Abstract: Lipases (E.C. 3.1.1.3) are serine-hydrolases, and act on long chain fatty acid ester bonds. They exhibit specific and enantioselective activities, which are desirable for many industrial applications. This study aimed at screening and optimizing the production of lipases by wild yeast strains from a variety of substrates, as well as characterizing the enzyme. An initial selection was made in oxygenated oil-supplemented minimum medium, and the enzymatic activity of the supernatant was tested over p- nitrophenyl palmitate. One-hundred and twenty-four yeast strains from different substrates were tested, and twenty-three showed significantly higher lipolytic activity (p <0.01). One yeast in particular, QU110, showed best lipase production and therefore was selected for the optimization and characterization processes. This yeast exhibits enzyme secretion in initial pH 6.0, with olive oil and tryptone as carbon and nitrogen sources, respectively. There was a strong interaction between nitrogen source and initial pH, and pH 9.0 seems to inhibit enzyme secretion. The crude enzyme (cell-free supernatant) shows stability in surfactants and n-hexane, but not in ethanol or methanol. A Response Surface Model was created and optimal enzyme activity conditions were observed at 36°C and pH 8.0. The lipase is appropriate for transesterification reactions, as the enzyme is more stable in strong apolar solvents than moderately apolar ones. Also, secretion by pH was not reported elsewhere, which should be further investigated and contribute for other yeast bioprocesses as well.
Keywords:p-NPPp-NPP,TryptoneTryptone,YeastYeast,PalmitatePalmitate,Response Surface ModelResponse Surface Model,Serine-hydrolaseSerine-hydrolase.
Biotecnologia
Nitrogen source and pH interact and modulate lipase secretion in a non-clinical strain of Candida parapsilosis
Universidade Estadual de Maringá
This work is licensed under Creative Commons Attribution 4.0 International.
Received: 31 January 2019
Accepted: 16 September 2019
Lipases (E.C. 3.1.1.3) catalyze hydrolysis and synthesis reactions over triacylglycerol esters. The typical structure involves a catalytic triad (Ser-His-Asp), and the main residue, Serine, is commonly found in a (Ser-X-His-X-Asp) sequence (Jain & Naik, 2018). Lipases are distinguished from other esterases especially by the interfacial activity, given by a hydrophobic “lid” that covers the catalytic center and prevents it from acting on water soluble substrates (Gupta, Kumari, Syal, & Singh, 2015). Nonetheless, lipases can hydrolyze many substrates of esterases, and the opposite also occurs (Lopes, Fraga, Fleuri, & Macedo, 2011). Besides acting on lipids, lipases possess interesting properties such as chemo-, regio- and stereoselectivity. Thus, a broad range of applications is possible, such as detergents and emulsifiers, biodiesel transesterification, paper pulp and leather cleaning, resolution of racemic solutions, food nutrition and flavor enhancement (Navvabi, Razzaghi, Fernandes, Karami, & Homaei, 2018; Sharma et al., 2012).
This enzyme is vastly distributed in nature, from Archaea to mammals, but microbial lipases are preferred since microorganisms secrete it to the outside of the cell, producing high yields of enzyme readily available to purification or direct utilization (Sharma et al., 2012). There are several reports of naturally occurring yeasts with high lipase production, especially belonging to the genera Candida and Yarrowia (Navvabi et al., 2018; Souza, Salgueiro, & Albuquerque, 2012; Thakur, 2012), and substrates like food, plants and soil are common sources of those organisms.
Candida parapsilosis is a cosmopolitan yeast, being reported associated with diverse substrates such as mayonnese and salad toppings (Pitt & Hocking, 2009), goat and cow milk and cheese (Landell, Hartfelder, & Valente, 2006; Spanamberg, Ramos, Leoncini, Alves, & Valente, 2009), Colombian chicha, a fermented beverage (López-arboleda & Ramírez-castrillón, 2010), soil and water (Gadanho & Sampaio, 2005; Wang, You, Bemis, Tegeler, & Brown, 2008). Its lipase production is also considered a virulence factor (Toth, Toth, Vagvolgyi, & Gacser, 2017; Trofa et al., 2011) as well as in other common industrial lipid-producing fungi, like Aspergillus niger (Costa, Hermann, Garcia-Roman, Valle, & Tavares, 2017) and Yarrowia lypolitica (Boyd, Wheless, Brady, & Ellis, 2017). Due to the ability of transesterification under water activities higher than 0.9 (Neang, Subileau, Perrier, & Dubreucq, 2014; Neugnot, Moulin, Dubreucq, & Bigey, 2002), C. parapsilosis lipase is considered a good choice for biodiesel transesterification and other biotechnological applications. It was successfully used for biodiesel transesterification, yielding more than 95% (Rodrigues, Perrier, Lecomte, Dubreucq, & Ferreira-Dias, 2016). Nonetheless, even when the transesterification reaction is desired, preliminary screening tests usually apply lipase hydrolysis as the evaluation parameter (Raoufi & Mousavi Gargari, 2018; Yan, Duan, Liu, Jiang, & Yang, 2016).
Given the interest in naturally produced lipases, the objective of this study was to find a lipase-producing wild yeast, optimize its production conditions and the enzymatic activity conditions.
The reagents were all of analytical grade.
One-hundred and twenty-four yeast strains were tested, previously isolated from cheese (Landell et al., 2006) and other substrates (Annex, supplementary material). All strains are maintained at the Department of Microbiology, Immunology and Parasitology of the Universidade Federal do Rio Grande do Sul, Brazil.
One-hundred µL from a suspension of 106 cells mL-1 were inoculated in 100 mL inductive medium (2% soybean oil, 0.5% peptone, 0.01% magnesium sulphate, 0.1% potassium phosphate), and grown in orbital shaker (Excella E24, New Brunswick, NJ, USA) at 200 rpm for 72 hours at 28°C for lipase induction. Culture supernatants (cell harboring and/or cell-free) were subjected to the p-nitrophenyl palmitate (pNPP) enzymatic assay in order to detect extracellular and cell-bound lipases. Cell-free supernatant was prepared by centrifugation at 5000 rpm for 5 min., and cell harboring supernatant was directly used.
Different pH values (3, 6 and 9), organic nitrogen sources (peptone and tryptone) and carbon sources (soybean and olive oils, tween 20 and tween 80) were tested in order to verify optimal conditions for lipase induction. The concentrations are the same as above; pH was adjusted by HCl or NaOH, as needed, but was not monitored during yeast growth. Lipase reactions were performed with cell harboring and cell free supernatants.
pNPP assays were performed in triplicate, in Tris-HCl 50 mM Buffer pH 8.0, containing 0.11% Arabic Gum, 0.44% Triton x-100 and 10% pNPP at 3 mg mL-1 of 2-propanol, according to Gupta et al. (2002). This substrate solution was added to supernatant (9:1) and kept for 1 hour at 37°C. The released product pNP exhibits yellow color, which absorbs light at 405-410 nm. Absorbance was then measured with Elisa microplate reader at 405 nm (ELx800 – BioTek Instruments Inc, VT USA). One unit of lipase (U) was defined as the amount of enzyme that releases 1 µmol p-nitrophenol min-1. A standard curve was prepared using p-nitrophenol in previously known concentrations.
A surface-response design was created using the Statistica 10 software (Statsoft Inc., 2011). The factors pH and Temperature were taken into account in this design. The pH/Temperature combinations were 14.6/8.0; 25.0/6.0; 25.0/10.0; 37.0/3.5; 37.0/14.14; 37.0/8.0; 37.0/8.0; 49.0/6.0; 49.0/10.0; 59.3/8.0. The reactions were performed as above, except for the buffers, which were either Tris-HCl 50mM for pH 7.5 or above, or Citrate-Phosphate 50mM for pH under 7.5.
The cell-free supernatant (crude enzyme) was co-incubated (concentration of 1:1 v:v) for one hour at 37°C with different Salts [50mM] (MgCl2, KCl, CaCl2, NaCl and EDTA), Solvents (n-Hexane, Acetone or Isopropanol 20%, 50% and 80%; ethanol 20%, 50% and 99.5%) and detergents (1% SDS, Triton X-100 or Tween 20). A control was made with distilled water (1:1 v:v). The residual activity was measured by the pNPP test.
Candida parapsilosis QU110 was aerobically grown in GYP broth (2% glucose, 1% peptone, 0.5% yeast extract) at 28ºC. Total genomic DNA was extracted and purified from 5 mL cultures as described by Osorio-Cadavid, Ramírez, López, and Mambuscay (2009). Sequencing of the D1/D2 domain of the large subunit (LSU) ribosomal DNA was performed according to Kurtzman and Robnett (1998), using the primers NL-1 (5'-GCATATCAATAAGCGGAGGAAAAG-3') and NL-4 (5'-GGTCCGTGTTTCAAGACGG-3'). Amplification conditions were: initial denaturation at 94ºC for 5 min., 30 cycles of denaturation at 94ºC for 1 min., annealing at 55ºC for 30 s, extension at 72ºC for 1 min., and final extension at 72ºC for 10 min. The PCR product was purified by the polyethylene glycol precipitation method (Lis, 1980), and sequenced at the Biotechnology Center of Universidade Federal do Rio Grande do Sul (Cbiot/UFRGS), Brazil. The sequence was assembled and compared with sequences reported in GenBank using the basic local alignment search tool (BLAST) algorithm. The sequence was deposited in GenBank under accession number MH938079.
Results of screening were subjected to Student’s t-test, and results of the univariate optimization were tested by Univariate Analysis of Variance (UNIANOVA) and GLM (Generalized Linear Model) applying hybrid estimation and robust estimation of covariance matrix, with Bonferroni correction for multiple comparisons. The SPSS v.18 was used. All graphic data show deviation bars corresponding to p =0.05.
Twenty-three strains showed significantly higher lipase activity (p <0.001; supplementary Annex). Candida parapsilosis QU110 was selected for optimization of lipase production due to its higher lipase activity when compared to the others, and consistency between the replicates. This yeast was isolated from an artisanal Caccio Cavalo cheese sample (Landell et al., 2006), and was identified as Candida parapsilosis by sequencing the D1/D2 region of the 26S rDNA.
All carbon sources tested showed different induction values (p <0.05) when cell-free supernatant was tested, but regarding cell-harboring supernatant, only olive oil induced significantly higher lipase production (p <0.01), while soybean oil, Tween 20 and Tween 80 showed no difference (p >0.4). The effect of different carbon sources on lipase production can be seen in Figure 1. Candida parapsilosis QU110 showed lipase production of 47.97 u L-1 in the presence of olive oil, more than ten times the activity in the presence of soybean oil, Tween 20 or Tween 80. However, the cell-free supernatant showed lipase activity of only 9.23 u L-1 (Figure 1).
Both data indicated olive oil as the best carbon source among all four tested, and no interaction with other variables over lipase production was observed.
Figure 1.
Effect of different carbon sources on lipase production. Tw20: Tween 20; Tw80: Tween 80; Soy: Soybean oil; Olive: Olive oil. CH: cell-harboring supernatant. CF: cell-free supernatant.
The effect of nitrogen source is strongly subjected to initial pH. Tryptone was the best nitrogen source for lipase production at pH 6.0, inducing an activity of 47.02 u L-1 in cell harboring supernatant and 36.98 u L-1 in cell-free supernatant (Figure 2). In pH 9.0, there was a slight reduction in lipase activity in the cell harboring supernatant (43.01 u L-1), and there was no lipase secretion (Figure 2).
Figure 2
Effect of different pH and nitrogen sources on lipase production. P: Peptone; T: Tryptone; 6 and 9: pH6 and pH 9, respectively; CH: cell-harboring supernatant CF: cell-free supernatant
The absence of lipase secretion at pH 9.0 was also found with peptone as the nitrogen source, while there was an increase in lipase activity in the cell-harboring supernatant (31.05 u L-1) in comparison to pH 6.0. These variations are corroborated by Generalized Linear Model statistics, which showed that pH and nitrogen sources have correlated effects, and cannot be estimated separately.
According to the Response Surface Model for lipase production, the best hydrolysis activity conditions for the lipase produced by C. parapsilosis QU110 were pH 8.0 and temperature of 36°C (Figure 3).
Figure 3.
Response surface model for lipase production (u L-1) considering pH and Temperature (°C). Green areas indicate lower lipase activity, and dark red, higher activities
The crude enzyme exhibited inhibition values greater than 50% for concentrated solvents, and good stability to anionic surfactants, retaining up to 80% activity in the presence of Tween 80 (Figure 4a). In the presence of mono- and divalent ions, the enzyme showed destabilization, with residual activities lower than 40% when treated with CaCl2. Most solvents showed strong inhibition and destabilization of the lipase, especially when concentrated. In contrast, n-Hexane 40% (v:v) increased lipase activity in about 5% (Figure 4c).
The preliminary screening step performed with 124 strains from different sources evidenced that, although lipase production is widespread, most wild yeast strains had low activities. Candida parapsilosis QU110 was selected as a good lipase-producing yeast.
It is known that oleic acid induces C. parapsilosis lipase gene CpLip2 (Neugnot et al., 2002), and this species has been identified in virgin oils as a spoilage organism (Zullo & Ciafardini, 2008). Recently, a good lipase producing yeast, Magnusiomyces capitatus was isolated from an Olive Mill Wastewater, indicating good inducing potential of olive oil (Salgado, Fonseca, Silva, Roseiro, & Eusébio, 2019).
No reports on gene CpLip1 activity were made so far. Since C. parapsilosis uses an alternative yeast genetic code, alternative translations are required for heterologous expression, which seems to be a setback in expressing LIP1 gene (Nosek, Holesova, Kosa, Gacser, & Tomaska, 2009).
In most conditions, we observed activity only in the cell harboring supernatant, indicating a cell wall or membrane-bound lipase. Interestingly, alkaline initial conditions seem to inhibit enzyme secretion.
The effect of the nitrogen source on lipase production was highly influenced by the medium pH. Although tryptone induced lipase secretion in pH 6.0 (cell-free supernatant), the same did not occur in pH 9.0. pH 9.0 allowed lipase production with both nitrogen sources, although it seemed to inhibit lipase secretion, probably remaining attached to the plasmatic membrane. To our knowledge, no reports have been made in this regard so far.
Figure 4.
Residual extracellular lipase activity (%) after exposure to chelating salts (A), surfactants (B) and several concentrations of different solvents (C) for 1 hour at 37°C
An alternative explanation would be that two different lipases (cell-bound and extracellular) are produced at different pH conditions. In accordance to this two-enzyme hypothesis, two lipase genes for C. parapsilosis have been described and characterized (Brunel et al., 2004; Subileau et al., 2015). Also, Hlavsová, Zarevúcka, Wimmer, Macková, and Sovová (2009) showed different conditions to induce extracellular and cell-bound lipases in Geotrichum candidum 4013, and Alonso, Oliveira, Dellamora-Ortiz, and Pereira-Meirelles (2005) stated that, in Yarrowia lipolytica IMUFRJ 50682, lipase secretion is dependent on the growth stage, with extracellular activity found at the late stationary phase, while late logarithmic phase is associated with cell-bound lipase activity.
It is remarkable that C. parapsilosis lipase, unlike classical lipases like CAL-A from Pseudozyma antarctica, retains its acyltransferase ability even at higher water activities, making it the best candidate for green biotechnology applications like biodiesel transesterification (Subileau et al., 2015). Wang, Chi, Wang, Liu, and Li (2007) showed in pH=7 optimal activity for cell-bound lipase from C. parapsilosis, similar to that observed for C. parapsilosis QU 110 crude lipase.
Stability characteristics seem to agree with typical lipases, showing stabilization against n-hexane and instability for solvents and ionic surfactants (Hama, Noda, & Kondo, 2018; Hasan, Shah, & Hameed, 2006;Nie, Xie, Wang, & Tan, 2006). Acetone 10% and 25% (v/v) show destabilization of about 50%, lower than other solvents tested, coherent with reports of acetone use for cell-preparation for interesterification and whole-cell biocatalysis (Lin & Tao, 2018)
It is known that lipase production is strongly influenced by culture conditions, which modulate its secretion. Our study showed that C. parapsilosis QU110, a wild strain, could be induced to produce lipases that are either secreted or bound to the cell, depending on the medium pH. This lipase shows typical optimal conditions for pNPP hydrolysis and good stability against some solvents. This yeast is a good candidate for further investigations in order to produce and/or degrade hydrophobic compounds and resolution of racemic mixtures, among other uses.
The authors acknowledge the financial support by FAPERGS, CNPq and CAPES.
List of yeasts screened for p-nitrophenyl palmitate essay indicating lipase activities (units L-1). The “t” student test was performed in order to highlight good lipase producing strains. Values over three standard deviations were considered high producing yeasts when compared to the pool of yeasts tested. All tests were performed in triplicates. Strain code names indicate substrate of origin (QU: artisanal cheese; FA: enrichment growth of soil samples; CB: fatty residues of restaurant exhaustion equipment; LV: raw bovine milk; EI: bromelid endophytic yeast).
Figure 1.
Effect of different carbon sources on lipase production. Tw20: Tween 20; Tw80: Tween 80; Soy: Soybean oil; Olive: Olive oil. CH: cell-harboring supernatant. CF: cell-free supernatant.
Figure 2
Effect of different pH and nitrogen sources on lipase production. P: Peptone; T: Tryptone; 6 and 9: pH6 and pH 9, respectively; CH: cell-harboring supernatant CF: cell-free supernatant
Figure 3.
Response surface model for lipase production (u L-1) considering pH and Temperature (°C). Green areas indicate lower lipase activity, and dark red, higher activities
Figure 4.
Residual extracellular lipase activity (%) after exposure to chelating salts (A), surfactants (B) and several concentrations of different solvents (C) for 1 hour at 37°C
