Thermostable recombinant xylanases from Nonomuraea flexuosa and Thermoascus aurantiacus show distinct properties in the hydrolysis of xylans and pretreated wheat straw
© Zhang et al; licensee BioMed Central Ltd. 2011
Received: 8 February 2011
Accepted: 18 May 2011
Published: 18 May 2011
In the hydrolysis of lignocellulosic materials, thermostable enzymes decrease the amount of enzyme needed due to higher specific activity and elongate the hydrolysis time due to improved stability. For cost-efficient use of enzymes in large-scale industrial applications, high-level expression of enzymes in recombinant hosts is usually a prerequisite. The main aim of the present study was to compare the biochemical and hydrolytic properties of two thermostable recombinant glycosyl hydrolase families 10 and 11 (GH10 and GH11, respectively) xylanases with respect to their potential application in the hydrolysis of lignocellulosic substrates.
The xylanases from Nonomuraea flexuosa (Nf Xyn11A) and from Thermoascus aurantiacus (Ta Xyn10A) were purified by heat treatment and gel permeation chromatography. Ta Xyn10A exhibited higher hydrolytic efficiency than Nf Xyn11A toward birchwood glucuronoxylan, insoluble oat spelt arabinoxylan and hydrothermally pretreated wheat straw, and it produced more reducing sugars. Oligosaccharides from xylobiose to xylopentaose as well as higher degree of polymerization (DP) xylooligosaccharides (XOSs), but not xylose, were released during the initial hydrolysis of xylans by Nf Xyn11A, indicating its potential for the production of XOS. The mode of action of Nf Xyn11A and Ta Xyn10A on glucuronoxylan and arabinoxylan showed typical production patterns of endoxylanases belonging to GH11 and GH10, respectively.
Because of its high catalytic activity and good thermostability, T. aurantiacus xylanase shows great potential for applications aimed at total hydrolysis of lignocellulosic materials for platform sugars, whereas N. flexuosa xylanase shows more significant potential for the production of XOSs.
Xylans represent a major source of plant cell wall polysaccharides with structural diversity and increasing application opportunities. Xylans in hardwoods and annual plants consist of a linear backbone of β-(1→4)-D-xylopyranosyl residues, substituted by α-L-arabinofuranosyl units in the positions of 2-O- and/or 3-O-, by 4-O-methyl-glucopyranosyl uronic acid in the position of 2-O, and/or by acetyl groups in the positions of 2-O and/or 3-O. Furthermore, some of the arabinofuranosyl units may be esterified with ferulic or p-coumaric acids . Complete hydrolysis of xylan involves the synergistic action of several main chain- and side group-cleaving enzymes, including endo-β-1,4-xylanases (EC 220.127.116.11), β-D-xylosidases (EC 18.104.22.168), α-L-arabinofuranosidases (EC 22.214.171.124), α-glucuronidases (EC 126.96.36.199), acetyl xylan esterases (EC 188.8.131.52) and feruloyl esterases (EC 184.108.40.206).
Endo-β-1,4-xylanases cleave randomly the internal β-1,4-glycosyl bonds in the xylan main chain. On the basis of the similarities in their amino acid sequences and hydrophobic cluster analysis, xylanases are currently classified into families 5, 8, 10, 11 and 43 of glycoside hydrolases . Xylanases from family 10 (GH10) and family 11 (GH11) of glycoside hydrolases are the major and best-studied xylanases. Enzymes from these two families differ in their physicochemical properties, as well as in their action on polysaccharides and xylooligosaccharides (XOSs) [4, 5]. GH10 xylanases have generally a higher molecular mass and lower isoelectric point than GH11 xylanases. GH 10 xylanases all have a catalytic domain which exhibits (β/α)8 architecture, whereas the GH11 xylanases have a β-jelly roll structure . GH10 xylanases are capable of cleaving glycosidic linkages in the xylan main chain closer to the substituents, such as the 4-O-methyl-glucuronic acid, α-L-arabinofuranose and acetyl groups. As a result, shorter hydrolysis products are released from xylan by GH10 xylanases as reported by Biely et al. .
Xylanases have raised interest because of their potential applications in various industrial fields, including the pulp and paper industries, bioethanol production and the feed industry [6–9]. Xylanases have been found to be important in the total hydrolysis of hemicelluloses containing lignocellulosic materials. In bioethanol production processes from lignocellulosic materials, xylanases can improve the hydrolysis of cellulose into fermentable sugars by removing xylans restricting the access of cellulases to cellulose surfaces . Thus, hydrolysis of pretreated lignocellulosic raw materials with even low residual xylan content by xylanases has been shown to improve the hydrolysis of cellulose significantly . Whereas extensive research on the partial hydrolysis of xylans in cellulosic pulps has been carried out, only a few reports are available on the mechanisms and efficiencies of various xylanases on complex lignocellulosic substrates. Xylanases can also be used for the production of XOSs, which exhibit a wide range of biological activities, including prebiotic effects, antioxidative and antimicrobial activities, as well as plant growth regulatory effects [11, 12]. Thus, XOSs show remarkable potential for practical utilization in many fields, including functional food, pharmaceuticals, feed formulations and agricultural applications. Enzymes with optimal catalytic properties for each application may be found among different families.
Thermostable enzymes have several generic advantages, allowing a decreased amount of enzyme needed because of higher specific activity and elongated hydrolysis time due to higher stability . In addition, thermostable enzymes are generally more tolerant and allow more flexibility in process configurations. Thermostable xylanases can be obtained from many bacterial and fungal sources [6, 8]. Several xylanases isolated from the thermophilic fungus Thermoascus aurantiacus belong to the GH10 family and have high specific activity and thermal stability. Xylanases from T. aurantiacus C-436 have been shown to be stable at 50°C for 12 weeks and to retain 90% of the initial activity. In addition, the half-lives of the xylanases at 70°C and 60°C were 1.5 hours and 4 days, respectively . Two xylanases from T. aurantiacus IMI 216529 were reported to have half-lives of 88 and 41 minutes at 80°C . Two family 11 xylanases purified from the thermophilic actinomycete Nonomuraea flexuosa (previously Microtetraspora flexuosa) SIIX had half-lives of about 5 minutes at 80°C in the absence of substrate and half-lives of about 25 minutes at 80°C in the presence of 1% substrate . The xylanase genes xyn11A from N. flexuosa and xyn10A from T. aurantiacus have been cloned and expressed in Trichoderma reesei[16, 17]. The three recombinant proteins from N. flexuosa (r33.4, r23.8 and r22.0 kDa) obtained were similar to each other in terms of temperature dependence, but the shorter polypeptides were more thermostable at 80°C than the full-length enzyme, especially at pH 5 . Both of the two shorter polypeptides from N. flexuosa and the xylanase 10A from T. aurantiacus lacked the C-terminal cellulose binding module (CBM). There are no reports, however, on the hydrolytic properties of the thermostable recombinant xylanases from N. flexuosa or on those of the thermostable recombinant Xyn10A xylanase from T. aurantiacus expressed in T. reesei.
For cost-efficient use of enzymes in large-scale industrial applications, high-level expression of enzymes in recombinant hosts is usually a prerequisite. In the present work, two thermostable recombinant xylanases from the two thermophilic organisms (N. flexuosa and T. aurantiacus), which were cloned and expressed in T. reesei, were purified and characterized. The hydrolytic properties of the two xylanases on xylans and lignocellulosic substrates were also investigated. The main aim of the present study was to compare the biochemical and hydrolytic properties of two thermostable recombinant GH11 and GH10 xylanases, both lacking the CBM, with respect to two potential application areas: for the production of XOSs and for the hydrolysis of lignocellulosic substrates. Isolated xylan substrates and hydrothermally pretreated wheat straw, a potential substrate for generating platform sugars, were used to compare the enzymes.
Birchwood glucuronoxylan was purchased from Sigma Chemical Co. (St. Louis, MO, USA). Oat spelt arabinoxylan was obtained from Serva (Heidelberg, Germany), and hydrothermally pretreated wheat straw was a kind gift of Inbicon (Fredericia, Denmark). The dry matter (DM) content of this wheat straw after being washed was 35.8%, and the contents of glucan and xylan were 58.9% and 3.2%, respectively, as determined by high-pressure liquid chromatography (HPLC) using the analytical CarboPac PA-1 column (Dionex Corp., Sunnyvale, CA, USA. D-xylose, D-arabinose, D-glucose (Merck, Darmstadt, Germany), 1,4-β-D-xylobiose, 1,4-β-D-xylotriose and 1,4-β-D-xylotetraose (Megazyme, Bray, Ireland) were used as carbohydrate standards. Arabinoxylobiose (AX) , aldotetrauronic acid (U4m2XX) and aldopentauronic acid (XU4m2XX) (S. Koutaniemi, unpublished data) were prepared by enzymatic endoxylanase hydrolysis of rye arabinoxylan and birchwood glucuronoxylan, respectively, followed by chromatographic purification. The nomenclature for oligosaccharides derived from xylan was derived from the naming system described by Fauré et al. . All other chemicals used were of analytical grade and purchased from Sigma or Merck.
Purification of N. flexuosa and T. aurantiacus xylanases
The two recombinant xylanases from N. flexuosa and T. aurantiacus were kindly provided by Roal Oy (Rajamäki, Finland). The enzymes were produced in a genetically modified T. reesei strain using a method whereby the genes cbh1, cbh2, egl1 and egl2 encoding for Cel7A, Cel6A, Cel7B and Cel5A, respectively, had been deleted according to a method described elsewhere [16, 17, 20]. To remove the less thermostable enzymes produced by the host strain T. reesei, the two xylanase preparations were adjusted to pH 6.0 and were treated at 60°C for 2 hours. The supernatants were further purified by gel permeation chromatography. The column with Sephacryl S-200 (1.6 × 60 cm; GE Healthcare Life Sciences, Uppsala, Sweden) was preequilibrated and run in 50 mM sodium citrate buffer (pH 5.0) with the addition of 100 mM NaCl at a flow rate of 0.5 ml/minute. Fractions of 2 ml were collected and analyzed for xylanase activity.
Xylanase activity was assayed using 1% (wt/vol) birchwood glucuronoxylan (Roth 7500, Karlsruhe, Germany) as a substrate in 50 mM sodium citrate buffer according to the method of Bailey et al. . The assay was performed at pH 5.0 and 50°C for 5 minutes. The amount of reducing sugars liberated was determined using the dinitrosalicylic acid (DNS) method with xylose used as standard . One nanokatal (1 nkat) of the enzyme activity was defined as the amount of enzyme that catalyzes the release of 1 nM reducing sugar per second. Activities of β-xylosidase and β-glucosidase were assayed using 5 mM p-nitrophenyl-β-D-xylopyranoside (N2132; Sigma Chemical Co.) and 1 mM p-nitrophenyl-β-D-glucopyranoside (N7006; Sigma) as substrates, respectively [23, 24]. Endoglucanase activity was determined using hydroxyl ethyl cellulose (Sigma-Aldrich, St. Louis, MO, USA) as substrate . The filter paper activity (FPA) was determined using Whatman 1 filter paper as substrate . All activities presented are average values of three separate determinations.
Protein was quantified by the Lowry method using bovine serum albumin (BSA) (Sigma Chemical Co.) as standard . Proteins in the column eluents were monitored by measuring the absorbance at 280 nm. The molecular masses of the purified xylanases were determined by matrix-assisted laser desorption/ionization time-of-flight mass spectrometry (MALDI-TOF-MS) (Bruker Daltonik, Bremen, Germany) at the Institute of Biotechnology (Helsinki, Finland). Sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) was performed on 12% polyacrylamide gel using the method of Laemmli . A prestained protein ladder (Invitrogen, Carlsbad, CA, USA) was used as a molecular weight standard. After electrophoresis, the gel was stained with Coomassie brilliant blue G-250 (Bio-Rad, Hercules, CA, USA).
N-terminal amino acid sequences of the enzymes were performed by Edman degradation at the Institute of Biotechnology (Helsinki, Finland). Apparent kinetic parameters were determined by incubating purified xylanases with different concentrations of birchwood glucuronoxylan in 50 mM sodium citrate buffer at pH 5.0 and 50°C. The Michaelis maximum velocity (Vmax) and constant (Km) values were determined by using the double-reciprocal plot method of Lineweaver-Burk.
Characterization of xylanases
The optimal pH for xylanase activity was determined by using McIlvaine buffer between pH 3 and pH 8 (50°C), and the optimal temperature for xylanase activity was determined to be between 30°C and 85°C (pH 5.0). The thermal stability of xylanases was determined after incubating the Nf Xyn11A (20.1 mg/mL) and Ta Xyn10A (20.1 mg/mL) samples without substrate in 50 mM sodium acetate buffer (pH 5.0) at 70°C and 80°C. The samples were removed after incubation for varying times (30 minutes and 1, 2, 3 and 4 hours) and immediately cooled on ice. The residual xylanase activity was determined using the standard assay.
Hydrolytic properties on polysaccharides
The hydrolysis of birchwood glucuronoxylan and insoluble oat spelt arabinoxylan (9 mg/mL) was carried out in test tubes with a working volume of 1 mL. Insoluble oat spelt arabinoxylan was prepared by using a modified method of Ryan et al. . Oat spelt arabinoxylan (4 g) was suspended in 400 mL of distilled water and stirred overnight at room temperature. The insoluble fraction was recovered by centrifugation for 20 minutes at 10,000 rpm and 4°C. The insoluble fraction was washed several times with Milli-Q water (Milli-Q Plus; Millipore, Billerica, MA, USA). After that, the sediment was lyophilized and used for hydrolysis. The enzyme dosage was 0.22 mg protein/g substrate. The hydrolysis of xylan substrates was carried out in 50 mM sodium citrate buffer (pH 5.0) at 55°C. Aliquots were removed periodically at different time intervals and boiled for 10 minutes to stop the enzymatic hydrolysis. Reducing sugars in supernatants were determined by using the DNS method . Xylose standard was used for calibration. Two replicates were carried out, and average values are presented.
To investigate the end products, birchwood glucuronoxylan and oat spelt arabinoxylan (5 g/L) were incubated with Nf Xyn11A (1.71 mg protein/g substrate, equal to 10,000 nkat/g substrate) and Ta Xyn10A (0.90 mg protein/g substrate, equal to 10,000 nkat/g substrate) in 50 mM sodium citrate buffer, pH 5.0, at 50°C for 48 hours, respectively. Hydrolysis was terminated by boiling the samples in a water bath for 10 minutes, after which the samples were analyzed by performing thin-layer chromatography (TLC) and high-performance anion exchange chromatography coupled with pulsed amperometric detection (HPAEC-PAD).
The hydrolysis of the hydrothermally pretreated, washed wheat straw was carried out by Nf Xyn11A and Ta Xyn10A in test tubes with a working volume of 2 mL in 50 mM sodium citrate buffer (pH 5.0) containing 0.02% NaN3 at 55°C. The DM content of substrate was 2%, and xylanases were dosed at 1 mg protein/g substrate. Samples were withdrawn at 4, 8 and 24 hours and boiled for 10 minutes to stop the enzymatic hydrolysis. After cooling, the samples were centrifuged and the supernatants were analyzed for reducing sugars using the DNS method with xylose as standard .
The hydrolysis products containing xylose and XOS were analyzed using TLC. TLC was carried out using Silica Gel 60 plates (Merck). A mixture of ethyl acetate, acetic acid, isopropanol, formic acid and water (25:10:5:1:15 vol/vol) was used as the running solution for analyzing hydrolysates of birchwood glucuronoxylan. A mixture of 1-butanol, ethanol and water (3:2:2 vol/vol) was used as the running solution for analyzing the hydrolysates of oat spelt arabinoxylan. The carbohydrates were detected by spraying with 2% (wt/vol) orsinol dissolved in a solution of ethanol, H2SO4 and H2O (80:10:10%), after which the plates were heated at 100°C for 10 minutes.
Oligosaccharides in the hydrolysates from birchwood glucuronoxylan and oat spelt arabinoxylan were analyzed using HPAEC-PAD . The HPAEC-PAD system was equipped with an SSI pulse equalizer (model LP 21; Scientific Systems, Inc., State College, PA, USA), two Waters 515 HPLC pumps, a PC Waters pump control module and a cooling Waters 717 autosampler using Millenium software (Waters Corp., Milford, MA, USA) for instrument control and data handling. The analytical CarboPac PA-100 column (250 × 4 mm) and the guard column PA-100 (25 × 3 mm) (Dionex Corp.) were maintained at 30°C. The eluents for gradient analysis were 100 mM NaOH and 100 mM NaOH/1 M NaOAc at a flow rate of 1 mL/minute as described by Rantanen et al. . D-xylose, linear XOS (X2-X4) and substituted XOS (AX, U4m2XX and XU4m2XX) were used as external standards.
Results and discussion
Purification of xylanases
Enzymatic activities of recombinant xylanase preparation from N. flexuosa (Nf), xylanase preparation from T. aurantiacus (Ta) and the corresponding two preparations after heat treatment for 2 hours at pH 6.0 and 60°C (Nf-H, Ta-H)
Family of GH
Gel permeation chromatography was used for further purification. Two peaks with xylanase activities were obtained when the xylanase preparation from N. flexuosa after heat treatment was fractionated by Sephacryl S-200. The peak with higher molecular weight was collected. A single peak with xylanase activity was obtained and collected from the xylanase preparations from T. aurantiacus after heat treatment by the same purification system. Both purified xylanases presented electrophoretic homogeneity by SDS-PAGE (Figure 1), which permitted physicochemical characterization of these enzymes.
Molecular weight and N-terminal amino acid sequence
Biochemical properties of recombinant Nf Xyn11A and Ta Xyn10A xylanasesa
Specific activity (nkat/mg)
(mg-1 s-1 ml)
The apparent kinetic parameters of Nf Xyn11A and Ta Xyn10A enzymes were determined at 50°C and pH 5.0 by using birchwood glucuronoxylan as substrate. For Nf Xyn11A, the values of Vmax and Km determined from Lineweaver-Burk plots were 5,862 nkat/mg and 6.0 mg/mL (Table 2). The Km of Nf Xyn11A was similar to the short proteins of r23.8 kDa and r22.0 kDa produced in T. reesei. The specific activity of Nf Xyn11A was 3,064 nkat/mg, which was lower than the r23.8 kDa reported by Leskinen et al. . The specific activity of Ta Xyn10A was 13,691 nkat/mg, which was higher than the activity of xylanase from T. aurantiacus Miehe, IMI 216529 and T. aurantiacus ALKO4242 [14, 17]. The Km of the Ta Xyn10A was 1.0 mg/mL, which was close to that of the GH10 xylanase from Streptomyces sp. QG-11-3 . The lower Km of Ta Xyn10A indicated that Ta Xyn10A had higher affinity than Nf Xyn11A for birchwood glucuronoxylan. The Ta Xyn10A had also a higher turnover number kcat and catalytic efficiency kcat/Km, indicating high catalytic activity.
Effect of pH and temperature on activity and thermostability
The thermal stabilities of the two xylanases were determined at 70°C and 80°C in the absence of substrate (Figure 2c). Ta Xyn10A had good stability at 70°C and retained approximately 77% of the activity after incubation for 4 hours. At 80°C, the xylanase activity of Ta Xyn10A decreased rapidly, and all activity was lost after 2 hours of incubation. Nf Xyn11A had slightly lower thermal stability than Ta Xyn10A at 70°C but, somewhat surprisingly, higher thermal stability than that of Ta Xyn10A at 80°C.
Mode action of the two xylanases on xylans
Hydrolysis of isolated xylans
End products of xylan hydrolysis
Nf Xyn11A released aldopentauronic acid (β-D-Xylp-(1→4) [4-O-methyl-α-D-Glcp A-(1→2)]-β-D-Xylp-(1→4)-β-D-Xylp -(1→4)-D-Xyl, XU4m2XX) as the shortest acidic fragment from birchwood glucuronoxylan (Figures 5a and 6a). The main acidic end product released by Ta Xyn10A was aldotetrauronic acid (4-O-methyl-α-D-Glcp A-(1→2)-β-D-Xylp-(1→4)-β-D-Xylp-(1→4)-D-Xyl, U4m2XX) (Figures 5a and 6b). The other two minor acidic oligosaccharides, eluting later in the HPAEC-PAD (between 35 and 45 minutes) corresponded to XOSs carrying 4-O-methyliduronic acid and hexenuronic acid, respectively, which were formed from the 4-O-methylglucuronic acid during the xylan isolation [41, 42]. Thus both enzymes acted on glucuronoxylan as typical GH11 and GH10 endoxylanases [4, 43].
The Nf Xyn11A enzyme released arabinoxylotetraose (β-D-Xylp-(1→4)[α-L-Araf-(1→3)]-β-D-Xylp-(1→4)-D-Xylp-(1→4)-D-Xyl, XA3XX) as the shortest arabinoxylan oligosaccharides (AXOS) from oat spelt arabinoxylan, whereas arabinoxylobiose (α-L-Araf-(1→3)-β-D-Xylp-(1→ 4)-D-Xylp, A3X) was the shortest AXOS liberated by Ta Xyn10A (Figures 5 and 6). For more precise identification of the shortest AXOS formed, TLC analysis would need to be performed, as some of the AXOSs, such as A3X and XA3X, coelute in the HPAEC-PAD . Thus, in addition to A3X, a longer XA3X was also clearly identified as a second AXOS end product by Ta Xyn10A (Figure 5b). The retention time in HPAEC-PAD is inversely correlated with pKa value and increases with increasing molecular mass of the carbohydrate. The peak of XA3XX shown in Figure 6c was tentatively identified on the basis of the longer retention time compared with A3X and XA3X, the elution order of different AXOSs and being the shortest AXOS from GH11 xylanases. It was previously reported that XA3XX was the shortest AXOS released from arabinoxylan by GH11 xylanase from Thermomyces lanuginosus and that A3X was the shortest AXOS from arabinoxylan by GH10 xylanase from Aspergillus aculeatus. These results are in accordance with present observations on the shortest AXOS formed from arabinoxylan by the Nf Xyn11A and Ta Xyn10A xylanases, respectively (Figures 5b, 6c and 6d). The Ta Xyn10A always released shorter acid XOSs and AXOSs from substituted xylans. Our results also confirmed that the endoxylanases from GH10 cleave the glycosidic linkages in the xylan main chain closer to the substituent, resulting in shorter products [4, 31, 37].
Hydrolytic properties on wheat straw
The two purified recombinant xylanases were shown to have good thermal stability at 70°C. As compared on the protein basis, the xylanase from T. aurantiacus was more efficient than the N. flexuosa xylanase in hydrolysis of isolated xylans and lignocellulosic biomass. The mode of action of the xylanases from T. aurantiacus and N. flexuosa on xylan was typical of enzymes belonging to the GH10 and GH11 families, respectively. Because of its high catalytic activity and good thermostability, the T. aurantiacus xylanase shows great potential for applications aimed at total hydrolysis of lignocellulosic materials for platform sugars, whereas the N. flexuosa xylanase has better potential as an enzyme for the production of XOSs.
glycosyl hydrolase family
high-performance anion exchange chromatography coupled with pulsed amperometric detection
The EU Commission is gratefully acknowledged for financial support (project number 213139, HYPE). This work was also supported by Natural Science Foundation of China (30700631) and Northwest A&F University Key Research Project for Young Staff. We thank Sun-Li Chong for assistance in thin-layer chromatography analysis and Henna Pynnönen for HPAEC-PAD analysis. We also thank Inbicon (Denmark) for providing pretreated wheat straw.
- Aspinall GO: Structural chemistry of the hemicelluloses. Adv Carbohydr Chem 1959, 14: 429-468.Google Scholar
- Mueller-Harvey I, Hartley RD, Harris PJ, Curzon EH: Linkage of p -coumaroyl and feruloyl groups to cell-wall polysaccharides of barley straw. Carbohydr Res 1986, 148: 71-85. 10.1016/0008-6215(86)80038-6View ArticleGoogle Scholar
- 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 Research 2009, (37 database):D233-D238.
- Biely P, Vršanská M, Tenkanen M, Kluepfel D: Endo-β-1,4-xylanase families: differences in catalytic properties. J Biotechnol 1997, 57: 151-166. 10.1016/S0168-1656(97)00096-5View ArticleGoogle Scholar
- Kolenová K, Vršanská M, Biely P: Mode of action of endo-β-1,4-xylanases of families 10 and 11 on acidic xylooligosaccharides. J Biotechnol 2006, 21: 338-345.View ArticleGoogle Scholar
- Collins T, Gerday C, Feller G: Xylanases, xylanase families and extremophilic xylanases. FEMS Microbiol Rev 2005, 29: 3-23. 10.1016/j.femsre.2004.06.005View ArticleGoogle Scholar
- Viikari L, Kantelinen A, Sundquist J, Linko M: Xylanase in bleaching: from an idea to the industry. FEMS Microbiol Rev 1994, 13: 335-350. 10.1111/j.1574-6976.1994.tb00053.xView ArticleGoogle Scholar
- Haki GD, Rakshit SK: Developments in industrially important thermostable enzymes: a review. Bioresour Technol 2003, 89: 17-34. 10.1016/S0960-8524(03)00033-6View ArticleGoogle Scholar
- Viikari L, Alapuranen M, Puranen T, Vehmaanperä J, Siika-aho M: Thermostable enzymes in lignocellulose hydrolysis. Adv Biochem Eng Biotechnol 2007, 108: 121-145.Google Scholar
- Öhgren K, Bura R, Saddler J, Zacchi G: Effect of hemicellulose and lignin removal on enzymatic hydrolysis of steam pre-treated corn stover. Bioresour Technol 2007, 98: 2503-2510. 10.1016/j.biortech.2006.09.003View ArticleGoogle Scholar
- Katapodis P, Kavarnou A, Kintzios S, Pistola E, Kekos D, Macris BJ, Christakopoulos P: Production of acidic xylo-oligosaccharides by a family 10 endoxylanase from Thermoascus aurantiacus and use as plant growth regulators. Biotechnol Lett 2002, 24: 1413-1416. 10.1023/A:1019898414801View ArticleGoogle Scholar
- Moure A, Gullón P, Domínguez H, Parajó JC: Advances in the manufacture, purification and applications of xylooligosaccharides as food additives and nutraceuticals. Process Biochem 2006, 41: 1913-1923. 10.1016/j.procbio.2006.05.011View ArticleGoogle Scholar
- Yu EKC, Tan LUL, Chan MKH, Deschatelets L, Saddler JN: Production of thermostable xylanase by a thermophilic fungus, Thermoascus aurantiacus . Enzyme Microbiol Technol 1987, 9: 16-24. 10.1016/0141-0229(87)90044-5View ArticleGoogle Scholar
- Kalogeris E, Christakopoulos P, Kekos D, Macris BJ: Studies on the solid-state production of thermostable endoxylanases from Thermoascus aurantiacus : characterization of two isozymes. J Biotechnol 1998, 60: 155-163. 10.1016/S0168-1656(97)00186-7View ArticleGoogle Scholar
- Berens S, Kaspari H, Klemme JH: Purification and characterization of two different xylanases from the thermophilic actinomycete Microtetraspora flexuosa SIIX. Antonie Van Leeuwenhoek 1996, 69: 235-241. 10.1007/BF00399612View ArticleGoogle Scholar
- Leskinen S, Mäntylä A, Fagerström R, Vehmaanperä J, Lantto R, Paloheimo M, Suominen P: Thermostable xylanases, Xyn10A and Xyn11A, from the actinomycete Nonomuraea flexuosa : isolation of the genes and characterization of recombinant Xyn11A polypeptides produced in Trichoderma reesei . Appl Microbiol Biotechnol 2005, 67: 495-505. 10.1007/s00253-004-1797-xView ArticleGoogle Scholar
- Vehmaanperä J, Alapuranen M, Puranen T, Siika-aho M, Kallio J, Hooman S, Voutilainen S, Halonen T, Viikari L: Treatment of cellulosic material and enzymes useful therein. Patent application FI 20051318, WO2007071818 Priority 22.12.2005Google Scholar
- Rantanen H, Virkki L, Tuomainen P, Kabel M, Schols H, Tenkanen M: Preparation of arabinoxylobiose from rye xylan using family 10 Aspergillus aculeatus endo-1,4-β-D-xylanase. Carbohydr Res 2007, 68: 350-359. 10.1016/j.carbpol.2006.11.022View ArticleGoogle Scholar
- Fauré R, Courtin CM, Delcour JA, Dumon C, Faulds CB, Fincher GB, Fort S, Fry SC, Halila S, Kabel MA, Pouvreau L, Quemener B, Rivet A, Saulnier L, Schols HA, Driguez H, O'Donohue MJ: A brief and informationally rich naming system for oligosaccharide motifs of heteroxylans found in plant cell walls. Aust J Chem 2009, 62: 533-537. 10.1071/CH08458View ArticleGoogle Scholar
- Suominen P, Mäntylä A, Karhunen T, Hakola S, Nevalainene H: High frequency one-step gene replacement in Trichoderma reesei : effects of deletions of individual genes. Mol Gen Genet 1993, 241: 523-530. 10.1007/BF00279894View ArticleGoogle Scholar
- Bailey MJ, Biely P, Poutanen K: Interlaboratory testing of methods for assay of xylanase activity. J Biotechnol 1992, 23: 257-270. 10.1016/0168-1656(92)90074-JView ArticleGoogle Scholar
- Miller GL: Use of dinitrosalicylic acid reagent for determination of reducing sugars. Anal Chem 1959, 31: 426-428. 10.1021/ac60147a030View ArticleGoogle Scholar
- Bailey MJ, Nevalainen KMH: Induction, isolation and testing of stable Trichoderma reesei mutants with improved production of solubilizing cellulase. Enzyme Microb Technol 1981, 3: 153-157. 10.1016/0141-0229(81)90076-4View ArticleGoogle Scholar
- Poutanen K, Puls J: Characteristics of Trichoderma reesei β-xylosidase and its use in the hydrolysis of solubilized xylans. Appl Microbiol Biotechnol 1988, 28: 425-432. 10.1007/BF00268208View ArticleGoogle Scholar
- Ghose TK: Measurement of cellulase activities. Pure Appl Chem 1987, 59: 257-268. 10.1351/pac198759020257Google Scholar
- Lowry OH, Roseborough NJ, Farr AL, Randall RJ: Protein measurement with the folin phenol reagent. J Biol Chem 1951, 193: 265-275.Google Scholar
- Laemmli UK: Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature 1970, 227: 680-685. 10.1038/227680a0View ArticleGoogle Scholar
- Ryan SE, Nolan K, Thompson R, Gubitz GM, Savage AV, Tuohy MG: Purification and characterization of a new low molecular weight endoxylanase from Penicillium capsulatum . Enzyme Microbiol Technol 2003, 33: 775-785. 10.1016/S0141-0229(03)00176-5View ArticleGoogle Scholar
- Pastell H, Virkki L, Harju E, Tuomainen P, Tenkanen M: Presence of 1→3 linked 2- O -β-D-xylopyranosyl-α-L-arabinofuranosyl side chains in cereal arabinoxylans. Carbohydr Res 2009, 344: 2480-2488. 10.1016/j.carres.2009.09.035View ArticleGoogle Scholar
- Georis J, Giannotta F, De Buyl E, Granier B, Frère JM: Purification and properties of three endo-β-1,4-xylanases produced by Streptomyces sp. strain S38 which differ in their ability to enhance the bleaching of kraft pulps. Enzyme Microb Technol 2000, 26: 178-186. 10.1016/S0141-0229(99)00141-6View ArticleGoogle Scholar
- Kalogeris E, Christakopoulos P, Vršanská M, Kekos D, Biely P, Macris BJ: Catalytic properties of the endoxylanase I from Thermoascus aurantiacus . J Mol Catal B: Enzym 2001, 11: 491-501. 10.1016/S1381-1177(00)00178-8View ArticleGoogle Scholar
- Natesh R, Bhanumoorthy P, Vithaythil PJ, Sekar K, Ramakumar S, Viswamitra MA: Crystal structure at 1.8 Å resolution and proposed amino acid sequence of a thermostable xylanase from Thermoascus aurantiacus . J Mol Biol 1999, 288: 999-1012. 10.1006/jmbi.1999.2727View ArticleGoogle Scholar
- Paloheimo M, Mäntylä A, Kallio J, Suominen P: High-yield production of a bacterial xylanase in the filamentous fungus Trichoderma reesei requires a carrier polypeptide with an intact domain structure. Appl Environ Microbiol 2003, 69: 7073-7082. 10.1128/AEM.69.12.7073-7082.2003View ArticleGoogle Scholar
- Srinivasa BR, Swaminathan KR, Ganapathy C, Roy RP, Murthy SK, Vithayathil PJ: The primary structure of xylanase from Thermoascus aurantiacus . Protein Seq Data Anal 1991, 4: 15-20.Google Scholar
- Beg QK, Kapoor M, Mahajan L, Hoondal GS: Microbial xylanases and their industrial applications: a review. Appl Microbiol Biotechnol 2001, 56: 326-338. 10.1007/s002530100704View ArticleGoogle Scholar
- Biely P, Kluepfel D, Morosoli R, Shareck F: Mode of action of three endo-β-1,4-xylanases for Streptomyces lividans . Biochim Biophys Acta 1993, 1162: 246-254. 10.1016/0167-4838(93)90288-3View ArticleGoogle Scholar
- Kalogeris E, Christakopoulos P, Kekos D, Macris BJ: Mode of action of a minor xylanase from Thermoascus aurantiacus on polysaccharides and model substrates. J Biosci Bioeng 1999, 87: 819-821. 10.1016/S1389-1723(99)80160-1View ArticleGoogle Scholar
- Vardakou M, Katapodis P, Samiotaki M, Kekos D, Panayotou G, Christakopoulos P: Mode of action of family 10 and 11 endoxylanases on water-unextractable arabinoxylan. Int J Biol Macromol 2003, 33: 129-134. 10.1016/S0141-8130(03)00077-1View ArticleGoogle Scholar
- Kaneko S, Kuno A, Muramatsu M, Iwamatsu S, Kusakabe I, Hayashi K: Purification and characterization of a family G/11 β-xylanase from Streptomyces olivaceoviridis E-86. Biosci Biotechnol Biochem 2000, 64: 447-451. 10.1271/bbb.64.447View ArticleGoogle Scholar
- Kim JH, Irwin D, Wilson DB: Purification and characterization of Thermobifida fusca xylanase 10B. Can J Microbiol 2004, 50: 834-843.View ArticleGoogle Scholar
- Teleman A, Harjunpää V, Tenkanen M, Buchert J, Hausalo T, Drakenberg T, Vuorinen T: Characterisation of 4-deoxy-α-L- threo -hex-4-enopyranosyluronic acid attached to xylan in pine kraft pulp and pulping liquor by 1 H and 13 C NMR spectroscopy. Carbohydr Res 1995, 272: 55-71. 10.1016/0008-6215(95)96873-MView ArticleGoogle Scholar
- Teleman A, Siika-aho M, Sorsa H, Buchert J, Perttula M, Hausalo T, Tenkanen M: 4- O -methyl-α-l-idopyranosyluronic acid linked to xylan from kraft pulp: isolation procedure and characterization by NMR spectroscopy. Carbohydr Res 1996, 293: 1-13. 10.1016/0008-6215(96)00170-XView ArticleGoogle Scholar
- Kolenová K, Vršanská M, Biely P: Purification and characterization of two minor endo-β-1,4-xylanases of Schizophyllum commune . Enzyme Microbiol Technol 2005, 36: 903-910. 10.1016/j.enzmictec.2005.01.006View ArticleGoogle Scholar
- Puchart V, Biely P: Simultaneous production of endo-β-1, 4-xylanase and branched xylooligosaccharides by Thermomyces lanuginosus . J Biotechnol 2008, 137: 34-43. 10.1016/j.jbiotec.2008.07.1789View ArticleGoogle Scholar
- Beaugrand J, Chambat G, Wong VWK, Goubet F, Rémond C, Paës G, Benamrouche S, Debeire P, O'Donohue M, Chabbert B: Impact and efficiency of GH10 and GH11 thermostable endoxylanases on wheat bran and alkali-extractable arabinoxylans. Carbohydr Res 2004, 339: 2529-2540. 10.1016/j.carres.2004.08.012View ArticleGoogle Scholar
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