- Open Access
Characterization of a highly stable α-galactosidase from thermophilic Rasamsonia emersonii heterologously expressed in a modified Pichia pastoris expression system
Microbial Cell Factories volume 18, Article number: 180 (2019)
Structurally stable α-galactosidases are of great interest for various biotechnological applications. More thermophilic α-galactosidases with high activity and structural stability have therefore to be mined and characterized. On the other hand, few studies have been performed to prominently enhance the AOX1 promoter activity in the commonly used Pichia pastoris system, in which production of some heterologous proteins are insufficient for further study.
ReGal2 encoding a thermoactive α-galactosidase was identified from the thermophilic (hemi)cellulolytic fungus Rasamsonia emersonii. Significantly increased production of ReGal2 was achieved when ReGal2 was expressed in an engineered Pastoris pichia expression system with a modified AOX1 promoter and simultaneous fortified expression of Mxr1 that is involved in transcriptionally activating AOX1. Purified ReGal2 exists as an oligomer and has remarkable thermo-activity and thermo-tolerance, exhibiting maximum activity of 935 U/mg towards pNPGal at 80 °C and retaining full activity after incubation at 70 °C for 60 h. ReGal2 is insensitive to treatments by many metal ions and exhibits superior tolerance to protein denaturants. Moreover, ReGal2 efficiently hydrolyzed stachyose and raffinose in soybeans at 70 °C in 3 h and 24 h, respectively.
A modified P. pichia expression system with significantly enhanced AOX1 promoter activity has been established, in which ReGal2 production is markedly elevated to facilitate downstream purification and characterization. Purified ReGal2 exhibited prominent features in thermostability, catalytic activity, and resistance to protein denaturants. ReGal2 thus holds great potential in relevant biotechnological applications.
In addition to glycoproteins and glycolipids, α-linked galactosyl residues are found in nature in two major forms: (1) as branched residues in galactomannans and galactoglucomannans that are classified into hemicellulose [1, 2], the second most abundant biopolymer on earth after cellulose, both of which are mainly present in plant cell walls, and (2) as moieties of oligosaccharides including melibiose, raffinose, and stachyose that are present in sugar beets and soys .
α-Galactosidases (α-d-galactoside galactohydrolase; EC 188.8.131.52) are exo-glycosidases that catalyze the removal of α-linked terminal non-reducing galactose residues from different galactoside-containing polymers or oligopolysaccharides . They are widely distributed in microorganisms, plants, and animals, and are classified into glycoside hydrolase (GH) families 4, 27, 36, 57, 97, and 110 . Whereas most bacterial α-galactosidases fall into GH family 36, most fungal α-galactosidases belong to GH27.
α-Galactosidases are of great interest in a variety of biotechnological applications [1, 3]. In pulp and paper manufacturing, α-galactosidases are used with other kinds of hemicellulases to enhance pulp bleaching [1, 5]. These enzymes are also conventionally applied in food and feed industries to process soy molasses and soybean milk to remove anti-nutritional factors such as raffinose family oligosaccharides (RFOs) that are mainly raffinose and stachyose , and to eliminate raffinose from sugar beet molasses to increase sucrose crystallization and consequently improve the yield .
Thermostable enzymes are frequently courted especially for processes running at elevated temperatures to achieve an overall high productivity . High structural stability is also an important and desirable feature of enzymes to resist toxic inhibitors either derived from the substrate or generated during the reaction. Compared to extensive studies on the mesophilic α-galactosidases, only a few thermophilic/thermostolerant α-galactosidases have been characterized, most of which are from thermophilic fungi (see a summary in Table 1), e.g., Neosarotrya fischeri [9, 10], Thermomyces lanuginosus , Talaromyces leycettanus , and Talaromyces emersonii . These α-galactosidases exhibit various degrees of thermo-activity and thermo-stability as well as resistance to a number of metal ions and some other chemicals (see a summary in Table 5). However, none has been found to be tolerant to protein denaturants such as SDS, urea, and guanidine hydrochloride (GdhHCl), implicating their structural fragility to these denaturants. Therefore, more thermophilic/thermotolerant α-galactosidases with desired properties including high structural stabilities have to be mined and characterized.
Rasamsonia emersonii (former name Talaromyces emersonii) is a (hemi)cellulolytic filamentous fungus with an optimum growth temperature of 40–45 °C and can even grow at up to 55 °C . Since its isolation, R. emersonii has become as a rich source of thermophilic polymer-degrading enzymes, e.g., β-glucosidase, endo-1,4-β-glucanase, and xylanase [15,16,17]. In particular, an α-galactosidase from this fungus exhibits remarkable thermostability and specific activities, which holds great potential for industrial application .
The methylotrophic yeast Pichia pastoris is one of the most commonly used expression systems for heterologous protein production, especially for eukaryotic proteins [18,19,20]. The highly inducible and tightly-regulated alcohol oxidase 1 gene (AOX1) promoter is extensively used to achieve high-level heterologous protein expression under methanol condition . In recent years, several strategies via engineering transcription factors exerting regulatory effects on the AOX1 promoter, including overexpression of the activators Mxr1 and Mit1 [21,22,23,24] and/or elimination of the repressors Mig1 and Mig2 , have been adopted to achieve the activation of the AOX1 promoter under non-inducing conditions (e.g., glucose and glycerol). Nevertheless, few studies have been performed to prominently enhance the AOX1 promoter activity on methanol, under which condition the production of some heterologous proteins is still too low to obtain decent amounts for further study.
In this study, four putative α-galactosidase encoding genes from R. emersonii were cloned and expressed in P. pastoris. ReGal2 displaying the highest optimum temperature was selected for further characterization. ReGal2 expression was significantly enhanced in an engineered P. pastoris expression system, wherein overexpression of the transcriptional activator Mxr1 was combined with the expansion of the corresponding cis-elements within the AOX1 promoter. Purified ReGal2 exhibited high hydrolytic activity as well as pronounced thermostability and tolerance to protein denaturants compared to the already reported fungal counterparts.
Strains and cultivation conditions
Rasamsonia emersonii was cultured on potato dextrose agar (PDA) plates at 45 °C. P. pastoris GS115 was cultured on yeast extract peptone dextrose (YPD) medium at 30 °C. Escherichia coli DH5α was routinely cultured at 37 °C on Luria–Bertani (LB) broth.
Heterologous expression of R. emersonii α-galactosidases in P. pastoris GS115
Rasamsonia emersonii was cultured in liquid potato dextrose medium at 45 °C for 2 days, and its mycelia was collected by filtration, and subsequently applied for extraction of genomic DNA using the E.Z.N.A. Fungal DNA Mini kit (Omega). The full-length coding sequences of ReGal2–ReGal4, but without introns and the corresponding sequences encoding N-terminal signal peptides that were predicted by SignalP (http://www.cbs.dtu.dk/services/SignalP/), were amplified from the R. emersonii genomic DNA, inserted into the pPICZαA vector (Invitrogen), and transformed into P. pastoris GS115, respectively. The heterologous expression of ReGal5 with removal of introns and the coding sequence for N-terminal transmembrane region predicted by TMHMM (http://www.cbs.dtu.dk/services/TMHMM/) was performed using the same strategy. Transformation of P. pastoris using electroporation was carried out according to the Pichia expression system manual (Invitrogen). The correct integration events occurred in the transformants were verified by anchored PCR. The crude culture supernatant of the correct transformants with 0.5% methanol induction was collected and subjected to enzymatic activity and SDS-PAGE analyses.
Engineering of P. pastoris GS115 to enhance AOX1 promoter activity
The transcriptional activators Mxr1 and Mit1 encoding genes were respectively overexpressed in P. pastoris GS115 under the control of the constitutive GAP promoter . Specifically, the amplified GAP promoter was inserted into the pPICZαA plasmid that was digested with BglII and KpnI to remove the original AOX1 promoter, generating pPICZαA-GAP. The full-length coding sequence of Mxr1 or Mit1 was inserted into the KpnI/XbaI-digested pPICZαA-GAP to construct pPICZαA-GAP-Mxr1 and pPICZαA-GAP-Mit1, respectively. To increase the activator response elements within the AOX1 promoter, the − 719 to − 503 promoter fragment upstream the initiation ATG codon, was amplified and fused to the 5′ end of the native AOX1 promoter (− 1 to − 936) via overlap extension PCR , generating the MBS-AOX1 promoter. To evaluate the activities of the native or engineered AOX1 promoter in P. pastoris, the enhanced green fluorescence protein encoding gene (egfp) was fused to the 3′ end of the promoters. Specifically, the full-length egfp fragment was inserted into the EcoRI-digested pPIC3.5 k*, which was derived from pPIC3.5 k (Invitrogen) by eliminating the BglII at the +6603 site and therefore retaining only one BglII at the +2 site. The resultant plasmid, pPIC3.5 k*-egfp, carrying the egfp gene readily behind the native AOX1 promoter, was transformed into P. pastoris GS115 cells, to result in the control-PAOX1 transformants. The plasmids pPICZαA-GAP-Mxr1 and pPICZαA-GAP-Mit1 were linearized with AvrII and transformed into the control-PAOX1 cells to result in the OEMxr1 and OEMit1 transformants, respectively. Moreover, the MBS-AOX1 promoter fragment was inserted into the plasmid pPIC3.5 k*-egfp that was simultaneously digested with BglII and EcoRI, to replace the native AOX1 promoter. The resultant plasmid was linearized with MssI and transformed into P. pastoris GS115 to generate the PMBS-AOX1 transformants. The plasmid pPICZαA-GAP-Mxr1 was further transformed into PMBS-AOX1 to generate the OEMxr1+PMBS-AOX1 transformants.
Quantification of fluorescence intensity from GFP was detected using a Nikon Eclipse 80i fluorescence microscope. P. pastoris transformants were cultured with 1% glycerol and then equally transferred to medium containing 0.5% methanol. Cells grown to late exponential phase were harvested and transferred to a black microtiter plate and measured using a 96-well spectrofluorometer at an excitation wavelength of 485 nm and an emission wavelength of 535 nm. An aliquot of each sample was diluted for OD600 determination, to calculate the relative fluorescence for each sample per OD.
Expression and purification of ReGal2 in the engineered P. pastoris expression system
Expression of ReGal2 in the engineered expression system
To compare ReGal2 production in the conventional and engineered P. pastoris expression systems, the α-factor signal sequence encoding sequence was amplified from the pPIC9 k vector (Invitrogen) and fused to the 5′ end of the coding sequence of ReGal2 with removal of introns and the first 69 bp encoding the putative N-terminal signal peptide. The resultant fragment was ligated into the EcoRI-digested pPIC3.5 k*, generating the pPIC3.5 k*-ReGal2 plasmid, which was transformed into P. pastoris GS115 to generate the control-ReGal2 transformants. Moreover, to drive the expression of ReGal2 via the MBS-AOX1 promoter, the − 936 to − 730 fragment of the native AOX1 promoter within pPIC3.5 k*-ReGal2 was replaced by the − 1152 to − 730 fragment from the MBS-AOX1 promoter via BglII/SacI-mediated ligation. The resultant plasmid and the pPICZαA-GAP-Mxr1 plasmid were then successively transformed into P. pastoris GS115.
Purification of ReGal2 in the engineered expression system
The crude culture supernatant of P. pastoris transformants with 0.5% methanol induction was fractioned through precipitation with ammonium sulfate ((NH4)2SO4). Briefly, 55.9 g of ground (NH4)2SO4 was added to 100 mL of fermentation broth. The mixture was maintained at 4 °C overnight and centrifuged at 10,000 rpm for 20 min. The supernatant was discarded and the pellet was resuspended with twofold volumes of 10 mM Tris–HCl buffer (pH 8.0) containing 100 mM NaCl. The mixture was dialyzed to remove (NH4)2SO4, and subjected to size exclusion chromatography using the ÄKTA™ system (GE Healthcare) equipped with a column of Superdex™ 200 Increase 10/300 Gl. Chromatography was performed using 10 mM Tris–HCl buffer (pH 8.0) plus 100 mM NaCl. Fractions were collected and subjected to enzymatic activity and SDS-PAGE analyses.
α-Galactosidase activity assays
The α-galactosidase activity was determined using the p-nitrophenyl-α-d-galactopyranoside (pNPGal) as substrate. The assays were performed in 200 μl of reaction mixtures containing 10 μl of diluted culture supernatant or purified enzyme and 190 μl pNPGal dissolved in 20 mM HAC-NaAC buffer (pH 4.8). The reaction mixture was then incubated at 50 °C for 10 min. The reaction was terminated by adding 50 μl of 10% Na2CO3. One unit of the enzyme activity (IU) was defined as the amount of enzyme releasing 1 μmol of pNP per minute. The kinetic parameters were determined at 80 °C using different pNPGal concentration (ranging from 0.25 to 2.0 mM). The Michaelis constant (Km) and Vmax were calculated by non-linear regression analysis using Origin 8.5 Pro software.
Purified protein concentration was determined using a Pierce™ BCA Protein Assay kit with standard bovine serum albumin (BSA) as the standard protein.
SDS-PAGE and semi-native PAGE
SDS-PAGE analyses were performed essentially as previously described , except for a modification in sample preheating time that was extended to 15 min. To analyze the polymeric state of ReGal2, samples treated with SDS and β-mercaptoethanol, but without 15-min boiling, were subjected to SDS-PAGE. To analyze the hydrolytic activity against methylumbelliferyl-α-d-galactopyranoside (MUG), ReGal2 with or without heating treatment was loaded to the polyacrylamide gel containing 25 μg ml−1 of MUG. After electrophoresis, the gel was immersed in 20 mM HAC-NaAC buffer at pH 4.8 and incubated for 30 min. The release of methylumbelliferone was visualized under ultraviolet light.
Molecular weight determination
The molecular weight of ReGal2 was determined using size exclusion chromatography with standards (GE Healthcare) as follows: ovalbumin (43 kDa), conalbumin (75 kDa), aldolase (158 kDa), ferritin (44 kDa) and thyroglobulin (669 kDa).
Determination of optimal temperature and pH as well as thermostability
The optimum temperature of the crude culture supernatant or purified ReGal2 was determined by measuring the hydrolytic activity toward pNPGal in 20 mM HAC-NaAC buffer (pH 4.8) at a temperature range from 40 to 100 °C. The thermostability of ReGal2 was determined by measuring the residual enzyme activity after incubation of the enzyme at different temperatures for the indicated time period. The optimum pH of purified ReGal2 was determined by measuring its hydrolytic activity toward pNPGal in different buffers of pH 2–10 at 50 °C. The Na2HPO4-citric acid and Tris–HCl buffers were used for pH 2.0–8.0 and pH 8.0–9.0, respectively.
Effect of the addition of metal ions, protein denaturants and other chemicals
The effect of metal ions on ReGal2 activity was determined by measuring the residual enzymatic activity at 50 °C in the presence of 0–20 mM of NiSO4, KCl, MnSO4, CuSO4, CoCl2, ZnSO4, or AgNO3. The effect of 0–3 M NaCl on ReGal2 activity was determined similarly. The effect of protein denaturants on ReGal2 activity was assessed by measuring the residual enzymatic activities at 50 °C in the presence of 0–200 mM of SDS, Urea, guanidine hydrochloride (GdnHCl), β-mercaptoethanol or EDTA.
Differential scanning calorimetry (DSC)
Thermal unfolding of ReGal2 was determined on a MicroCal VP-Capillary DSC calorimeter (Malvern, UK) with a range of 20–110 °C at a scan rate of 90 °C h−1. The protein concentration was 0.5 mg ml−1.
Soybean treatment with ReGal2
One gram of defatted and ground soybean flour was suspended in 4 ml of 20 mM HAC-NaAC buffer (pH 4.8), shaken for 10 min, and centrifuged at 10,000 rpm for 20 min. After removal of undissolved residues, 300 μl of soymilk was treated with 100 μl of 2 U ml−1 ReGal2 at 50 °C or 70 °C for continuous time periods. The mixture was boiled for 15 min to terminate the reaction, followed by centrifugation at 10,000 rpm for 10 min. The resultant supernatant was subjected to high-performance liquid chromatography (HPLC) analysis that was performed on a REZEX ROA (0138) column with a mobile phase of 0.5632:1000 (v/v) H2SO4:H2O at a flow rate of 0.5 ml min−1 and an injection volume of 10 μl.
Amino acid sequences of α-galactosidases were retrieved from the NCBI database (https://www.ncbi.nlm.nih.gov/). Protein domain organization was analyzed on NCBI. The phylogenetic tree was generated with MEGA 7 .
Results and discussion
Identification of a thermophilic α-galactosidase ReGal2 from the thermophilic fungus R. emersonii
In order to mine α-galactosidases with ideal properties, the genome of the thermophilic (hemi)cellulolytic fungus R. emersonii were analyzed, and five putative α-galactosidase-encoding genes (ReGal1–ReGal5) were retrieved. The five corresponding proteins, ReGal1–ReGal5, are predicted to have a catalytic domain of GH27 family although their overall sequence identify is relatively low (< 34%; Fig. 1). All proteins except ReGal5 have putative signal peptides, suggesting that these enzymes may be secreted extracellularly. ReGal5 instead contains a putative N-terminal transmembrane region and was therefore predicted to be anchored to cell membrane in R. emersonii.
Of the five ReGal genes, ReGal1 has been previously reported to encode a thermophilic α-galactosidase . We therefore performed the heterologous expression of ReGal2–ReGal5. These four genes without coding sequences for signal peptide or N-terminal transmembrane helix were individually expressed under the control of the AOX1 promoter with methanol induction in P. pastoris. The resulting recombinant proteins all exhibited α-galactosidase activities as demonstrated by the remarkable hydrolytic activities toward pNPGal in the culture supernatant of the respective P. pastoris transformants (Table 2). However, SDS-PAGE analysis showed that the extracellular amounts of these recombinant α-galactosidases varied. The lowest production was observed for ReGal2 with barely detectable protein band on SDS-PAGE (Fig. 2a).
The optimum temperature of each recombinant α-galactosidase was measured with the crude culture supernatant. As shown in Fig. 2 and Table 2, while ReGal3 and ReGal4 showed their maximum activity at 50 °C, ReGal2 and ReGal5 exhibited their highest activity at 80 °C and 65 °C, respectively, suggesting that ReGal2 and ReGal5 are potential thermophilic enzymes. The observation that these enzymes showed varying optimum temperatures may implicate a cooperative division of action among them, allowing the fungus to achieve the efficient degradation when confronted with changing environmental conditions. Given that ReGal2 is the most thermoactive enzyme among these α-galactosidases, we next focused on the purification and characterization of ReGal2.
Improved expression and purification of recombinant ReGal2 in an optimized P. pastoris expression system with enhanced AOX1 promoter activity
As shown above, the production yield of ReGal2 in P. pastoris is too low to obtain decent amounts of purified proteins for further characterization. Attempts were therefore made to improve protein production by enhancing the AOX1 promoter activity via 1) overexpressing the transcriptional activators, Mxr1 and Mit1 [21, 22], and 2) expanding their putative binding elements within the AOX1 promoter [22, 29] (Fig. 3a). The reporter gene gfp was fused to the native or the engineered AOX1 promoter for evaluation of their activities via fluorescence intensity analysis. As shown in Fig. 3b, overexpression of Mxr1 or Mit1 driven by the constitutive GAP promoter markedly enhanced the AOX1 promoter activity on methanol, with a more pronounced enhancement (4.5-fold in fluorescence intensity) resulted from Mxr1 expression. To make the most of the overexpressed Mxr1 or Mit1, we purposedly placed the − 719 to − 503 promoter region that contains putative binding motifs of Mxr1 or Mit1, but without the binding motif of the transcription repressor PpNrg1 , at the 5′ end of the AOX1 promoter. This modified promoter resulted in a 4.4-fold increase in the fluorescence intensity compared to that driven by the native promoter (Fig. 3b). Combining these two strategies to further elevate the engineered AOX1 promoter activity resulted in an overall 7.5-fold increase in the fluorescence intensity, compared to that in the conventional P. pastoris system (Fig. 3b, c).
ReGal2 was then expressed in the optimized P. pastoris expression system. Compared with the conventional system, ReGal2 production was markedly enhanced, as shown by the significantly increased extracellular α-galactosidase activity and the readily detected protein band resolved by SDS-PAGE (Fig. 3d, e). The enhanced ReGal2 production facilitated the following two-step purification via ammonium sulfate precipitation and size-exclusion chromatography, with a final yield of ~ 15 mg l−1.
Biochemical characteristics of the recombinant ReGal2
ReGal2 is an oligomer
In most cases, the recombinant ReGal2 migrated on SDS-PAGE as a single, homogenous band with an estimated molecular weight (MW) of 66 kDa, which is a little higher than the predicted MW of a 6 × His-tagged monomer (54 kDa). However, an additional band with a much higher estimated MW, which was verified to be ReGal2 by mass spectrometry, was also observed (Fig. 3e), suggesting that ReGal2 may adopt an oligomeric structure. Further analysis revealed that ReGal2 heat-treated for up to 15 min is present mainly in monomeric forms whereas the untreated enzyme essentially forms the higher MW oligomers (Fig. 4a). Moreover, semi-native PAGE with MUG as the substrate indicated that the active form of ReGal2 is the oligomer but not the monomer (Fig. 4b). The native MW of ReGal2 as determined by gel filtration is 362 kDa (Fig. 4c), suggesting that ReGal2 may be a hexamer.
Catalytic properties of ReGal2
The purified ReGal2 was active over a broad temperature range (50–100 °C) and exhibited an optimum temperature at 80 °C (Fig. 5a). ReGal2 showed the maximum activity at pH 4.0 (Fig. 5b), which is consistent with an acidic optima for most fungal α-galactosidases (optimum pH 4–6) (Table 1). Under the optimum temperature and pH, ReGal2 showed the highest specific activity of 935 U mg−1 toward pNPGal, which is among the most effiencient fungal α-galactosidases that have been reported (Table 1). Using pNPGal as substrate, the Km, Vmax, and kcat values of ReGal2 were determined to be 0.19 ± 0.04 mM, 566.5 ± 15.9 µmol−1min−1mg−1, and 623.1 ± 17.5 s−1, respectively. The catalytic efficiency (kcat/Km) of ReGal2 was 3279.7 s−1 mM−1, which is much higher than the reported thermophilic fungal counterparts, including the first characterized α-galactosidase (ReGal1 in our study) from R. emersonii .
Thermostability of ReGal2
ReGal2 displayed remarkable tolerance to high temperature, retaining 20% of the maximum activity even at 100 °C (Fig. 5a). Further thermal inactivation analyses demonstrated that ReGal2 was 100% active after incubation at 50–70 °C for 3 h (Fig. 5c), and full activity was still maintained after up to 60 h of incubation at 70 °C (data not shown). This is in sharp contrast with the so far characterized thermostable fungal counterparts, which usually lost hydrolytic activities after incubation at 70 °C (Table 1). Of note, ReGal2 retained 80% of its initial activity after incubation of 3 h at 80 °C, whereas TtGalA, one of the most thermophilic α-galactosidase from the thermophilic bacterium Thermus thermophiles, retains only 9.7% of its initial activity after the same treatment . Consistently, DSC analysis showed that ReGal2 had a high melting temperature of 97.9 °C (Fig. 5d), an excellent trait that is frequently observed in thermophilic proteins. The above results indicate that ReGal2 is highly thermostable.
Effect of metal ions and chemical reagents on the activity of ReGal2
The effect of different metal ions or chemical reagents on the activity of ReGal2 is shown in Tables 3 and 4. Like many other thermophilic fungal counterparts, ReGal2 was remarkably resistant to most metal ions tested, including Ni2+, K+, Mn2+, Cu2+, Co2+, Zn2+, and Mg2+, but was sensitive to Ag+ (Table 5). ReGal2 also exhibited a relatively high tolerance to NaCl, keeping 76% of its activity with up to 3 M NaCl (Table 6).
On the other hand, as with other thermophilic counterparts, the enzymatic activity of ReGal2 was hardly affected in the presence of EDTA (Table 5), suggesting that ReGal2 may not have a specific requirement for divalent metal ions as cofactors. Notably, ReGal2 exhibited a significant tolerance to SDS and β-mercaptoethanol with hardly any activity lost when treated with SDS or β-mercaptoethanol up to 200 mM, which is in agreement with the observation that it retained the active oligomeric state during electrophoresis in the presence of these two denaturants. This is quite unique among the so far characterized α-galactosidases, which markedly lost activities in the presence of SDS (Table 5) [9, 10, 12, 31,32,33]. Even more surprisingly, ReGal2 did not show reduced activity in the presence of urea (up to 200 mM), and maintained approximately up to 80% of its initial activity in the presence of GdnHCl (200 mM), which is a stronger denaturant than urea. This is in sharp contrast with the thermophilic and oligomeric TtGalA, which lost 40% and 64% activities even in the presence of 5 mM urea and GdnHCl, respectively . Together these results indicate that ReGal2 is capable of maintaining its active state even in the presence of potent protein structural denaturants.
Given the many reports indicating that oligomerization stabilizes protein structure, it is reasonably to speculate that oligomerization of ReGal2 contributes to its outstanding tolerance to high temperature and a number of chemicals, especially protein denaturants. Notwithstanding this, exception to this rule does exist wherein two oligomeric thermophilic α-galactosidases, one from Ganoderma lucidum and the other from Thermus thermophilus, have been reported to be highly sensitive to protein denaturants [31, 34]. We therefore speculated that additional structural features unique to ReGal2 may account for its exceptional structural stability, which merits further investigation.
Elimination of RFOs from soybean with ReGal2
Soybeans rich in vegetable proteins are used in a variety of food and fodder fields. However, high concentrations of flatulence-causing RFOs have to be removed to improve the soybean utilization efficiency. To test the efficiency of ReGal2 in removing RFOs from soybean materials, we determined changes of stachyose and raffinose content in defatted soybean meal upon treatment with ReGal2. The original amount of stachyose and raffinose in untreated soybean substrate was determined to be 10.37 mg ml−1 and 2.96 mg ml−1, respectively. A time-course of stachyose and raffinose hydrolysis upon treatment with ReGal2 were analyzed (Fig. 6). Stachyose was found to decrease by 45% and 71% after treatment for 1 h at 50 °C and 70 °C, respectively. The residual stachyose was completely hydrolyzed in 12 h at 50 °C, which was dramatically shortened to 3 h at 70 °C. As a result of stachyose hydrolysis, the raffinose content increased during the early reaction period, but was later on decreased by 55% in 12 h, and completely removed in 24 h after treatment with ReGal2 at 70 °C. These data thus indicate that ReGal2 is able to efficiently remove RFOs from soybeans, and therefore holds great promise in beet sugar processing as well as in food and feed industries for improving the nutritive quality of soybean and other legumes.
In this study, a thermophilic α-galactosidase encoding gene (Regal2) was identified from the thermophilic (hemi)cellulolytic fungus, R. emersonii, expressed and purified from an optimized P. pastoris expression system with significantly increased production yield. ReGal2 exhibited remarkable thermostability and superior resistance to protein denaturants, e.g., SDS, urea, and GdnHCl. ReGal2 possessed high specific catalytic activity and efficiently removed the anti-nutrient RFOs in soybean. The identified ReGal2 thus holds great potential in relevant biotechnological applications. The optimized P. pastoris expression system would also be widely used to increase production yield of heterologous proteins, and therefore contributes to mining more enzymes with desired features.
Availability of data and materials
All data generated or analyzed during this study are included in this published article.
Aulitto M, Fusco S, Limauro D, Fiorentino G, Bartolucci S, Contursi P. Galactomannan degradation by thermophilic enzymes: a hot topic for biotechnological applications. World J Microbiol Biotechnol. 2019;35:32.
Aulitto M, Fusco FA, Fiorentino G, Bartolucci S, Contursi P, Limauro D. A thermophilic enzymatic cocktail for galactomannans degradation. Enzyme Microb Technol. 2018;111:7–11.
Katrolia P, Rajashekhara E, Yan Q, Jiang Z. Biotechnological potential of microbial alpha-galactosidases. Crit Rev Biotechnol. 2014;34:307–17.
Cantarel BL, Coutinho PM, Rancurel C, Bernard T, Lombard V, Henrissat B. The Carbohydrate-Active EnZymes database (CAZy): an expert resource for Glycogenomics. Nucleic Acids Res. 2009;37:D233–8.
Clarke JH, Davidson K, Rixon JE, Halstead JR, Fransen MP, Gilbert HJ, Hazlewood GP. A comparison of enzyme-aided bleaching of softwood paper pulp using combinations of xylanase, mannanase and alpha-galactosidase. Appl Microbiol Biotechnol. 2000;53:661–7.
Ghazi S, Rooke JA, Galbraith H. Improvement of the nutritive value of soybean meal by protease and alpha-galactosidase treatment in broiler cockerels and broiler chicks. Br Poult Sci. 2003;44:410–8.
Kobayashi H, Suzuki H. Studies on the decomposition of raffinose by alpha–galactosidase of mold. II. Formation of mold pellet and its enzyme activity. J Ferment Technol. 1972;50:625–9.
Sharma S, Vaid S, Bhat B, Singh S, Bajaj BK. Thermostable enzymes for industrial biotechnology. In advances in enzyme technology. New York: Elsevier; 2019. p. 469–95.
Wang H, Shi P, Luo H, Huang H, Yang P, Yao B. A thermophilic alpha-galactosidase from Neosartorya fischeri P1 with high specific activity, broad substrate specificity and significant hydrolysis ability of soymilk. Bioresour Technol. 2014;153:361–4.
Wang H, Ma R, Shi P, Huang H, Yang P, Wang Y, Fan Y, Yao B. Insights into the substrate specificity and synergy with mannanase of family 27 alpha-galactosidases from Neosartorya fischeri P1. Appl Microbiol Biotechnol. 2015;99:1261–72.
Puchart V, Vrsanska M, Bhat MK, Biely P. Purification and characterization of alpha-galactosidase from a thermophilic fungus Thermomyces lanuginosus. Biochim Biophys Acta. 2001;1524:27–37.
Wang C, Wang H, Ma R, Shi P, Niu C, Luo H, Yang P, Yao B. Biochemical characterization of a novel thermophilic alpha-galactosidase from Talaromyces leycettanus JCM12802 with significant transglycosylation activity. J Biosci Bioeng. 2016;121:7–12.
Simila J, Gernig A, Murray P, Fernandes S, Tuohy MG. Cloning and expression of a thermostable alpha-galactosidase from the thermophilic fungus Talaromyces emersonii in the methylotrophic yeast Pichia pastoris. J Microbiol Biotechnol. 2010;20:1653–63.
Maheshwari R, Bharadwaj G, Bhat MK. Thermophilic fungi: their physiology and enzymes. Microbiol Mol Biol Rev. 2000;64:461–88.
Murray P, Aro N, Collins C, Grassick A, Penttila M, Saloheimo M, Tuohy M. Expression in Trichoderma reesei and characterisation of a thermostable family 3 beta-glucosidase from the moderately thermophilic fungus Talaromyces emersonii. Protein Expr Purif. 2004;38:248–57.
Wang K, Luo H, Bai Y, Shi P, Huang H, Xue X, Yao B. A thermophilic endo-1,4-beta-glucanase from Talaromyces emersonii CBS394.64 with broad substrate specificity and great application potentials. Appl Microbiol Biotechnol. 2014;98:7051–60.
Tuohy MG, Puls J, Claeyssens M, Vrsanska M, Coughlan MP. The xylan-degrading enzyme system of Talaromyces emersonii: novel enzymes with activity against aryl beta-d-xylosides and unsubstituted xylans. Biochem J. 1993;290(Pt 2):515–23.
Juturu V, Wu JC. Heterologous protein expression in Pichia pastoris: latest research progress and applications. ChemBioChem. 2018;19:7–21.
Ahmad M, Hirz M, Pichler H, Schwab H. Protein expression in Pichia pastoris: recent achievements and perspectives for heterologous protein production. Appl Microbiol Biotechnol. 2014;98:5301–17.
Zhu T, Sun H, Wang M, Li Y. Pichia pastoris as a versatile cell factory for the production of industrial enzymes and chemicals: current status and future perspectives. Biotechnol J. 2019;14:e1800694.
Lin-Cereghino GP, Godfrey L, de la Cruz BJ, Johnson S, Khuongsathiene S, Tolstorukov I, Yan M, Lin-Cereghino J, Veenhuis M, Subramani S, Cregg JM. Mxr1p, a key regulator of the methanol utilization pathway and peroxisomal genes in Pichia pastoris. Mol Cell Biol. 2006;26:883–97.
Wang X, Wang Q, Wang J, Bai P, Shi L, Shen W, Zhou M, Zhou X, Zhang Y, Cai M. Mit1 transcription factor mediates methanol signaling and regulates the alcohol oxidase 1 (AOX1) promoter in Pichia pastoris. J Biol Chem. 2016;291:6245–61.
Wang J, Wang X, Shi L, Qi F, Zhang P, Zhang Y, Zhou X, Song Z, Cai M. Methanol-independent protein expression by AOX1 promoter with trans-acting elements engineering and glucose-glycerol-shift induction in Pichia pastoris. Sci Rep. 2017;7:41850.
Vogl T, Sturmberger L, Fauland PC, Hyden P, Fischer JE, Schmid C, Thallinger GG, Geier M, Glieder A. Methanol independent induction in Pichia pastoris by simple derepressed overexpression of single transcription factors. Biotechnol Bioeng. 2018;115:1037–50.
Turkanoglu Ozcelik A, Yilmaz S, Inan M. Pichia pastoris promoters. Methods Mol Biol. 1923;2019:97–112.
Heckman KL, Pease LR. Gene splicing and mutagenesis by PCR-driven overlap extension. Nat Protoc. 2007;2:924–32.
Laemmli UK. Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature. 1970;227:680–5.
Kumar S, Stecher G, Tamura K. MEGA7: molecular evolutionary genetics analysis version 7.0 for bigger datasets. Mol Biol Evol. 2016;33:1870–4.
Kranthi BV, Kumar R, Kumar NV, Rao DN, Rangarajan PN. Identification of key DNA elements involved in promoter recognition by Mxr1p, a master regulator of methanol utilization pathway in Pichia pastoris. Biochim Biophys Acta. 2009;1789:460–8.
Wang X, Cai M, Shi L, Wang Q, Zhu J, Wang J, Zhou M, Zhou X, Zhang Y. PpNrg1 is a transcriptional repressor for glucose and glycerol repression of AOX1 promoter in methylotrophic yeast Pichia pastoris. Biotechnol Lett. 2016;38:291–8.
Aulitto M, Fusco S, Fiorentino G, Limauro D, Pedone E, Bartolucci S, Contursi P. Thermus thermophilus as source of thermozymes for biotechnological applications: homologous expression and biochemical characterization of an alpha-galactosidase. Microb Cell Fact. 2017;16:28.
Katrolia P, Jia H, Yan Q, Song S, Jiang Z, Xu H. Characterization of a protease-resistant alpha-galactosidase from the thermophilic fungus Rhizomucor miehei and its application in removal of raffinose family oligosaccharides. Bioresour Technol. 2012;110:578–86.
Hu Y, Tian G, Geng X, Zhang W, Zhao L, Wang H, Ng TB. A protease-resistant α-galactosidase from Pleurotus citrinopileatus with broad substrate specificity and good hydrolytic activity on raffinose family oligosaccharides. Process Biochem. 2016;51:491–9.
Sripuan T, Aoki K, Yamamoto K, Tongkao D, Kumagai H. Purification and characterization of thermostable alpha-galactosidase from Ganoderma lucidum. Biosci Biotechnol Biochem. 2003;67:1485–91.
Larkin MA, Blackshields G, Brown NP, Chenna R, McGettigan PA, McWilliam H, Valentin F, Wallace IM, Wilm A, Lopez R, et al. Clustal W and Clustal X version 2.0. Bioinformatics. 2007;23:2947–8.
Cavazzoni V, Adami A, Craveri R. α-Galactosidase from the yeast Candida javanica. Appl Microbiol Biotechnol. 1987;26:555–9.
Shankar SK, Kumar SK, Mulimani VH. Calcium alginate entrapped preparation of alpha-galactosidase: its stability and application in hydrolysis of soymilk galactooligosaccharides. J Ind Microbiol Biotechnol. 2011;38:1399–405.
Sinitsyna OA, Fedorova EA, Vakar IM, Kondratieva EG, Rozhkova AM, Sokolova LM, Bubnova TM, Okunev ON, Chulkin AM, Vinetsky YP, Sinitsyn AP. Isolation and characterization of extracellular alpha-galactosidases from Penicillium canescens. Biochemistry (Mosc). 2008;73:97–106.
Hu Y, Zhu M, Tian G, Zhao L, Wang H, Ng TB. Isolation of a protease-resistant and pH-stable alpha-galactosidase displaying hydrolytic efficacy toward raffinose family oligosaccharides from the button mushroom Agaricus bisporus. Int J Biol Macromol. 2017;104:576–83.
Jang JM, Yang Y, Wang R, Bao H, Yuan H, Yang J. Characterization of a high performance alpha-galactosidase from Irpex lacteus and its usage in removal of raffinose family oligosaccharides from soymilk. Int J Biol Macromol. 2019;131:1138–46.
This work is supported by grants from the National Key Research and Development Program of China (2018YFA0900501 and 2018YFA0900503), National Natural Science Foundation of China (31770047 and 31670040), and Shandong Technology Innovation Center of Synthetic Biology (sdsynbio-2018PY-01).
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An, J., Zhang, W., Wu, W. et al. Characterization of a highly stable α-galactosidase from thermophilic Rasamsonia emersonii heterologously expressed in a modified Pichia pastoris expression system. Microb Cell Fact 18, 180 (2019). https://doi.org/10.1186/s12934-019-1234-6
- Rasamsonia emersonii
- Structural stability
- Pichia pastoris AOX1 promoter