Production and Characterization of Partially Purified Thermostable Endoxylanase and Endoglucanase from Novel Actinomadura geliboluensis and the Biotechnological Applications in the Saccharification of Lignocellulosic Biomass
Ali Osman Adıgüzel * and Münir Tunçer
Extracellular endoxylanase and endoglucanase from halo- and thermo-tolerant Actinomadura geliboluensis were produced, purified, characterized, and used in the saccharification of native and pretreated lignocellulosic biomasses. The molecular mass of endoxylanase and endoglucanase were 30 and 38 kDa, respectively. The optimum pH and temperature values for both endoxylanase and endoglucanase activities were pH 6.0 and 60 °C, respectively. They were both stable within a pH range of 4.0 to 8.0 and up to 70 °C. The half-lives of endoxylanase and endoglucanase at 70 °C were calculated as 180 min and 60 min, while their half-lives at 80 °C were detected as 60 min and 50 min, respectively. Both the endoxylanase and endoglucanase obeyed Michaelis-Menten kinetics. The endoxylanase and endoglucanase from A. geliboluensis were strongly inhibited by Hg2+. Endoxylanase was activated by Mg2+ and Ca2+ and endoglucanase was activated by Fe2+ and Ca2+. The potential application of endoxylanase and endoglucanase in saccharification of lignocellulosic biomass was further evaluated. The reduced sugar was 265.12 mg/g biomass after both endoxylanase and endoglucanase were incubated with wheat straw, which was pretreated by 1 % NaOH at 121 °C for 15 min. Endoxylanase and endoglucanase were produced from novel A. geliboluensis, which could potentially be used in biotechnological applications.
Keywords: Actinomadura; Endoglucanase; Endoxylanase; Reducing Sugar; Thermostable
Contact information: Department of Biology, Faculty of Science and Letters, University of Mersin, Turkey; * Corresponding author: email@example.com
Lignocellulose, which is the most abundant biopolymer on earth, consists of three major components: lignin (10% to 25%), hemicellulose (20% to 40%), and cellulose (35% to 55%) (Nanda et al. 2013). Composition of lignocellulose depends on biomass source (Beg et al. 2001; Ang et al. 2015; Pellegrini et al. 2015). Cellulose is a major structural component of lignocellulosic biomass and is composed of repeating (1,4)-D-glucopyranose units numbering from 100 to 20,000. Unlike cellulose, hemicellulose is a branched heteropolysaccharide. The main components of hemicellulose are xylan, xyloglucan, glucomannan, mannan, and galactomannan (Pérez et al. 2002). Agricultural, forestry, and municipal wastes comprise most of the abundant and cheap lignocellulosic biomass sources (Chandra et al. 2012). The production of microbial enzymes by using wastes, which contains lignocellulose, as carbon sources reduces the fermentation cost (Ravindran and Jaiswal 2013).
Endoglucanases (EC 188.8.131.52; 1,4-β-D-glucan 4-glucanohydrolase), which hydrolyze β-1,4-glucosidic bonds of cellulose chains and create reducing and non-reducing ends, are used in some biotechnological applications such as bioethanol production, pulp and paper biobleaching, fruit juice clarification, food processing, and animal feed improvement (Pellegrini et al. 2015). Endoxylanases (EC 184.108.40.206; 1,4-β-D-xylan xylanohydrolase) that hydrolyze xylan chains in hemicellulose have biotechnological potential in various industries, including bioethanol, food, animal feed, textile, and paper (Beg et al. 2001).
The market value of strong, thermostable, and specific industrial enzymes was 3.6 billion U.S. dollars in 2010. Approximately 75% of these enzymes are hydrolases such as cellulases, xylanases, amylases, and pectinases (Ang et al. 2015). The cost of carbon sources plays a main role in the economics of endoglucanase and endoxylanase production. In this study, the production of endoglucanase and endoxylanase from halo- and thermo-tolerant Actinomadura geliboluensis was investigated. The enzymes were partially purified, characterized, and used in the saccharification of raw and pretreated wheat straw, banana leaves, and R.communis stalks from agricultural waste.
Chemicals and Raw Materials
The chemicals used in this study were purchased from Merck (Darmstadt, Germany), Sigma (Missouri, USA), and Alfa Easer (Karlsruhe, Germany). Lentil straw, banana leaves, barley straw, corn stover, and sawdust were obtained from a local market in Mersin, Turkey. Pine needle, pine wood, and R. communis stalk were collected from a local forest in Mersin, Turkey. These lignocellulosic biomasses were chopped, milled, washed twice with distilled water, and dried at 80 °C before use.
Microorganism and Culture Conditions
The microorganism used in this study was a novel actinobacterium Actinomadura geliboluensis. The strain was isolated and identified by Sazak et al. (2012). The strain was grown on a yeast extract-malt extract agar (ISP2) medium that contained 4 g/L yeast extract, 10 g/L malt extract, 4 g/L glucose, and 20 g/L agar. The final pH of the medium was adjusted to 7.2 ± 0.2. One loop of A. geliboluensis colonies was inoculated to a minimal salts-yeast extract nutrient medium (MS-YEM) (pH 7.0 ± 0.2) that contained 6 g/L yeast extract, 0.1 g/L ammonium sulphate, 0.3 g/L sodium chloride, 0.1 g/L magnesium sulphate, 0.02 g/L calcium carbonate, and 1 mL of trace-elements solution. The culture was incubated at 30 °C and 150 rpm for 7 days. One mL of culture was used as a preculture. All fermentation experiments were performed in 50 mL of the MS-YEM in 250-mL flasks.
Measurement of Enzyme Activity and Protein Content
The culture was centrifugated at 10,000 x g for 5 min at 4 °C at the end of the incubation and then 100 µL of the supernatant and 100 µL of 1% substrate were incubated in 50 mM phosphate buffer (pH 7.0) at 37 °C for 10 min. Birchwood xylan and carboxymethylcellulose (CMC) were used as substrates for determining the endoxylanase and endoglucanase activities, respectively. The amount of reducing sugar was calculated using the 3,5-dinitrosalysilic acid (DNS) method (Miller 1959). One unit of enzyme activity was defined as the amount of enzyme required to liberate 1 µmol xylose or glucose equivalent per minute under the conditions described above. The protein content was estimated according to the Bradford method (Bradford 1976). The standard curve was plotted by using bovine serum albumin.
Determining the Lignocellulosic Structure of Biomass
The hemicellulose, lignin, and cellulose contents of wheat straw, banana leaves, and R. communis stalks were estimated according to Ali et al. (2012).
Optimization of Endoglucanase and Endoxylanase Production
The effect of different nutritional, physical, and environmental parameters such as incubation time (0 to 120 h), carbon source (lentil straw, banana leaves, barley straw, corn stover, sawdust, pine needle, pine wood, and R. communis stalk), particle size of the carbon source (0.25 to 1.00 mm), nitrogen source (asparagine, glycine, casein, peptone, yeast extract, soybean meal, urea, and gelatin), incubation temperature (25 to 40 °C), the initial pH of the medium (4.0 to 9.0), and agitation rate (50 to 250 rpm) on endoxylanase and endoglucanase production were studied. Each parameter studied was incorporated into subsequent experiments.
The crude extract was concentrated 20-fold by a 100,000 molecular weight cut-off ultra-filtration membrane before purification. The concentrated sample was loaded on to the gel filtration column that was packed with Sephadex G-100 column material according to the manufacturer’s instructions. The sample was eluted with 50 mM potassium phosphate buffer (pH 7.0). Fractions (1.5 mL) were collected at a flow rate of 30 mL/h. Endoxylanase and endoglucanase activities and absorbance at 280 nm of each fraction were determined.
Native- and SDS-PAGE
Native polyacrylamide gel electrophoresis (Native PAGE) and SDS-PAGE was performed using an OmniPAGE mini vertical electrophoresis unit (Cleaver Scientific LTD). The resolving gel was composed of 0.375 M Tris HCl buffer (pH 8.8), acrylamide (10%), bis-acrylamide (0.27%), SDS (10%), ammonium persulfate (0.006%), and tetramethylethylenediamine (TEMED) (0.15%). The stacking gel consisted of 0.125 M Tris HCl buffer (pH 6.8), acrylamide (4%), bis-acrylamide (0.105%), SDS (10%), ammonium persulfate (0.012%), and TEMED (0.30%). The reservoir buffer consisted of 0.25 M Trisma base, and 1.92 M glycine and SDS (10%). The sample buffers were prepared with 0.625 M Tris-HCl (pH 6.8), glycerol (50 %), SDS (10%), 2-mercaptoethanol (25%), and bromophenol blue (0.05%) (Laemmli 1970). The protein bands were displayed with rapid silver staining protocol (Nesterenko et al. 1994). Native PAGE was performed with SDS-free resolving gel, stacking gel, reservoir buffer, and sample buffer, similarly. The gel was incubated into a 3% substrate solution that was prepared with 50 mM phosphate buffer (pH 6.0) at 60 °C for 30 min, Congo red solution at room temperature for 15 min, and 1 M NaCl solution at room temperature for 30 min for zymography.
Characterization of Partially Purified Endoxylanase and Endoglucanase
The effect of temperature on endoxylanase and endoglucanase activities was determined at 30 to 90 °C (pH 7.0). The thermostability was assessed at 30 to 90 °C for 0 to 6 h in a 50 mM phosphate buffer (pH 7.0). The optimum pH of the enzyme was determined by carrying out the reaction in the pH range of 3.0 to 9.0 using different assay buffers for 10 min each: 50 mM sodium acetate buffer (pH 4.0 to 6.0), phosphate buffer (pH 6.0 to 7.0), and Tris-HCl (pH 7.0 to 9.0) at 60 °C.
The effects of various metal ions and inhibitors, including Mn+2, Ca+2, Mg+2, Cu+2, Zn+2, Fe+2, Hg+2, Ag+, NaCl, EDTA, DTT, and SDS, on endoxylanase and endoglucanase activities were also examined. Each enzyme with substance (1 and 10 mM) was incubated for 1 h in a phosphate buffer at optimum pH before performing the standard enzyme assay. The relative activity was calculated by comparing with a control without metal ions and inhibitors. The enzyme was pre-incubated in the presence of 20% (v/v) of different substances including formaldehyde, methanol, acetone, ethanol, isopropanol, glycerol, tween 80, isoamyl alcohol, butanol, triton X-100, toluene, and benzene at 60 °C for 1 h to determine the effects of organic solvents and chemical reagents on activity. The relative activity was calculated by comparison on the control without substance.
Application of Endoxylanase and Endoglucanase in Biomass Hydrolysis
Crude and pretreated wheat straw, banana leaves, and R. communis stalk was used in the hydrolysis experiment. Pretreatment was carried out with 1% NaOH (solid to liquid ratio of 1/10) at 121 °C for 15 min using an autoclave. Pretreated biomass was washed by distilled water four times and dried overnight at 80 °C before hydrolysis. Hydrolysis was performed in 100 mM phosphate buffer (pH 6.0) containing 2.5% biomass, 0.005% sodium azide, 20 U/mL (800 U/g biomass) endoxylanase, and 10 U/mL (400 U/g biomass) endoglucanase. During hydrolysis (0 to 6 h), sufficient hydrolysis liquid was taken at regular intervals and then reducing sugar was estimated by the DNS method (Miller 1959). The saccharification percentage was calculated as the amount of sugar after enzymatic hydrolysis divided by the amount of carbohydrate in the substrate.
RESULTS AND DISCUSSION
Optimization of Endoglucanase and Endoxylanase Production
The use of pure xylan and cellulose as carbon sources is not economical for production of endoxylanase and endoglucanase. Therefore, cost-effective and easily available lignocellulosic wastes as primary the carbon source were used for endoxylanase and endoglucanase production. Enzyme production was performed in MS-YEM supplemented with different carbon sources (5 g/L) at 30 °C and 150 rpm for 3 days. Actinomadura geliboluensis showed the highest endoxylanase (170.91 U/mL) and endoglucanase (6.20 U/mL) production when wheat straw was used as the primary carbon source (Fig. 1). Actinomadura geliboluensis produced 164.98, 122.37, and 100.47 U/mL endoxylanase in MS-YEM supplemented with corn stover, R. communis stalk, and Lolium sp., respectively. Endoglucanase activities were 5.47 and 5.41 U/mL in MS-YEM supplemented with barley straw and corn stover, respectively. Similarly, wheat straw has been reported as a good substrate for enzyme production from some actinomycetes (Kohli et al. 2001; Nadia et al. 2010; Kumar et al. 2012).
The particle size of the substrate is another important parameter for endoxylanase and endoglucanase production. In this study, the highest endoxylanase (192.76 U/mL) and endoglucanase (7.27 U/mL) production were obtained with the smallest particle size of wheat straw (≤ 0.25 mm) (Fig. 2).
Fig. 1. Effect of different lignocellulosic carbon sources on (a) endoxylanase and (b) endoglucanase production. Incubation was performed in MS-YEM supplemented with different lignocellulosic substances such as lentil straw (LS), banana leaves (BL), barley straw (BS), wheat straw (WS), corn stover (CS), Ricinus communis stalk (RCS), pine needle (PN), pine wood (PW), Lolium sp. (L), and sawdust (S) as primary carbon sources at 30 °C and 150 rpm for 3 days. The data are presented as means of three replicates with SE.
The lowest endoxylanase (77.15 U/mL) and endoglucanase (0.77 U/mL) production were recorded when wheat straw that was passed through the 1-mm IS sieve was used in a medium as the primary carbon source. Consequently, the enzyme production decreased when the particle size of wheat straw was increased due to the decrease in the surface area of the straw for microbial attack.
Fig. 2. Effect of the particle size of wheat straw on endoxylanase (a) and endoglucanase (b) production. Incubation was carried out in MS-YEM supplemented with wheat straw of different particle sizes as the primary carbon source at 30 °C and 150 rpm for 3 days. Data are presented as means of three replicates with SE.
The effect of nitrogen sources on endoxylanase and endoglucanase production was evaluated. The highest endoxylanase (193.27 U/mL) and endoglucanase (8.04 U/mL) activities were determined in a medium containing yeast extract as a nitrogen source. Also, noticiable endoxylanase (144.55 U/mL) and endoglucanase (6.98 U/mL) production were obtained when the medium was supplemented with peptone as a nitrogen source. In contrast, relatively low endoxylanase activity was determined when glycine (80.94 U/mL), casein (76.25 U/mL), asparagine (62.64 U/mL), or gelatine (46.27 U/mL) was used in the medium. The lowest endoglucanase production occurred when casein (2.47 U/mL) and gelatine (2.66 U/mL) were used in the medium (Fig. 3). Similarly, Streptomyces thermovulgaris TISTR1948 (Chaiyaso et al. 2011) and Streptomyces sp. B-PNG23 (Bettache et al. 2013) secreted high amounts of enzyme when the yeast extract was used in the medium.
Fig. 3. The effect of different nitrogen sources on (a) endoxylanase and (b) endoglucanase production; incubation was carried out in MS-YEM supplemented with wheat straw (≤0.25 mm) as the primary carbon source and with different nitrogen sources (Asparagine: ASP; Glycine: GLY; Casein: CS; Peptone: PEP; Yeast extract: YE; Soybean meal: SM; Urea: UR; Gelatine: GEL) at 30 °C and 150 rpm for 3 days; data are presented as means of three replicates with SEs
The suitable incubation temperature for endoxylanase and endoglucanase production from A. geliboluensis was determined. Actinomadura geliboluensis showed the maximum production of endoxylanase (189.26 U/mL) and endoglucanase (7.76 U/mL) at 30 °C. The enzyme production increased with the increase in incubation temperature from 25 to 30 °C (Fig. 4). Actinomadura geliboluensis produced 127.58 and 32.21 U/mL endoxylanase when incubation was carried out at 35 and 40 °C, respectively. Similarly, the endoglucanase production decreased drastically when the incubation temperature was increased to 40 °C (0.64 U/mL). Generally, microorganisms produce high amounts of enzyme at their optimum growth temperature (Nagar et al. 2010).
Fig. 4. Effect of incubation temperature on endoxylanase (a) and endoglucanase (b) production. Incubation was carried out in MS-YEM supplemented with wheat straw (≤ 0.25 mm) as the primary carbon source at different temperatures and 150 rpm for 3 days. Data are presented as means of three replicates with SE.
The effect of the culture medium initial pH on endoxylanase and endoglucanase production was investigated. The highest endoxylanase production (200.71 U/mL) was observed when the initial pH of culture medium was adjusted to 6.0. Endoxylanase production was 195.31 and 155.58 U/mL at pH 7.0 and 8.0, respectively. However, endoxylanase production decreased drastically at pH 5.0 (55.35 U/mL) and 4.0 (5.11 U/mL) (Fig. 5). The culture medium of Streptomyces olivaceoviridis E-86 demonstrated a similar optimum initial pH for endoxylanase production (Ding et al. 2004). There are, however, also some reports of endoxylanase production at neutral and alkali conditions (Nawel et al. 2011). The best initial pH of the culture medium for endoglucanase production was 7.0 (9.33 U/mL). A. geliboluensis produced 4.40, 7.25, and 7.48 U/mL endoglucanase when the initial pH of the culture was adjusted to 5.0, 6.0, and 8.0, respectively.
Fig. 5. Effect of the incubation medium initial pH on endoxylanase (a) and endoglucanase (b) production. Incubation was carried out in MS-YEM supplemented with wheat straw (≤ 0.25 mm) as the primary carbon source at 30 °C and 150 rpm for 3 days. Data are presented as means of three replicates with SE.
Agitation affected the endoxylanase and endoglucanase production notably. The highest endoxylanase (199.63 U/mL) and endoglucanase (11.98 U/mL) production were obtained at an agitation speed of 200 rpm. Endoxylanase (150.56 U/mL) and endoglucanase (7.24 U/mL) production decreased as the agitation speed increased from 200 to 250 rpm (Fig. 6). However, when the agitation speed was less than 200 rpm, noticeable reduction in both endoxylanase and endoglucanase production occurred. Observations showed that agitation speed was one of the remarkable physicochemical parameters for enzyme production. The results of this study showed that suitable agitation speed might promote enzyme production by increasing the availbility of nutrients and soluble oxygen into the medium.
Fig. 6. Effect of the agitation rate on the endoxylanase (a) and endoglucanase (b) production. A. geliboluensis incubated in MS-YEM supplemented with wheat straw (≤ 0.25 mm) as the primary carbon source at different agitation rates at 30 °C for 3 days
Purification of Endoxylanase and Endoglucanase
For the purification experiment, A. geliboluensis was incubated in MS-YEM medium supplemented with 5 g/L wheat straw (0.25 mm particle size) at 30 °C and 200 rpm for 3 days. After centrifugation of culture liquid at 10,000 x g for 5 min, supernatant was used for crude enzyme preparation. Endoxylanase and endoglucanase activities of the supernatant were 232.55 U/mL and 17.76 U/mL, respectively, and the protein content of the supernatant was 2.39 mg/mL. The supernatant was concentrated 20-fold by an Amicon ultrafiltration chamber using 10 kDa cut-off ultrafiltration membrane, and 1 mL of concentrated sample was loaded onto the gel filtration column that was packed with Sephadex G-100. Phosphate buffer (pH 7.0 and 50 mM) was used to elute the proteins at 30 mL/h. Fractions containing endoxylanase (fraction numbers 130 to 135) and endoglucanase (fraction numbers 125 to 129) were pooled and concentrated (Fig. 7). Specific activities of purified endoxylanase and endoglucanase were 182.23 U/mg and 17.65 U/mg, respectively. The purities of the endoxylanase and endoglucanase were calculated as approximately 1.87- and 2.37-fold greater than that of the crude sample. Molecular masses of enzymes were estimated as 30 kDa for endoxylanase and 38 kDa for endoglucanase by SDS-PAGE (Fig. 8).
Fig. 7. Gel filtration chromatography with Sephadex G-100. The flow rate was 30 mL/h and the size of the fractions were 1.5 mL.
Fig. 8. Electrophoretic analyses of partially purified endoxylanase and endoglucanase produced by A. geliboluensis: (a) SDS-PAGE (Lane 1: crude enzyme; Lane 2: endoglucanase; Lane 3: endoxylanase). (b) Zymogram of endoxylanase and endoglucanase. The clear band that resulted from CMC and birchwood xylan hydrolysis from purified endoglucanase and endoxylanase is visible against a red background.
Characterization of Endoxylanase and Endoglucanase
The relative activities of the endoxylanase and endoglucanase at different temperatures were determined at pH 7.0 using a standard assay method. The relative endoxylanase activity at 30 °C, 40 °C, and 50 °C was 51.80 %, 62.60 %, and 97.15 %, respectively. The optimum temperature for endoxylanase was 60 °C. Endoxylanase retained up to 50% activity at temperatures ranging from 60 °C to 90 °C (Fig. 9). Xylanases derived from actinomycetes such as Streptomyces sp. RCK-2010 (Kumar et al. 2012), Streptomyces sp. SWU10 (Deesukon et al. 2011), Streptomyces matensis (Yan et al. 2009), Streptomyces cyaneus SN32 (Ninawe et al. 2008), Streptomyces actuosus A-151 (Wang et al. 2003), and Streptomyces althioticus LMZM (Luo et al. 2016) have the same optimal temperature. However, the relative activity of xylanases from these microorganisms decreased rapidly when the temperature was increased from 60 °C to 90 °C. The optimum temperature of endoglucanase was 60 °C at pH 7.0, but it retained over 70% maximum activity in a broad temperature range (40 to 80 °C) (Fig. 9). The relative activity of endoglucanase decreased at 90 °C (56.28%). The optimum temperature of the A. geliboluensis endoglucanase was higher than some other endoglucanases obtained from Streptomyces sp. B-PNG23 (Bettache et al. 2013), Bacillus subtilis (Asha and Sakthivel 2014), and Bacillus mycoides S122C (Balasubramanian et al. 2012). Some researchers have also recently reported that endoglucanases showed maximum activity at 60 °C and above 60 °C (Saratale et al. 2012; Dipasquale et al. 2014).
Fig. 9. Effect of the reaction temperature on endoxylanase and endoglucanase activity. After substrates (CMC and birchwood xylan) and enzymes incubated at specified temperatures for 10 min at pH 7.0, the DNS method was used to measure enzyme activity. Data are presented as means of three replicates with SE.
The effect of pH on endoxylanase and endoglucanase activities was determined at standard conditions at 60 °C. Endoxylanase exhibited its maximum activity at pH 6.0 (Fig. 10). Also, relative activities of endoxylanase at pH 4.0, 5.0, 7.0, and 8.0 were 70.98%, 81.31%, 77.50%, and 56.99%, respectively. Endoxylanase activity sharply decreased above pH 8.0. Similar pH optima have been previously reported for other endoxylanases (Nascimento et al. 2002; Bajaj and Singh 2010; Kim et al. 2010; Kumar et al. 2012). Endoglucanase also showed optimal activity at pH 6.0. Endoglucanase showed considerable activity in a pH range from 4.0 (73.93%) to 8.0 (86.74%) (Fig. 10). Similarly, endoglucanase that was obtained from Streptomyces sp. showed optimal activity at pH 6.0 to 8.0 (Jang and Chen 2003).
The therrmostability of endoxylanase and endoglucanase was studied at 40 to 80 °C for 6 h. The maximum stability for endoxylanase was observed at 40 °C. The relative activities of endoxylanase were 99.61%, 95.62%, 93.28%, 88.81%, 84.46%, and 74.46% after the preincubation at 40 °C for 1, 2, 3, 4, 5, and 6 h, respectively. However, endoxylanase was moderately stable when the enzyme was pre-incubated at 50 °C (63.01%) and 60 °C (51.11%) for 5 h (Fig. 11a). Remarkable loss in endoxylanase activity was observed at 70 °C and 80 °C. The half-lives of endoxylanase at 70 °C and 80 °C were approximately 3 h and 1 h, respectively. The thermostability exhibited by endoxylanase that was observed from A. geliboluensis was higher than endoxylanase from Streptomyces cyaneus SN32 (Ninawe et al. 2008), but it was lower than Actinomadura sp. Cpt20 (Taibi et al. 2012). The relative endoglucanase activities at 40, 50, and 60 °C for 3 h incubation were 77.24%, 73.87%, and 53.05%, respectively. The half-lives of endoglucanase at 70 °C and 80 °C were approximately 60 and 50 min, respectively (Fig. 11b). The thermostability of endoglucanase that was produced by A. geliboluensis was better than that of some actinomycetes such as Streptomyces malaysiensis (Nascimento et al. 2009), Streptomyces viridobrunnes SCPE-09 (Da Vinha et al. 2011), and Streptomyces drozdowiczii (De Lima et al. 2005). However, endoglucanase that was produced by Thermomonospora sp. was more stable between 50 and 70 °C (George et al. 2001). In another study, the half-life of endoglucanase was obtained from Streptomyces sp. SLBA-08 at 8 h and 50 °C (Macedo et al. 2013).
Fig. 10. Effect of incubation pH on endoxylanase and endoglucanase activity. Reactions were performed at specified pH and 60 °C for 10 min; enzyme activity was calculated using the DNS method. Data are presented as means of three replicates with SE.
Fig. 11. The thermostability profiles of (a) endoxylanase and (b) endoglucanase. The enzymes were incubated at 40 °C (●), 50 °C (■), 60 °C (▲), 70 °C (◆), and 80 °C (x) for 6 h, and residual activities were detected at 1 h intervals. Data are presented as means of three replicates with SE.
The effect of certain metal ions and inhibitors at the concentration of 1 mM and 10 mM on the stability of endoxylanase and endoglucanase was studied at pH 6.0 and 60 °C. As shown in Table 1, some metal ions and inhibitors at 1 mM and 10 mM concentration, such as Mn+2, Cu+2, Zn+2, Ag+, EDTA, DTT, and SDS, did not affect endoxylanase activity (80% to 100% relative activity) notably. Endoxylanase activity was enhanced (100% to 110%) by Ca+2 and Mg+2 at 1 mM and 10 mM concentrations. On the other hand, Hg+2 (1 and 10 mM) showed inhibitor effects on endoxylanase that was obtained from A. geliboluensis. Similarly, some researchers reported that Hg+2 showed inhibitor effects on endoxylanases (Sharma and Bajaj 2005; Taibi et al. 2012; Luo et al. 2016). Some metal ions and inhibitors at 1 mM and 10 mM concentrations, such as Mn+2, Cu+2, Mg+2, Zn+2, Ag+, EDTA, DTT, and SDS, inhibited the endoglucanase moderately. The endoglucanase activity decreased after preincubation of enzyme with 1 mM and 10 mM Hg+2 while it was stimulated in the presence of Ca+2 and Fe+2 ions. Inhibition by Hg+2 and stimulation by Ca+2 and Fe+2 has also been indicated in previous reports (De Lima et al. 2005; Lee et al. 2008; Wang et al. 2008).
Table 1. Effect of Metal Ions and Reagents on Enzyme Activity*
*The enzyme reaction mixture without metal ions and reagents was taken as the control (100%). Data are presented as means of three replicates with SD.
The effects of various organic solvents and chemical reagents (20%) on endoxylanase and endoglucanase activities are shown in Table 2. Formaldehyde, methanol, isopropanol, glycerol, and toluene stimulated endoxylanase at 60 °C. However, acetone, ethanol, tween 80, isoamyl alcohol, butanol, triton X-10, and benzene slightly inhibited the endoxylanase activity. The endoglucanase activity was enhanced by acetone, glycerol, and tween 80, and it was inhibited by formaldehyde, methanol, ethanol, isopropanol, isoamyl alcohol, and butanol.
The kinetic parameters Km and Vmax were determined from Lineweaver-Burk double reciprocal plots of endoxylanase and endoglucanase activities at 60 °C using various concentrations (0 to 10 mg/mL) of birchwood xylan and CMC as substrates. The Vmax and Km values of endoxylanase were 292.2 (± 5.72) U/min and 3.87 (± 0.16) mg/mL, and the Vmax and Km values of endoglucanase were 18.03 (± 0.35) U/min and 3.57 (± 0.22) mg/mL, respectively. The Km value of endoxylanase from A. geliboluensis was lower than endoxylanase obtained from Streptomyces cyaneus SN32 (11.1 mg/mL) (Ninawe et al. 2008) and Streptomyces althioticus LMZM (43.03 mg/mL) (Luo et al. 2016). The Km value of endoglucanase has been reported in the range of 3.0 to 4.0 mg/mL for CMC (Wang et al. 2009; Rastogi et al. 2010). The kinetics of endoglucanase obtained from Actinomadura sp. have not been previously characterized. Lower Km values were important for the industrial application of enzymes due to increasing substrate affinity.
Table 2. Effect of Organic Solvents and Chemical Reagents on Enzyme Activity*
*The enzyme reaction mixture without organic solvents and chemical reagents was taken as the control (100%). Data are presented as means of three replicates with SD.
Hydrolysis of Biomass
Second generation biomasses include agricultural and municipal lignocellulosic waste. They are preferable in the production of value-added products, such as bioethanol and some organic acids, because they are cheap and abundant. Also, the use of lignocellulosic waste can decrease environmental problems. Because wheat straw, banana leaves, and R. communis stalks are cheap and abundant, they are good candidates for the production of reducing sugar with hydrolysis. For this reason, this study evaluated milled (0.25 mm particle size) wheat straw, banana leaves, and R. communis stalks with endoxylanase and endoglucanase that were obtained from A. geliboluensis.
The maximum reducing sugar was obtained from the hydrolysis of pretreated wheat straw (265.1 mg/g biomass). Reducing sugars were obtained via the enzymatic hydrolysis of native wheat straw, pretreated banana leaves, pretreated R. communis stalk, native banana leaves, and native R. communis stalk, which after 6 h were 138.3, 120.0, 82.1, 57.5, and 51.4 mg/g biomass, respectively (Fig. 12a). The lignocellulosic content of biomass (Table 3) was taken into consideration when saccharification was calculated.
Table 3. Contents of Natural Wheat Straw (NWS), Pretreated Wheat Straw (PWS), Natural Banana Leaves (NBL), Pretreated Banana Leaves (PBL), Natural R. communis Stalk (NRC), and Pretreated R. communis Stalk (PRC)*
*Data are presented as means of three replicates with SD.
The saccharification yields of native wheat straw, pretreated wheat straw, native banana leaves, pretreated banana leaves, native R. communis stalk, and pretreated R. communis stalk were 21.0%, 35.6%, 9.5%, 16.1%, 7.1%, and 10.3%, respectively (Fig. 12b). After pretreatment, the hemicellulose and cellulose content increased, and lignin content decreased (Table 3). Therefore, the reducing sugar yield increased with pretreatment of the biomass after hydrolysis. Table 4 shows compares the reducing sugar yields that were determined previously.
Table 4. Comparison of Reducing Sugar Yields Obtained by Enzymatic Hydrolysis of Different Biomass Materials
|Biomass||Enzymes||Enzyme Source||Pretreatment||Hydrolysis Yield||Hydrolysis Time||Ref.|
|Parthenium hysterophorus||CMCase (10 U/g biomass)||Bacillus amyloliquefaciens SS35||130 min autoclaving with 1 % (v/v) H2SO4||271.5 mg TRS/g biomass||120 h||(Singh et al. 2015)|
|Maize straw (80 g/L)||20 FPU/g substrate||T. reesei ZU-02||2% NaOH at 80 °C for 1 h||50 g/L (400 mg/g biomass) (approximately)||48 h||(Chen et al. 2008)|
|2.0%(w/v) wheat bran||0.5 U/mL xylanase||Recombinant xylanase from Bacillus sp. HJ14||None||19.0 μmol/mL reducing sugar||12 h||(Zhou et al. 2014)|
|Wheat straw||500 IU of xylanase, 80 FPU of FPase, 160 IU β-glucosidase||B. pumilus VLK-1||0.1 N NaOH for 2 h at room temperature||553 ± 12 mg sugars/g biomass||6 h||(Kumar et al. 2013)|
|Sorghum straw||Crude enzyme||Bacillus altitudinis DHN8||3% alkaline hydrogen per- oxide||34.94 mg/g biomass||36 h||(Adhyaru et al. 2014)|
|Water hyacinth biomass||Cellulase (103.75 U/g) and xylanase (650.18 U/g||Commercial||5 % NaOH for 1 h at room temperature and for 10 min at 150 °C||465 mg/g||36 h||(Ganguly et al. 2013)|
|Sugarcane bagasse||Cellulase(25 FPU/g)||Penicillium oxalicum EU2106||10 % NaOH + 10 % peracetic acid||30 g/L||96 h||(Huang et al. 2015)|
|Wheat straw||Celluclast 1.5 L (0.24 FPU/mL)||Commercial||Thermomechanical pretreatment||31 g reducing sugar/ 100 g straw||18h||(Pierre et al. 2011)|
|Wheat straw||2.5 U/mLCMCase||Commercial||Fungal pretreatment||225 mg/g straw (approximately)||35 days||(Dias et al. 2010)|
|Wheat straw||Endoxylanase (800 U/g biomass) and endoglucanase (400 U/g biomass)||A. geliboluensis||%1 NaOH for 15 min at 121 °C.||265.12 mg/g biomass||6 h||This study|
|Banana leaves||Endoxylanase (800 U/g biomass) and endoglucanase (400 U/g biomass)||A. geliboluensis||%1 NaOH for 15 min at 121 °C.||119.97 mg/g biomass||6 h||This study|
|R. communis stalk||Endoxylanase (800 U/g biomass) and endoglucanase (400 U/g biomass)||A. geliboluensis||%1 NaOH for 15 min at 121 °C.||82.14 mg/g biomass||6 h||This study|
Fig. 12. (a) The reducing sugar and (b) saccharification rates, after hydrolysis of natural wheat straw (NWS), pretreated wheat straw (PWS), natural banana leaves (NBL), pretreated banana leaves (PBL), natural R. communis stalk (NRC), and pretreated R. communis stalk (PRC). Hydrolysis was performed at 60 °C for 6 h. Data are presented as means of three replicates with SE.
- This study showed that novel A. geliboluensis can produce endoxylanase and endoglucanase using lignocellulosic wastes in submerged fermentation.
- The molecular mass of endoxylanase and endoglucanase purified by gel filtration chromatography were found to be approximately 30 kDa and 38 kDa. Endoxylanase and endoglucanase display thermotolerant characteristics and promising activity in the broad range of pH. Kinetic analysis of endoxylanase showed that Vmax and Km values of endoxylanase were 292.2 (±5.72) U/min and 3.87 (±0.16) mg/mL. The endoglucanase exhibited maximum activity (Vmax) of 18.03 (±0.35) U/min with its corresponding Km value of 3.57 (±0.22).
- Hydrolysis experiment in this study revealed that endoxylanase and endoglucanase obtained from A. geliboluensis may be useful in saccharification of lignocellulosic feedstocks.
The authors are grateful to Prof. Dr. Nevzat Şahin for the microorganism used in this study.
Adhyaru, D. N., Bhatt, N. S., and Modi, H. A. (2014). “Enhanced production of cellulase-free, thermo-alkali-solvent-stable xylanase from Bacillus altitudinis DHN8, its characterization and application in sorghum straw saccharification,” Biocatalysis and Agricultural Biotechnology 3(2), 182-190. DOI: 10.1016/j.bcab.2013.10.003
Ali, S. S., Khan, M., Mullins, E., and Doohan, F. (2012). “The effect of wheat genotype on ethanol production from straw and the implications for multifunctional crop breeding,” Biomass and Bioenergy 42, 1-9. DOI: 10.1016/j.biombioe.2012.03.020
Ang, S. K., Yahya, A., Aziz, S. A., and Salleh, M. M. (2015). “Isolation, screening, and identification of potential cellulolytic and xylanolytic producers for biodegradation of untreated oil palm trunk and its application in saccharification of lemongrass leaves,” Preparative Biochemistry and Biotechnology 45(3), 279-305. DOI: 10.1080/10826068.2014.923443
Asha, B. M., and Sakthivel, N. (2014). “Production, purification and characterization of a new cellulase from Bacillus subtilis that exhibit halophilic, alkalophilic and solvent-tolerant properties,” Annals of Microbiology 64(4), 1839-1848. DOI: 10.1007/s13213-014-0835-x
Bajaj, B. K., and Singh, N. P. (2010). “Production of xylanase from an alkalitolerant Streptomyces sp. 7b under solid-state fermentation, its purification, and characterization,” Applied Biochemistry and Biotechnology 162(6), 1804-1818. DOI: 10.1007/s12010-010-8960-x
Balasubramanian, N., Toubarro, D., Teixeira, M., and Simõs, N. (2012). “Purification and biochemical characterization of a novel thermo-stable carboxymethyl cellulase from Azorean isolate Bacillus mycoides S122C,” Applied Biochemistry and Biotechnology 168(8), 2191-2204. DOI: 10.1007/s12010-012-9929-8
Beg, Q., Kapoor, M., Mahajan, L., and Hoondal, G. (2001). “Microbial xylanases and their industrial applications: A review,” Applied Microbiology and Biotechnology 56(3), 326-338. DOI: 10.1007/s002530100704
Bettache, A., Messis, A., Copinet, E., Kecha, M., Boucherba, N., Belhamiche, N., Duchiron, F., and Benallaoua, S. (2013). “Optimization and partial characterization of endoglucanase produced by Streptomyces sp. B-PNG23,” Archives of Biological Science 65(2), 549-558. DOI: 10.2298/ABS1302549A
Bradford, M. M. (1976). “A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding,” Analytical Biochemistry 72(1-2), 248-254. DOI: 10.1016/0003-2697(76)90527-3
Chaiyaso, T., Kuntiya, A., Techapun, C., Leksawasdi, N., Seesuriyachan, P., and Hanmoungjai, P. (2011). “Optimization of cellulase-free xylanase production by thermophilic Streptomyces thermovulgaris TISTR1948 through Plackett-Burman and response surface methodological approaches,” Bioscience, Biotechnology, and Biochemistry 75(3), 531-537. DOI: 10.1271/bbb.100756
Chandra, R., Takeuchi, H., and Hasegawa, T. (2012). “Methane production from lignocellulosic agricultural crop wastes: A review in context to second generation of biofuel production,” Renewable and Sustainable Energy Reviews 16(3), 1462-1476. DOI: 10.1016/j.rser.2011.11.035
Chen, M., Zhao, J., and Xia, L. (2008). “Enzymatic hydrolysis of maize straw polysaccharides for the production of reducing sugars,” Carbohydrate Polymers 71(3), 411-415. DOI: 10.1016/j.carbpol.2007.06.011
Da Vinha, F. N., Oliveira, M. P. G., Franco, M. N., Macrae, A., Bon, E. P. S., Nascimento, R. P., and Coelho, R. R. (2011). “Cellulase production by Streptomyces viridobrunneus SCPE-09 using lignocellulosic biomass as inducer substrate,” Applied Biochemistry and Biotechnology 164(3), 256-267. DOI: 10.1007/s12010-010-9132-8
De Lima, A. L. G., do Nascimento, R. P., da Silva Bon, E. P., and Coelho, R. R. R. (2005). “Streptomyces drozdowiczii cellulase production using agro-industrial by-products and its potential use in the detergent and textile industries,” Enzyme and Microbial Technology 37(2), 272-277. DOI: 10.1016/j.enzmictec.2005.03.016
Deesukon, W., Nishimura, Y., Harada, N., Sakamoto, T., and Sukhumsirichart, W. (2011). “Purification, characterization and gene cloning of two forms of a thermostable endo-xylanase from Streptomyces sp. SWU10,” Process Biochemistry 46(12), 2255-2262. DOI: 10.1016/j.procbio.2011.09.004
Dias, A. A., Freitas, G. S., Marques, G. S. M., Sampaio, A., Fraga, I. S., Rodrigues, M. A. M., Evtuguin, D. V., and Bezerra, R. M. F. (2010). “Enzymatic saccharification of biologically pre-treated wheat straw with white-rot fungi,” Bioresource Technology 101(15), 6045-6050. DOI: 10.1016/j.biortech.2010.02.110
Ding, C. H., Jiang, Z. Q., Li, X. T., Li, L. T., and Kusakabe, I. (2004). “High activity xylanase production by Streptomyces olivaceoviridis E-86,” World Journal of Microbiology and Biotechnology 20(1), 7-10. DOI: 10.1023/B:WIBI.0000013278.24679.ed
Dipasquale, L., Romano, I., Picariello, G., Calandrelli, V., and Lama, L. (2014). “Characterization of a native cellulase activity from an anaerobic thermophilic hydrogen-producing bacterium Thermosipho sp. strain 3,” Annals of Microbiology 64(4), 1493-1503. DOI: 10.1007/s13213-013-0792-9
Ganguly, A., Halder, S., Laha, A., Saha, N., Chatterjee, P. K., and Dey, A. (2013). “Effect of alkali preteatment on water hyacinth biomass for production of ethanol,” Advanced Chemical Engineering Research 2(2), 40-44.
George, S. P., Ahmad, A., and Rao, M. B. (2001). “Studies on carboxymethyl cellulase produced by an alkalothermophilic actinomycete,” Bioresource Technology 77(2), 171-175. DOI: 10.1016/S0960-8524(00)00150-4
Huang, Y., Qin, X., Luo, X. M., Nong, Q., Yang, Q., Zhang, Z., Gao, Y., Lv, F., Chen, Y., Yu, Z., Liu, J. L., and Feng, J. X. (2015). “Efficient enzymatic hydrolysis and simultaneous saccharification and fermentation of sugarcane bagasse pulp for ethanol production by cellulase from Penicillium oxalicum EU2106 and thermotolerant Saccharomyces cerevisiae ZM1-5,” Biomass and Bioenergy 77, 53-63. DOI: 10.1016/j.biombioe.2015.03.020
Jang, H. D., and Chen, K. S. (2003). “Production and characterization of thermostable cellulases from Streptomyces transformant T3-1,” World Journal of Microbiology and Biotechnology 19(3), 263-268. DOI: 10.1023/A:1023641806194
Kim, D. Y., Han, M. K., Oh, H. W., Park, D. S., Kim, S. J., Lee, S. G., Shin, D. H., Son, K. H., Bae, K. S., and Park, H. Y. (2010). “Catalytic properties of a GH10 endo-β-1,4-xylanase from Streptomyces thermocarboxydus HY-15 isolated from the gut of Eisenia fetida,” Journal of Molecular Catalysis B: Enzymatic 62(1), 32-39. DOI: 10.1016/j.molcatb.2009.08.015
Kohli, U., Nigam, P., Singh, D., and Chaudhary, K. (2001). “Thermostable, alkalophilic and cellulase free xylanase production by Thermoactinomyces thalophilus subgroup C,” Enzyme and Microbial Technology 28(7-8), 606-610. DOI: 10.1016/S0141-0229(01)00320-9
Kumar, A., Gupta, R., Shrivastava, B., Khasa, Y. P., and Kuhad, R. C. (2012). “Xylanase production from an alkalophilic actinomycete isolate Streptomyces sp. RCK-2010, its characterization and application in saccharification of second generation biomass,” Journal of Molecular Catalysis B: Enzymatic 74(3-4), 170-177. DOI: 10.1016/j.molcatb.2011.10.001
Kumar, L., Kumar, D., Nagar, S., Gupta, R., Garg, N., Kuhad, R. C., and Gupta, V. K. (2013). “Modulation of xylanase production from alkaliphilic Bacillus pumilus VLK-1 through process optimization and temperature shift operation,” 3 Biotech 4(4), 345-356.
Laemmli, U. K. (1970). “Cleavage of structural proteins during the assembly of the head of bacteriophage T4,” Nature 227, 680-685. DOI: 10.1038/227680a0
Lee, Y. J., Kim, B. K., Lee, B. H., Jo, K. I., Lee, N. K., Chung, C. H., Lee, Y. C., and Lee, J. W. (2008). “Purification and characterization of cellulase produced by Bacillus amyoliquefaciens DL-3 utilizing rice hull,” Bioresource Technology 99(2), 378-386. DOI: 10.1016/j.biortech.2006.12.013
Luo, L., Cai, J., Wang, C., Lin, J., Du, X., Zhou, A., and Xiang, M. (2016). “Purification and characterization of an alkaliphilic endo-xylanase from Streptomyces althioticus LMZM and utilization in the pulp paper industry,” Journal of Chemical Technology and Biotechnology 91(4), 1093-1098. DOI: 10.1002/jctb.4690
Macedo, E. P., Cerqueira, C. L. O., Souza, D. A. J., Bispo, A. S. R., Coelho, R. R. R., and Nascimento, R. P. (2013). “Production of cellulose-degrading enzyme on sisal and other agro-industrial residues using a new Brazilian actinobacteria strain Streptomyces sp. SLBA-08,” Brazilian Journal of Chemical Engineering 30(4), 729-735. DOI: 10.1590/S0104-66322013000400005
Miller, G. L. (1959). “Use of dinitrosalicylic acid reagent for determination of reducing sugar,” Analytical Chemistry 31(3), 426-428. DOI: 10.1021/ac60147a030
Nadia, H., El-Nassar, A., Amal, M. A., and Abeer, A. K. (2010). “Xylanase production by Streptomyces lividans (NRC) and it’s application on waste paper,” Australian Journal of Basic and Applied Sciences 4(6), 1358-1368.
Nagar, S., Gupta, V. K., Kumar, D., Kumar, L., and Kuhad, R. C. (2010). “Production and optimization of cellulase-free, alkali-stable xylanase by Bacillus pumilus SV-85S in submerged fermentation,” Journal of Industrial Microbiology and Biotechnology 37(1), 71-83. DOI: 10.1007/s10295-009-0650-8
Nanda, S., Mohanty, P., Pant, K. K., Naik, S., Kozinski, J. A., and Dalai, A. K. (2013). “Characterization of North American lignocellulosic biomass and biochars in terms of their candidacy for alternate renewable fuels,” Bioenergy Research 6(2), 663-677. DOI: 10.1007/s12155-012-9281-4
Nascimento, R. P., Coelho, R. R. R., Marques, S., Alves, L., Gírio, F. M., Bon, E. P. S., and Amaral-Collaço, M. T. (2002). “Production and partial characterisation of xylanase from Streptomyces sp. strain AMT-3 isolated from Brazilian cerrado soil,” Enyzme and Microbial Technology 31(4), 549-555. DOI: 10.1016/S0141-0229(02)00150-3
Nascimento, R. P., Junior, N. A., Pereira, N., Jr., Bon, E. P. S., and Coelho, R. R. R. (2009). “Brewer’s spent grain and corn steep liquor as substrates for cellulolytic enzymes production by Streptomyces malaysiensis,” Letters in Applied Microbiology 48(5), 529-535. DOI: 10.1111/j.1472-765X.2009.02575.x
Nawel, B., Said, B., Estelle, C., Hakim, H., and Duchiron, F. (2011). “Production and partial characterization of xylanase produced by Jonesia denitrificans isolated in Algerian soil,” Process Biochemistry 46(2), 519-525. DOI: 10.1016/j.procbio.2010.10.003
Nesterenko, M. V., Tilley, M., and Upton, S. J. (1994). “A simple modification of Blum’s silver stain method allows for 30 minute detection of proteins in polyacrylamide gels,” Journal of Biochemical and Biophysical Methods 28(3), 239-242. DOI: 10.1016/0165-022X(94)90020-5
Ninawe, S., Kapoor, M., and Kuhad, R. C. (2008). “Purification and characterization of extracellular xylanase from Streptomyces cyaneus SN32,” Bioresource Technology 99(5), 1252-1258. DOI: 10.1016/j.biortech.2007.02.016
Pellegrini, V. O. A., Serpa, V. I., Godoy, A. S., Camilo, C. M., Bernardes, A., Rezende, C. A., Perieira, N., Jr., Cairo, J. P. L. F., Squina, F. M., and Polikarpov, I. (2015). “Recombinant Trichoderma harzianum endoglucanase I (Cel7B) is a highly acidic and promiscuous carbohydrate-active enzyme,” Applied Microbiology and Biotechnology 99(22), 9591-9604. DOI: 10.1007/s00253-015-6772-1
Pérez, J., Muñoz-Dorado, J., de la Rubia, T., and Martínez, J. (2002). “Biodegradation and biological treatments of cellulose, hemicellulose and lignin: An overview,” International Microbiology 5(2), 53-63. DOI: 10.1007/s10123-002-0062-3
Pierre, G., Maache-Rezzoug, Z., Sannier, F., Rezzoug, S. A., and Maugard, T. (2011). “High-performance hydrolysis of wheat straw using cellulase and thermomechanical pretreatment,” Process Biochemistry 46(11), 2194-2200. DOI: 10.1016/j.procbio.2011.09.002
Rastogi, G., Bhalla, A., Adhikari, A., Bischoff, K. M., Hughes, S. R., Christopher, L. P., and Sani, R. K. (2010). “Characterization of thermostable cellulases produced by Bacillus and Geobacillus strains,” Bioresource Technology 101(22), 8798-8806. DOI: 10.1016/j.biortech.2010.06.001
Ravindran, R., and Jaiswal, A. K. (2016). “Exploitation of food industry waste for high-value products,” Trends in Biotechnology 34(1), 58-69. DOI: 10.1016/j.tibtech.2015.10.008
Saratale, G. D., Saratale, R. G., and Oh, S. E. (2012). “Production and characterization of multiple cellulolytic enzymes by isolated Streptomyces sp. MDS,” Biomass and Bioenergy 47, 302-315. DOI: 10.1016/j.biombioe.2012.09.030
Sazak, A., Camas, M., Spröer, C., Klenk, H. P., and Sahin, N. (2012). “Actinomadura geliboluensis sp. nov., isolated from soil,” International Journal of Systematic and Evolutionary Microbiology 62(8), 2011-2017. DOI: 10.1099/ijs.0.036145-0
Sharma, P., and Bajaj, B. K. (2005). “Production and partial characterization of alkali-tolerant xylanase from an alkalophilic Streptomyces sp. CD3,” Journal of Scientific and Industrial Research 64(9), 688-697.
Singh, S., Dikshit, P. K., Moholkar, V. S., and Goyal, A. (2015). “Purification and characterization of acidic cellulase from Bacillus amyloliquefaciens SS35 for hydrolyzing Parthenium hysterophorus biomass,” Environmental Progress and Sustainable Energy 34(3), 810-818. DOI: 10.1002/ep.12046
Taibi, Z., Saoudi, B., Boudelaa, M., Trigui, H., Belghith, H., Gargouri, A., and Ladjama, A. (2012). “Purification and biochemical characterization of a highly thermostable xylanase from Actinomadura sp. strain Cpt20 isolated from poultry compost,” Applied Biochemistry and Biotechnology 166(3), 663-679. DOI: 10.1007/s12010-011-9457-y
Wang, C. M., Shyu, C. L., Ho, S. P., and Chiou, S. H. (2008). “Characterization of a novel thermophilic, cellulose-degrading bacterium Paenibacillus sp. strain B39,” Letters in Applied Microbiology 47(1), 46-53. DOI: 10.1111/j.1472-765X.2008.02385.x
Wang, C. Y., Hsieh, Y. R., Ng, C. C., Chan, H., Lin, H. T., Tzeng, W. S., and Shyu, Y. T. (2009). “Purification and characterization of a novel halostable cellulase from Salinivibrio sp. strain NTU-05,” Enzyme and Microbial Technology 44(6-7), 373-379. DOI: 10.1016/j.enzmictec.2009.02.006
Wang, S. L., Yen, Y. H., Shih, I. L., Chang, A. C., Chang, W. T., Wu, W. C., and Chai, Y. D. (2003). “Production of xylanases from rice bran by Streptomyces actuosus A-151,” Enzyme and Microbial Technology 33(7), 917-925. DOI: 10.1016/S0141-0229(03)00246-1
Yan, Q., Hao, S., Jiang, Z., Zhai, Q., and Chen, W. (2009). “Properties of a xylanase from Streptomyces matensis being suitable for xylooligosaccharides production,” Journal of Molecular Catalysis B: Enzymatic 58(1-4), 72-77. DOI: 10.1016/j.molcatb.2008.11.010
Zhou, J., Wu, Q., Zhang, R., Mo, M., Tang, X., Li, J., Xu, B., Ding, J., Lu, Q., and Huang, Z. (2014). “A thermo-halo-tolerant and proteinase-resistant endoxylanase from Bacillus sp. HJ14,” Folia Microbiologica 59(5), 423-431. DOI: 10.1007/s12223-014-0316-4
Article submitted: November 20, 2016; Peer review completed: January 21, 2017; Revised version received and accepted: February 5, 2017; Published: February 15, 2017.