studies
Maximum enzyme stability was observed in the pH range of 6-8. Incubation in pH 10 buffer resulted in 49% activity loss of the free enzyme. However, the polymer-adsorbed enzyme suffered a substantially lower activity loss of 28%, which further came down to 24% upon cross-linking (Figure 1A). In the case of temperature stability, while the free lipase showed good stability (87% relative activity) in the range of 30 -50ºC, the immobilized enzyme exhibited good activity retention upon exposure to an elevated temperature of 60ºC. Moreover, stability at a much higher temperature of 80ºC had nearly doubled for the cross-linked and adsorbed enzyme (Figure 1B). Similarly, while the free enzyme was less stable in the presence of organic solvents such as n-hexane and toluene, the stability increased remarkably after adsorption onto the hydrophobic resin. Gluteraldehyde cross-linking led to a marginal increase in this adsorption conferred stability. A minimum of 20% increase in relative activity was observed as a result of immobilization. Specifically, the relative activity in the presence of methanol was shifted from 53% to 81%, after the immobilization, thereby favoring the enzyme’s application in FAME synthesis (Figure 2). The storage stability of the free enzyme was poor, with it retaining only 18.36% of its initial activity after a month’s storage in pH 7 phosphate buffer. However, adsorption of the enzyme molecules onto the Sty-Dvb resin increased their stability dramatically, with 50.23% activity retention after a similar period of time. This was further augmented to75.97% upon cross-linking with gluteraldehyde (3a). The immobilized enzyme molecules also showed good reusability. The cross-linked lipase retained 77.5% of its original activity after 20 uses, while the non-cross-linked enzyme was able to retain only 60.03% of its activity after the same number of repetitive uses (3b).
3.3. Kinetic Constants
The Km values of the free and immobilized (Sty-Dvb-Glu) lipase preparations were calculated to be 6.24±0.14 and 6.91±0.13 mM, respectively. Their Vmax values were determined to be 16.87±0.34 and 15.34±0.16 mM/min, respectively from the Lineweaver-Burk plot (not shown).
3.4. Biodiesel Production Using Immobilized C-4 Lipase
Preliminary trials on palm oil methanolysis under arbitrarily fixed conditions of single step methanol addition in a molar ratio of 4:1 and incubation temperature of 40ºC resulted in FAME yield of 62.53%. When single factor optimization of process parameters was performed, the yield was considerably improved. Methanol and oil molar ratio of 5:1, three step methanol additions, and an incubation temperature of 50ºC were established to be the ideal conditions conducive for the transesterification reaction. A maximum of 97% conversion was observed under these optimal conditions. The methyl ester, glycerides (mono, di, and triglycerides), free glycerol and fatty acid contents of the biodiesel are listed in (Table 1).
While single step methanol addition resulted in only a low ME yield of 56.47%, it was amply improved in two-step addition, yielding 73.12% esters. This was further enhanced to 89.32% in three-step addition (Figure 4A). When the impact of methanol and oil molar ratio was investigated, highest FAME accumulation of 97.01% was observed at a ratio of 5:1. A lower yield of 78.63% was noticed at a molar ratio of 4:1. When the ratio was increased further to 6:1, the yield was comparable up to 36h, after which the reaction slowed down and the final yield after 96 h incubation amounted to only 89% (Figure 4B). Lowest ME yield of 37.23% was obtained in the total absence of water. Increasing the water content to 10% hiked the ester yield to a maximum of 96.87% (Figure 4C). However, a further increase in water content to 20% was not helpful for the reaction and the ester yield fell down to 48.53%. Incubation temperature also impacted the lipase catalysed transesterification reaction tremendously. FAME formation at 40ºC was 73.97%, which was increased to 88.74% at 45ºC, and further to 96.12% at 50ºC (Figure 4D).
4.1. Immobilization Efficiency
Immobilized lipase preparations, especially the cross-linked ones, showed good performance in terms of enzyme activity, specific activity, protein loading, as well as activity yield. The high activity yield obtained means that this method of immobilization is suitable for the enzyme’s application in heterogenousbiocatalysis. Gluteraldehyde cross-linking has also been shown to increase the efficiency of Burkholderia cepacia lipase entrapped in alginate and k-carrageenan hybrid matrix (9)
4.2. Stability Studies
Culture medium pH can have a profound impact on the charged groups present on the enzyme surface, which in turn may influence its structure and function. If the charges on the amino acid residues in the active site are altered, substrate binding may be considerably affected. Thus, H+ ions and OH- ions can modify the enzyme’s activity as a result of changes in the three dimensional structure of the enzyme, that especially occur at the active site. The immobilized enzymes were stable in a broader pH range, which enhance their industrial applicability. Adsorption onto the support could have minimized the changes in stereo configurations occurring in the immediate vicinity of the active site and contributed to enzyme stability. Better pH stability of immobilized enzymes has been established in several studies. For instance, Rhizopus oryzae lipase immobilized on silica aerogels by adsorption had retained 95% of its activity within a pH range of 5-9, while the soluble enzyme had lost 60% of its activity at pH 5 and 30% of its activity at pH 9 (10).
Thermal stability is another important requirement which enables the enzyme to function as a biocatalyst at elevated temperatures that may be required for certain reactions to proceed, such as the synthesis of FAME. Immobilized enzymes are known to have better thermal stability than free enzymes. This has been corroborated by results from the present investigation, as well as certain earlier studies. Upon incubation for 24h at 50°C, free lipase from Pseudomonas gessardii had retained an activity of 52% while its immobilized counterpart had displayed a residual activity of 79% (11). Organic solvent stability of the lipase is of paramount importance, if it is to be applied for catalysing esterification, transesterification and interesterification reactions in water restricted environments. Although the free enzyme was less stable in the presence of organic solvents such as n-hexane and toluene, the stability increased remarkably after adsorption onto the hydrophobic resin. Such observations have also been reported elsewhere in literature (12). Accentuated thermostability and organic solvent stability conferred on the lipase by immobilization were particularly handy in catalysing the transesterification reaction.
Enhancement of storage stability is often a prime objective to be met by immobilized enzymes, so as to make them more attractive for commercial applications (13). Immobilization conditions determine enzyme stability, as it depends on the interactions between the enzyme and the support matrix (14). Reusability is another desired attribute for immobilized enzymes, making the process more economical for the industry that applies them (15). Immobilized C-4 lipase exhibited these desirable traits, which enhanced its prospects of being applied in biodiesel production. Earlier, Pseudomonas gessardii lipase immobilized on mesoporous activated carbon had retained 54% of its activity after 30 days of storage (11). Thermomyces lanuginosus and Pseudomonas fluorescens lipases immobilized on epoxy-chitosan/alginate support had retained 95% of their activities after the fifth reuse in butyl oleate synthesis (16). Lipases immobilized on regenerated cellulose and glass fiber membranes have been shown to retain 16 and 41% of their original activities, respectively, after 10 repetitive uses (17).
Enzyme leakage is a pressing problem that often undermines the performance of enzymes that are immobilized by physical adsorption or entrapment. This has been attributed to the larger pore size of the resin in comparison with the size of the enzyme molecules. When the enzyme molecules are cross-linked with bifunctional reagents such as glutaraldehyde, their increased size minimizes leakage (18). Glutaraldehyde is present in the solution in different forms that are in equilibrium with each other at a specific pH. Even though different models have been put forth to explain the chemical basis of cross-linking, the mechanism has not been entirely elucidated (19).
4.3. Kinetic Constants
Immobilization may alter the enzyme kinetic constants favorably or otherwise. For instance, an increase in Km value for the immobilized enzyme has been reported, which translates into a decreased affinity for the substrate. This may be due to the support posing steric hindrance and blocking access to the active site or a loss of the much needed substrate flexibility. Problems associated with diffusional limitations may also be encountered, thereby affecting the reaction rate (20). The Km value for Burkholderia lipase immobilized on celite carrier has been reported to be much higher than that for free lipase, suggesting diffusion resistance. Also, the Vmax was lesser, probably due to blocking of the active site (21). However, in case of the C-4 lipase the kinetic constants of the immobilized enzyme were not significantly altered.
4.4. Biodiesel Production Using the Immobilized Lipase
The chemical composition of the biodiesel was in agreement with the EN 14214 standards. The incubation time and methyl ester yield obtained were comparable to other reports. A period of 72-96 h has generally been reported for maximum methyl ester formation (22). Bulk addition of large amounts of organic solvent had inhibitory effects on the enzyme, while adding the same amount in small increments was well tolerated by the enzyme. Methanol addition pattern and its effect on ester content have been studied extensively and in one such study involving packed bed reactor, 4-4.5 molar equivalents of methanol had been added totally and the optimal amount of methanol per pass was found to be dependent on the reaction stage (23). Methanol and oil molar ratio also influenced the FAME yield from the process. A whole cell biocatalyst Rhodotorula mucilagenosa yielded 83.29% FAME with a 6:1 molar ratio of methanol and palm oil (24). Water activity in the reaction mixture was another factor that impacted the process outcome significantly. Other researchers have also reported 10% to be the optimum water content for palm oil transesterification (24). Incubation temperature was also observed to play a key role in the reaction. In previous studies, application of Aspergillus oryzae whole cell biocatalyst expressing Geobacillus thermocatanulatus lipase (r-BTL) for palm oil methanolysis had resulted in near 100% FAME formation at 40-50ºC (25). Hence, this study has facilitated the optimization of process parameters and ascertained the conditions that are conducive for maximizing the ME yield from palm oil.
To sum up, this work has enabled the immobilization of lipase from Bacillus sp. PS35 on a hydrophobic support that is beneficial for its catalytic action. This might be due to the enzyme being fixed in a perpetually open conformation, obviating the necessity for interfacial activation. The styrene-divinyl benzene resin has shown good immobilization efficiency and the immobilized enzyme has displayed superior characteristics in terms of pH, temperature, organic solvent and storage stabilities, with prior gluteraldehyde cross-linking further enhancing the stability of the adsorbed enzyme molecules. The enzyme has also been successfully applied in an emerging area of green chemistry, namely, enzymatic biodiesel production. With biodiesel being widely acclaimed as an environmentally sound replacement to the non-renewable and much polluting fossil fuels, the enzymatic route to its synthesis needs to be thoroughly explored. Ability to perform under high temperatures and in the presence of organic solvents are much needed criteria for such enzymes and C-4 lipase has fulfilled these criteria, more so upon immobilization onto an appropriate support. It could hence serve as a suitable biocatalyst for the enzymatic biodiesel production.
The authors are thankful to the management of Kumaraguru College of Technology, Coimbatore, India, for providing the laboratory facilities to carry out this work.
Conflict of interest
The authors have no substantial financial or commercial conflicts of interest with the current work or its publication.