Random mutagenesis is a powerful technique to obtain mutant proteins with different properties from the wild-type molecule. Error-prone PCR is often employed for random mutagenesis in bacterial protein expression systems, but has rarely been used in the methylotrophic yeast Pichia pastoris system, despite its significant advantages, mainly because large (μg-level) amounts of plasmids are required for transformation.
We developed a quick and easy technique for random mutagenesis in P. pastoris by sequential Phi29 DNA polymerase-based amplification methods, error-prone rolling circle amplification (RCA) and multiple displacement amplification (MDA). The methodology was validated by applying it for random mutation of the gene encoding cellulase from the basidiomycete Phanerochaete chrysosporium (PcCel6A), a key enzyme in degradation of cellulosic biomass. In the error-prone RCA step, the concentrations of manganese ion (Mn2+) and cellulase gene-containing plasmid were varied, and the products obtained under each condition were subjected to the second MDA step in the absence of Mn2+. The maximum error rate was 2.6 mutations/kb, as evaluated from the results of large-scale sequencing. Several μg of MDA products was transformed by electroporation into Pichia cells, and the activities of extracellularly expressed PcCel6A mutants towards crystalline and amorphous celluloses were compared with those of wild-type enzyme to identify key amino acid residues affecting degradation of crystalline cellulose.
We present a rapid and convenient random mutagenesis method that does not require laborious steps such as ligation, cloning, and synthesis of specific primers. This method was successfully applied to the protein expression system in P. pastoris.
Mutagenesis is an important technique in protein engineering to modify properties such as thermostability, optimum pH and specific activity, or to understand structure–function relationships of target proteins. There are two main approaches, i.e., rational design and random mutagenesis. Rational design is attractive when sufficient information is available about the protein structure, for example, if the key active-site amino acid residue(s) have been identified, even if their function is not fully established. On the other hand, random mutagenesis, i.e., introducing random mutations into the protein-coding gene and then screening the expressed mutant proteins, provides access to proteins having altered properties without human bias. Many proteins have been successfully engineered by means of random mutagenesis methods .
It is important that random mutagenesis methodology should be simple, because it is often necessary to screen large numbers of mutants, in contrast to the case of rational design. Escherichia coli and Saccharomyces cerevisiae are generally used as protein expression hosts for random mutagenesis because of the availability of various plasmids. However, heterologous expression of eukaryotic genes is often restricted in these organisms [2–4]. The methylotrophic yeast Pichia pastoris is a useful alternative, as it can perform many of the post-translational modifications found in higher eukaryotic cells, and it has been used to express proteins from a variety of different organisms, including human, vertebrates, fungi, plants and bacteria, in milligram-to-gram quantities . Furthermore, P. pastoris is able to secrete heterologous proteins directly into the culture medium, which enables easy screening of mutant libraries and simplifies downstream purification. Despite these advantages, however, P. pastoris has rarely been used in random mutagenesis , mainly because the transformation efficiency is usually several orders of magnitude lower than that for E. coli and other yeasts . Microgram amounts of plasmids are required for integration into the P. pastoris genome via homologous recombination, and therefore expression plasmids are often designed as shuttle vectors to enable rapid amplification in bacterial cloning hosts . This technique is feasible for low-throughput analyses, but is too time-consuming for high-throughput experiments because of the need for thousands of bacterial transformations and plasmid isolations. To date, there are only a few established methods of random mutagenesis in this host [8–11].
Cellulase plays a key role in producing fermentable glucose from lignocellulosic biomass by hydrolyzing glycosidic bonds of cellulose, a linear biopolymer of β-1,4-linked d-glucose units. Cellulase has recently attracted much attention because of its enormous potential for application in commercial-scale biofuel production. However, the slow hydrolysis rate is still a bottleneck of this technology, because cellulose, especially crystalline cellulose, is quite resistant to hydrolysis. Therefore, improvement of cellulase performance has been a focus of research for many years and many researchers have attempted to engineer cellulase to improve the enzyme activity, thermal stability, or pH range [12–16]. Error-prone PCR and DNA shuffling have been used successfully in random mutagenesis of cellulases, but the limited host range for expression remains a key issue, especially for fungal cellulases. Other challenges include the complexity of transformation and screening operations with yeast or other eukaryotic host organisms, and low productivity of recombinant proteins. We have reported heterologous expression of many biomass utilization-related enzymes from the basidiomycete Phanerochaete chrysosporium in P. pastoris at the gram per liter of culture level [17–19]. In addition, utilization of P. pastoris for cellulase production would be advantageous for biofuel production, because this organism is able to ferment glucose to ethanol, and therefore it could be used in a consolidated bioprocess (CBP) involving simultaneous production of enzyme protein for sugar formation and fermentation of the sugar to obtain ethanol.
We describe here a simple random mutagenesis method for the P. pastoris expression system. To obtain microgram amounts of randomly mutated DNA, Phi29 DNA polymerase was repeatedly used (Fig. 1). This polymerase has strong strand displacement activity, and has been used for exponential amplification of circular DNA or genomic DNA [20–22]. The first step in our method is introduction of random mutations using the error-prone rolling circle amplification (RCA) method reported by Fujii [23, 24]. The second step is amplification of mutated DNA by Phi29 DNA polymerase, which is generally called multiple displacement amplification (MDA). The combination of these methods provide sufficient DNA to enable the P. pastoris expression system to be used easily for random mutagenesis experiments.
Pichia pastoris KM71H strain and the expression vector pGAPZαA were purchased from Invitrogen (Carlsbad, CA, USA). TempliPhi 100 DNA amplification kit was purchased from GE Healthcare (Buckinghamshire, UK). RepliPHI™ Phi29 Reagent Set and thiophosphate-modified random hexamer primer were bought from Epicentre (Madison, WI, USA) and Sigma-Aldrich (St. Louis, MO, USA), respectively. The restriction enzyme BlnI was purchased from TaKaRa (Shiga, Japan). Amorphous cellulose, phosphoric acid-swollen cellulose (PASC), was prepared from Avicel cellulose powder Funacel II from Funakoshi Ltd (Tokyo, Japan) . Crystalline cellulose IIII was prepared from green algae Cladophora spp. as described previously . Novozyme 188 β-glucosidase and Glucose CII Test Wako were purchased from Novozymes (Bagsværd, Denmark) and Wako Pure Chemical Industries (Osaka, Japan), respectively. MightyPrep reagent for DNA and KOD plus version 2 DNA polymerase were bought from TaKaRa (Shiga, Japan) and Toyobo (Osaka, Japan), respectively.
Error-prone rolling circle amplification
The gene encoding PcCel6A from P. chrysosporium (cel6A) was cloned into the pGAPZαA vector based on the previous report . The purified pGAPZα/cel6A vector was dissolved in water at the concentration of 100, 200, 500 or 1000 pg/μl and used as a template for the RCA reaction. RCA was performed using the Templiphi 100 DNA amplification kit based on the method described by Fujii et al. [23, 24]. In brief, 0.5 μl of the template was mixed with 5 μl of sample buffer containing random hexamers, and the mixture was heated at 95 °C for 3 minutes to denature the plasmid, and then immediately cooled to room temperature. The amplification reaction was started by addition of 1 μl of MnCl2 solution (0, 20, 40 mM), 5 μl of reaction buffer and 0.2 μl of enzyme mix. After 24-hours incubation at 30 °C, the mixture was heated at 65 °C for 10 minutes to inactivate the enzyme, and the amplification of DNA was confirmed by electrophoresis in a 0.8 % agarose gel. To estimate the amount of amplified vectors, the error-prone RCA product was treated with restriction enzyme BlnI for 3 hours and then subjected to 1 % agarose gel electrophoresis.
Multiple displacement amplification of the error-prone RCA product
After error-prone RCA under 12 conditions (0, 1.0, 2.0 mM Mn2+ versus 50, 100, 250, and 500 pg of template), the second amplification by Phi29 DNA polymerase was conducted with the RepliPHI™ Phi29 Reagent Set. The error-prone RCA product was diluted 10 times with water and a 2.5 μl aliquot of the diluted product was mixed with 5 μl of 10× reaction buffer and 5 μl of 100 μM random hexamer. The mixture was heated at 95 °C for 3 minutes, then cooled to room temperature, and the amplification reaction was started by adding dNTPs, DTT and Phi29 DNA polymerase (total volume 50 μl). The final concentrations were 2 U/μl of Phi29 DNA polymerase, 10 μM of random hexamers, 5 mM DTT, and 0.25 mM each dNTP in 40 mM Tris–HCl buffer (pH 7.5) containing 10 mM MgCl2, 5 mM (NH4)2SO4 and 50 mM KCl. After incubation at 30 °C for 18 hours, the mixture was heated at 65 °C for 10 minutes to inactivate the enzyme and DNA amplification was confirmed by electrophoresis in 0.8 % agarose gel. To estimate the amount of amplified plasmids in the total amplified DNA, the product was digested with restriction enzyme BlnI for 3 hours and subjected to 1 % agarose gel electrophoresis.
Large-scale sequencing of a mutant library
Twelve samples of MDA products obtained above were purified with a MinElute PCR purification kit (QIAGEN, Hilden, Denmark) after digestion with restriction enzyme BlnI. Sequencing was performed using an Illumina HiSeq 2000 according to the standard protocol of Illumina Inc. Briefly, library construction was performed according to the Illumina TruSeq™ DNA Sample Preparation Guide. Cluster generation took place on the Illumina cBot by using a TruSeq™ Rapid PE Cluster Kit. The libraries were then subjected to Illumina HiSeq 2000 sequencing according to standard procedures. Paired-end 100-bp reads were generated and the raw sequencing data was processed with the Illumina analysis pipeline (CASAVA ver. 1.8). Short reads were filtered and trimmed with the qtrim program (Genaris, Inc., Yokohama, Japan) to increase analytical precision. These short reads were aligned to the sequence data of pGAPZα/cel6A (4.4 kbp) using the Burroughs–Wheeler Aligner (BWA; Cambridge, UK) with default parameter settings.
Mutation frequency analysis
The sequence data was analyzed to compare the mutation frequencies obtained under various conditions of error-prone RCA. Mutation frequency was calculated at each reference base of cel6A (1320 bp, A:255 T:256 G:330 C:479) by dividing the number of mismatches (substitutions, insertions and deletions) by the number of total sequenced bases. A histogram was generated with IGOR Pro software (Ver. 6.1) by plotting mutation frequency at each reference base. Curve fittings were performed by using the log-normal distribution of Multi-peak fit function (Ver. 2.00). Heat maps were drawn by Microsoft Excel. The GC content was defined as the percentage of GC in 6 neighbor sequences. The heat map was also drawn for the whole vector pGAPZα/cel6A in a similar way with the cel6A region analysis.
Production of enzymes in Pichia pastoris
Approximately 5 μg of the MDA product (50 μl of the MDA product) was digested with BlnI prior to transformation of P. pastoris. After purification of DNA by ethanol precipitation, electroporation was carried out according to the instruction manual of the EasySelect™ Pichia expression kit. The plasmids were also prepared by the usual preparation method described in the manual, including E. coli transformation and plasmid isolation by miniprep, and were transformed as a control. The transformed cells were plated in YPDS agar (1 % yeast extract, 2 % polypeptone, 2 % glucose, 1 M sorbitol, 1.5 % agar) plus zeocin (100 μg/ml) and incubated at 30 °C. Single colonies of the transformants were transferred into deep-well microtiter plates containing 1 ml of YPDZ media per well (1 % yeast extract, 2 % polypeptone, 2 % glucose, 100 μg/ml zeocin) and incubated at 30 °C for 3 days with shaking at 1400 rpm. Gene expression was driven by the constitutive GAP promoter, and the protein was accumulated during 3 days cultivation without addition of any inducer.
Characterization of mutant enzymes
All hydrolysis experiments were performed in 96-well Multiscreen HTS plates (Millipore), of which the bottoms were sealed. Ten μl aliquots of yeast culture supernatants were incubated with PASC (0.05 %, w/v) or cellulose IIII (0.05 %, w/v) for 2 hours at 40 °C with shaking at 1000 rpm. Each well contained 100 mM sodium acetate buffer (pH 5.0), and Novozyme 188 β-glucosidase was added to the mixture to convert cellooligosaccharides to glucose. The mixture was filtered through the plates to terminate the reaction. The amount of released sugars was determined using Glucose CII Test Wako: 50 μl of filtrate was mixed with 150 μl of the test kit and the absorbance of 492 nm was measured with a Multiskan FC (Thermo Fisher Scientific, USA).
The PASC-degrading activity was measured for 87 transformants obtained by the error-prone RCA-MDA under the conditions of 2 mM Mn2+ and 100 pg template, 100 transformants under the conditions of 2 mM Mn2+and 250 pg template, and 96 colonies obtained by the usual plasmid preparation method. For further characterization, 87 transformants whose activity was more than 10 % of the wild-type activity were randomly selected from those obtained by error-prone RCA-MDA listed above. The PASC- and cellulose IIII-degrading activities were measured for all 87 selected colonies and the cel6A region was sequenced as follows. Colonies on the plate were picked up, suspended in 100 µl MightyPrep reagent and incubated at 95 °C for 10 minutes for DNA extraction. PCR were performed using KOD plus DNA polymerase. The PCR products were purified and the inserted cel6A region was sequenced using the Eurofins sequencing service (Eurofins MWG Operon). Total protein concentration of each culture supernatant was determined by Bradford assay (Bio-rad, Hercules CA, USA) with bovine serum albumin (BSA) as a standard. The three-dimensional structure of PcCel6A catalytic domain was determined (submitted elsewhere) and the structure of CBM was predicted by using Protein Homology/analogy Recognition Engine (Phyre) version 2.0 (http://www.sbg.bio.ic.ac.uk/phyre2/). Figures for molecular models were prepared using the PyMOL Molecular Graphics System, Version 1.7 Schrödinger, LLC .
Results and discussion
We have developed a novel, rapid random mutagenesis strategy that enables the P. pastoris expression system to be used for directed evolution of eukaryotic proteins, despite its low transformation efficiency. This method is composed of sequential plasmid amplification by means of error-prone RCA and MDA of the error-prone RCA products, followed by protein expression in P. pastoris (Fig. 1).
Error-prone rolling circle amplification
Phi29 DNA polymerase amplifies circular DNAs isothermally and yields linear DNAs composed of tandem repeats of the circular DNA plasmids . In error-prone RCA, the gene coding a target protein is first cloned into an expression vector and then the whole vector is amplified in the presence of Mn2+ to introduce mutations of the target gene [23, 24]. In this study, various amounts of circular pGAPZα vectors including cel6A gene (50–500 pg) were amplified in the presence of 0–2 mM MnCl2.
The products thus obtained appeared at positions corresponding to more than 10 kbp in agarose gel electrophoresis. Therefore, the products were digested with restriction enzyme (BlnI) to afford linear fragments of 4.4 kbp, which is identical to the sum of vector and insert. The yield of the products decreased with increase of Mn2+ concentration and also with decrease of the initial amount of template, as shown in Fig. 2a. The largest amount of amplified plasmids estimated from gel electrophoresis was ~1 μg in a total volume of 10 μl. However, plasmids obtained in the presence of 2 mM Mn2+ were less than 10 ng/µl, and no band of the expected size appeared in the presence of 4 mM Mn2+ (data not shown).
The amount of the error-prone RCA products shown in Fig. 2a is more than enough for transformation in the E. coli expression system, as reported by Fujii and coworkers . E. coli needs only a ng-level amount of plasmids for transformation, but on the other hand, it is not enough for the Pichia expression system. The transformation efficiency of E. coli is generally 108–1011 transformants per µg of DNA, on the other hand, the electroporation of P. pastoris yields 103–104 transformants per µg of linearized DNA [6, 29]. The low transformation efficiency of P. pastoris is unavoidable because the yeast cell has thicker walls compared with Bacteria and plasmid must enter through the walls and be integrated into specific locations in the chromosome. The difference in the vector integration results in the increased stability of expression strains but the reduced transformation efficiency.
Multiple displacement amplification of the error-prone RCA product
To obtain plasmids with random mutation on a larger (μg) scale, we used Phi29 DNA polymerase again for amplification of the linear DNA by means of MDA. Twelve samples of the error-prone RCA product (0, 1, 2 mM Mn2+ versus 50, 100, 250, 500 pg of template) were diluted 10-fold and directly used as templates for MDA amplification. As shown in Fig. 2b, almost the same level of amplification was obtained for all samples, indicating that the initial RCA products are long enough to serve as templates of MDA. The amount of linear plasmids obtained after restriction enzyme treatment was about 5 μg in a total volume of 50 μl, which is enough for P. pastoris transformation.
Analysis of mutation frequency using large-scale sequencing
To evaluate the mutation frequency after the two-step amplification, the MDA products were sequenced with an Illumina sequencer. The number of sequenced bases for each error-prone RCA condition was 0.6–4 gb/sample for the 4.4 kbp vector (Additional file 1: Table S1). After removal of low-quality bases, we analyzed errors in the cel6A region. As we used large-scale sequencing, we could calculate the mutation frequency at each base (cel6A 1320 bp, A:255 T:256 G:330 C:479) for detailed analysis.
The minimum and maximum of total sequenced bases at each base of cel6A and the averaged mutation frequencies are shown in Table 1. The maximum mutation frequency (2.60 kb−1) was obtained with 2 mM Mn2+ and 100 pg template. The mode and distribution of mutation frequency were also analyzed and the results are shown as a histogram in Fig. 3. Under all conditions, the bases of cel6A were log-normally distributed. The number of errors increased with increasing concentration of Mn2+ in accordance with Fujii’s findings . Surprisingly, at high template concentration (500 pg), the averaged mutation frequency was high (2.07 kb−1) even in the absence of Mn2+ in the reaction mixture. Thus, higher concentrations of Mn2+ and templates tended to result in higher error ratios.
The types of substitution mutation varied, as shown in Additional file 1: Tables S2–S5. The mutation frequency of each substitution is shown on the left side of each column to illustrate any inherent bias of this error-prone RCA-MDA method, and the proportion of the total mutations in cel6A is shown in parentheses. The exchange of A to C revealed an overall trend towards high mutation frequency, reaching 1.44–1.65 kb−1 under 9 conditions. The transition/transversion ratio was 0.4–0.6, except for the condition with 1 mM Mn2+ and 50 pg templates. These results are different from Fujii’s findings, in which mutations were strongly biased in favour of C to T and G to A (66 %) and the transition/transversion ratio was 2.7 . The distribution of mutations is analysed and shown in relation to GC content at each base of cel6A (Additional file 1: Figure S1). There were some regions where mutations continuously appeared (positions 770–830, 1000–1050), indicating that errors were more frequently distributed in GC-rich regions (Additional file 1: Figures S2–S3). The mutations were also found in the whole vector regions including promoter regions and selection marker gene (Additional file 1: Figure S4), which potentially affect the transformation efficiency or protein productivity.
Transformation, enzyme production, and measurements of cellulase activities
Error-prone RCA-MDA products obtained under two conditions (2 mM manganese and 100, 250 pg template) were successfully transformed into P. pastoris after restriction enzyme digestion. The number of colonies was ~100 per plate, which is slightly fewer than the plates of wild-type colonies obtained by the usual plasmids preparation protocol (100–300 colonies per plate).
All colonies from error-prone RCA-MDA plates, excluding small colonies, and 96 colonies from the control plate were incubated in liquid culture for cellulase production. Then the amorphous cellulose (PASC)-degrading activity of the crude enzymes was measured, and the results obtained for the transformants of error-prone RCA-MDA are shown with those of wild-type in Fig. 4. The activity of wild-type transformants were dispersed (Fig. 4c), indicating that the activities would be influenced by differing amounts of enzymes in the culture resulting from the different productivity of the enzymes. Especially, multiple gene integration events occur with detectable frequency and greatly enhance the expression level of a target protein [30, 31]. The numbers of transformants whose activities were less than 10 % of that of wild-type PcCel6A (the median activity of 96 control transformants was 0.37 mM glucose in 2-hour incubation) were 40 and 37 % under the conditions with 100 and 250 pg template, respectively (Fig. 4a, b). In contrast, the corresponding number for wild-type PcCel6A was 2 % (2 of 96 colonies, Fig. 4c). We consider that the high levels of transformants with markedly lowered activity from the error-prone RCA-MDA plates are mainly due to the introduction of mutations.
Degradation of amorphous and crystalline celluloses by mutants
Next, we compared the activities of the crude mutant enzymes to degrade amorphous and crystalline celluloses. Figure 5a shows the amorphous cellulose (PASC)-degrading versus crystalline cellulose (cellulose IIII)-degrading activities of 87 randomly selected transformants from error-prone RCA-MDA plates, which had activities of more than 10 % of that of the wild type in Fig. 4. The data points in blue in Fig. 5a shows the transformants for which DNA sequencing revealed no mutation or no change in amino acid sequence. Mutants that had at least one mutation in the cel6A gene are shown in red in Fig. 5a. The activities of these mutants were affected by relatively large difference in protein expression levels, as the total protein concentrations of culture supernatants were varied from 0.01 to 0.2 mg/ml. The results of SDS-PAGE analysis of some mutants were shown in Additional file 1: Figure S5.
Most of the mutants had an amorphous/crystalline cellulose-degrading activity ratio similar to that of the wild type, though two mutants revealed a clearly different character. Mutants #13 and #15 had lowered degrading activity towards crystalline cellulose IIII while retaining activity towards amorphous cellulose. The DNA sequencing of #15 revealed a single mutation, W267C. This tryptophan residue is located at the entrance of the active site tunnel of PcCel6A (Fig. 5b), and the importance of the residue has been demonstrated in Trichoderma reesei Cel6A: it is not necessary for hydrolysis, but is requisite for loading a cellulose chain from the crystalline surface . On the other hand, the DNA sequencing of #13 revealed several mutations: C25Y, A105D, G346D, as well as two mutations that would not cause any amino acid substitution. The most influential mutation is probably C25Y, because C25 is expected to form a disulfide bridge with C8 in the carbohydrate-binding module (CBM) of PcCel6A (Fig. 5b), and this mutation is expected to result in reduced affinity and adsorption on the crystalline surface . However, the DNA sequencing traces of #13 showed overlaps with the wild-type sequence, probably due to multiple-copy gene integration, while the multiple integration event occurs less than 10 % of transformed colonies . It might result in the production of different proteins in a single Pichia cell, and the activity would be a mixture of mutants. Interestingly, deletion of 17 amino acids at the C-terminus did not cause a significant change of activity, as seen in the case of mutant #23 with a stop codon at W423 and two silent mutations.
A major advantage of the P. pastoris expression system is that the enzyme is secreted extracellularly, so that the cellulase activity of PcCel6A mutants can be easily measured by the direct use of culture filtrates. In the present study, we found two mutants with altered crystalline cellulose degradation by PcCel6A in relatively small libraries, supporting the idea that P. pastoris is a useful system for screening of secreted proteins. The use of P. pastoris could be especially advantageous for screening of enzymes with insoluble substrates or substrates that are unable to diffuse through cell membranes. Moreover, by utilizing β-glucosidase-producing P. pastoris, direct screening in terms of growth difference might be possible.
The goal of this study was to establish the suitability of P. pastoris as an expression system for random mutagenesis, because this organism has the capability to perform many eukaryotic post-translational modifications. Furthermore, P. pastoris is an excellent choice for the production of secreted proteins on account of its limited endogenous protein secretion. To obtain sufficient amounts of mutated DNA, we developed a rapid and convenient random mutagenesis method that does not require laborious steps such as ligation, cloning, and synthesis of specific primers (Fig. 6). This method uses widely available kits and takes the advantage of the fact that cloned DNA is typically obtained in circular vectors. Each experimental step takes only a few minutes, and microgram amounts of mutated DNA can be obtained within 3 days. Mutation frequencies were consistently in the range of 2–3 base substitutions per kb in the presence of 2 mM manganese ions, and this error rate is considered to be favorable for accumulation of adaptive mutations . The prepared DNAs performed normally as vectors for transformation of P. pastoris. This method was successfully applied to the P. pastoris system, but should also be applicable to many other transformation systems that employ linear vectors.
multiple displacement amplification
phosphoric acid-swollen cellulose
rolling circle amplification
Bloom JD, Meyer MM, Meinhold P, Otey CR, MacMillan D, Arnold FH. Evolving strategies for enzyme engineering. Curr Opin Struct Biol. 2005;15:447–52.
Bulter T, Alcalde M, Sieber V, Meinhold P, Schlachtbauer C, Arnold FH. Functional expression of a fungal laccase in Saccharomyces cerevisiae by directed evolution. Appl Environ Microbiol. 2003;69:987–95.
Liu Z, Pscheidt B, Avi M, Gaisberger R, Hartner FS, Schuster C, et al. Laboratory evolved biocatalysts for stereoselective syntheses of substituted benzaldehyde cyanohydrins. ChemBioChem. 2008;9:58–61.
Igarashi K, Maruyama M, Nakamura A, Ishida T, Wada M, Samejima M. Degradation of crystalline celluloses by Phanerochaete chrysosporium cellobiohydrolase II (Cel6A) heterologously expressed in methylotrophic yeast Pichia pastoris. J Appl Glycosci. 2012;59:105–10.
Kawai R, Yoshida M, Tani T, Igarashi K, Ohira T, Nagasawa H, et al. Production and characterization of recombinant Phanerochaete chrysosporium beta-glucosidase in the methylotrophic yeast Pichia pastoris. Biosci Biotechnol Biochem. 2003;67:1–7.
Igarashi K, Yoshida M, Matsumura H, Nakamura N, Ohno H, Samejima M, et al. Electron transfer chain reaction of the extracellular flavocytochrome cellobiose dehydrogenase from the basidiomycete Phanerochaete chrysosporium. FEBS J. 2005;272:2869–77.
Nelson JR, Cai YC, Giesler TL, Farchaus JW, Sundaram S, Ortiz-rivera M, et al. TempliPhi, phi29 DNA polymerase based rolling circle amplification of templates for DNA sequencing. Biotechniques. 2002;32:S44–7.
Nakamura A, Tsukada T, Auer S, Furuta T, Wada M, Koivula A, et al. The tryptophan residue at the active site tunnel entrance of Trichoderma reesei cellobiohydrolase Cel7A is important for initiation of degradation of crystalline cellulose. J Biol Chem. 2013;288:13503–10.
Clare J, Rayment F, Ballantine S, Sreekrishna K, Romanos M. High-level expression of tetanus toxin fragment C in Pichia pastoris strains containing multiple tandem integrations of the gene. Biotechnology. 1991;9:455–60.
Koivula A, Kinnari T, Harjunpää V, Ruohonen L, Teleman A, Drakenberg T, et al. Tryptophan 272: an essential determinant of crystalline cellulose degradation by Trichoderma reesei cellobiohydrolase Cel6A. FEBS Lett. 1998;429:341–6.
Tomme P, Van Tilbeurgh H, Pettersson G, Van Damme J, Vandekerckhove J, Knowles J, et al. Studies of the cellulolytic system of Trichoderma reesei QM 9414. Analysis of domain function in two cellobiohydrolases by limited proteolysis. Eur J Biochem. 1988;170:575–81.
MT performed major part of the experiments, MT and KI wrote the manuscript, NSugimoto guided RCA and MDA experiments, AN contributed cellulase assays and NSunagawa, TI and TU supported the cultivation of P. pastoris, and KI and MS designed the experiments. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Availability of supporting data
The datasets generated during and/or analyzed during the current study are available from the corresponding author on reasonable request.
This work was supported by a grant for Development of an Innovative and Comprehensive Production System for Cellulosic Bioethanol from the New Energy and Industrial Technology Development Organization (NEDO) to MS [09000833-0]; by an Impulsing Paradigm Change through Disruptive Technologies (ImPACT) Program from the Japan Science and Technology Agency (JST) to KI; by a Grant-in-Aid for Innovative Areas from the Japanese Ministry of Education, Culture, Sports, and Technology (MEXT) to KI [Nos. 24114001 and 24114008]; by a Grant-in-Aid for Scientific Research from the Japan Society for the Promotion of Science (JSPS) to KI [B: No. 24380089]; by a Grant-in-aid for JSPS Fellows 15J10657 from the JSPS to MT; and partially supported by the Asahi Glass Foundation to KI.
Present address: Biomaterial in Tokyo Co., Ltd., Fukuoka Lab, Ōnojō, Fukuoka, 816-0905, Japan
Present address: Institute for Molecular Science, National Institute of Natural Sciences, Okazaki, 444-8787, Japan
Authors and Affiliations
Department of Biomaterial Sciences, Graduate School of Agricultural and Life Sciences, The University of Tokyo, Yayoi 1-1-1, Bunkyo-ku, Tokyo, 113-8657, Japan
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Tachioka, M., Sugimoto, N., Nakamura, A. et al. Development of simple random mutagenesis protocol for the protein expression system in Pichia pastoris
Biotechnol Biofuels9, 199 (2016). https://doi.org/10.1186/s13068-016-0613-z