NC State
Knob, A., Fortkamp, D., Prolo, T., Izidoro, S. C., and Almeida, J. M. (2014). "Agro-residues as alternative for xylanase production by filamentous fungi," BioRes. 9(3), 5738-5773.


Agro-industrial wastes are the most abundant renewable resource on earth and are available in large quantities. However, the disposal of these wastes presents an increasing environmental problem. Recently, there has been a great interest in the exploitation of these wastes as low-cost raw materials for the production of value-added compounds as microbial enzymes by submerged or solid-state fermentation systems. This review focuses on alternatives for xylanase production using agro-residues as substrates. In recent years, the interest in xylanase, which plays an important role in the breakdown of xylan, has markedly increased due to its wide variety of biotechnological applications. Among several agro-industrial residues that have been intensively investigated, many, such as wheat bran, wheat straw, and sugarcane bagasse, are suitable and result in high yields of xylanase, leading to low production costs. In addition, many relatively unexplored residues, such as oil palm wastes, sorghum straw, and coffee by-products, are some of the most promising substrates for xylanase production, requiring further assessment.

Download PDF

Full Article

Agro-residues as Alternative for Xylanase Production by Filamentous Fungi

Adriana Knob,* Diana Fortkamp, Thaiane Prolo, Simone C. Izidoro, and Janaína M. Almeida

Agro-industrial wastes are the most abundant renewable resource on earth and are available in large quantities. However, the disposal of these wastes presents an increasing environmental problem. Recently, there has been a great interest in the exploitation of these wastes as low-cost raw materials for the production of value-added compounds as microbial enzymes by submerged or solid-state fermentation systems. This review focuses on alternatives for xylanase production using agro-residues as substrates. In recent years, the interest in xylanase, which plays an important role in the breakdown of xylan, has markedly increased due to its wide variety of biotechnological applications. Among several agro-industrial residues that have been intensively investigated, many, such as wheat bran, wheat straw, and sugarcane bagasse, are suitable and result in high yields of xylanase, leading to low production costs. In addition, many relatively unexplored residues, such as oil palm wastes, sorghum straw, and coffee by-products, are some of the most promising substrates for xylanase production, requiring further assessment.

Keywords: Xylanolytic enzymes; Lignocellulosic materials; Solid-state fermentation; Submerged fermentation

Contact information: Biological Sciences Department, Midwest State University, 03 Camargo Varela de Sá Street, Guarapuava, PR, Brazil; *Corresponding author:


Environmental issues and concerns aimed at reducing ambient pollution have prompted an increase in the search for environmentally friendly technologies to be used in the production of many commodities (Martins et al. 2011). White biotechnology, which can be defined as the use of biotechnology for industrial production, remains a challenge because new biocatalytic processes have to compete economically with well-established chemical processes that have been optimized for years (Otten and Quax 2005). In this context, agricultural waste utilization for industrial development has emerged as an important area in industrial biotechnology. These residues are abundant sources of lignocellulose, are treated as waste in many countries, and are available worldwide (Dashtban et al. 2009).

The conversion of lignocellulosic biomass into valuable enzymes is of strategic importance for the sustainability and advancement of several industries. These materials may be used by microorganisms as a carbon source, which results in the production of cellular proteins, enzymes, organic acids, biologically important secondary metabolites, and prebiotic oligosaccharides. In addition, agro-industrial wastes can be used as source of fermentable sugars in second generation ethanol production (Anwar et al. 2014; Chandel et al. 2012; Mussato and Teixeira 2010; Sanchéz 2009). Regardless of a worldwide and enormous utilization of natural cellulosic sources, there are still abundant quantities of cellulose-containing raw materials and waste products that are not exploited or which could be used more efficiently (Sethi et al. 2013).

Successful biotechnological applications require low cost enzymes. Thus, the use of purified xylan as an inducer for enhanced xylanase production is unviable. One recent trend in this area is to use lignocellulosic residues, which not only serve as cost-effective substrates but also offer environmental advantages. Because of their biotechnological importance, significant progress has been made in the use of agro-residues for microbial enzyme production. In the present review, the main efforts for xylanase production by filamentous fungus, as have been described to date, are presented.


As the most abundant and renewable source on earth, lignocellulosic biomass includes various agro-industrial wastes (straws, hulls, stems, and stalks), deciduous and coniferous woods, waste from pulp and paper industry, municipal biodegradable wastes, and herbaceous energy crops (Limayema and Rickea 2012). With the increasing expansion of agro-industrial activities, large quantities of lignocellulosic residues are generated annually worldwide (Sanchéz 2009). Disposal of these wastes causes serious environmental problems. In addition, the non-use of agro-industrial residues constitutes a loss of potentially valuable resources (Mussato and Teixeira 2010). These potentially valuable materials were treated as waste in many countries in the past (and still are today in some developing countries) and disposed of in the environment, many times without an adequate counteractive measure, increasing environmental damage (Palacios-Oureta 2005; Dashtban et al. 2009). In other countries, they are also used to generate thermal energy by traditional means, such as fire for cooking and heat, or in modern ways, including the production of electricity, steam, and liquid biofuels (Dawson and Boopathy 2007; Kim and Dale 2004).

Agro-residues serve as low-cost raw material for other processes and can be purchased in regions that are located close to the local processing of the material. Because these wastes are rich in sugars, which are easily assimilated by microorganisms, they are very appropriate for use as raw materials in the production of industrially relevant compounds by fermentation (Mussato and Teixeira 2010).

Average values of the main components in some lignocellulose wastes are shown in Table 1. Like other lignocellulosic materials, agro-residues are composed primarily of structural, cellular-wall polysaccharides. In such residues, cellulose is usually the dominant polysaccharide (35 to 50%), followed by hemicellulose (20 to 35%), and lignin (10 to 25%).

Table 1. Composition of Some Lignocellulosic Materials

Proteins, oils, and ash make up the remaining fraction of lignocellulosic biomass. Nevertheless, amounts of cellulose, hemicellulose, and lignin vary from one plant species to another. In addition, many factors influence the ratio between various constituents in a single plant, such as age, stage of growth, and other conditions (Saha 2003; Zhu et al. 2009).


Xylan is a major structural polysaccharide of plant-cell walls and is the second most prevalent in nature after cellulose, representing up to 30 to 35% of a plant’s total dry weight. It is a heterogeneous polymer composed primarily of a linear -(1,4)-D-xylose backbone that is partially acetylated and substituted at different degrees by a variety of side chains, mostly -D-glucuronosyl and -L-arabinosyl units (Collins et al. 2005; Knob et al. 2010). The frequency and composition of the branches are dependent on the xylan source (Saha 2003). In addition, the side chains determine the solubility, physical conformation, and reactivity of the xylan molecule with the other hemicellulosic components. This greatly influences the mode and extent of enzymatic cleavage (Shallom and Shoham 2003).

Because of its heterogeneity and structural complexity, complete degradation of xylan involves the synergistic action of several hemicellulases, including endo--1,4-xylanases (EC, which attack the main chain of xylan, and -D-xylosidases (EC, which hydrolyze xylooligossacharides into D-xylose. Moreover, several accessory enzymes, such as -L-arabinofuranosidases (EC, -glucuronidases (EC, acetylxylan esterases (EC, ferulic acid esterases (EC, and p-coumaric acid esterases (EC 3.1.1-), are required to achieve the complete degradation of complex, substituted xylans (Collins et al. 2005; Knob et al. 2010; Shallom and Shoham 2003).


Xylanase is a key enzyme in the xylanolytic system with a great potential in many biotechnological applications. The use of xylanases as bleaching agents of wood kraft pulps has been considered the main industrial application of these enzymes. Currently, some of the bleaching processes commonly employed for the brightening and further delignifcation of kraft pulp call for large amounts of chlorine-based chemicals, which are toxic, mutagenic, and persistent; they also cause numerous harmful disturbances in biological systems (Yeasmin et al. 2011). Many studies have demonstrated that the pulp treatment with xylanases contributes to reduce the chlorine required in this process (Khandeparker and Numan 2008; Gupta and Kar 2009; Albert et al. 2011). Xylanases cleave the glycosidic bonds in the macromolecular chains of the xylan present in the wood pulp, facilitating the release of lignin, which is then readily available for further bleaching and thereby increasing the efficiency of this process (Birijlall et al. 2011; Dehia et al. 2013; Yeasmin et al. 2011). However, for application in biobleaching process, an ideal xylanase should be cellulase-free, alkali and thermo-stable enzyme, which requires minimum downstream processing for its production (Chapla et al. 2012; Saleem et al. 2012; Yeasmin et al. 2011).

Enzymes are widely added to feeds, and these have contributed to the substantial gains in feed conversion efficiency that have been achieved. Several studies have demonstrated that the use of xylanases can result in improvement of nutritive values of feed and performance of animals such as poultry, piggery, and fishery (Alpine et al. 2012; Bobeck et al. 2014; Guo et al. 2014; Lin et al. 2007; Omogbenigun et al. 2004). The mode of action of xylanases has been described as being predominately associated with hydrolysis of high molecular weight non-starch polysaccharides in cereals and, to a lesser extent, in vegetable protein meals, with a reduction in luminal viscosity and an improved access for endogenous enzymes to cell contents (Bedford and Cowieson 2012). Since only a partial hydrolysis of xylan is needed for viscosity reduction, the xylanase addition to feed is already highly effective. Many current studies are focusing on the development of enzymes that are resistant to natural inhibitors, as well as high temperatures, while at the same time being well suited for the conditions in the digestive tract of the target animal.

Another biotechnological application of xylanases is the bioconversion of lignocellulosic residues in the constituent sugars of xylan, which can be converted into bioethanol and xylitol (Dhiman et al. 2008; Polizeli et al. 2005; Sharma and Kumar 2013). The ethanol production from pentoses, such as xylose, has received renewed interest from researchers in recent years. As some of the most promising native strains for pentose fermentation, Scheffersomyces stipitis (formerly known as Pichia stipitis) and Scheffersomyces shehatae have been widely studied for their xylose fermentation capabilities, which provide high ethanol productivities (Liang et al. 2013; Martiniano et al. 2014). Great progress has also been achieved in the last decade by genetic engineering to make S. cerevisiae able to ferment xylose (Diao et al. 2013; Kuyper et al. 2005; Zhou et al. 2012). Moreover xylose has also been used by microorganisms for production of xylitol, a polyalcohol which finds wide application as a natural food sweetener, a dental caries reducer, and a sugar substitute for diabetics (Chandel et al. 2012; Ghosh and Sudha 2012; Sarrouh et al. 2009). Furthermore, as mentioned above, the lignocellulosic residues can be converted into other high value-added chemicals, with extensive applications in food, feed, pharmaceutical, and cosmetics industries, such as 2,3-butanediol, lactic, itaconic and ferulic acids (Mazzaferro et al. 2011; Sanchéz 2009).

Xylooligosaccharides are sugar oligomers consisting of xylose units, with different polymerization degrees, usually showing 2 to 5 residues, naturally occurring in fruits, vegetable, milk, and honey (Kumar et al. 2012). The industrial production of xylooligosaccharides is obtained through xylan-rich lignocellulosic raw materials that are partially hydrolyzed either by acids or specific enzymes (Yang et al. 2007). The latter process is preferred in the industry because of the lack of undesirable side reactions and products. Xylooligosaccharides have a sweet taste and are used as an alternative sweetener (Lachke 2006; Kumar et al. 2012). They also function as a prebiotic by stimulating the growth of healthy microflora, such as bifidobacteria (Aachary and Prapulla 2012; Childs et al. 2014). Xylooligosaccharides are also widely employed in fields of medicine and in health products, foods, beverages, and feed (Aachary and Prapulla 2012; Kumar et al. 2012; Moure et al. 2006).

In the baking industry, xylanases are used for their ability to improve textural properties of bread (Santala et al. 2011). The beneficial role of xylanases is generally attributed to their ability to hydrolyze the cell wall polysaccharides. These enzymes degrade the insoluble xylans in such a way that they become more soluble, which results in a higher viscosity of the dough (Polizeli et al. 2005; Sharma and Kumar 2013). The monomers and oligomers resulting from enzyme activity affect the water balance and modify the protein-starch interaction during bread storage. The effects on the arabinoxylan structure and functionality result in better crumb structure, improvement of texture profile, crumb porosity, firmness, higher moisture retention, and extended shelf-life of the bread (Collins et al. 2005; Butt et al. 2008; Harris and Ramalingam 2010). Xylanases that are only able to degrade water-soluble xylans to smaller parts are less suitable for use in baking industries, since small xylan molecules result in slackening and softening of the dough. Moreover, for use in biobleaching processes, xylanases should preferably be insensitive to inhibition by proteinaceous xylanase inhibitors present in wheat to display good efficiency (Courtin et al. 2001; Butt et al. 2008). In these cases, the use of xylanase in combination with other enzymes is a good strategy, because the synergistic effects of these enzymes provide better results as compared to the sole use of an isolated enzyme (Butt et al. 2008).

Other industrial applications include the clarification of wines, juices and beers, bio-processing of fabrics, and plant product processing (Harris and Ramalingam 2010; Goswami et al. 2013; Sharma and Kumar 2013). Because of the immense application possibilities, xylanase is regarded as industrially important and research has been conducted for its production using different strategies.


Microorganisms are primarily responsible for xylan degradation in nature. Thus, xylanases have been isolated from a variety of fungi and bacteria such as AspergillusTrichodermaStreptomycesPhanerochaeteChytridiomycesFibrobacterClostridiumBacillus, and Pichia (Collins et al. 2005). Microorganisms differ considerably in their ability to produce these enzymes in terms of their activities, as well as the spectrum of different xylanases (Hinz et al. 2009). However, the majority of industrially applicable sources of xylanase are limited to fungi. Currently, most commercial xylanolytic preparations are produced by genetically modified Trichoderma or Aspergillus strains (Mussatto and Teixeira 2010).

Filamentous fungi are the most distinguished producers of enzymes involved in the decomposition of lignocellulosic material. In recent decades, the use of fungi in bioprocesses has grown in importance because of the production of numerous enzymes with different biochemical properties and excellent potential for biotechnological application. According to Polizeli et al. (2005), filamentous fungi are widely utilized as enzyme producers and are generally considered more potent xylanase producers than bacteria or yeast. Xylanases in bacteria are not only produced at lower activity levels than in fungi, but they are also restricted to the intracellular or periplasmic fractions (Knob et al. 2010). Furthermore, enzymes produced by bacteria are not subjected to post-translational modifications such as glycosylation, which is an important process that affects the stability of protein conformation, protects proteins from proteolysis, and improves protein solubility (Polizeli et al. 2005).

One must also consider the fact that fungal xylanases are highly advantageous for their elevated activity levels and specificity (Knob et al. 2010). Nevertheless, the major problem associated with fungi is their reduced enzyme yield in bioreactor studies. With agitation, the shearing forces in the fermenter can disrupt the fragile fungal biomass, resulting in low productivity (Motta et al. 2013; Subramaniyan and Prema 2002).

Several mesophilic fungal species have been evaluated in relation to xylanase production, including members of AspergillusTrichoderma, and PenicilliumAspergillus niger has been one of the most investigated microorganisms as a xylanase producer, regardless of carbon source or system used (submerged or solid state fermentations). On the other hand, thermophilic microorganisms such as Thermomyces lanuginosusThermoascus aurantiacus, Talaromyces thermophiles, and Myceliophthora thermophila have been widely investigated, due to the increased biotechnological importance of thermostable xylanases (Maalej et al. 2009; Milagres et al. 2004; Moretti et al. 2012; Yang et al. 2006).

Many of the xylanase-producing fungi express multiple isoforms. These enzymes exhibit a diversity of physicochemical properties, structures, specific activities, yields, and particular specificity, leading to an increment in xylan degradation. Various mechanisms have been suggested to account for the multiplicity of function and specificity of xylan degrading enzymes, such as heterogeneity and complexity of the xylan structure, genetic redundancy, and post-translational modifications (Ghotora et al. 2006).

New Xylanase-Producing Fungal Strains

The search for new strains that display high enzyme production potential is of great biotechnological importance. Thus, the selection of the new fungal strains with high enzyme synthesis ability as well as the need to be germ-free, stable, easily preserved, and produced are of strategic importance. According to Narasimnha et al. (2006), the use of modern techniques to improve the production of metabolites does not invalidate the search for wild organisms producing useful metabolites. In fact, the screening of naturally occurring microorganisms may be the best way to obtain new strains and/or enzymes for industrial purposes.

Nevertheless, the enzymes produced by wild microorganisms are not always sufficient to meet the demand, due to low yields and incompatibility of the standard industrial fermentation processes (Ahmed et al. 2009). Therefore, several attempts have been made to increase fungal xylanase production by fungal strains, through mutagenesis and recombinant DNA technology. According to Otten and Quax (2005), large-scale production of xylan-degrading enzymes has been facilitated with genetic engineering. Additionally, recent advances in genomics have helped to overcome problems such as limited enzyme availability, substrate scope, and operational stability.

Some fungal xylanase encoding genes have been cloned in homologous and heterologous hosts, in order to overproduce the xylanolytic enzymes and modify its properties to suit commercial needs (Ahmed et al. 2009). As industrial applications require cheaper enzymes, high-level expression of enzymes in recombinant hosts is essential for ensuring the viability of the process (Juturu et al. 2011). Usually, higher production levels have been obtained when the expressed genes were from organisms taxonomically related to the host (Ahmed et al. 2009). Nevertheless, Escherichia coli (Le and Wang 2014; Yi et al. 2010; Xie et al. 2012), Pichia pastoris (Damaso et al. 2003; Driss et al. 2012; Fan et al. 2012; He et al. 2009) and, to a lesser extent, Saccharomyces cerevisiae (La Grange et al. 2001; Tian et al. 2013) have been used as hosts for expression of filamentous fungal xylanase genes.

Filamentous fungi are attractive hosts for recombinant DNA technology because of their natural ability to secrete large amounts of proteins in the medium with post-translational processing such as glycosylation (Demain and Vaishnav 2009). Regardless of the considerable amount of work dedicated to the topic and rapid development of new techniques, only a few articles concerned with the cloning of fungal xylanases genes into filamentous fungal host have been published in recent decades.

A. niger is one of the fungi that dominate the scene as a xylanase recombinant production host. Three Phanerochaete chrysosporium endo-1,4-beta-xylanase genes are cloned and expressed in A. niger. The levels of xylanase activity presented by the XynA, XynB, and XynC transformants in medium containing sacarose correspond to 0.47, 3.17, and 1.22 U/mL, respectively (Decelle et al. 2004). The xylanase II (xyn2)-encoding region of Trichoderma reesei QM6a was also successfully expressed in A. niger D15 under the transcriptional control of the glyceraldehyde-6-phosphate dehydrogenase promoter from A. niger and the glaA terminator of Aspergillus awamori. A stable Xyn2 transformant produced xylanase activity of 8,000 nkat/ml in shake-flask cultures containing molasses medium (Rose and van Zyl 2002).

A homologous expression system in A. niger was used by Levasseur et al. (2005). The authors cloned the gene xynB of A. niger under the control of the strong and constitutive glyceraldehyde-3-phosphate dehydrogenase (gpdA) gene promoter from Aspergillus nidulans. Overproduction of XynB was achieved in shake flask cultures with minimal medium containing glucose, and the secretion yield was estimated to be 625 U/mL.

The fungus T. reesei is an attractive host for expression of homologous or heterologous genes, and the inducible CBHI promoter is generally used. A xyn2 gene (cDNA) from Humicola grisea was cloned under the CBHI promoter and secretion signal and overexpressed in T. reesei (de Faria et al. 2002). The highest xylanase activity was exhibited by the transformant T2-8 (12,700 nkat mL-1) cultivated on avicel-celulose that might have activated the CBHI promoter. Salles et al. (2007) describe the heterologous expression of the Acrophialophora nainiana xyn6 gene in T. reesei Rut C-30 also under CBHI promoter. Conversely, Li et al. (2012) utilized constitutive promoters for high level homologous expression of xylanase II in T. reesei. The recombinant T. reesei strains were able to produce 9,266 U/mL and 8,866 U/mL of xylanase activities when grown in a medium with high glucose concentration.

A. nidulans and Aspergillus oryzae are also common choices as hosts to express recombinant xylanases. The xylanase activity was enhanced up to 40-fold by the introduction of multiple copies of xylanase gene exlA from A. awamori in A. nidulans (Hessing et al. 1994). The xynF1 gene was overexpressed under a strong A. oryzae TEF1 gene promoter that gives high expression levels even in the glucose-containing medium (Kitamoto et al. 1999), while the gene encoding xylanase F3 (xynF3) was successfully expressed in A. oryzae when grown in the medium containing wheat bran as a carbon source (Kimura et al. 2002).

Furthermore, Osipov et al. (2011) obtained an increased heterologous expression of Xyl-31 xylanase gene from Penicillium canescens in Penicillium verruculosum strains. The authors achieved enzymatic preparations that are biocatalysts for the hydrolysis of wastes from wood processing industries. Despite the good prospects on enzyme development provided by developments of mutations and genetic engineering studies, suitable fermentation strategies need to be developed for xylan-degrading enzyme production by cloning hosts at the industrial level.


Submerged and Solid-state Fermentations

Submerged fermentation (SmF) and solid state fermentation (SSF) systems are currently employed to produce compounds of industrial interest from lignocellulose, as an alternative for valorization of these wastes and also to solve environmental problems caused by their disposal (Kumar et al. 2012). Both systems have been used at the research level, but some techniques yielded better results than others. Because the metabolism exhibited by microorganisms is different in both systems and the influx of nutrients and efflux of waste materials needs to be carried out based on these metabolic parameters, any slight deviation from the specified parameters will result in an undesirable product (Subramaniyam and Vimala 2012).

Submerged fermentation is also known as submerged culture, and its main characteristic is the use of a liquid fermentation media with soluble nutrients. In this type of fermentation, the substrate is dissolved or suspended in a water source that is not a limiting factor. Submerged fermentation is generally used in industrial processes, as modern methods of control are more easily adapted to fermentation, the yields are higher, and the costs and risks of contamination are lower (Krishna 2005). Nevertheless, it has some drawbacks, such as physical space and requirements for energy and water (Jain et al. 2013). For this reason, interest in solid state fermentation (SSF) has increased in the last years, as it provides various advantages from both practical and economic perspectives.

Solid state fermentation has been defined as any fermentation process that involves a solid matrix acting as both a physical support and source of nutrition that allows the development of microorganisms in the absence of free flowing liquid (Pandey et al. 2000; Singhania et al. 2009). This system provides many advantages, such as mimicking the natural habitat in which the microorganism grows and reducing water activity, which can reduce microbial contaminations, and limit water consumption and equipment size. Also, it has been reported that solid-state cultures present higher volumetric yield, greater end-product stability, and less energy requirements than submerged cultures (Ayyachamy and Vatsala 2007; Jain et al. 2013; Singhania et al. 2009).

However, scaling up represents another obstacle to be overcome in SSF processes once different gradients (moisture, temperature, substrate concentration, and others) form along the bioreactor, especially the static bed ones, which may negatively influence the process. Heat dissipation, mass transfer, and control of fermentative parameters are the main challenges to be overcome in this process (Hölker and Lenz 2005; Khanahmadia et al. 2006; Singhania et al. 2009). In this respect, more research on design, modeling, operation, and scaling up are necessary to allow the employment of SSF processes involving bioreactors.

Fungi and yeast are the most suitable microorganisms for SSF, while bacteria have been considered unsuitable, according to the theoretical concept of water activity (Chinn et al. 2007). According to Orozco et al. (2008), some bacterial strains may be adapted to this type of process, although many advantages can be obtained with SSF systems when fungi are used. Unlike other microorganisms, fungi are normally found in nature growing on solid substrates such as seeds, roots, pieces of wood, stems, and dried parts of animals, such as skin and bones, and on fecal matter (Bhargav et al. 2008). Since SSF provides an environment closer to the natural habitat of fungi, these microorganisms can be stimulated to produce more xylanolytic enzymes. The highest xylanase yields have been obtained under solid-state conditions, rather than liquid state conditions (Assamoi et al. 2008; Nair et al. 2008; Kulkarni and Gupta 2013; Roy et al. 2013; Singh et al. 2013). The findings of Jin et al. (2012) also support the use of SSF bioreactors and suggest that they are good not only for the control of microbial fermentation that affect the growth of some important parameters, but also for substantially increasing xylanase production as well.

Despite the potential advantages presented by SFF, more than 75% of industrial enzymes are produced using SmF. This can be explained by the fact that SmF supports the utilization of genetically modified organisms to a greater extent than SSF. Moreover, SmF is widely used due to the lack of equipment required for the production of various enzymes under SSF (Subramaniyam and Vimala 2012). However, current trends emphasize that solid-state fermentation systems have potential for increased xylanase production.

Induction of Xylanases by lignocellulosic materials

The capacity of a particular microorganism to grow in lignocellulosic substrates is directly related to the production of a broad spectrum of enzymes that act synergistically to deconstruct the plant cell wall by substrate depolymerization of varying complexity (Siqueira et al. 2010; Moreira et al. 2012). It has been proposed that substrates containing xylan are necessary for xylanase production because its hydrolysis products serve both as inducers as well as a carbon source for the organism (Haltrich et al. 1996). In most of the fungi studied, xylanolytic enzymes expression regulation is mediated by the transcriptional activator XlnR, which regulates the expression of a number of genes involved in xylan degradation (Hasper et al. 2002; Stricker et al. 2008). The xlnR gene transcription is modulated by carbon sources, such as xylan and xylose (de Vries et al. 1999; Tamayo et al. 2008; Mandal et al. 2012). Xylan was found to be the best inducer of most microbial xylanases (Khucharoenphaisan et al. 2010; Joshi and Khare 2012) followed by the monosaccharides xylose and arabinose (Mandal et al. 2012), medium- to large-sized xylooligosaccharides (Miyazaki et al. 2005), xylitol, and arabinol (Mach-Aigner et al. 2011). In many cases, basal constitutive synthesis was detected in absence of an inducer added, leading to the formation of easily metabolizable compounds (Mandal et al. 2012).

Several studies have demonstrated that xylanase-encoding genes are subject to catabolic repression. This mechanism alters transcription and it is regulated by CreA protein, a transcriptional repressor of glucose-repressible genes (de Vries et al. 1999; Sun et al. 2011). The repression of xylan-degrading enzymes by preferred carbon sources such as glucose is an efficient energy-conserving mechanism, once when glucose is abundant in the environment; the xylan degrading enzymes are unnecessary (Amore et al. 2013; Sun and Glass 2011). In spite of being an inducer of xylanolytic gene expression, xylose also represses the expression of xylanolytic genes. In T. reesei and Neurospora crassa, it has been reported that xylose can function as both a repressor and an inducer of xylanase expression, depending on concentration (Mach-Aigner et al. 2010; Sun et al. 2012). In A. niger, CreA mediates carbon repression of xylanolytic enzymes by xylose, beginning at 1 mM and increases in strength up to in the area between 30-70 mM (de Vries et al. 1999).

According to Glass et al. (2013), despite recent progress, knowledge on the order of events, the timing, and the regulatory mechanism behind the induction of genes encoding plant polysaccharide-degrading enzymes during the exposure of fungi to complex lignocellulosic substrates remains poorly understood. However, recent studies have been able to elucidate part of this intricate process.

When saprophytic fungus such as A. niger and N. crassa are exposed to complex lignocellulosic materials, their response is complex and leads to the up-regulated transcription of several carbohydrate active enzymes and accessory proteins (Coradetti et al. 2012; Znameroski and Glass 2013; Benz et al. 2014; van Munster et al. 2014). It has been shown that carbon starvation plays a major role in the induction or initial fungal response. The relief of carbon catabolite repression, by glucose depletion or deletion of creA, activate the expression of genes of the early degradative response, including genes that encode enzymes that are active on arabinan or arabinogalactan side chains of pectin, as well as (arabino)xylan and galacto(gluco)mannan. On the other hand, expression levels of genes of the major, later, degradative response were not affected (Nakari-Setälä et al. 2009; Delmas et al. 2012). The enzymes encoded by the genes that have increased transcription levels under early lignocellulose degradation can be responsible for release of small inducers from substrates in the environment of the fungus, acting either alone or together with enzymes encoded by constitutively expressed genes (Martens-Uzunova and Schaap 2009; Glass et al. 2013; van Munster et al. 2014).

Thus, this model of induction suggests that both types of enzymes (constitutively expressed and up-regulated by carbon starvation) contribute to the release of inducing molecules. The early up-regulation of the xylanolytic genes that are transcriptionally activated by the xylanolytic regulator XlnR could be related to the early release of xylose, arabinose, and (arabino)xylan oligosaccharides from the substrate by these enzymes. Alternatively, it could be related to the presence of low amounts of xylose in the cultivation medium containing the lignocellulosic substrate (Delmas et al. 2012).

Agro-Residues Used for Fungal Xylanase Production

The market demand for xylanases has significantly increased during the past few decades. The practical application of these enzymes cannot be achieved unless they are available in sufficient amounts. Because biotechnological applications require large quantities of low-cost enzymes, several approaches for xylanase production have been applied. The use of agro-residues as substrates for the microbial production of xylanase has shown promise as an alternative that could substantially reduce enzyme costs and increase productivity.

The nature of particles and moisture content of the agro-industrial waste utilized in fermentation systems are critical factors (Singhania et al. 2009). The choices of suitable agro-industrial waste for the fermentation process have indicated the types of a lignocellulosic material that favor both fungal growth and product formation (Kumar and Kanwar 2012). The evaluation of this parameter and other process conditions, such as temperature, pH, and aeration, has encouraged the screening of several agricultural-residues for the production of xylanase (Singhania et al. 2009). However, because the growth of microorganisms in different carbon sources is associated with a differential expression of functionally distinct xylanases (Badhan et al. 2007), much exploration still needs to be carried out to identify sustainable substrates that allow production of xylanases with desirable characteristics.

Since compounds derived from xylan are required for xylanase induction, several reports evaluated the xylanase production using isolated xylans as substrate. Higher xylanases titers obtained with oat spelt xylan (a highly substituted xylan) were produced by T. aurantiacus, corresponding to 575.9 U/mL (Yu et al. 1987), whereas Ghatora et al. (2007) achieved notable xylanase levels using birchwood xylan (a less-branched xylan) with Melanocarpus sp. (264.2 U/mL). However, the high cost of xylans has limited their applications for large-scale production processes. In this context, some lignocellulolytic substrates, such as sawdust, sugarcane bagasse, soy flour, maize straw, or wheat bran, have been compared in relation to purified xylans (Okafor et al. 2007; Goyal et al. 2008; Jhosi and Khare 2012; Guimaraes et al. 2013). Many of these have performed significantly better than isolated xylans with respect to the yields of xylanase in large-scale production processes. However, the successful application of enzymes depends not only on the substrate choice but on the optimization of production, which may directly result in cost reduction.

A comparison of the production levels of fungal xylanase reported in the literature of recent years was performed. The greatest xylanase yields for several agro-residues that were evaluated in SSF and SmF are shown in Tables 2 and 3, respectively.

Table 2. Comparisons of Xylanase Production Levels from Different Filamentous Fungi Grown on Agro-residues in SSF

In general, the values ​​in Table 2 were obtained after optimizing the xylanase production process. It is emphasized that this comparison may not reflect the real differences between the levels produced, as no standard enzyme substrate has yet been adopted. Historically, xylanase activity has been measured by the DNS-method using purified xylan from several sources, such as oat spelt, larch wood, birch wood, or beech wood, as a substrate. In addition, other variables such as inoculum size, experimental design, and operational conditions directly affect the levels of xylanase produced. However, it still is possible to infer from the data which of the raw materials may be the most promising.

Table 3. Comparisons of Xylanase Production Levels from Different Filamentous Fungi Grown on Agro-residues in SmF

A greater number of agro-residues are currently being exploited by both systems. The different production levels observed among the lignocellulosic materials that have been evaluated are likely related to the differences in composition and the accessibility of the substrates to the fungi. Additionally, each fungal species shows an intrinsic ability to produce xylanases in the presence of specific substrates. Interestingly, high titers of xylanase have been obtained with some substrates not commonly explored for xylanase production, such as soya oil cake, coffee husk, and sorghum straw. In addition, lignocellulosic materials such as maize straw, sawdust, grape pomace, citrus peel, soybean meal, and barley bran provided low levels of xylanases when compared to other materials. These substrates have not been extensively exploited, possibly due to lower observed yields in comparison with other substrates.

In most cases, agro-residues used to produce enzymes by SSF or SmF either do not contain all the necessary nutrients for this purpose or they may be available but in sub-optimal concentrations. In these circumstances, the substrate must be supplemented to stimulate or improve enzyme production by the addition of extra carbon or nitrogen sources (Galiotou-Panayotou and Kapantai 1993; Patil and Dayanand 2006; Ritter et al. 2013). Supplementation can also be carried out by using a mineral salt solution to adjust the initial moisture content of the residue (Khandeparkar and Bhosle 2006; Papinutti and Forchiassin 2007). Moreover, for each organism or strain to have its own special conditions, including specific carbon sources for maximum yields, other fungal strains must be evaluated to verify the real potential of these substrates as xylan-degrading enzyme inductors. The representative studies on agro-residues that have been concerned with fungal xylanase productivity are described below.

Wheat bran

Wheat bran, produced worldwide in large quantities as a by-product of the wheat milling industry, constitutes a significant underutilized source of sugars. Annually, over 650 million tons of wheat is produced in the world. The accumulated biomass of wheat bran can be estimated at 150 million tons, which is predominantly used in the feed industry (Prückler et al. 2014).

Recently, there has been an increase in attempts to produce xylanases, especially through SSF, using wheat bran. It is interesting to note that, although a number of substrates have been employed for cultivating different fungi, wheat bran has been the preferred choice in most of these studies. This substrate shows a natural ability to induce xylanase synthesis. This quality is attributed to its cell-wall polysaccharides that contain 40% xylan, favorable degradability, and the presence of some nutrients in the carbon source. Additionally, wheat bran is able to remain loose in moist conditions, thereby providing a large surface area (Betini et al. 2009; Dhillon et al. 2011; Singh et al. 2008). On the other hand, it can be an expensive carbon source for large scale usage, which can represent problems for its industrial application (Virupakshi et al. 2005; Yang et al. 2006).

The biochemical composition of wheat bran indicates that when this material is hydrolyzed, it contains a considerable amount of soluble sugars, such as glucose (42.5% dry wt), xylose (15.4% dry wt), arabinose (3.1% dry wt), and galactose (2.7% dry wt), which are required to initiate micro-organism growth and replication (Archana and Sathyanarayana 1997). In the literature, many works have reported the use of wheat bran to produce xylanase by several fungal species. These fungi, such as those belonging to the genera Aspergillus (Li et al. 2006; Betini et al. 2009; Dhillon et al. 2011; Sorgatto et al. 2012; Guimaraes et al. 2013), Penicillium chrysogenum (Okafor et al. 2007), Sclerotinia sclerotiorum (Ellouze et al. 2008), Fusarium solani (Bakri et al. 2013), and Simplicillium obclavatum (Roy et al. 2013), have exhibited different levels of enzyme production.

Remarkable xylanase levels were produced by A. niger XY-1, when grown under SSF in the presence of wheat bran. After 48 h of fermentation, xylanase activity reached 14,637 U/g dry substrate (Xu et al. 2008). With a shortened fermentation time, higher xylanase production, and no need for the addition of expensive mediums, this process shows the potential ability to be utilized for industrial purposes. Among the lignocellulosic substrates tested by Kamra and Satyanarayana (2004), wheat bran supported a high xylanase secretion (7,832 U/g of dry carbon source) by H. lanuginosa in SSF after parametric optimization. It is also important to highlight the xylanase production titers of A. foetidus MTCC 4898, which corresponded to 8,450 U/g dry substrate after optimizing the xylanase production process (Chapla et al. 2010).

In relation to SmF, significant levels of xylanase were produced by A. niger (74.5 U/mL) and A. terreus (68.9 U/mL) using wheat bran after optimization of process parameters, such as moistening agent, level of initial moisture content, temperature of incubation, inoculum size, and incubation time (Gawande and Kamat 1999). Gottschalk et al. (2013) evaluated xylanase production by A. awamori 2B.361 U2/1 in the presence of wheat bran. An improved yield was achieved with the use of poor nitrogen sources, such as sodium nitrate, corresponding to 44.88 U/mL. Efficient production was also obtained with Penicillium sp. WX-Z1, using Plackett-Burman and Box-Behnken designs (46.5 U/mL) (Cui and Zao 2012).

Wheat straw

Wheat straw is one of the most abundant crop residues in the world. It is estimated that 354 million of tons of wheat straw may be available globally (Bhatia et al. 2012). The huge amount of this residue may constitute a promising raw material that could potentially be transformed into a more edible feed for ruminants (Rodrigues et al. 2008) or, alternatively, it could also be used for microbial enzyme production. Wheat straw is also one of the substrates that has been extensively investigated as a carbon source for xylanase production (Narang et al. 2001; Gupta et al. 2009; Sanghvi et al. 2010; Liao et al. 2012; Pandya and Gupte 2012). The high xylan content in wheat straw makes it an accessible and cheap inducer source that can be applied in large volumes for fermentation, such as in industrial bioreactors (Michelin et al. 2012).

P. thermophila J18, a thermophilic fungus, was able to produce substantial quantities of xylanase under SSF in the presence of wheat straw. The production was enhanced by optimizing the particle size of wheat straw, nitrogen source, initial moisture level, growth temperature, and initial pH level. Under optimized conditions, yields as high as 18,580 U/g dry substrate were achieved (Yang et al. 2006). M. albomyces IIS-68, Aspergillus tubingensis JP-1, and T. aurantiacus also showed promising xylanase activity in the presence of wheat straw, with yields of 7,760 U/g, 6,887 U/g, and 6,193 U/g dry substrate, respectively (Kalogeris et al. 1998; Narang et al. 2001; Pandya and Gupte 2012).

Under SmF, high amounts of xylanase ​​were produced by M. albomyces IITD3A when cultivation was performed with wheat straw (550 U/mL). The statistical optimization of the process parameters by response surface methodology revealed that xylanase production was most affected by fungus morphology and changes in the pH medium (Biswas et al. 2010). A similar level of production by M. albomyces was verified by Gupta et al. (2013). The authors found that xylanase production is influenced by the synergic effect of nitrogen sources in the fermentation medium, reaching a production of 520 U/mL.

Sugarcane bagasse

Sugarcane plays a vital economic role as one of the main crops cultivated in countries such as Brazil, India, and China (Chandel et al. 2012). The remnants left over after the juice extraction from the sugarcane stem are called sugarcane bagasse (Pandey et al. 2000). Sugarcane bagasse represents a sizeable portion of annually collected agro-residues. Approximately 1.6 billion tons of sugarcane is collected annually from around the world. This production yields approximately 279 million metric tons of sugarcane waste (Krishnan et al. 2010; Chandel et al. 2012). This waste is typically used as a source of fuel for heat and electricity in sugar mills.

The use of SSF for enzymes production is an interesting alternative for the valorization of sugarcane bagasse. Consequently, various reports on the production of xylanases using this lignocellulosic material have been published. High xylanase yields under SSF using sugarcane bagasse as a substrate were described by Manimaran et al. (2009) with T. lanuginosus SSBP (19,320 U/g dry substrate). Expressive xylanase titers (2,600 U/g dry substrate) were also obtained when T. reesei and A. niger were co-cultured (Gutierrez-Correa and Tengerdy 1998). In addition, Milagres et al. (2004) used sugarcane bagasse in xylanase production with a T. aurantiacus strain and obtained levels of 1,597 U/g dry substrate. Similar xylanase production was recorded by Ghoshal et al. (2012). The SSF of sugarcane bagasse by Penicillium citrinum MTCC 2553 was optimized, resulting in 1,645 U/g dry substrate.

Many investigations have also been carried out to evaluate xylanase production when employing sugarcane bagasse under SmF. Optimization of growth conditions for xylanase production by T. lanuginosus resulted in substantial xylanase activity of 946 U/mL (Ali et al. 2013). Rezende et al. (2002) showed that T. harzianum produced high levels of xylanase with sugarcane bagasse, reaching 288 U/mL.

Rice straw

Rice straw, a renewable lignocellulosic biomass, is an attractive feedstock because it is one of the most abundant lignocellulosic waste materials in the world (Binod et al. 2010). About 60% of the mass produced by rice crops is rice straw, which has high cellulose and hemicellulose contents that can be hydrolyzed into fermentable sugars. The annual global generated amount of this residue is 685 million tons (Lim et al. 2012).

Usually, rice straw is removed from the field at harvest time and is subjected to open field burning. However, this practice creates serious environmental, safety, and health issues (Sarkar and Aikat 2012; Shafie et al. 2012). For this reason, there is a strong desire to find alternative ways to remove the rice straw after each harvest season. Recent research findings have provided new options for the reutilization of rice straw as a feedstock for enzyme and monosaccharide production (Sarkar and Aikat 2012).

Rice straw is ostensibly a feasible medium for xylanase production under SFF, as has been demonstrated in recent research. Kang et al. (2004) reported a total xylanase production of 5,070 U/g dry substrate by A. niger KK2 in a basal medium that was supplemented with rice straw as a carbon source. Soroor et al. (2013) described xylanase production by T. reeseiF418 when cultivated on a medium containing rice straw, corresponding to 2,232 U/g dry carbon source.

Under SmF, substantial amounts of xylanase have also been obtained with rice straw. The xylanase production by A. fumigatus NITDGPKA3 was statistically optimized by response surface methodology based on a central composite design. A significant titer of xylanase was obtained, corresponding to 1,040 U/mL (Sarkar and Aikat 2012). Among several fungal strains that were isolated from paper mill effluent, A. fumigatus produced high levels of xylanase in the presence of rice straw (135 U/mL) and negligible levels of endocellulase (Anthony et al. 2003).

Corn cob

Agricultural residues such as corn cob represent large, renewable sources of lignocellulosic biomass. Corn cob is an important by-product of the sweet corn processing industry (Kumar et al. 2008). For every 100 kg of corn grain that is processed, approximately 18 kg of corn cobs is generated. The large quantities of corn cob produced have negligible value and are mostly discarded, with small quantities sold at very low prices for supplementary animal feed or used as fertilizer (Topakas et al. 2004; Ashour et al. 2013).

Because of its nutritional content, corn cob can be used as a medium to cultivate microorganisms, or it may be converted into added-value chemicals, such as lactic acid, citric acid, sugars, and ethanol (Ashour et al. 2013). In addition, the elevated xylan content in corn cob (40%), the highest among all agricultural waste, makes it a potential substrate for xylanase production. Remarkable xylanase production by A. foetidus, 3065 U/g dry substrate, was achieved by Shah and Madamwar (2005) using corn cob under optimized growth conditions, taking into account the parameters of temperature, pH, moistening agents, moisture level, and nitrogen sources. The xylanase production process by A. niger CECT 2700 was successful established in a laboratory-scale horizontal tube bioreactor, achieving the highest xylanase activity of 2.926 U/g of corn cob (Pérez-Rodríguez et al. 2014).

Moreover, corn cob has potential as a substrate for SmF xylanase production. T. lanuginosus has been reported to be one of the best producers of xylanase when grown on corn cob (3,575 U/mL) (Singh et al. 2000). Similar quantities of xylanase were produced by T. lanuginosus MC 134 (3,399 U/mL), according to a report by Kumar et al. (2009), showing the xylanase production potential of these strains using corn cobs.

Other potential substrates

Among the substrates evaluated for fungal xylanase production, oil palm wastes are one of the least explored, but one of the most promising. Remarkably, an A. terreus strain showed xylanase activity corresponding to 115,000 U/g after optimization, using palm fiber as a carbon source. Expressive production was also obtained with oil palm waste by A. terreus(41,000 U/g dry substrate) and A. fumigatus (35,380 U/g dry substrate) (Lakshmi et al. 2011). In addition, oil palm leaf has also been shown to be a promising raw material for xylanase production by A. niger under SmF, reaching 1,906 U/mL (Norazlina et al. 2013). These substrates are a by-product from extracting the oil of palm fruits that are normally burned as fuel to provide energy for the palm oil mills (Neoh et al. 2011) and have only recently been explored as a viable alternative for xylanase production.

Sorghum straw is a renewable and cheap resource, commonly used as livestock feed. However, it has scarcely been studied as a raw material for biological processes (Sene et al. 2011). Nevertheless, because of the high xylose content of sorghum straw (19.16 % dry weight) (Téllez-Luis et al. 2002), it may be explored as a xylanase inducer. Sonia et al. (2005) have reached notable xylanase levels using sorghum straw with T. lanuginosus D2 W3 via SSF (48,000 U/g dry substrate), after optimizing conditions using Box-Behnken methodology.

Oil cakes are by-products obtained after oil is extracted from seeds. These materials have been explored by several researchers for their employability as substrates in SSF or as supplements for production media (Ramachandran et al. 2007). Soya oil cakes, however, have occasionally been used for enzyme production (Assamoi et al. 2010), the potential for which was demonstrated by Antoine et al. (2010). Various fermentation parameters were optimized for enhanced xylanase production by P. canescens under SSF, with production amount of 18,895 U/g dry substrate. Assamoi et al. (2008) also reported high xylanase production by P. canescens 10-10c when cultivation was performed with soya oil cake, which corresponded to 14,000 U/g dry substrate.

Coffee, after petroleum, is the second largest traded commodity in the world. Therefore, the coffee industry is responsible for the generation of large amounts of residue (Nabais et al. 2008). Despite the large quantities of coffee wastes that are generated, there are few studies focusing on their use in other, profitable applications (Mussatto et al. 2011b). However, the chemical composition data (Table 1) suggest that coffee husk and spent coffee grounds can be of value as raw material for biotechnological processes, including xylanase production.

The feasibility of using coffee by-products for xylanase production under SFF by Penicillium sp. has recently been studied. The process parameters, such as fermentation time, carbon source, nitrogen source, moisture, particle size, and inoculum size were optimized, resulting in an expressive production of 20,388 U/g dry substrate when coffee husk was employed as carbon source. Xylanase titers were further improved to 23,494 U/g dry substrate with a steam pre-treatment (Murthy and Naidu 2012). The high enzyme titers obtained with coffee husk proved it to be a promising substrate for xylanase production.

Combinations of agro-industrial residues as carbon sources for xylanase production

In recent research, agro-industrial residues combinations being used as carbon sources for xylanase production have been reported for several types of fungi. However, there have been very few reports concerning the production of xylanases on mixed agro-industrial wastes in SmF. Mostly, mixed agro-industrial wastes are employed in SSF processes. In general, good levels of productivity have been obtained through these combinations, many times exceeding the titers obtained with the use of substrates alone (Pang et al. 2006; Betini et al. 2009; Su et al. 2011). Despite the limited attention devoted to the development of enzyme production processes employing mixed agro- residues, this is an important and emerging area for waste management.

Among several lignocellulosic substrates that have been evaluated, a mixture of corn cob and wheat bran supported a high xylanase secretion by H. lanuginosa in SSF, corresponding to 8,237 U/g dry substrate (Yang et al. 2011). The xylanase production by the thermotolerant fungus A. fumigatus was substantially enhanced through media optimization process. The combination of corn straw and wheat bran yielded enzyme levels of 7,232 U/g dry substrate (Moretti et al. 2012).

A. niger DFR-5 exhibited its highest xylanase production (2,596 U/g dry substrate) in media containing a mixture of wheat bran and soybean powder in a ratio 7:3 (Pal and Khanum 2010), while a combination of rice straw and wheat bran (3:2) was found to be the best substrate for xylanase production by A. niger mixed with T. reesei. (Dhillon et al. 2011). Among a few easily available lignocellulosic substrates that were tested, a combination of soybean meal and crushed corn cob increased xylanase activity by Aspergillus japonicas C03 (Facchini et al. 2011), while a mixture of wheat bran and rice straw improved the xylanase production by A. fumigatus ABK9, reaching 1,130 U/g dry substrate (Das et al. 2013).

Xylanase production by A. awamori in both SSF and SmF was stimulated by mixing grape pumice with orange peels. The enzyme synthesis was similar to or higher than those produced by other agro-industrial residues (Díaz et al. 2012). In addition, high quantities of xylanase were obtained by T. lanuginosus SDYKY-1 under SmF. The adjustment of corn cob and soybean meal concentrations resulted in maximum enzyme production of 3,078 U/mL (Su et al. 2011).


Recently, many efforts have been made to convert lignocellulosic residues into valuable products. For this reason, a number of such substrates have been evaluated for their potential as a carbon source for xylanase production, and many benefits have been obtained by these processes, such as high productivity and low production cost. So far, lignocellulosic biomass has been the most promising source to be employed as feedstock for microbial xylanase production. However, taking into account the variability of waste composition as well the optimization of the production process, larger studies are needed to determine if these wastes are suitable for pilot-scale production of the same or at even an industrial scale.

Molecular techniques developed during the past few decades have improved characteristics of the xylan degrading enzymes and increased its expression rates. However, the search for new microbial strains with improved enzyme expression profiles or higher protein secretion levels should be intensified in order to develop viable enzymatic production technologies that employ agro-industrial wastes as substrates.

Finally, in relation to environmental questions, it is necessary to emphasize the importance of removing wastes from the environment and adding value to them, allowing various industrial sectors to benefit from the use of xylanases that are obtained from lignocellulosic materials.


The authors would like to thank CAPES (Coordination for the Improvement of Higher Education Personnel) and Fundação Araucária for their financial support to the project on fungal xylanases and the scholarship awarded to the authors.


Aachary, A. A., and Prapulla, S. G. (2012). “Xylooligosaccharides (XOS) as an emerging prebiotic: Microbial synthesis, utilization, structural characterization, bioactive properties, and applications,” Comp. Rev. Food Sci. Food Saf. 10(1), 2-16.

Abbas, A. A., Obeid, R. K., Assmaeel, H. H, and Abdulatif, M. O. (2011). “Optimal conditions for production acidic D-xylanase by Aspergillus niger in submerged fermentation,” J. Biotechnol. Res. C. 5(3), 14-21.

Adapa, P. K., Tabil, L. G., Schoenau, G. J., Canam, T., and Dumonceaux, T. (2011). “Quantitative analysis of lignocellulosic components of non-treated and steam exploded barley, canola, oat and wheat straw using Fourier transform infrared spectroscopy,” J. Agr. Sci. Technol. B1, 177-188.

Ahmed, S., Riaz, S., and Jamil, A. (2009). “Molecular cloning of fungal xylanases: An overview,” Appl. Microbiol. Biotechnol. 84(1), 19-35.

Akpinar, O., Erdogan, K., and Bostanci, S. (2009). “Production of xylooligosaccharides by controlled acid hydrolysis of lignocellulosic materials,” Carbohydr. Res. 344(5), 660-666.

Albert S., Chauhan, D., Pandya, B., and Padhiar, A. (2011). “Screening of Trichoderma spp. as potential fungal partner in co-culturing with white rot fungi for efficient bio-pulping,” Global J. Biotechnol. Biochem. 6(3), 95-101.

Ali, U. F., Ibrahim, Z. M., and Isaac, G. S. (2013). “Ethanol and xylitol production from xylanase broth of Thermomyces lanuginosus grown on some lignocellulosic wastes using Candida tropicalis EMCC2,” Life Sci. J. 10(1), 968-978.

Alpine, P. O. Mc., O’Shea, C. J., Varley, P. F., and O’Doherty, J. V. (2012). “The effect of protease and xylanase enzymes on growth performance and nutrient digestibility in finisher pigs,” J. Amin. Sci. 90(4), 375-377.

Amore, A., Giacobbe, S., and Faraco, V. (2013). “Regulation of cellulase and hemicellulase gene expression in fungi,” Curr. Genomics 14(4), 230-249.

Anthony, T., Raj, K. C., Rajendran, A., and Gunasekaran, P. (2003). “High molecular weight cellulase-free xylanase from alkali-tolerant Aspergillus fumigatus AR1,” Enzyme Microbial. Technol. 32(6), 647-654.

Antoine, A. A., Jacqueline, D., and Thonart, P. (2010). “Xylanase production by Penicillium canescens on soy oil cake in solid-state fermentation,” Appl. Biochem. Biotechnol. 160(1), 50-62.

Anwar, Z., Gulfraz, M., and Irshad, M. (2014). “Agro-industrial lignocellulosic biomass a key to unlock the future bio-energy: A brief review,” J. Rad. Res. Appl. Sci. 7(2), 163-173.

Archana, A., and Satyanarayana, T. (1997). “Xylanase production by thermophilic Bacillus licheniformis A99 in solid-state fermentation,” Enzyme Microb. Technol. 21(1), 12-17.

Ashour, A., Amer, M., Marzouk, A., Shimizu, K., Kondo, R., and El-Sharkawy, S. (2013). “Corn cobs as a potential source of functional chemicals,” Molecules 18(11), 13823-13830.

Assamoi, A. A., Destain, J., Delvigne, F., Lognay, G., and Thonart, P. (2008). “Solid-state fermentation of xylanase from Penicillium canescens 10-10c in a multi-layer-packed bed reactor,” Appl. Biochem. Biotechnol. 145, 87-97.

Ayyachamy, M., and Vatsala, T. M. (2007). “Production and partial characterization of cellulase free xylanase by Bacillus subtilis C01 using agro-residues and its application in bio-bleaching of non-woody plant pulps,” Lett. Appl. Microbiol. 45(5), 467-472.

Bajaj, B. K., Sharma, M., and Sharma, S. (2011). “Alkalistable endo--1,4-xylanase production from a newly isolated alkalitolerant Penicillium sp. SS1 using agro-residues,” Biotech 1, 83-90.

Bakri, Y., Jawhar, M., and Arabi, M. I. E. (2013). “Xylanase production by Fusarium solani in solid state fermentation,” Res. Biotechnol. 4(1), 31-37.

Bathia, L., Johri, S., and Ahmad, R. (2012). “An economic and ecological perspective of ethanol production from renewable agro waste: A review,” ABM Express 2(1), 2-19.

Battan, B., Sharma, J., Dhiman, S. S., and Kuhad, R. C. (2007). “Enhanced production of cellulase-free thermostable xylanase by Bacillus pumilus ash and its potential application in paper industry,” Enzyme Microbial. Technol. 41(6-7), 733-739.

Bedford, M. R., and Cowieson, A. J. (2012). “Exogenous enzymes and their effects on intestinal microbiology,” Anim. Feed Sci Technol. 173(1-2), 76-85.

Benz, J. P., Chau, B. H., Zheng, D., Bauer, S., Glass, N. L., and Somerville, C. R. (2014). “A comparative systems analysis of polysaccharide-elicited responses in Neurospora crassa reveals carbon source-specific cellular adaptations,” Mol. Microbiol. 91(2), 275-299.

Betini, J. H. A., Michelin, M., Peixoto-Nogueira, S. C., Jorge, J. A., Terenzi, H. F., and Polizeli, M. L. T. M. (2009). “Xylanases from Aspergillus niger, Aspergillus niveus and Aspergillus ochraceus produced under solid-state fermentation and their application in cellulose pulp bleaching,” Bioprocess Biosyst. Eng. 32(6), 819-824.

Bhargav, S., Panda, B. P., Ali, M., and Javed, S. (2008). “Solid-state fermentation: An overview,” Chem. Biochem. Eng. 22(1), 49-70.

Bhatt, N., Dharmesh, A., and Priti, T. (2012). “Production of xylanase by Aspergillus flavus FPDN1 on pearl millet bran: Optimization of culture conditions and application in bioethanol production,” Int. J. Res. Chem. Environ. 2(3), 204-210.

Binod, P., Sindhu, R., Singhania, R. R., Vikram, S., Devi, L., Nagalakshmi, S., Kurien, N, Sukumaran, R. K., and Pandey, A. (2010). “Bioethanol production from rice straw: An overview,” Bioresour. Technol. 101(13), 4767-4774.

Birijlall, N., Manimaran, A., Kumar, K. S., Permaul, K., and Singh, S. (2011). “High level expression of a recombinant xylanase by Pichia pastoris NC38 in a 5 L fermenter and its efficiency in biobleaching of bagasse pulp,” Bioresour. Technol. 102(20), 9723-9729.

Biswas, R., Sahai, V., Mishra, S., and Bisaria, V. S. (2010). “Bioprocess strategies for enhanced production of xylanase by Melanocarpus albomyces IITD3A on agro-residual extract,” J. Biosci. Bioeng. 110(6), 702-708.

Bobeck, E. A., Nachtrieb, N. A., Batal, A. B., and Persia, M. E. (2014). “Effects of xylanase supplementation of corn-soybean meal-dried distiller’s grain diets on performance, metabolizable energy, and body composition when fed to first-cycle laying hens,” J. Appl. Poult. Res. 23(2), 174-180.

Botella, C., Diaz, A., Ory, I., Webb, C., and Blandino, A. (2007). “Xylanase and pectinase production by Aspergillus awamori on grape pomace in solid state fermentation,” Process Biochem. 42(1), 98-101.

Butt, M. S., Tahir-Nadeem, M., Ahmad, Z., and Sultan, M. T. (2008). “Xylanases and their application in baking industry,” Food Technol. Biotechnol. 46(1), 22-31.

Chandel, A. K., Silva, S. S., Carvalho, W., and Singh, O. V. (2012). “Sugarcane bagasse and leaves: Foreseeable biomass of biofuel and bio-products,” J. Chem. Technol. Biotechnol. 87(1), 11-20.

Chapla, D., Divecha, J., Madamwar, D., and Shah, A. (2010). “Utilization of agro-industrial waste for xylanase production by Aspergillus foetidus MTCC 4898 under solid state fermentation and its application in saccharification,” Biochem. Eng. J. 49(3), 361-369.

Chapla, D., Patel, H., Madamwar, D., and Shah, A. (2012). “Assessment of a thermostable xylanase from Paenibacillus sp. ASCD2 for application in prebleaching of eucalyptus kraft pulp,” Waste Biomass Valor 3(3), 269-274.

Childs, C. E., Röytiö, H., Alhoniemi, E., Fekete, A. A., Forssten, D. S., Hudjec, N., Lim, Y. N. Steger, C. J., Yagoob, P., Tuohy, K. M., Rastall, R. A., Ouwehand, A. C., and Gibson, G. R. (2014). “Xylo-oligosaccharides alone or in symbiotic combination with Bifidobacterium animalis subsp. lactis induce bifidogenesis and modulate markers of immune function in healthy adults: A double-blind, placebo-controlled, randomized, factorial cross-over study,” B. J. Nutr. 111(11), 1945-1956.

Chinn, M. S., Nokes, S. E., and Strobel, H. J. (2007). “Influence of process conditions on end product formation from Clostridium thermocellum 27405 in solid substrate cultivation on paper pulp sludge,” Bioresour. Technol. 98(11), 2184-2193.

Collins, T., Gerday, C., and Feller, G. (2005). “Xylanases, xylanase families and extremophilic xylanases,” FEMS Microbiol. Rev. 29(1), 3-13.

Coradetti, S. T., Craig, J. P., Xiong, Y., Shock, T., Tian, C., and Glass, N. L. (2012). “Conserved and essential transcription factors for cellulase gene expression in ascomycete fungi,” Proc. Natl. Acad. Sci. U.S.A. 109(19), 7397-7402.

Courtin C. M., and Delcour, J. A. (2001). “Relative activity of endoxylanases towards water-extractable and water-unextractable arabinoxylan,” J. Cer. Sci. 33(3), 301-312.

Cui, F., and Zhao, L. (2012). “Optimization of xylanase production from Penicillium sp.WX-Z1 by a two-step statistical strategy: Plackett-Burman and Box-Behnken experimental design,” Int. J. Mol. Sci. 13(8), 10630-10646.

Dai, X.-J., Liu, M.-Q., Jin, H.-X., and Jing, M.-Y. (2011). “Optimization of solid-state fermentation of Aspergillus niger JL-15 for xylanase production and xylooligosaccharides preparation,” Czech. J. Food Sci. 29(5), 557-567.

Damaso, M. C. T., Almeida, M. S., Kurtenbach, E., Martins, O. B., Pereira, J. R. N., Andrade, C. M. M. C., and Albano, R. M. (2003). “Optimized expression of a thermostable xylanase from Thermomyces lanuginosus in Pichia pastoris,” Appl. Environ. Microbiol. 69(10), 6064-6072.

Das, A., Paul, T., Halder, S. K., Jana, A., Maity, C., Mohapatra, P. K. D., Pati, B. R., and Mondal, K. C. (2013). “Production of cellulolytic enzymes by Aspergillus fumigatus ABK9 in wheat bran-rice straw mixed substrate and use of cocktail enzymes for deinking of waste office paper pulp,” Bioresour. Technol. 128, 290-296.

Dashtban, M., Schraft, H., and Qin, W. (2009). “Fungal bioconversion of lignocellulosic residues; Opportunities & perspectives,” Int. J. Biol. Sci. 5(6), 578-595.

Dawson, L., and Boopathy, R. (2007). “Use of post-harvest sugarcane residue for ethanol production,” Bioresour. Technol. 98(9), 1695-1699.

Decelle, B., Tsang, A., and Storms, R. K. (2004). “Cloning, functional expression and characterization of three Phanerochaete chyrsosporium endo-1,4-β-xylanases,” Curr. Genet. 46(3), 166-175.

de Faria, F. P., Teo, V. S. J., Bergquist, P. L., Azevedo, M. O., and Nevalainen, K. M. (2002). “Expression and processing of major xylanase (XYN2) from the thermophilic fungus Humicola grisea var. thermoidea in Trichoderma reesei,” Lett. Appl. Microbiol. 34(2), 119-123.

Dehia, B. S., Vetal, M. D., Rathod, V. K., and Levent, C. (2013). “Xylanase and laccase aided bio-bleaching of wheat straw pulp,” Can. J. Chem. Eng. 92(1), 131-138.

Delmas, S., Pullan, S. T., Gaddipati, S., Kokolski, M., Malla, S., Blythe, M. J., Ibbett, R., Campbell, M., Liddell, S., Aboobaker, A., Tucker, G. A., and Archer, D. B. (2012). “Uncovering the genome-wide transcriptional responses of the filamentous fungus Aspergillus niger to lignocellulose using RNA sequencing,” PLoS Genet. 8(8), e1002875.

Demain, A. L., and Vaishnav, P. (2009) “Production of recombinant proteins by microbes and higher organisms,” Biotechnol. Adv. 27(3), 297-306.

Deshpande, S. K., Bhotmange, M. G., Chakrabarti, T., and Shastri, P. N. (2008). “Production of cellulase and xylanase by Trichoderma reesei (QM9414 mutant), Aspergillus niger and mixed culture by solid state fermentation (SSF) of water hyacinth (Eichhornia crassipes),” Indian J. Chem. Technol. 15, 449-456.

de Vries, R. P., Visser, J., and de Graaff, L. H. (1999). “CreA modulates the XlnR-induced expression on xylose of Aspergillus niger genes involved in xylan degradation,” Res. Microbiol. 150(4), 281-285.

Dhillon, G. S., Oberoi, H. S, Kaur, S., Bansal, S., and Brar, S. K. (2011). “Value-addition of agricultural wastes for augmented cellulase and xylanase production through solid-state tray fermentation employing mixed-culture of fungi,” Ind. Crops Prod. 34(1), 1160-1167.

Dhiman, S. S., Sharma, J., and Battan, B. (2008). “Industrial application and future prospect of microbial xylanases: A review,” BioResources 3(4), 1377-1402.

Diao, L., Yingmiao, L, Qian, F., Yang, J., Yiang, Y., and Yang, S. (2013). “Construction of fast xylose-fermenting yeast based on industrial ethanol-producing diploid Saccharomyces cerevisiae by rational design and adaptive evolution,” BMC Biotecnol. 13, article 110.

Díaz, A. B., de Ory, I., Caro, I., and Blandino, A. (2012). “Enhance hydrolytic enzymes production by Aspergillus awamori on supplemented grape pomace,” Food Bioprod. Process 90(1), 72-78.

Dogaris, I., Vakontios, G., Kalogeris, E., Mamma, D., and Kekos, D. (2009). “Induction of cellulases and hemicellulases from Neurospora crassa under solid-state cultivation for bioconversion of sorghum bagasse into ethanol,” Ind. Crops Prod. 29(2-3), 404-411.

Driss, D., Bhiri, F., Ghorbel, R., and Chaabouni, S. E. (2012). “Cloning and constitutive expression of His-tagged xylanase GH 11 from Penicillium occitanis Pol6 in Pichia pastorisX33: Purification and characterization,” Protein Expr. Purif. 83(1), 8-14.

Elisashvili, V. V., Kachlishvili, E., Tsiklauri, N., Metreveli, E., Khardziani, T., and Agathos, S. N. (2009). “Lignocellulose-degrading enzyme production by white-rot Basidiomycetes isolated from the forests of Georgia,” World J. Microbiol. Biotechnol. 25(2), 331-339.

Ellouze, O., Fattouch, M., Mestiri, F., Aniba M. R., and Marzouki, M. N. (2008). “Optimization of extracellular xylanase production by Sclerotinia sclerotiorum S2 using factorial design,” Indian J. Biochem. Biophys. 45(6), 404-409.

El-Tayeb, T. S., Abdelhafez, A. A., Ali, S. H., and Ramandan, E. M. (2012). “Effect of acid hydrolysis and fungal biotreatment on agro-industrial wastes for obtainment of free sugars for bioethanol production,” Braz. J. Microbiol. 43(4), 1523-1535.

Facchini, F. D., Vici, A. C., Reis, V. R., Jorge, J. A., Terenzi, H. F., Reis, R. A., and Polizeli, M. L. T. M. (2011). “Production of fibrolytic enzymes by Aspergillus japonicus C03 using agro-industrial residues with potential application as additives in animal feed,” Bioprocess Biosyst. Eng. 34(3), 347-355.

Fan, G., Katrolia, P., Jia, H., Yang, S., Yan, Q., and Jiang, Z. (2012). “High-level expression of a xylanase gene from the thermophilic fungus Paecilomyces thermophila in Pichia pastoris,” Biotechnol. Lett. 34(11), 2043-2048.

Fang, T. J., Liao, B. C., and Lee, S. C. (2010). “Enhanced production of xylanase by Aspergillus carneus M34 in solid-state fermentation with agricultural waste using statistical approach,” New Biotechnol. 27(1), 25-32.

Fortkamp, D., and Knob, A. (2014). “High xylanase production by Trichoderma viride using pineapple peel as substrate and its application in pulp biobleaching,” Afr. J. Biotech. 13(22), 2248-2259.

Galiotou-Panayotou, M., Rodis, P., and Kapantai, M. (1993). “Enhanced polygalacturonase production by Aspergillus niger NRRL-364 grown on supplemented citrus pectin,” Lett. Apl. Microbiol. 17(4), 145-148.

Gattinger, L. D., Duvnjak, Z., and Khan, A. W. (1990). “The use of canola meal as a substrate for xylanase production by Trichoderma reesei,” Appl. Microbiol. Biotechnol. 33(1), 21-25.

Gawande, P. V., and Kamat, M. Y. (1999). “Production of Aspergillus xylanase by lignocellulosic waste fermentation and its application,” J. Appl. Microbiol. 87(4), 511-519.

Ghatora, S. K., Chadha, B. S., Badhan, A. K., Saini, H. S., and Bhat, M. K. (2007). “Identification and characterization of diverse xylanases from thermophilic and thermotolerant fungi,” BioResources 1(1), 18-33.

Ghosh, S., and Sudha, M. L. (2012). “A review on polyols: News frontiers for health-based bakery products,” Int. J. Food Sci. Nutr. 63(3), 372-379.

Ghoshal, G., Banerjee, U. C., Chisti, Y., and Shivharea, U. S. (2012). “Optimization of xylanase production from Penicillium citrinum in solid state fermentation,” Chem. Biochem. Eng. Q. 26(1), 61-69.

Ghotora, S. K., Chada, B. S., Badhan, A. K., Saini, H. S., and Bhat, M. K. (2006). “Identification and characterisation of diverse xylanases from thermophilic and thermotolerant fungi,” BioResources 1(1), 18-33.

Gilleran, C. T., Hernon, A. T., Murray, P. G., and Tuohy, M. G. (2010). “Induction of enzyme cooktails by low cost carbon sources for production of monosaccharide-rich syrups from plant materials,” BioResources 5(2), 634-649.

Glass, N. L., Schmoll, M., Cate, J. H. D., and Coradetti, S. (2013). “Plant cell wall deconstruction by Ascomycete fungi,” Ann. Rev. Microbiol. 67(1), 477-498.

Goswami, G. K., and Pathak, R. R. (2013). “Microbial xylanases and their biomedical applications: A review,” Int. J. Basic Clin. Pharmacol. 2(3), 237-246.

Gottschalk, L. M. F., Paredes, R. S., Teixeira, S. S., Silva, A. S. A., and Bon, E. P. S. (2013). “Efficient production of lignocellulolytic enzymes xylanase, β-xylosidase, ferulic acid esterase and β-glucosidase by the mutant strain Aspergillus awamori 2B.361 U2/1,” Braz. J. Microbiol. 44(2), 569-576.

Goyal, M., Kalra, K. L., Sarren, V. K., and Soni, G. (2008). “Xylanase production with xylan rich lignocellulosic wastes by a local soil isolate of Trichoderma viride,” Braz. J. Microbiol.39(3), 535-541.

Graminha, E. B. N., Gonçalvez, A. Z. L., Pirota, R. D. P. B., Balsalobre, M. A. A., da Silva, R., and Gomes, E. (2008). “Enzyme production by solid-state fermentation: Application to animal nutrition,” Anim. Feed Sci. Technol. 144(1-2), 1-22.

Guimaraes, N. C. A., Sorgatto, M., Peixoto-Nogueira, S. C., Betini, J. H. A., Zanoelo, F. F., Marques, M. R., Polizeli, M. L. T. M., and Giannesi, G. C. (2013). “Xylanase production from Aspergillus japonicus var aculeatus: Production using agroindustrial residues and biobleaching effect on pulp,” J. Biocatal. Biotransformation 2(1), 1-6.

Guo, S., Liu, D., Zhao, Z., Li, C., Guo, Y. (2014). “Xylanase supplementation of a wheat-based diet improved nutrient digestion and mRNA expression of intestinal nutrient transporters in broiler chickens infected with Clostridium perfringens,” Poult Sci. 93(1), 94-103.

Gupta, G., Sahai, V., and Gupta, R. K. (2013). “Optimization of xylanase production from Melanocarpus albomyces using wheat straw extract and its scale up in stirred tank bioreactor,” Indian J. Chem. Tech. 20(4), 282-289.

Gupta, U., and Kar, R. (2009). “Xylanase production by a thermo-tolerant Bacillus species under solid-state and submerged fermentation,” Braz. Arch. Biol. Technol. 52(6), 1363-1371.

Gutierrez-Correa, M., and Tengerdy, R. P. (1998). “Xylanase production by fungal mixed culture solid substrate fermentation on sugar cane bagasse,” Biotechnol. Lett. 20(1), 45-47.

Haltrich, D., Nidetzky, B., Kulbe, K. D., Steiner, W., and Zupancic, S. (1996). “Production of fungal xylanases,” Bioresour. Tech. 58, 137-161.

Harris, A. D., and Ramalingam, C. (2010). “Xylanases and its application in food Industry: A review,” J Exper. Sci. 1(7), 1-11.

Hasper, A, A., Dekker, E., van Mil, M., van de Vondervoort, P. J. I., and de Graaff, L. H. (2002). “EglC, a new endoglucanase from Aspergillus niger with major activity towards xyloglucan,” Appl. Environ. Microbiol. 68(4), 1556-1560.

He, J., Yu, B., Zhang, K., Ding, X., and Chen, D. (2009). “Expression of endo-1,4-beta xylanase from Trichoderma reesei in Pichia pastoris and functional characterization of the produced enzyme,” BMC Biotecnol. 9, article 56.

Hessing, J. G., Rotterdam, C. V., Verbake, J. M., Roza, M., Maat, J., Gorcom, R. F. V., and Hondel, C. A. V. D. (1994). “Isolation and characterization of a 1,4-β-endoxylanase gene of A. awamori,” Curr. Genet. 26(3), 228-232.

Hinz, S. W. A., Pouvreau, L., Joosten, R., Bartels, J., Jonathan, M. C., Wery, J., and Schols, H. (2009). “Hemicellulase production in Chrysosporium lucknowense C1,” J. Cereal Sci. 50(3), 318-323.

Hölker, U., and Lenz, J. (2005). “Solid-state fermentation – Are there any biotechnological advantages?,” Curr. Opin. Microbiol. 8(3), 301-306.

Howard, R. L., Abotsi, E., Jansen van Rensburg, E. L., and Howard, S. (2003). “Lignocellulose biotechnology: Issues of bioconversion and enzyme production,” African J. Biotechnol. 2(12), 602-619.

Huitron, C., Perez, R., Sanchez, A. E., Lappe, P., and Rocha Zavaleta, L. (2008). “Agricultural waste from the tequila industry as substrate for the production of commercially important enzymes,” J. Environ. Biol. 29(1), 37-41.

Isil, S., and Nilufer, A. (2005). “Investigation of factors affecting xylanase activity from Trichoderma harzianum 1073 D3,” Braz. Arch. Biol. Biotechnol. 48(2), 187-193.

Jain, A., Morlok, C. K., and Henson, J. M. (2013). “Comparison of solid-state and submerged-state fermentation for the bioprocessing of switchgrass to ethanol and acetate by Clostridium phytofermentans,” Appl. Microbiol. Biotechnol. 97(2), 905-917.

Jin, N., Ma, S., Liu, Y., Yi, X., He, R., Xu, H., Qiao, D. R., and Cao, Y. (2012). “Thermophilic xylanase production by Aspergillus niger in solid state fermentation using wheat straw and corn cob,” African J. Microbiol. Res. 6(10), 2387-2390.

Joshi, C., and Khare, S. K. (2012). “Induction of xylanase in thermophilic fungi Scytalidium thermophilum and Sporotrichum thermophile,” Braz. Arch. Biol. Biotechnol. 55(1), 21-27.

Juturu, V., and Wu, J. C. (2011). “Microbial xylanases: Engineering, production and industrial applications,” Biotechnol. Adv. 30(6), 1218-1227.

Kalogeris, E.; Christakopoulos, P., Kekos, D., and Macris, B. J. (1998). “Studies on the solid-state production of thermostable endoxylanases from Thermoascus aurantiacus: Characterization of two isozymes,” J. Biotechnol. 60(3), 155-163.

Kamra, P., and Satyanarayana, T. (2004). “Xylanase production by the thermophilic mold Humicola lanuginosa in solid state fermentation,” Appl. Biochem. Biotechnol. 119(2), 145-158.

Kang, S. W., Park, Y. S., Lee, J. S., Hong, S. I., and Kim, S. W. (2004). “Production of cellulases and hemicellulases by Aspergillus niger KK2 from lignocellulosic biomass,” Bioresour. Technol. 91(2), 153-156.

Kanmani, P., Karuppasamy, P., Pothiraj, C., and Arul, V. (2009). “Studies on lignocellulose biodegradation of coir waste in solid state fermentation using Phanerocheate chrysosporiumand Rhizopus stolonifer,” African J. Biotechnol. 8(24), 6880-6887.

Kanna, M., Yano, S., and Sawayama, S. (2011). “Enhancement of -xylosidase productivity in cellulase producing fungus Acremonium cellulolyticus,” AMB Express 30(1), 1-13.

Khanahmadi, M., Mitchell, D. A., Beheshti, M., Roostaazad, R., and Sanchez, R. L. (2006). “Continuous solid-state fermentation as affected by substrate flow pattern,” Chem. Eng. Sci. 61(8), 2675-2687.

Khandeparkar, R., and Bhosle, N. B. (2006). “Isolation, purification, and characterization of the xylanase produced by Arthrobacter sp. MTCC 5214 when grown in solid-state fermentation,” Enzyme Microb. Technol. 39(4), 732-742.

Khandeparker, R., and Numan, M. T. (2008). “Bifunctional xylanases and their potential use in biotechnology,” J. Ind. Microbiol. Biotechnol. 35(7), 635-644.

Khucharoenphaisan, K., Tokuyama, S., Ratanakhanokchai, K., and Kitpreechavanich, V. (2010). “Induction and repression of β-xylanase ofThermomyces lanuginosus TISTR 3465,” Pak. J Biol. Sci. 13(5), 209-215.

Kim, S., and Dale, B. E. (2004). “Global potential bioethanol production from wasted crops and crop residues,” Biomass Bioenerg. 26(4), 361-375.

Kimura, T., Suzuki, H., Furuhashi, H., Aburatani, T., Morimoto, K., Sakka, K., and Ohmiya K. (2002). “Molecular cloning, characterization and expression analysis of the xynF3 gene from Aspergillus oryzae,” Biosci. Biotechnol. Biochem. 66(2), 285-292.

Kitamoto, N., Yoshino, S., Ohmiya, K., and Tsukagoshi, N. (1999). “Purification and characterization of the overexpressed Aspergillus oryzae xylanase, xynF1,” Biosci. Biotechnol. Biochem. 63(10), 1791-1794.

Knob, A., Beitel, S. M., Fortkamp, D., Terrasan, C. R., and de Almeida, A. F. (2013). “Production, purification, and characterization of a major Penicillium glabrum xylanase using Brewer’s spent grain as substrate,” Biomed Res. Int. 2013(2013), 1-8.

Knob, A., Terrasan, C. R. F., and Carmona, E. C. (2010). “-Xylosidases from filamentous fungi: An overview,” World J. Microbiol. Biotechnol. 26(3), 389-407.

Krishna, C. (2005). “Solid-state fermentation systems: An overview,” Crit. Rev. Biotechnol. 25(1-2), 1-30.

Kulkarni, P., and Gupta, N. (2013). “Screening and evaluation of soil fungal isolates for xylanase production,” Recent Res. Sci. Technol. 5(2), 33-36.

Kumar, A., and Kanwar, S. S. (2012). “Lipase production in solid state fermentation (SSF): recent developments and biotechnological applications,” Dyn. Biochem. Process Biotechnol. Mol. Biol. 6(1), 13-27.

Kumar, D., Yaday, K. K., Singh, M., and Garg, M. (2012). “Biochemical utilization of agro-industrial lignocelluloses rich waste for cellulase production,” Res. J. Agri. Sci. 44(2), 184-190.

Kumar, G. P., Pushpa, A., and Prabha, H. (2012). “A review on xylooligosscharadies,” Int. Res. J. Pharm. 3(8), 71-74.

Kumar, K. S., Manimaran, A., Permaul, K., and Singh, S. (2009). “Production of beta-xylanases by a Thermomyces lanuginosus MC 134 mutant on corn cobs and its application in biobleaching of bagasse pulp,” J. Biosci. Bioeng. 107(5), 494-498.

Kumar, R., Singh, S., and Singh, O. V. (2008). “Bioconversion of lignocellulosic biomass: Biochemical and molecular perspectives,” J. Ind. Microbiol. Biotechnol. 35(5), 377-391.

Kuyper, M., Hartog, M. M. P., Toirkens, M. J., Almering, M. J. H., Winkler, A. A., van Dijken, J. P., Pronk, J. T. (2005). “Metabolic engineering of a xylose-isomerase-expressing Saccharomyces cerevisiae strain for rapid anaerobic xylose fermentation,” FEMS Yeast Res. 5(4-5), 399-409.

Lachke, A. (2006). “Xylitol: A sweetener with special qualities,” Resonance 11(9), 90-92.

La Grange, D. C., Claeyssens, I. M., Pretorius, I. S., and van Zyl, W. H. (2001). “Degradation of xylan to D-xylose by recombinant Saccharomyces cerevisie co-expressing the Aspergillus niger -xylosidase (xlnD) and the Trichoderma reesei xylanase II (xyn2) genes,” Appl. Environ. Microbiol. 67(12), 5512-5519.

Lakshmi, G. S., Rao, C. S., Rao, R. S., Hobbs, P. J., and Prakasham, R. S. (2009). “Enhanced production of xylanase by a newly isolated Aspergillus terreus under solid state fermentation using palm industrial waste: A statistical optimization,” Biochem. Eng. J. 48(1), 51-57.

Lakshmi, G. S., Lakshmi, B. P., and Prakasham, R. S. (2011). “Sustainable bioprocess evaluation for xylanase production by isolated Aspergillus terreus and Aspergillus fumigatus under solid-state fermentation using oil palm empty fruit bunch fiber,” Curr. Trends Biotechnol. Pharm. 5(4), 1434-1444.

Laxmi, G. S., Sathish, T., Rao, C. H. S., Brahmaiah, P., Hymavathi, M., and Prakasham, R. S. (2008). “Palm fiber as novel substrate for enhanced xylanase production by isolated Aspergillus sp. RSP-6,” Curr. Trends Biotechnol. Pharm. 2(3), 447-455.

Le, Y., and Wang, H. (2014). “High-level soluble expression of a thermostable xylanase from thermophilic fungus Thermomyces lanuginosus in Escherichia coli via fusion with OsmY protein,” Protein Expr. Purif. 99, 1-5.

Le, Y., Peng, J., Wu, H., Sun, J., and Shao, W. (2009). “An approach to the production of soluble protein from a fungal gene encoding an aggregation-prone xylanase in Escherichia coli,” Plos One 6(4), e18489.

Levasseur, A., Asther, M., and Record, E. (2005). “Overproduction and characterization of xylanase B of Aspergillus niger,” Can. J. Microbiol. 51(2), 177-183.

Li, J., Wang, J., Wang, S., Xing, M., Yu, S., and Liu, G. (2012). “Achieving efficient protein expression in Trichoderma reesei by using strong constitutive promoters,” Microb. Cell Fact. 11, article 84.

Li, Y., Lin, J., Meng, D., Lu, J., Gu, G., and Mao, Z. (2006). “Effect of pH, cultivation time and substrate concentration on the endoxylanase production by Aspergillus awamori ZH-26 under submerged fermentation using central composite rotary design,” Food Technol. Biotechnol. 44(4), 473-477.

Liang, M., Damiani, A., He, Q. P., and Wang, J. (2013). “Elucidating xylose metabolism of Scheffersomyces stipitis for lignocellulosic ethanol production,” ACS Sustain. Chem. Eng. 2(1), 38-48.

Liao, H., Xu, C., Tan, S., Wei, Z., Ling, N., Yu, G., Raza, W., Zhang, R., Shen, Q., and Xu, Y. (2012). “Production and characterization of acidophilic xylanolytic enzymes from Penicillium oxalicum GZ-2,” Bioresour. Technol. 123, 117-124.

Lim, J. S., Manan, Z. A., Alwi, S. R. W., and Hashim, J. (2012). “A review on utilization of biomass from rice industry as a source of renewable energy,” Renew. Sustain. Energ. Rev. 16(5), 3084-3094.

Limayema, A., and Ricke, S. C. (2012). “Lignocellulosic biomass for bioethanol production: current perspectives, potential issues and future prospects,” Progress Energ. Comb. Sci. 38(4), 449-467.

Lin, S., Kangsen, M., and Tan, B. (2007). “Effect of exogenous enzyme supplementation in diets on growth and feed utilization in tilapia, Oreochromis niloticus x O. aureus,” Aquacult. Res. 8(15), 1645-1653.

Lio, J., and Wang, T. (2012). “Solid-state fermentation of soybean and corn processing coproducts for potential feed improvement,” J. Agric. Food Chem. 60(31), 7702-7709.

Liu, C., Sun, Z. T., Du, J. H., and Wang, J. (2008). “Response surface optimization of fermentation conditions for producing xylanase by Aspergillus niger SL-05,” J. Ind. Microbiol. Biotechnol. 35(7), 703-711.

Maalej, I., Belhaj, I., and Belghith, H. (2009). “Highly thermostable xylanase of the thermophilic fungus Talaromyces thermophilus: Purification and characterization,” Appl. Biochem. Biotechnol. 158(1), 200-212.

Mach-Aigner, A. R., Gudynaite-Savitch, L., and Mach, R. L. (2011). “l-Arabitol is the actual inducer of xylanase expression in Hypocrea jecorina (Trichoderma reesei),” Appl. Environ. Microbiol. 77(17), 5988-5994.

Mach-Aigner, A. R., Pucher, M. E., and Mach, R. L. (2010). “D-Xylose as a repressor or inducer of xylanase expression in Hypocrea jecorina (Trichoderma reesei),” Appl. Envirom. Microbiol. 76(6), 1770-1776.

Mandal, A., Kar, S., Das Mahapatra, P. K., Maity, C., Pati, B. R., and Mondal, K. C. (2012). “Regulation of xylanase biosynthesis in Bacillus cereus BSA1,” Appl. Biochem. Biotechnol. 167(5), 1052-1060.

Manimaran, A., Kumar, K. S., Permaul, K., and Singh, S. (2009). “Hyper production of cellulase-free xylanase by Thermomyces lanuginosus SSBP on bagasse pulp and its application in biobleaching,” Appl. Microbiol. Biotechnol. 81(5), 887-893.

Martens-Uzunova, E. S., and Schaap, P. J. (2009). “Assessment of the pectin degrading enzyme network of Aspergillus niger by functional genomics,” Fungal Genet. Biol. 46(1), S170-S179.

Martiniano, S. E., Philippini, R. R., Chandel, A. K., Rosa, C. A., and Silva, S. S. (2014). “Evaluation of rice bran extract as a nitrogen source for improved hemicellulosic ethanol production by new xylose fermenting yeasts, isolated from Brazilian forests,” Sugar Tech. 16(1), 1-8.

Martins, D. A., Prado, H. F. A., Leite, R. S. R., Ferreira, H., Moretti, M. S., Silva, R., and Gomes, E. (2011). “Agro-industrial wastes as substrates for microbial enzymes production and source of sugar for bioethanol production,” in: Integrated Waste Management, S. Kulmar (ed.), InTech, Shangai, pp. 319-360.

Mazzaferro, L. S., Cuña, M. M., and Breccia, J. D. (2011). “Production of xylo-oligosaccharides by chemo-enzimatic treatment of agricultural by-products,” BioResources 6(4), 5050-5061.

Megawati, Sediawan, W. B., Sulistyo, H., and Hidayat, M. (2011). “Kinetics of sequential reaction of hydrolysis and sugar degradation of rice husk in ethanol production: Effect of catalyst concentration,” Biores. Technol. 102(2), 2062-2067.

Michelin, M., Polizeli, M. L. T. M., Ruzene, D. S., Silva, D. P., Vicente, A. A., Jorge, J. A., Terenzi, H. F., and Teixeira, J. A. (2012). “Xylanase and β-xylosidase production by Aspergillus ochraceus: New perspectives for the application of wheat straw autohydrolysis liquor,” Appl. Biochem. Biotechnol. 166(2), 336-347.

Milagres, A. M. F., Santos, E., Piovan, T., and Roberto, I. C. (2004). “Production of xylanase by Thermoascus aurantiacus from sugar cane bagasse in an aerated growth fermentor,” Process Biochem. 39(11), 1387-1391.

Miyazaki, K., Hirase, T., Kojima, Y., and Flint, H. J. (2005). “Medium- to large-sized xylo-oligosaccharides are responsible for xylanase induction in Prevotella bryantii B14,” Microbiology 151(12), 4121-4125.

Mohamed, S. A., Al-Malki, A. L., Khan, J. A., Kabli, S. A., and Al-Garni, S. M. (2013). “Solid state production of polygalacturonase and xylanase by Trichoderma species using cantaloupe and watermelon rinds,” J. Microbiol. 51(5), 605-611.

Monte, J. R., Carvalho, W., and Milagres, A. M. F. (2010). “Use of a mixture of thermophilic enzymes produced by the fungus Thermoascus aurantiacus to enhance the enzymatic hydrolysis of the sugarcane bagasse cellulose,” American J. Agri. Biol. Sci. 5(4), 468-476.

Moreira, L. R. S., Ferreira, G. V., Santos, S. S. T., Ribeiro, A. P. S., Siqueira, F. G., and Filho, E .X. F. (2012). “The hydrolysis of agro-industrial residues by holocellulose-degrading enzymes,” Braz. J. Microbiol. 43(2), 498-505.

Moretti, M. M. S., Bocchini-Martins, D. A., Silva, R., Rodrigues, A., Sette, L. D., and Gomes, E. (2012). “Selection of thermophilic and thermotolerant fungi for the production of cellulases and xylanases under solid-state fermentation,” Braz. J. Microbiol. 43(3), 1062-1071.

Motta, F. L., Andrade, C. C. P., and Santana, M. H. A. (2013). “A review of xylanase production by the fermentation of xylan: Classification, characterization and applications,” in: Sustainable Degradation of Lignocellulosic Biomass – Techniques, Application and Commercialization,A. K. Chandel and S. S. da Silva (eds.), InTech, Shangai, pp. 251-275.

Moure, A., Gullón, P., Domínguez, H., and Parajó, J. C. (2006). “Advances in the manufacture, purification and applications of xylo-oligosaccharides as food additives and nutraceuticals,” Process Biochem. 4(9), 1913-1923.

Murthy, P. S., and Naidu, M. M. (2012). “Production and application of xylanase from Penicillium sp. utilizing coffee by-products,” Food Bioprocess Technol. 5(2), 657-664.

Mussatto, S. I., and Teixeira, J. A. (2010). “Lignocellulose as raw material in fermentation processes,” in: Current Research, Technology and Education Topics in Applied Microbiology and Microbial Biotechnology, A. Méndez-Vilas (ed.), Formatex Research Center, Badajoz, pp. 897-907.

Mussatto, S. I., Carneiro, L. M., Silva, J. P. A., Roberto, I. C., and Teixeira, J. A. (2011a). “A study on chemical constituents and sugars extraction from spent coffee grounds,” Carbohy. Polymers 83(2), 368-374.

Mussatto, S. I., Machado, E. M. S., Martins, S., and Teixeira, J. A. (2011b). “Production, composition, and application of coffee and its industrial residues,” Food Bioprocess. Technol. 4(5), 661-672.

Nabais, J. M. V., Nunes, P., Carrott, P. J. M., Carrot, M. R., Garcia, A. M., and Díez, M. A. D. (2008). “Production of activated carbons from coffee endocarp by CO2 and steam activation,” Fuel Processing Technol. 89(3), 262-268.

Nakari-Setälä, T., Kallio, J., Vehmaanperä, J., Penttilä, M., Saloheimo, K. (2009). “Genetic modification of carbon catabolite repression in Trichoderma reesei for improved protein production,” Appl. Environ. Microbiol. 75(14), 4835-4860.

Nair, S. G., and Shashidhar, S. (2008). “Fungal xylanase production under solid state and submerged fermentation conditions,” African J. Microbiol. Res. 2(4), 82-86.

Narang, S., Sahai, V., and Bisaria, V. S. (2001). “Optimization of xylanase production by Melanocarpus albomyces IIS-68 in solid state fermentation using response surface methodology,” J. Biosci. Bioeng. 91(4), 425-427.

Narasimnha, G., Sridevi, A., Buddolla, V., Chandra, M. S., and Reddy, B. R. (2006).” Nutrient effects on production of cellulolytic enzymes by Aspergillus niger,” Afr. J. Biotechnol. 5(5), 472-476.

Ncube, T., Howard, R. L., Abotsi, E. K., Van Rensburg, E. L. J., and Ncube, I. (2012). “Jatropha curcas seed cake as substrate for production of xylanase and cellulase by Aspergillus niger FGSCA733 in solid-state fermentation,” Ind. Crops Prod. 37(1), 118-123.

Neoh, B. K., Thang, Y. M., Zain, M. Z. M., and Junaidi, A. (2011). “Palm pressed fibre oil: A new opportunity for premium hardstock?,” Int. Food Res. J. 18(2), 769-773.

Neves, M. L. C, Silva, M. F., Souza-Motta, C. M., Spier, M. R., Soccol, C. R., Porto, T. S., Moreira, K. A., and Porto, A. L. F. (2011). “Lichtheimia blakesleeana as a new potencial producer of phytase and xylanase,” Molecules 16(6), 4807-4817.

Nigam, P. S., Gupta, N., and Anthwal, A. (2009). “Pre-treatment of agro-industrial residues,” in: Biotechnology for Agro-industrial Residues Utilization, P. S. Nigam, and A. Pandey (eds.), Springer, Netherlands, pp. 13-33.

Norazlina, I., Pushpahvalli, B., Ku Halim, K. H., and Norakma, M. N. (2012). “Comparable study of xylanase production from Aspergillus niger via solid state culture,” J. Chem. Chemical Eng. 6(12), 1106-1113.

Okafor, U. A., Emezue, T. N., Okochi, V. I., Onyegeme-Okerenta, B. M., and Nwodo-Chinedu, S. (2007). “Xylanase production by Penicillium chrysogenum (PCL501) fermented on cellulosic wastes,” African J. Biochem. Res. 1(4), 48-53.

Omogbenigun, F. O., Nyachoti, C. M., Slominski, B. A. (2004). “Dietary supplementation with multienzyme preparations improves nutrient utilization and growth performance in weaned pigs,” J. Anim. Sci. 82(4), 1053-1061.

Orozco, A. L., Pérez, M. I., Guevara, O., Rodríguez, J., Hernández, M., González-Vila, F. J., Polvillo, O., and Arias, M. E. J. (2008). “Biotechnological enhancement of coffee pulp residues by solid-state fermentation with Streptomyces,” J. Anal. Appl. Pyrolysis 81(2), 247-252.

Osipov, D. O., Rzhkova, A. M., Matys, V. Yu., Koshelev, A. V., Okuney, O. N., Rubtsova, E. A., Pravil’nikov, A. G., Zorov, I. N., Sinitsyna, O. A., Oveshnikov, I. N., Davidov, E. R., and Sinitsyn, A. P. (2011). “Production of biocatalysts on the basis of recombinant heterologous xylanase producer strains in the Penicillium verruculosum fungus: Their application in the hydrolysis of timber and wood processing industry wastes,” Catalysis Ind. 3(1), 34-40.

Otte, L. G., and Quax, W. J. (2005). “Direct evolution: Selecting today’s biocatalysts,” Biomol. Eng. 22(1-3), 1-9.

Pal, A., and Khanum, F. (2010). “Production and extraction optimization of xylanase from Aspergillus niger DFR-5 through solid-state-fermentation,” Bioresour. Technol. 101(19), 7563-7569.

Palacios-Orueta, A., Chuvieco, E., Parra, A., and Carmona-Moreno, C. (2005). “Biomass burning emissions: A review of models using remote-sensing data,” Environ. Monit. Assess 104(1-3), 189-209.

Palaniswamy, M., Arulanandham, T. V., and Angayarkanni, J. (2012). “Production of xylanase by litter degrading fungal species using agro-industrial wastes as substrates by solid state fermentation,” RJPBCS 3(1), 143-149.

Panagiotou, G., Kekos, D., Macris, B. J., and Christakopoulos, P. (2003). “Production of cellulolytic and xylanolytic enzymes by Fusarium oxysporum grown on corn stover in solid state fermentation,” Ind. Crops Products 18(1), 37-45.

Pandey, A., Soccol, C. R., and Mitchell, D. (2000). “New developments in solid state fermentation, I: Bioprocess and products,” Process Biochem. 35(10), 153-169.

Pandya, J. J., and Gupte, A. (2012). “Production of xylanase under solid-state fermentation by Aspergillus tubingensis JP-1 and its application,” Bioprocess Biosyst. Eng. 35(5), 769-779.

Pang, P. K., Darah, I., Poppe, L., Szakacs, G., and Ibrahim, C. O. (2006). “Xylanase production by a local isolate, Trichoderma spp. FETL c3‐2 via solid state fermentation using agricultural wastes as substrates,” Malaysian J. Microbiol. 2(1), 7‐14.

Papinutti, V. L. and Forchiassin, F. (2007). “Lignocellulolytic enzymes from Fomes fomentarius growing in solid-state fermentation,” J. Food Eng. 81(1), 54-59.

Patil, S. R., and Dayanand, A. (2006). “Exploration of regional agrowastes for the production of pectinase by Aspergillus niger,” Food Technol. Biotechnol. 44(2), 289-292.

Pérez-Rodríguez, N., Oliveira, F., Pérez-Bibbins, B., Belo, I., Agrasar, A. T., Domínguez, J. M. (2014). “Optimization of xylanase production by filamentous fungi in solid-state fermentation and scale-up to horizontal tube bioreactor,” Appl. Biochem. Biotechnol. 173(3), 803-825.

Polizeli, M. L. T. M., Rizzati, A. C. S., Monti, R., Terenzi, H. F., Jorge, J. A., and Amorin, D. S. (2005). “Xylanases from fungi: Properties and industrial applications,” Appl. Microbiol. Biotechnol. 67(5), 577-591.

Prückler, M., Siebenhandl-Ehn, S., Apprich, S., Höltinger, S., Hass, C., Schmid, E., and Kneifel, W. (2014). “Wheat bran-based biorefinery 1: Composition of wheat bran and strategies of functionalization,” LWT-Food Sci. Technol. 56(2), 211-221.

Rajoka, M. I., Huma, T., Khalid, A. M., and Latif, F. (2005). “Kinetics of enhanced substrate consumption and endo--xylanase production by a mutant derivative of Humicola lanuginosa in solid-state fermentation,” World J. Microbiol. Biotechnol. 21(6-7), 869-876.

Ramachandran, S., Singh, S. K., Larroche, C., Soccol, C. R., and Pandey, A. (2009). “Oil cakes and their biotechnological applications – A review,” Bioresour. Technol. 98(10), 2000-2009.

Rezende, M. I., Barbosa, A. M., Vasconcelos, A. F. D., and Endo, A. S. (2002). “Xylanase production by Trichoderma harzianum rifai by solid state fermentation on sugarcane bagasse,” Braz. J. Microbiol. 33(1), 67-72.

Ritter, C. E. T., Camassola, M., Zampieri, D., Silveira, M. M., and Dillon, A. J. P. (2013). “Cellulase and xylanase production by Penicillium echinulatum in submerged media containing cellulose amended with sorbitol,” Enzyme Res. 2013, 1-9.

Rodrigues, M. A. M., Pinto, P., Bezerra, R. M. F., Dias, A. A., Guedes, C. V. M., Cardoso, V. M. G., Cone, J. W., Ferreira, L. M. M., Colaco, J., and Sequeira, C. A. (2008). “Effect of enzyme extracts isolated from white-rot fungi on chemical composition and in vitro digestibility of wheat straw,” Anim. Feed Sci. Technol. 141(3-4), 326-338.

Rose, S. H., and van Zyl, W. H. (2002). “Constitutive expression of the Trichoderma reesei beta-1,4-xylanase gene (xyn2) and the beta- 1,4-endoglucanase gene (egl) in Aspergillus nigerin molasses and defined glucose media,” Appl. Microbiol. Biotechnol. 58(4), 461-468.

Roy, S., Durra, T., Sarkar, T. S., and Ghosh, S. (2013). “Novel xylanase from Simplicillium obclavatum 9604: Comparative analysis of production, purification and characterization of enzymes from submerged and solid state fermentation,” SpringerPlus 2(1), 1-10.

Ruiz, E., Cara, C., Manzanares, P., Ballesteros, M., and Castro, E. (2008). “Evaluation of steam explosion pretreatment for enzymatic hydrolysis of sunflower stalks,” Enzyme Microb. Technol. 42(2), 160-166.

Saad, M. B. W., Oliveira, L. R. M., Cândido, R. G., Quintana, G., Rocha, G. J. M., and Gonçalves, A. R. (2008). “Preliminary studies on fungal treatment of sugarcane straw for organosolv pulping,” Enzyme Microbial Technol. 43(2), 220-225.

Saha, B. C. (2003). “Hemicellulose bioconversion,” J. Ind. Microbiol. Biotechnol. 30(5), 279-291.

Sakthiselvan, P., Naveena, B., and Partha, N. (2012). “Effect of medium composition and ultrasonication on xylanase production by Trichoderma harzianum MTCC 4358 on novel substrate,” African J. Biotechnol. 11(57), 12067-12077.

Saleem, M., Aslam, F., Akhtar, M. S., Tariq, M., and Rajoka, M. I. (2012). “Characterization of thermostable and alkaline xylanase from Bacillus sp. and its bleaching impact on wheat straw pulp,” Word J. Microbiol. Biotechnol. 28(2), 513-522.

Salles, B. C., Teo, V. S. J., Gibbs, M. D., Bergquist, P. L., Filho, E. X. F., Ximenes, E. A., and Nevalainen, K. M. (2007). “Identification of two novel xylanase-encoding genes (xyn5 and xyn6) from Acrophialophra nainiana and hetrologous expression of xyn6 in Trichoderma reesei,” Biotechnol. Lett. 29(8), 1195-1201.

Sanchéz, C. (2009). “Lignocellulosic residues: Biodegradation and bioconversion by fungi,” Biotechnol. Adv. 27(2), 185-194.

Santala, O., Lehtinen, P., Nordlund, E., Suortti, T., and Poutanen, K. (2011). “Impact of water content on the solubilization of arabinoxylan during treatment of wheat bran,” J. Cer. Sci.54(2), 187-194.

Shafie, S. M., Mahlia, T. M. I., Masjuki, H. H., and Ahmad-Yazid, A. (2012). “A review on electricity generation based on biomass residue in Malaysia,” Renew Sustain. Energ. Rev 16(8), 5879-5889.

Shah, A. R., and Madamwar, D. (2005). “Xylanase production under solid-state fermentation and its characterization by an isolated strain Aspergillus foetidus in India,” World J. Microbiol. Biotechnol. 21(3), 233-243.

Shallom, D., and Shoham, Y. (2003). “Microbial hemicellulases,” Curr. Opinion Microbiol. 6(3), 219-228.

Sanghvi, G. V., Koyani, R. D., and Rajput, K. S. (2010). “Thermostable xylanase production and partial purification by solid-state fermentation using agricultural waste wheat straw,” Mycology 1(2), 106-112.

Sarkar, N., and Aikat, K. (2012). “Cellulase and xylanase production from rice straw by a locally isolated fungus Aspergillus fumigatus NITDGPKA3 under solid state fermentation – Statistical optimization by response surface methodology,” J. Technol. Innovat. Renewable Energ. 1(1), 54-62.

Sarrouh, B. F., Branco, R. F., and Silva, S. S. (2009). “Biotechnological production of xylitol: enhancement of monossacharide production by post-hydrolysis of dilute acid sugarcane hydrolysate,” Appl. Biochem. Biotechnol. 153(1-3), 163-170.

Sene, L., Arruda, P. V., and Felipe, M. G. A. (2011). “Evaluation of sorghum straw hemicellulose hydrolysate for biotechnological production of xylitol by Candida guilliermondii,” Braz. J. Microbiol. 42(3), 1141-1146.

Sethi, S., Datta, A. P., Gupta, B. L., and Gupta, S. (2013). “Optimization of cellulase production from bacteria isolated from soil,” ISRN Biotechnol. 2013(2013), 1-7.

Sharma, M., and Kumar, A. (2013). “Xylanases: An overview,” British Biotechnol. J. 3(1), 1-28.

Silva, C. A. A., Lacerda, M. P., Leite, R. S. R., and Fonseca, G. G. (2013). “Production of enzymes from Lichtheimia ramosa using Brazilian savannah fruit wastes as substrate on solid state bioprocesses,” Electron J. Biotechnol. 16(5), 1-9.

Silveira, M. L. L., Furlan, S. A., and Ninow, J. L. (2008). “Development of an alternative technology for the oyster mushroom production using liquid inoculum,” Cienc. Tecnol. Aliment. 28(4), 858-862.

Singh, S., Reddy, P., Haarhoff, J., Biely, P., Janse, B., Pillay, B., Pillay, D., and Prior, B. A. (2000). “Relatedness of Thermomyces lanuginosus stains producing a thermostable xylanase,” J. Biotechnol. 81(2-3), 119-128.

Singh, S. K., Sczakas, G., Soccol, C. R., and Pandey, A. (2008). “Production of enzymes by solid-state fermentation,” in: Current Developments in Solid State Fermentation, A. Pandey, C. R. Soccol, and C. Larroche (eds.), Springer, New York, pp. 183-204.

Singh, S., Dutt, D., and Tyagi, C. H. (2013). “Screening of xylanases from indigenously isolated white rot fungal strains for possible application in pulp biobleaching,” Open Access Sci. Rep. 2(1), 262.

Singhania, R. R., Patel, A. K., Soccol, C. R., and Pandey, A. (2009). “Recent advances in solid-state fermentation,” Biochem. Eng. J. 44(1), 13-18.

Siqueira, F. G., Siqueira, A. G., Siqueira, E. G., Carvalho, M. A., Peretti, B. M. P., Jaramilho, P. M. D., Teixeira, R. S. S., Dias, E. S., Félix, C. R., and Filho, E. X. F. (2010). “Evaluation of holocellulase production by plant-degrading fungi grown on agro-industrial residues,” Biodegradation 21(5), 815-824.

Smith, D. C., and Wood, T. M. (1991). “Xylanase production by Aspergillus awamori. Development of a medium and optimization of the fermentation parameters for the production of extracellular xylanase and β-xylosidase while maintaining low protesase production,” Biotechnol. Bioeng. 38(8), 883-890.

Soliman, H. M., Sherief, A. A. D., and El-Tanash, A. B. (2012). “Production of xylanase by Aspergillus niger and Trichoderma viride using some agriculture residues,” In. J. Agri. Res.7(1), 46-57.

Sonia, K. G., Chadha, B. S., and Saini, H. S. (2005). “Sorghum straw for xylanase hyper-production by Thermomyces lanuginosus (D2 W3) under solid-state fermentation,” Bioresour. Technol. 96(14), 1561-1569.

Sørensen, H. R., Pedersen, S., Vikso-Nielsen, A., and Meyer, A. S. (2005). “Efficiencies of designed enzyme combinations in releasing arabinose and xylose from wheat arabinoxylan in an industrial ethanol fermentation residue,” Enzyme Microb. Technol. 36(5-6), 773-784.

Sorgatto, M., Guimarães, N. C. A., Zanoelo, F. F., Marques, M. R., Peixoto-Nogueira, S. C., and Giannesi, G. C. (2012). “Purification and characterization of an extracellular xylanase produced by the endophytic fungus Aspergillus terreus, grown in submerged fermentation,” Afr. J. Biotechnol. 11(32), 8076-8084.

Soroor, M. A. M., Ghazy, A.-E.-H. M., Mahdy, E.-S. M. S., El-badry, M. O., Shousha, W. G., and EL-Khonezy, M. I. (2013). “Purification and characterization of cellulase-poor xylanases from Trichoderma reesei F418 grown on rice straw by solid-state fermentation,” J. Appl. Sci. Res. 9(3), 1702-1713.

Stricker, A., Mach, R., and de Graaff, L. H. (2008). “Regulation of transcription of cellulase and hemicellulase-encoding genes in Aspergillus niger and Hypocrea jecorina (Trichoderma reesei),” Appl. Microbiol. Biotechnol. 78(2), 211-220.

Su, Y., Zhang, X., Hou, Z., Zhu, X., Guo, X., and Ling, P. (2011). “Improvement of xylanase production by thermophilic fungus  Thermomyces lanuginosus SDYKY-1 using response surface methodology,” New Biotechnol. 31(1), 40-6.

Subramaniyam, R., and Vimala, R. (2012). “Solid state and submerged fermentation for the production of bioactive substances: A comparative study,” Int. J. Sci. Nat. 3(3), 480-486.

Subramaniyan, S., and Prema, P. (2002). “Biotechnology of microbial xylanases: Enzymology, molecular biology, and application,” Crit. Rev. Biotechnol. 22(1), 33-64.

Sun, J., and Glass, N. L. (2011) “Identification of the CRE-1 cellulolytic regulon in Neurospora crassa,” PLoS ONE 6(9), e25654.

Sun, J., Tian, C., Diamond, S., and Glass, N. L. (2012). “Deciphering transcriptional regulatory mechanism associated with hemicellulose degradation in Neurospora crassa,” Eucaryot. Cell. 11(4), 482-493.

Sun, Y., and Cheng, J. (2002). “Hydrolysis of lignocellulosic materials for ethanol production: A review,” Bioresour. Technol. 83(1), 1-11.

Tamayo, E. N., Villanuevaa, A., Hasper, A. A., de Graaff, L. H., Ramóna, D., and Orejas, M. (2008). “CreA mediates repression of the regulatory gene xlnR which controls the production of xylanolytic enzymes in Aspergillus nidulans,” Fungal Genet. Biol. 45(6), 984-993.

Tao, N.-G., Shi, W.-Q., Liu, Y.-J., and Huang, S.-R. (2011). “Production of feed enzymes from citrus processing waste by solid-state fermentation with Eupenicillium javanicum,” Int. J. Food Sci. Technol. 46(5), 1073-1079.

Téllez-Luiz, S. J., Ramirez, J. A., and Vazquez, M. (2002). “Mathematical modeling of hemicellulose sugar production from sorghum straw,” J. Food Eng. 52(3), 285-291.

Tian, B., Xu, Y., Cai, W., Huang, Q., Gao, Y., Li, X., and Huang, J. (2013). “Molecular cloning and overexpression of an endo--1,4-xylanase gene from Aspergillus niger in industrial Saccharomyces cerevisiae YS2 strain,” Appl. Biochem. Biotechnol. 170(2), 320-8.

Topakas, E., Kalogeris, E., Kekos, D., Macris, B. J., and Christakopoulos, P. (2004). “Production of phenolics from corn cobs by coupling enzymatic treatment and solid state fermentation,” Eng. Life Sci. 4(3), 283-286.

Umsza-Guez, M. A., Díaz, A. B., Ory, I., Blandino, A., Gomes, E., and Caro, I. (2011). “Xylanase production by Aspergillus awamori under solid state fermentation conditions on tomato pomace,” Braz. J. Microbiol. 42(4), 1585-1597.

van Munster, J. M., Daly, P., Delmas, S., Pullan, S. T., Dlythe, M. J., Malla, S., Kokolski, M., Noltorp, E. C., Wennberg, K., Fetherston, R., Beniston, R., Yu, X., Dupree, P., and Archer, D. B. (2014). “The role of carbon starvation in the induction of enzymes that degrade plant-derived carbohydrates in Aspergillus niger,” Fungal Genet. Biol. DOI: 10.1016/j.fgb.2014.04.006, in press.

Venegas, I. M., Fuentes-Hernández, J. F., Rivero, M. G., and Trujillo, A. M. (2013). “Characteristics of Aspergillus niger xylanases produced on rice husk and wheat bran in submerged culture and solid-state fermentation for an applicability proposal,” Int. J. Food Sci. Technol. 48(9), 1798-1807.

Virupakshi, S., Babu, K. G., Gaikwad, S. R., and Naik, G. R. (2005). “Production of a xylanolytic enzyme by a thermoalkaliphilic Bacillus sp. JB-99 in solid state fermentation,” Process Biochem. 40(1), 431-435.

Vitcosque, G. L., Fonseca, R. F., Rodríguez-Zúñiga, U. F., Bertucci Neto, V., Couri, S., and Farinas, C. S. (2012). “Production of biomass-degrading multienzyme complexes under solid-state fermentation of soybean meal using a bioreactor,” Enzyme Res. 2012(2012), 1-9.

Yang, C. H., Yang, S. F., and Liu, W. H. (2007). “Production of xylooligosaccharides from xylans by extracellular xylanases from Thermobifida fusca,” J. Agric. Food Chem. 55(10), 3955-3959.

Yang, S. Q., Yan, Q. J., Jiang, Z. Q., Li, L. T., Tian, H. M., and Wang, Z. (2006). “High-level of xylanase production by the thermophilic Paecilomyces themophila J18 on wheat straw in solid-state fermentation,” Bioresour. Technol. 97(15), 1794-1800.

Yang, G., Hou, L. L., and Zhang, F. L. (2011). “Study on the solid-state fermentation conditions for producing thermostable xylanase feed in a pressure pulsation bioreactor,” Adv. Mater. Res. 236-238, 72-76.

Yeasmin, S., Kim, C. H., Park, H. J., Sheikh, M. I., Lee, J. Y., Kim, J. W., Back, K. K., and Kim, S. H. (2011). “Cell surface display of cellulase activity-free xylanase enzyme on Saccharomyces cerevisiae EBY100,” Appl. Biochem. Biotechnol. 164(3), 294-304.

Yi, X., Shi, Y., Xu, H., Li, W., Xie, J., Yu, R., Zhu, J., Cao, Y., and Qiao, D. (2010). “Hyperexpression of two Aspergillus niger xylanase genes in Escherichia coli and characterization of gene products,” Braz. J. Microbiol. 41(3), 778-786.

Yu, K. C. E., Tan, L. U. L., Chan, M. K. H., Deschatelets, L., and Saddler, J. N. (1987). “Production of thermostable xylanase by a thermophilic fungus Thermoascus aurantiacus,” Enzyme Microb. Technol. 9(1), 16-24.

Xie, Z-L., Gao, H-Y., Zhang, Q., Wang, H., Liu, Y. (2012). “Cloning of a novel xylanase gene from a newly isolated Fusarium sp. Q7-31 and its expression in Escherichia coli,” Braz. J. Microbiol. 43(1), 405-417.

Xiros, C., Topakas, E., Katapodis, P., and Christakopoulos, P. (2008). “Hydrolysis and fermentation of brewer’s spent grain by Neurospora crassa,” Bioresour. Technol. 99(13), 5427-5435.

Xu, Y-X., Li, Y-L., and Tang, J.-W. (2008). “Improvement of xylanase production by Aspergillus niger XY-1 using response surface methodology for optimizing the medium composition,” J. Zhejiang Univ. Sci. B. 9(7), 558-566.

Zhao, X., Peng, F., Cheng, K., and Liu, D. (2009). “Enhancement of the enzymatic digestibility of sugarcane bagasse by alkali-peracetic acid pretreatment,” Enzyme Microb. Technol. 44(1), 17-23.

Zhou, H., Cheng, J. S., Wang, B. L., Fink, G. R., and Stephanopoulos, G. (2012). “Xylose isomerase overexpression along with engineering of the pentose phosphate pathway and evolutionary engineering enable rapid xylose utilization and ethanol production by Saccharomyces cerevisiae,” Metab. Eng. 14(6), 611-622.

Zhu, Z. G., Sathitsuksanoh, N., Vinzant, T., Schell, D. J., McMillan, J. D., and Zhang, Y.-H. P. (2009). “Comparative study of corn stover pretreated by dilute acid and cellulose solvent-based lignocellulose fractionation: Enzymatic hydrolysis, supramolecular structure, and substrate accessibility,” Biotechnol. Bioeng. 103(4), 715-724.

Znameroski, E. A., and Glass, N. L. (2013). “Using a model filamentous fungus to unravel mechanisms of lignocellulose deconstruction,” Biotechnol. Biofuels 6(1), 1-7.

Article submitted: February 24, 2014; Peer review completed: June 18, 2014; Revised version received and accepted: July 1, 2014; Published: July 15, 2014.