Enhancement of β-xylosidase productivity in cellulase producing fungus Acremonium cellulolyticus
© Kanna et al; licensee Springer. 2011
Received: 9 May 2011
Accepted: 30 June 2011
Published: 30 June 2011
Enzymatic hydrolysis is one of the most important processes in bioethanol production from lignocellulosic biomass. Acremonium cellulolyticus is a filamentous fungus with high cellulase production but productivity of hemicellulase, especially β-xylosidase, is lower than other filamentous fungi. We identified 2.4 Kb β-xylosidase gene in the A. cellulolyticus genome sequence information and it encoded 798 amino acids without introns. To enhance hemicellulase productivity in A. cellulolyticus, we transformed this fungus with the identified β-xylosidase gene driven by the cellobiohydrolase Ι (cbh1) promoter, using the protoplast-polyethyleneglycol (PEG) method, and obtained a transformant, YKX1. Hydrolysis rate of xylooligosaccharides was more than 50-fold higher using culture supernatant from YKX1 than that from the parental strain, Y-94. Total cellulase activity (measured by filter paper assay) in YKX1 was not affected by the cbh1 promoter used for expression of β-xylosidase, and induced by cellulose. Since YKX1 can produce larger amount of β-xylosidase without affecting cellulase productivity, it is considered to be beneficial for practical monosaccharide recoveries from lignocellulosic biomass.
Ethanol produced from lignocellulosic biomass is a second-generation biofuel which does not compete with food resources (Sims et al. 2010) and is expected to be an alternative to gasoline that reduces dependence on fossil fuels. Bioethanol can be produced from lignocellulosic biomass via several processes; pretreatment, enzymatic hydrolysis, and fermentation. In these processes, effective enzymatic hydrolysis of cellulose and hemicellulose is the most important step. Therefore, we focused on the enzyme activities that catalyze the saccharification of cellulose and hemicellulose.
Cellulose is the primary component of lignocellulosic biomass. After cellulose, hemicellulose is t he second most abundant component of the plant cell wall, and accounts for 20-30% of lignocellulosic biomass (Girio et al. 2010). Glucuronoxylans (O-acetyl-4-O-methylglucuronoxylan) are the most abundant type of hemicellulose, and they make up 15-30% of the dry mass in hardwoods (Girio et al. 2010). Although conventional ethanol fermenting yeasts cannot utilize xylose, we have developed efficient xylose-fermentable Saccharomyces cerevisiae strains (Matsushika et al., 2009). Hence, effective saccharification of xylan is practically important for attaining higher yields of monosaccharides.
Endo-β-1, 4-xylanase and β-xylosidase catalyze the production of xylooligosaccharides from xylan and xylose from xylooligosaccharides, respectively. β-xylosidase hydrolyzes the non-reducing end of xylooligosaccharides. Although purified β-xylosidase is commercially available, it is too costly for practical large-scale applications. It will be beneficial if cellulase-producing filamentous fungi also produce hemicellulase for efficient and cost-effective hydrolysis of lignocellulosic biomass.
The β-xylosidase genes have been sequenced and characterized from many species of filamentous fungi. xylA of Aspergillus oryzae (Kitamoto et al. 1999) and xyl I of Aureobasidium pullulans strain ATCC 20524 (Ohta et al. 2010) belong to the glycosyl hydrolase (GH) 3 family. xylB in A. oryzae belongs to the GH43 family (Suzuki et al. 2010). Based on amino acid sequence, Bxl1 of Trichoderma reesei RutC-30 (Margolles-Clark et al. 1996), XlnD of Aspergillus nidulans (Perez-Gonzalez et al. 1998), and Aspergillus niger (van Peij et al. 1997) belong to the GH 3 family (Suzuki et al. 2010). Furthermore, heterologous expression of xylB of A. oryzae in Escherichia coli was more stable than endogenous XylB expression in A. oryzae (Suzuki et al. 2010) or heterologous expression of xlnD from A. n iger strain ATCC 10864 in Aspergillus awamori, which has similar activity on 4-nitrophenyl-β-D-xyloopyranoside to A. niger XlnD (Selig et al. 2008).
Acremonium cellulolyticus is a cellulase-producing filamentours fungus isolated in Japan (Yamanobe et al., 1987). Repeated UV and/or nitrosoguanidine (NTG) mutagenesis of the wild strain Y-94 was used to enhance cellulase productivity, and strains with high cellulase productivity (TN, C-1, and CF-2612) have been selected. Although the productivity of cellulase is quite high in A. cellulolyticus, its hemicellulase production is not sufficient. Recently, we have sequenced the whole genome of A. cellulolyticus (unpublished data) and could deduce many genes for saccharifying enzymes. Although there are only a few reports of successful transformation in A. cellulolyticus, we could successfully obtain many transformants with protoplast- PEG method. Therefore, we tried to enhance β-xylosidase productivity of this fungus by introducing its β-xylosidase gene under strong promoter.
Among strains of A. cellulolyticus, CF-2612 has the highest cellulase productivity (Fang et al. 2009), but it underwent random mutagenesis and may have mutations at every site as well as cellulase related genes. And apparently random mutagenesis affected the growth rates of CF-2612 because it grows more slowly than other strains. Therefore, we used the wild type strain, Y-94, in our study.
Materials and methods
Fungal strain and culture condition
A. cellulolyticus Y-94 (FERM Number BP-5826) was cultured in 10 ml of medium in 100 ml flasks at 30°C with shaking at 200 rpm. The composition of the culture medium for A. cellulolyticus was described previously (Fang et al. 2009). Sampling was performed at 1, 3, and 7 days for analysis of gene expression using real-time PCR and/or enzyme activity. A. cellulolyticus strains were cultured in potato dextrose (PD) medium for cloning and transformation.
Measurement of the amount of ATP, β-xylosidase and β-mannosidase activity, and saccharification efficiency
The amount of ATP measured based on fluorescence using a Rucifel-250 kit (Kikkoman, Tokyo Japan) and Lumitester C-100 (Kikkoman) according to the manufacturers' instructions.
Activities for β-xylosidase and β-mannosidase were measured using 100 μl of 10 mM 4-nitrophenyl-β-D-xyloopyranoside (PNP-Xyl, Sigma, MO USA) or 4-nitrophenyl-β-D-mannopyranoside (PNP-Man, Sigma) as the substrates (final concentration is 1 mM), respectively. Fifty μl of enzymes were incubated with 1 mM PNP-Xyl or PNP-Man at 45°C for 10 minutes in 850 μl of 50 mM acetic acid buffer (pH.5). After 10 minutes, 500 μl of 1 M NaCO3 was added. Because 4-nitrophenol which will be generated from substrates by enzymatic hydrolysis is a chromogenic substance, enzyme activities were assayed by measuring absorbance at 420 nm by UV-2550 Spectrophotometer (Shimadzu, Kyoto, Japan). One unit of the enzyme activity is defined as the amount of enzyme that produces 1 μmol of p-nitrophenol per minute. For analysis of saccharification efficiency, culture medium was centrifuged at 9,000 g for 10 min to collect the supernatant containing the secreted enzyme. Enzyme solutions were incubated at 45°C in 50 mM acetic acid buffer with 4% xylooligosaccharides (Wako Pure Chemicals, Osaka JAPAN). The xylose concentration was measured using a high performance liquid chromatography system (JASCO, Tokyo, Japan), under the conditions described previously (Buaban et al. 2010).
Cloning β-xylosidase gene from A. cellulolyticus
A putative β-xylosidase gene, bxy3A, was identified in A. cellulolyticus genome sequence information using A. nidulans xlnD sequence as the query for a homology search. In silico molecular cloning (in silico biology, Yokohama Japan) which is a software for gene analysis was used for homology search. Augstus 2.2 http://augustus.gobics.de/ which is a program for eukaryotic genome sequence was used for the prediction of genes. The β-xylosidase coding region was amplified using A. cellulolyticus CF-2612 genomic DNA as the template, and the cellobiohydrolase Ι (cbh1) promoter was amplified from Y-94 genome. For the extraction of genomic DNA, cells cultured in PD medium were collected by centrifugation, and 3 volumes of TE (10 mM Tris-HCl, 1 mM EDTA, pH 8.0) with 2% sodium dodecyl sulfate (SDS) were added to the cell pellet. The cell suspension was incubated at 50°C for 1 hr. Potassium acetate (5 M) was added to the cell suspension at one-tenth of total volume, and this mixture was incubated on ice for 1 hr. The mixture was centrifuged at 13,000 g for 10 min, and the supernatant was subjected to two rounds of phenol-chloroform treatment, and ethanol precipitation was performed to obtain genomic DNA. The DNA was incubated with RNaseA (Nippon gene, Toyama, Japan) at 37°C for 1 hr to degrade contaminating RNA.
To amplify β-xylosidase open reading frame from A. cellulolyticus DNA, the forward primer with engineered Spe Ι site (5'-GCACTAGTATGGTCTACACCACG) and the reverse primer with engineered Kpn Ι site (5'-GCGGTACCTCAATTAGAATCAGGC) were designed based on sequence from the A. cellulolyticus genome sequence information (unpublished data) using Augustus 2.2 software The promoter from the cellobiohydrolase Ι (cbh1) gene (GenBank Accession number; E39854) was amplified with the forward primer with an Xho Ι site (5'-GCCTCGAG AAGCTTGGAAGCT) and the reverse primer with a Spe Ι site (5'-TACCATGGCTGCACTAGT GTGTCGATTGCTT). The amplified fragment of the cbh1 promoter was connected to β-xylosidase gene in frame, and incorporated into a shuttle vector pLD10 provided by Dr. H. Corby Kistler (University of Minnesota, USA), and the resulting plasmid, pLcbX-1, was obtained. E. coli DH5α cells (Takara Bio, Shiga, Japan) were used to maintain the plasmid.
Transformation of A. cellulolyticus
The parental strain, Y-94, was transformed using a slightly modified protoplast-PEG method (Fincham et al. 1989). An overnight culture of A. cellulolyticus was treated with in 10 mM KH2PO4, 0.8 M NaCl, and 0.2% Yatalase (Takara Bio) to prepare protoplasts. The protoplasts were washed with 0.8 M NaCl and suspended in Solution A (1.2 M Sorbitol, 10 mM Tris-HCl, 10 mM CaCl2). Plasmid (10 μg) was added to the protoplast suspension, then 50 μl of Solution B (40% PEG4000, 10 mM Tris-HCl, 10 mM CaCl2) was added to the protoplast suspension, and the suspension was incubated on ice for 30 min and RT for 15 min. Then, 8.5 ml of solution A was added to the cell suspension to dilute Solution B. The protoplasts suspension was spread on YPSA plate (1% Bacto yeast extract, 1% Bacto tryptone, 1 M Sucrose, and 2% Agar) and incubated overnight at 30°C. PD medium with 0.2% agar with 500 μg hygromycin was piled on to the YPSA plate. A single colony was isolated 3 days after the addition of PD medium. To confirm the presence of hygromycin phosphotransferase (hph) gene, transformant was checked by PCR using the forward (5'-ATGCCTGAACTCACCGCGAC-3') and the reverse (5'-CTATTCCTTTGCCCTCGGAC-3') primers.
Measurement of FPU, xylanase, and mannanase activities
The FPU activity assay described by Ghose (1987) was performed as a reference for cellulase activity. Whatman NO.1 filter paper (paper size; 1 cm × 6 cm, Whatman, Kent UK) was used as the substrate. Culture medium was centrifuged at 9,000 g for 10 min to collect the supernatant with the secreted enzyme. Enzyme solution in 1 ml of 50 mM citric acid buffer, pH4.8, was incubated with the substrate at 50°C for 60 min. DNS solution (3 ml; 1% 3, 5-dinitrosalycilic acid (Sigma), 1.2% NaOH, 0.05% sodium sulfate, and 20% potassium sodium tartrate tetrahydrorate) was added to the enzyme solution, and the mixture was boiled for 5 min, then the reaction mixture was put on ice. The amount of glucose was measured with the absorbance at 540 nm with UV-2550 Spectrophotometer as a reducing sugar.
For assay of xylanase and mannanase, 2% birch-wood xylan (Sigma) or 1% Konjac Glucomannan (Megazyme, Wicklow, Ireland) were used as substrates, respectively. The incubation time for enzymatic reaction was 30 min and activities were assayed according to the previously described method (Bailey et al. 1991).
Measurement of gene expression by real-time PCR
For analyzing expression of the β-xylosidase gene, we performed real-time PCR. RNA was extracted with Fast RNA Pro Red kit (MP biomedicals CA USA) at one day after starting the cultures. The extracted RNA was cleaned using the RNeasy mini kit (Qiagen, Hilden Germany). cDNA was prepared using the M-MLV reverse transcriptase (Takara Bio) and oligo (dT) 20 (Toyobo, Osaka Japan). Samples were labeled by iQ SYBR Green (Bio-Rad, CA USA). Primers used for real-time PCR were as follows: For β-xylosidase: 5'-TTCCCGGTTAGGGTTTGATG-3' (forward) and 5'-GGGACACCATTCACCGAGTT-3' (reverse), for cellobiohydrolase I: 5'-ACTGCCTCCTTCAGCAAACAC-3' (forward) and 5'-GGCGTAGTCGTCCCACAAA-3' (reverse), for β-actin (the internal control): 5'-CAACTGGGACGACATGGAGA-3' (forward) and 5'-GTTGGACTTGGGGTTGATGG-3' (reverse).
Nucleotide sequence accession number
The DDBJ accession number of bxy3A sequence is AB613265.
A putative β-xylosidase gene, bxy3A, was identified in A. cellulolyticus genome sequence information using the A. nidulans xlnD sequence as the query for a homology search. The size of the gene was 2.4-Kb and it encoded 798 amino acids without introns. The amino acid sequence deduced from bxy3A was aligned with other β-xylosidase sequences (data not shown). This protein had 74% identity to T. reesei Bxl1 (Margolles-Clark et al. 1996) and 61% identity to A. nidulans XlnD (Perez-Gonzalez et al. 1998).
Gene expression in Y94 and YKX1 was analyzed one day after the cultures were started.
0.02 ± 0.004
3.3 ± 0.509
15.78 ± 3.316 *
11.16 ± 2.321 *
Enzyme activity 3 days after the cultures were started.
56.68 ± 4.13
59.59 ± 2.96
4.21 ± 0.29
3.76 ± 0.21
0.0071 ± 0.00042
0.0063 ± 0.00042
In filamentous fungi, β-xylosidase of each species belongs to one of 3 GH families, 3, 43, or 54 (Knob et al. 2010). The putative β-xylosidase gene in A. cellulolyticus, bxy3A, showed high homology to β-xylosidase of the GH 3 family, and Bxy3A shared a conserved motif with the GH 3 family.
In this study, to increase hemicellulase productivity, the cbh1 promoter was used to drive overexpression of BXY3A. CBH1, which is one of major cellulase, cleaves cellulose at the non-reducing end and produces cellobiose. CBH1 protein accounts for about 60% of all secreted proteins in T. reesei. Therefore, the cbh1 promoter is widely used as a promoter for overexpression of homologous or heterologous gene (Keränen and Penttilä 1995). However, expression cassettes containing the cbh1 promoter might integrate at the cbh1 loci by homologous recombination. Actually, it was reported that expression of cbh1 was abolished by homologous recombination, pcbh1-gus in T. reesei PC-3-7 (Rahman et al. 2009). Moreover, the value of cellulase activity of Pcbh1-gus, in which uidA encoding β-glucuronidase is ligated between the cbh1 promoter and the cbh1 terminator, was half of that in wild type (Rahman et al. 2009). In this study, FPU activity of YKX1 was similar to that of Y-94. In most transformation experiments in filamentous fungi, a terminator is added downstream of the open reading frame. We did not ligated the terminator of cbh1 at downstream of bxy3A. Therefore, the expression cassette was less likely to induce a double crossover. However, it is possible that a single crossover could have occurred at cbh1 gene. Although cbh1 gene of YKX1 was slightly lower than that of Y-94, expression cassette did not disrupt the original cbh1 gene.
β-xylosidase gene in the integrated transformation cassette was expressed and the produced enzyme functioned. Xylosidase activity in YKX1 was higher than that in Y-94 grown in PD medium (data not shown), while activity of YKX1 was much higher than that of Y-94 in medium with 4%Solcaflock (Figure 3). Another potential problem with using the cbh1 promoter was a possible titration effect; the cellulase genes may have bound most of the transcription factor, xyr1, in T. reesei (Stricker et al. 2006). In A. niger, xlnR which is an ortholog of xyr1, induces expression of the cellulase gene (Stricker et al. 2008). In both cases, expression from the endogenous cbh1 gene might decrease by an additional cbh1 promoter due to competition for the transcription factor. However, we found that FPU activity of YKX1 was similar to Y-94, which suggests titration effect did not occur in YKX1.
We were also concerned that a titration effect might decrease expression from the endogenous β-xylosidase gene because xyr1 induces bxl1 and xlnR induces xlnD in T. reesei and A. niger, respectively (Stricker et al. 2006, Stricker et al. 2008). It was difficult to determine whether the endogenous β-xylosidase was influenced by a titration effect because YKX1 was transformed with the open reading frame from the endogenous β-xylosidase gene. However, expression of bxy3A driven by the cbh1 promoter in YKX1 was higher than expression of the endogenous bxy3A in the parental strain (Table 1). Because there was no evidence of any titration effect in YKX1, it is appropriate to use the cbh1 promoter to enhance hemicellulase activity in the strain A. cellulolyticus Y-94.
Expression of the xylanolytic gene, bxl1, is induced by xylobiose in T. reesei (Margolles-Clark et al. 1997). In A. nidluns, D-xylose induces xylanolytic enzymes via the regulatory gene, xlnR (Tamayo et al. 2008). Although D-xylose and xylobiose can induce xylanolytic enzymes, another report indicates that the activity of β-xylosidase depends on the concentration of D-xylose in T. reesei (Mach-Aigner et al. 2010). β-xylosidase activity of YKX1 might have no effect in the presence of D-xylose because YKX1 used cbh1 promoter.
YKX1 grew faster than Y-94 in the same medium measured by ATP amount (Figure 2). In a previous study, cellulase activity increased gradually as the amount of ATP decreased (Fang et al. 2009). Similarly in YKX1, xylosidase activity was highest at 7 days, which was when ATP concentrations decreased. The behavior of the enzymatic activity was similar to other cellulolytic enzyme in this previous report (Fang et al. 2009) because the promoter used was from cellulolytic enzyme expression. Furthermore, the amount of ATP in YKX1 was higher than that in Y-94 at 3 and 7 days (Figure 2). In contrast, the values of cellulase activity in CF-2612 and C-1 are negatively correlated ATP concentrations (Fang et al. 2009). However, ATP levels in YKX1 were consistently high than those in Y-94.
Furthermore, the activities of other hemicellulolytic enzymes were similar in YKX1 and Y-94 (Table 2), indicating that the transformation was not affected by other hemicellulase. We generated a transformant of A. cellulolyticus that has higher β-xylosidase productivity than the parental strain without affecting cellulase or other hemicellulase productivity. We confirmed xylose yield improved by adding enzyme solution of YKX1, in saccharification experiments using rice straw (data not shown). Therefore, YKX1 should be useful for enzyme production in practical applications that convert both cellulose and xylan into fementable monosaccharides.
This work was supported by New Energy and Industrial Technology Development Organization (NEDO) of Japan. We would like to thank to Dr. Min-tian Gao for helpful discussion and Ms. Miyu Sumii and Ms. Reiko Yoshii for technical assistance.
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