Scholarly article on topic ' Analysis of a conserved cellulase transcriptional regulator reveals inducer-independent production of cellulolytic enzymes in Neurospora crassa '

Analysis of a conserved cellulase transcriptional regulator reveals inducer-independent production of cellulolytic enzymes in Neurospora crassa Academic research paper on "Biological sciences"

Share paper
Academic journal
OECD Field of science

Academic research paper on topic " Analysis of a conserved cellulase transcriptional regulator reveals inducer-independent production of cellulolytic enzymes in Neurospora crassa "



Analysis of a conserved cellulase transcriptional regulator reveals inducer-independent production of cellulolytic enzymes in Neurospora crassa

Samuel T. Coradetti, Yi Xiong & N. Louise Glass

Plant and Microbial Biology Department, The University of California, Berkeley, CA 94720-3102


Aspergillus, biofuels, cellulase, Neurospora, transcriptional regulation.


N. Louise Glass, Plant and Microbial Biology Department, University of California, 341 Koshland Hall, Berkeley, CA 94720-3102. Tel:+1 510 643-2546; Fax: +1 510 642-4995; E-mail:

Funding Information

This work was supported by a grant from Energy Biosciences Institute to N. L. G. and National Institutes of Health (NIH) NRSA Trainee Grant #2 T32 GM 7127-36 A1 to S. T. C.

Received: 23 April 2013; Accepted: 2 May 2013

MicrobiologyOpen 2013; 2(4): 595-609

doi: 10.1002/mbo3.94


Cellulose is recalcitrant to deconstruction to glucose for use in fermentation strategies for biofuels and chemicals derived from lignocellulose. In Neurospora crassa, the transcriptional regulator, CLR-2, is required for cellulolytic gene expression and cellulose deconstruction. To assess conservation and divergence of cellulase gene regulation between fungi from different ecological niches, we compared clr-2 function with its ortholog (clrB) in the distantly related species, Aspergillus nidulans. Transcriptional profiles induced by exposure to crystalline cellulose were similar in both species. Approximately 50% of the cellulose-responsive genes showed strict dependence on functional clr-2/clrB, with a subset of 28 genes encoding plant biomass degrading enzymes that were conserved between N. crassa and A. nidulans. Importantly, misexpression of clr-2 under noninducing conditions was sufficient to drive cellulase gene expression, secretion, and activity in N. crassa, to a level comparable to wild type exposed to Avicel. However, misexpression of clrB in A. nidulans was not sufficient to drive cellulase gene expression under noninducing conditions, although an increase in cellulase activity was observed under crystalline cellulose conditions. Manipulation of clr-2 orthologs among filamentous fungi may enable regulated cellu-losic enzyme production in a wide array of culture conditions and host strains, potentially reducing costs associated with enzyme production for plant cell wall deconstruction. However, this functionality may require additional engineering in some species.


Saprotrophic fungal species are major agents of plant decay in the environment (Kominkova et al. 2000; Hieber and Gessner 2002), with influences on the global carbon cycle (Heimann and Reichstein 2008), local nutrient flows (Frey et al. 2003), and the historic accumulation of fossil fuel deposits (Floudas et al. 2012). Depolymerization of cellulose for biotechnological applications is currently assisted by large-scale production of fungal enzyme mixtures and their application to pretreated plant biomass. However, commercially available enzyme mixtures for cellulose degradation remain prohibitively expensive for current saccharification processes (Margeot et al. 2009). A greater understanding of fundamental aspects of fungal enzyme synthesis and secretion is required, including

defining regulatory networks that control enzyme production. Regulated control of cellulase gene expression across divergent fungal species would allow for high productivity of varied enzyme mixtures under a range of growth conditions and media compositions.

To elucidate the fungal potential for plant cell wall deconstruction and explore how environmental factors affect the production of enzymes mediating decay, we study regulatory mechanisms associated with cellulose degradation in two distantly related model filamentous fungi, Neurospora crassa and Aspergillus nidulans. In nature, N. crassa is associated with plant material that has been killed by fire (Perkins and Turner 1988). A. nidulans is a more cosmopolitan species and has been isolated from a variety of substrates including dead plant matter (Klich 2002). Both N. crassa and A. nidulans have a wide

© 2013 The Authors. MicrobiologyOpen published by John Wiley & Sons Ltd. This is an open access article under the terms of the Creative Commons Attribution License, which permits use, distribution and reproduction in any medium, provided the original work is properly cited.

array of genomic, genetic, and biochemical tools that make these two species an ideal platform for comparative analyses of processes associated with plant cell wall deconstruction.

The production of hydrolytic plant cell wall degrading enzymes in filamentous fungi, including N. crassa and A. nidulans is dependent upon a release from carbon catabolite repression (CCR) as well as induction in response to the presence of plant cell wall material (Ruij-ter and Visser 1997; Mach and Zeilinger 2003; Aro et al. 2005; Andersen et al. 2008; Portnoy et al. 2011; Sun and Glass 2011; Zhou et al. 2012). In a previous study, we identified a zinc binuclear cluster transcription factor, CLR-2 (NCU08042), that is essential for induction of genes encoding cellulases (Coradetti et al. 2012); the expression of clr-2 is induced in the presence of plant cell walls (Miscanthus), cellulose, or cellodextrins (Tian et al. 2009; Znameroski et al. 2012). An N. crassa strain containing a deletion of clr-2 is unable to utilize cellulose as a sole carbon source and fails to induce ~2/3 of the genes identified in the "Avicel regulon" (Coradetti et al. 2012). clr-2 is highly conserved in filamentous ascomycete fungi; a strain carrying a deletion of the A. nidulans ortholog of clr-2 (clrB) also failed to induce a number of cellulolytic genes and lacked cellulase activity (Coradetti et al. 2012).

Here, we generated the first set of RNA-seq data from both wild-type A. nidulans and a AclrB mutant in response to carbon starvation or crystalline cellulose. In-depth comparative analyses of these data with published N. crassa wild type and Aclr-2 data unraveled both conserved and divergent genes associated with the CLR-2 versus the ClrB regulons in these two distantly related species. Importantly, we found that misexpression of clr-2 in N. crassa induced cellulase gene expression and activity under noninducing conditions and also increased cellulase activity when the misexpression strain was exposed to crystalline cellulose. To our knowledge, this is first report of that the manipulation of one gene can circumvent the dependence of inducers for cellulase production. Our experiments suggest that the manipulation of clr-2 ortho-logs among filamentous fungi holds great potential for the identification and characterization of new enzymes. These studies will increase our understanding of mechanistic aspects of plant cell wall deconstruction and the development of optimal enzyme cocktails for cellulose degradation.

Experimental Procedures


The wild-type N. crassa reference strain and background for mutant strains were OR74A (FGSC 2489) (Colot et al.

2006). The deletion strains for clr-2 (FGSC 15,835) were obtained from the Fungal Genetics Stock Center (http:// (McCluskey 2003). The clr-2 misexpres-sion strain was constructed by transforming a his-3 rid-1 Asad-1; Aclr-2 A mutant with a variant of plasmid pMF272, where the open reading frame and 3' untranslated region (UTR) of clr-2 were placed under the control of the promoter and 5' UTR of the clock-controlled gene 1 (ccg-1). Transformants were selected for histidine proto-trophy and backcrossed to a his-3; Aclr-2 A strain to obtain a his-3::pccg-1-clr-2 rid-1 Asad-1; Aclr-2 A homok-aryotic strain.

The A. nidulans reference strain was FGSC 4A. The DclrB deletion strain was constructed previously (Coradetti et al. 2012). The clrB misexpression strains were constructed by transforming a AclrB mutant (AclrB::pyrG, pyroA4, pyrG89) with a DNA fragment consisting of the Aspergillus fumiga-tus pyroA gene, the gpdA (Punt et al. 1990) or the alcA (Waring et al. 1989) promoter and the coding region, and 3' UTR of either clrB or clr-2 inserted into the pyrG locus. Transformants were selected for pyridoxine prototrophy (Nayak et al. 2006). The DNA fragments were generated by fusion PCR and transformation was carried out as described previously (Szewczyk et al. 2006).

Culture conditions

N. crassa cultures were grown on Vogel's minimal medium (VMM) (Vogel 1956); carbon sources were 2% w/v unless otherwise noted. Strains were inoculated into 3 mL VMM slants and grown at 30°C in the dark for 48 h, then at 25°C in constant light for 4-10 days to stimulate conidia production. Conidia were inoculated into 100 mL of liquid media at 106 conidia/mL and grown at 25°C in constant light and shaking (200 rpm).

A. nidulans cultures were grown on A. nidulans minimal medium (MM) (Vishniac and Santer 1957). Carbon sources were 2% w/v unless otherwise noted. Conidia were grown on sucrose MM slants, then inoculated into 100 mL liquid media at 3 x 106 conidia/mL and grown at 37°C in constant light and shaking (200 rpm). These culture conditions were optimal for cellulose utilization by each species in pilot experiments and are in line with previous studies on each species. The higher temperature and inoculum used for A. nidulans allowed for comparable biomass accumulation to N. crassa cultured over the same period, which was chosen as the best practical basis comparison between the two species.

Media shift experiments

Cultures were grown 16 h on sucrose (or 1% glucose for the A. nidulans RNA-seq experiments), centrifuged at

2000 g for 10 min, and washed in VMM or MM (Vogel 1956) without a carbon source. Mycelia were resuspended in 100 mL VMM or MM with 2% carbon source (sucrose, cellulose [Avicel® PH-101, Sigma Aldrich, MO]) or with no carbon source added. Total RNA was extracted as described in Tian et al. (2009) at 4 h after shift for N. crassa cultures and 6 h after shift for A. nidu-lans cultures. These time points were selected as the earliest points of full cellulase gene induction by preliminary RT-PCR time course experiments. For enzyme activity assays, culture supernatants were sampled at 6, 12, 24, 36, 48, and 72 h (and 96 h for A. nidulans), centrifuged at 3000 g twice to remove mycelia, and stored at 4°C for prior to analysis. At the end of the time course experiments, fungal biomass was harvested, dried, and weighed. The relative proportion of mycelia to residual Avicel was calculated by solubilizing fungal biomass in boiling acetic nitric reagent as in Updegraff (1969), washing the residual mass thoroughly, then drying, and reweighing.

One mutant strain (Pg2) required alternate media switch conditions due to low growth and conidiation. Pg2 conidia were inoculated in 3 mL 1% glucose MM and grown 3 days at 37°C in constant light and shaking (200 rpm). Cultures were then washed in MM with no carbon and switched to 3 mL MM with 2% Avicel, 2% glucose, or no carbon source. Other A. nidulans strains used in RT-PCR experiments were cultured similarly, but with only 24 h pregrowth in 1% glucose to achieve similar biomass to Pg2.

RNA sequencing and transcript abundance

Libraries were prepared with standard protocols from Illumina Inc (San Diego, CA) and sequenced on the Illumina Genome Analyzer IIx and HiSeq 2000 platforms. Sequenced libraries were mapped against predicted transcripts from the N. crassa OR74A genome (Galagan et al. 2003) ( neurospora/MultiHome.html) or the A. nidulans FGSC A4 genome (Galagan et al. 2005) with Tophat v2.0.4 (Langmead et al. 2009). Transcript abundance (Fragments per Kilobase exon length per Megabase mapped, FPKM) was estimated with Cufflinks v2.0.2 (Roberts et al. 2011) mapping against reference isoforms. Profiling data are available as a supplemental Data S1 and at the GEO (http://www.ncbi.; Series Record GSE44100). Raw counts for reads mapping to unique exons were tallied with HTSeq (Anders and Huber 2010) and used as inputs for the DESeq software packages. Genes with a multiple hypothesis-adjusted p-value below 0.05 and at least fourfold induction on Avicel were selected as belonging to the Avicel regulon and used for further analyses.

Orthologous gene pairs were taken from the fungal orthogroups repository ( regev/orthogroups/) and supplemented by a best reciprocal blast search for recently added or revised gene models in the N. crassa and A. nidulans genomes. In few cases, Avicel-induced genes had an ortholog listed in the repository with very low expression and a second close homolog with similar sequence conservation which showed specific induction. In those cases, the induced homolog was selected as the likely ortholog. For each species, specifically induced genes without a clear ortholog were used as BLAST queries against the other genome. The most significant alignment (E-value <10—50) was taken as a possible paralog. In some cases this procedure matched several paralogs in one species to a single gene in the other. These pairings were treated as distinct entries for clustering analysis. Genes with very low expression (FPKM <5 on Avicel) were filtered from the cross-species clustering analysis. For clustering of or-thologous and paralogous pairs of genes, FPKM were log transformed and normalized on a per gene basis such that the highest value recorded in any sample for either member of the pairing was set to 1. The normalized values were then scaled and centered to set 1 FPKM to —1 and the maximal FPKM to 1 for clustering. Average linkage clustering was performed with Cluster 3.0 (de Hoon et al. 2004) using Pearson correlation as the similarity metric.

For clustering of WT and mutant clr-2/clrB libraries in each species, FPKM were log transformed then normalized and centered on per gene basis with Cluster 3.0 standard settings, such that values from each gene ranged from —1 (minimum/uninduced value) to 1 (maximum/ induced value) and clustered with K-means clustering with Euclidean distance as the similarity metric.

Enzyme activity assays

CMCase and xylanase activity of culture supernatants was assayed with Remazolbrilliant Blue R-conjugated carboxy-methyl cellulose (CMC) and xylan (birchwood) kits from Megazyme (Wicklow, Ireland). Briefly, in these assays enzyme activity is measured by the release of ethanol soluble short-chain dye-conjugated oligomers from the long-chain substrates, followed by quantification with a UV spectro-photometer. Total protein was determined with the Bradford assay from BioRad (Hercules, CA). Cellulase activity was measured as previously reported (Tian et al. 2009) with minor adjustments. A 200 iL aliquot of culture supernatant was added to a final volume of 1 mL 1% Avicel in 50 mmol/L sodium acetate and incubated with shaking at 37°C overnight. Released glucose and cellobiose levels were measured by high performance liquid chromatography.

Variation and statistical significance

All error bars on charts and figures represent standard deviation from biological triplicate samples unless otherwise noted.


A comparison of the Avicel regulons of A. nidulans and N. crassa reveals conserved clusters of genes

To comprehensively compare the CLR-2/ClrB regulons in these two evolutionarily divergent species, we first characterized the transcriptional response of A. nidulans to Avicel. To compare its Avicel regulon with that of N. crassa, A. nidulans wild-type strains were switched from a simple carbon source, glucose to Avicel, or no carbon source media; transcriptional profiles of the switched cultures were analyzed with RNA-seq. Genes strongly induced on Avicel (>fourfold transcript abundance with a statistical significance beyond a 5% false discovery rate, as calculated with DESeq) were compared between the two species (Fig. 1; Data S1).

Both N. crassa and A. nidulans exhibited a broad and similar transcriptional response to Avicel with several hundred genes meeting the conservative criteria for specific induction (Fig. 1C, D). The magnitude of this induction was greater in N. crassa, however, particularly for enzyme classes with predicted function in the degradation of crystalline cellulose, such as genes encoding enzymes in the glycoside hydrolase (GH; (Cantarel et al. 2009)) 7 family (cellobiohydrolase I), GH6 family (cello-biohydrolase II), polysaccharide monooxygenases (formerly GH61 family), and GH5 family (endoglucanases) (Fig. 1E). To compare enzyme activity and protein secretion, supernatants from N. crassa and A. nidulans cultures shifted to either Avicel or sucrose were evaluated. Enzyme activity on amorphous cellulose (carboxymethyl cellulose) and xylan was significantly higher from A. nidulans Avicel-grown supernatants as compared with N. crassa (Fig. 2A, B). However, enzyme activity on crystalline cellulose was significantly higher for Avicel su-pernatants from N. crassa (Fig. 2D, F). N. crassa also secreted more protein, consumed more cellulose, and accumulated more biomass on Avicel than A. nidulans (Fig. 2C, E). These results reflected the observed tran-scriptional differences between N. crassa and A. nidulans in genes encoding enzymes with predicted activity on crystalline cellulose (Fig. 1E).

To assess the conservation of the Avicel regulon between N. crassa and A. nidulans on a gene-by-gene basis, expression of orthologous and paralogous gene pairs was sorted

with hierarchical clustering. Among genes with likely or-thologs in each species, 10 gene expression clusters were identified (Fig. 3; Data S1). Cluster O1 consisted of genes strongly induced in N. crassa under Avicel conditions, but with very low expression in A. nidulans. This cluster included genes encoding two putative transporters (NCU01633/AN4277 and cdr4 NCU05591/AN0771), a ß-glucosidase gh3-6/bglB (NCU07487/AN0712), as well genes encoding six additional secreted carbohydrate-active enzymes (CAZy;, an acetylcholine esterase (NCU08752/AN7407), and a monooxygenase (NCU7055/AN8199).

Cluster O2 consisted of 29 genes strongly and specifically induced on Avicel in both species, 25 of which encoded secreted CAZy proteins (Data S1). These included the most highly expressed and well-characterized cellulases: cbh-1 (NCU07340, orthologous to both cbhA AN5176 and cbhB AN0494), gh6-2 (NCU09680 orthologous to both cbhC AN5282 and cbhD AN1273), gh5-1/ eglA (NCU00762/AN1285), and multiple polysaccharide monooxygenases (PMO). Cluster O3 consisted of 9 genes strongly induced on Avicel, but with higher expression under starvation conditions than genes in cluster O2 (Data S1). Most of these genes are implicated in pectin or hemicellulose deconstruction. Also included were two transporters: cellodextrin transporter cdt-1 (NCU00801/ AN2814) and a less strongly expressed putative sugar transporter NCU06384/AN3498.

Clusters O4 and O5 consisted of genes with specific induction under Avicel conditions in N. crassa, but relatively constant expression at an intermediate level in A. nidulans. These clusters were differentiated mostly by their relative transcript abundances in N. crassa under starvation conditions. They included several genes that function in xylose utilization: xylose reductase NCU08384/AN0423, xylitol dehydrogenase NCU00891/ AN9064, xylulose kinase NCU11353/AN8790, ribose-5-phosphate isomerase NCU10107/AN5907, mitochondrial triose phosphate isomerase NCU10106/AN5908, and a xylose-specific transporter NCU06138/AN0250 (Du et al. 2010). Six genes with known or suspected roles in protein secretion and trafficking also clustered tightly in O5: hsp70-6 NCU09485/AN0847, calreticulin/calnexin homolog clxA NCU09265/AN3592, sec61-1 NCU08897/AN7721, grp78/bipA NCU03982/AN2062, SEC62 homolog NCU06333/AN6269, and protein disulfide isomerase A pdiA NCU09223/AN7436. Also prominent in these clusters were several genes involved in aspartate/aspara-gine and aromatic amino acid biosynthesis. The cellulo-lytic regulators clr-1/clrA (NCU07705/AN5808) and clr-2/clrB also clustered in O5 and O4, respectively. They showed specific induction in both species, but the magnitude of the change was more dramatic in N. crassa.


г - P < 0.05 & Av/NC > 4 (193 genes) P < 0.01 (60 genes) P < 0 05 (47 genes) '

10"' 10" 10' 10z 10J 10" 10° 10° Expression maximum (Normalized counts)

10 103 102 101 10° 10' 10'

Г • P < 0.05 & Av/NC > 4 (295 genes) P < 0.01 (1080 genes) P < 0.05 (737 genes) .

. :• . Y.'^'. '. '-V

10"' 10u 10' 10^ 10J 10* 10° 10° Expression maximum (Normalized counts)


GH28 GH5.7

GH5 GH74

GH62 GH131

GH51 GH12



CE4 GH5.5





No C I Avi A. nidulans A4

Figure 1. The Avicel regulons of N. crassa and A. nidulans. (A) Photograph of N. crassa grown on a Petri dish showing mycelia and conidia (orange). (B) Photograph of A. nidulans grown on a Petri dish showing mycelia and conidia (green). (C) Relative mRNA abundance of N. crassa exposed to Avicel versus no carbon conditions. Genes showing significant differential expression are colored by adjusted P-value. (D) Relative mRNA abundance of A. nidulans exposed to Avicel versus no carbon source conditions. Genes showing significant differential expression are colored by adjusted P-value. (E) Total expression from RNA-seq data of genes encoding the major classes of plant cell wall carbohydrate-active enzymes (CAZy; (Cantarel et al. 2009)) from a WT N. crassa culture shifted to media with no carbon source or to Avicel and from a WT A. nidulans culture shifted to media with no carbon source or to Avicel. FPKM (Fragments Per Kilobase per exon per Megabase mapped) for individual genes were averaged between biological replicates and pooled by CAZy class. Classes acting primarily on crystalline cellulose are shown in blue, classes acting primarily on hemicellulose are shown in brown and orange, and classes acting primarily on pectin are colored in purple.

Clusters O6 and O7 (Data S1) consisted of 23 and 14 genes, respectively, with specific induction under Avicel conditions in A. nidulans, but with relatively constitutive expression in N. crassa. They included a few secreted pectinases (arabinosidase gh43-7 NCU05965/AN7781, exopolygalacturonase gh28-2 NCU06961/AN8891, GDSL lipase/acylhydrolase NCU06364/AN1792) and intracellular enzymes with activity on pectin breakdown products (L-galactonate dehydratase NCU07064/AN6035, b-xylosidase gh43-5/bxlD NCU09652/AN7864, b-galactosidase gh2-3/

lacD NCU00810/AN3201, and UDP-glucose 4-epimerase NCU05133/AN2951).

Cluster O8 had generally higher expression in A. nidulans, but more specific induction under Avicel conditions in N. crassa. It was most dominated by genes encoding predicted pectinases and hemicellulases (rhamnogalactu-ronan acetylesterase ce12-1 NCU09976/AN2528, faeC NCU08785/AN5267, acetylxylan esterase ce5-3 NCU09664/AN5309, gh11-1/xlnA NCU02855/AN3613, and mixed-linked glucanase NCU01353/AN0245) and


N.c. Avi

24 48 72 Hours after shift

24 48 72 Hours after shift

(E) 1 N. crassa

■ A. nidulans

Avicel Sucrose

■£■ 2

24 48 72 Hours after shift

24 48 72 Hours after shift

"О re 10

¿с 0


Figure 2. Time course of enzyme activity from N. crassa and A. nidulans culture supernatants. (A) CMCase activity of culture supernatants from N. crassa or A. nidulans cultures shifted to either Avicel or sucrose, as measured by cleavage of dye-conjugated CMC. (B) Xylanase activity of culture supernatants from N. crassa or A. nidulans cultures shifted to either Avicel or sucrose, as measured by cleavage of dye-conjugated xylan.

(C) Secreted protein in N. crassa or A. nidulans supernatants from cultures shifted to either Avicel or sucrose, as determined by Bradford assay.

(D) Cellulase activity, as determined by sugar release from Avicel, of N. crassa or A. nidulans supernatants from cultures shifted to either Avicel or sucrose. (E) Final mycelia dry weights 72 and 96 h after shift of N. crassa and A. nidulans cultures to sucrose or Avicel. Biomass in Avicel cultures was estimated by degrading mycelia and weighing the recalcitrant fraction (Updegraff 1969). (F) Cumulative breakdown of Avicel normalized to final dry weight of cultures. (A-D) All data points normalized to final culture biomass as in (E).

hypothetical proteins. It also included the major secreted ß-glucosidase gh3-4/bglL NCU04952/AN2828. Clusters O9 and O10 were induced in A. nidulans, but not in N. crassa. Cluster O9 included several stress response genes (hsp30-like proteins AN3555 and AN2530 orthologous to hsp30 NCU09364, hsp78 NCU02630/AN1163, a MFS multidrug transporter NCU00306/AN0732, and a mito-chondrial hypoxia-responsive gene NCU02623/AN1066).

Genes with uncertain orthology relations were matched as pairs of cross-species paralogs and clustered by FPKM with the same parameters as the orthologous pairs, yielding 6 major clusters (Fig. 3B; Data S1). Most of the genes encoding CAZy proteins in this set clustered together in P2 and P3. Genes in P2 showed some induction in both species, but with greater magnitude in N. crassa. Most notable in this group were an expansion of highly expressed PMOs in N. crassa and an expansion of endo-ß-mannanases (GH5.7) in A. nidulans. Genes in cluster P3 were comparably expressed in both species. Most prominent in P3 were several ß-glucosidases and ß-xylo-sidases and the highly expressed CBHII homolog gh6-3

NCU07190, most closely related to cbhD AN1273. Cluster P5 genes were induced on Avicel in A. nidulans, and included 3 paralogous genes encoding enzymes associated with hemicellulose and/or pectin breakdown. Cluster P6 included A. nidulans paralogs that were induced under Avicel conditions, but not in N. crassa.

Polysaccharide monooxygenases (GH61) oxidatively cleave cellulose (Phillips et al. 2011a; Quinlan et al. 2011; Beeson et al. 2012). Based on phylogenetic analyses, three PMO enzyme classes have been identified in N. crassa (Li et al. 2012); these genes had a particularly distinct pattern of expression between the two species. In N. crassa, 10 of 14 predicted PMO genes met our criterion for specific induction on Avicel, with no particular gene accounting for more than 27% of total FPKM among this class. In A. nidulans, 5 of 9 predicted PMO genes were specifically induced, but just one type-3 PMO, AN3860, accounted for more than 93% of total FPKM under Avicel conditions.

N. crassa genes without clear homologs in A. nidulans that were induced on Avicel were dominated by hypothetical

(A) Orthologs A.n. N.c. A N A N


GH3 PM0 CE5 CE8 GH74 GH51


GH43 GH18


GH5.7 GH1 GH131 GH13


GH7 CE1 CE16

CEnc GH5.5 GH131

GH7 GH10 GH3

GH43 PL4 GH53

Paralogs A.n. N.c. A N A N

P1 ■ =

P2 I i ■

P4 1 1 ■■

P5 k i i

P6 1". 3 II

Figure 3. Hierarchical clustering of orthologous and paralogous genes induced by exposure to Avicel in N. crassa and A. nidulans. (A) Hierarchical clusters of FPKM for ortholog pairs (O1-O10) for which at least one member passed criteria for specific induction under either Avicel [A] or no carbon source [N] conditions. A.n. = Aspergillus nidulans; N.c. = Neurospora crassa. (B) Hierarchical clusters of FPKM for paralogous pairs (P1-P6) of genes induced under Avicel [A] or no carbon source [N] conditions (see methods for details on paralog selection). Heat maps display log (FPKM) scaled from 1 (bright blue) to the maximal value for each pair (bright yellow). CAZy genes in each cluster are marked with small arrows and listed in order to the right of each cluster.

proteins (34 of 39; Data S1); 12 were predicted to be secreted and may have novel functions in plant cell well deconstruction. A. nidulans genes without clear homologs in N. crassa that were induced on Avicel included genes encoding predicted pectinases and enzymes with roles in secondary metabolism (sterigmatocystin/aflatoxin, terreq-uinone A, and penicillin biosynthesis).

Conservation of gene regulation by CLR-2 and ClrB

To assess conservation of function and respective target genes of CLR-2 and ClrB, we analyzed expression patterns

of the Avicel regulon (295 genes total) in WT A. nidulans transferred to Avicel or no carbon source media versus the AclrB mutant transferred to Avicel. We identified 4 clusters of genes in A. nidulans (An1-An4; Fig. 4A; Data S1). Cluster An1 was comprised of 141 genes strictly dependent on clrB. It was dominated by highly expressed genes encoding the core enzymes associated with crystalline cellulose degradation: the CDH, PMO, GH7, GH6, and GH5.5 families. Although genes encoding cellulases were not induced in AclrB on Avicel, expression of some genes associated with hemicellulose degradation showed an increased expression level in the AclrB mutant on Avicel over WT under no carbon conditions (Fig. 4B).

Cluster An2 was composed of 40 genes with intermediate transcript abundance in AclrB strains on Avicel as compared with WT, indicating a partial or indirect requirement for functional ClrB for induction on Avicel (Data S1). This cluster included several genes with predicted function in secondary metabolite biosynthesis, including several robustly expressed genes of the sterig-matocystin biosynthesis gene cluster. Genes implicated in monodictyphenone and penicillin biosynthesis and a putative polyketide synthase (AN12331) also showed clrB-dependent induction, but were expressed at lower levels.

Genes in clusters An3 and An4 (61 and 53 genes) reached full induction in Avicel in the AclrB mutant, although variance in expression was high between biological replicates (Fig. 4; Data S1). This cluster was dominated by expression of the GH10, GH11, GH43, and GH62 gene families, which encode the major enzyme

(A) A. nidulans

Avicel No C WT AclrB WT

An2 An3 An4

Min 1 1 Max


GH28 GH5.7

GH5 GH74

GH62 GH131

GH51 GH12



CE4 GH5.5



GH43 PM0



Figure 4. Dependence of Avicel-induced genes on functional ClrB in A. nidulans. (A) K-means clusters of Avicel-induced genes in an A. nidulans AclrB mutant strain on Avicel as compared to a WT strain on Avicel or media with no carbon source. Heat map displays log (FPKM) scaled from minimal expression (bright blue) to the maximal expression (bright yellow). (B) Total expression of genes encoding major CAZy classes in the AclrB mutant on Avicel as compared to a WT strain on Avicel or media with no carbon source. Note the absence of expression of genes encoding predicted cellulases in the AclrB mutant (PMO, GH6, GH7, and GH5.5 classes, shown in blue).

classes dedicated to hemicellulose degradation. Several of these genes or their orthologs have been identified as targets of the transcriptional regulator XlnR in Aspergilli (van Peij et al. 1998), and also had variable expression in A. nidulans when induced by xylose (Andersen et al. 2008).

The genes identified as ClrB dependent in A. nidulans were compared with those identified as CLR-2 dependent in N. crassa in response to Avicel (Coradetti et al. 2012). Twenty-eight orthologous pairs of genes with conserved regulation by CLR-2/ClrB were identified (Table 1). All of these genes encode proteins with some functional annotation (no hypothetical), although some are based solely on homology to enzymes with limited experimental data. The majority encoded secreted proteins that represent the conserved core of enzymes for cellulose degradation, including well-studied endoglucanases, exoglucanases, and b-glucosidases, as well as the newly characterized polysac-charide monooxygenases. The conserved list also included xylan and pectin degrading enzymes, including NCU00449 and NCU09764, orthologs to AN7598

(GH131; b-glucanase), and which have sequence similarity to a characterized glucuronan lyase from T. reesei (Konno et al. 2009). A conserved CLR-2/ClrB target NCU07143/AN2112 is homologous to a recently characterized extracellular aldonolactonase from M. thermophila (Beeson et al. 2011) and was identified in N. crassa secretome studies on Avicel (Phillips et al. 2011b). The expression of genes encoding several intracellular enzymes had conserved modulation by CLR-2/ClrB, including an intracellular b-glucosidase (NCU00130) and a b-mannosidase (NCU00890), as well as the cellodextrin transporter, cdt-1 (NCU00801) (Galazka et al. 2010). Finally, one transcriptional regulator was conserved (clr-1/clrA). In N. crassa, clr-1 is required for the induction of clr-2 in response to cellulose (Coradetti et al. 2012).

Inducer-independent expression of cellulases in N. crassa

Transcripts of clr-2 and clrB accumulate under cellulolytic conditions (Coradetti et al. 2012). To test whether clr-2

Table 1. Conserved orthologous genes in the CLR-2 and ClrB regulons.

Gene and annotation

Orthologs with conserved dependence on clr-2/clrB



NCU00762 NCU07760 NCU00206

NCU07143 NCU08412 NCU03328 NCU02344 NCU04952 NCU09664 NCU00449 NCU09764 NCU06326 NCU03181 NCU00972 NCU04997 NCU07705 NCU05598 NCU09976 NCU08176 Orthologs with conserved NCU00130 NCU00801 NCU04854 NCU00890 NCU09416

cbh-1 cellobiohydrolase 1

gh6-2 cellobiohydrolase 2

gh5-1 endoglucanase 2 gh61-2 PMO cdh-1 cellobiose dehydrogenase lac-2 aldonolactonase endo-b-1,4-mannanase gh61-6 PMO gh61-12 PMO

gh3-4 secreted b-glucosidase ce5-3 acetylxylan esterase glycoside hydrolase gh61-14 glycoside hydrolase pectate lyase 1 acetylxylan esterase

arabinogalactan endo-1,4-b-galactosidase gh10-3 xylanase

clr-1 cellulose degradation regulator 1 asd-1 rhamnogalacturonase B ce12-1 rhamnogalacturonan acetylesterase ply-2 pectate lyase A modulation by clr-2/clrB gh1-1 cytoplasmic b-glucosidase cdt-1 cellodextrin transporter gh7-2 endoglucanase gh2-1 b-mannosidase cellulose-binding GDSL lipase/acylhydrolase




CBM1, GH131

CBM1, GH10


CBM1, CE16

AN5176 AN0494 AN1273 AN5282 AN1285 AN3860 AN7230

AN2112 AN6427 AN6428

AN2828 AN5309 AN7598

AN0741 AN5320 AN5727 AN7401 AN5808 AN7135 AN2528 AN6106






cbhA cbhB cbhD cbhC eglA

gala xlnE clrA rglA

eglB mndB

expression alone was sufficient for cellulase enzyme secretion in N. crassa, we placed a copy of the clr-2 coding region under control of the promoter from clock-controlled gene 1 (Pccg-1) in a Aclr-2 (strain Pc2; see Experimental Procedures). Under our culture conditions of vegetative growth in constant light and temperature, circadian rhythm is dampened (Elvin et al. 2005) and Pccg-1 is essentially a constitutive promoter.

Expression patterns of the Avicel regulon (193 genes total) were compared in WT N. crassa on Avicel and no carbon media, the Aclr-2 strain on Avicel, and the Pc2 strain on no carbon media. Four major expression clusters were identified in WT (Fig. 5A; Nc1-Nc4); the Nc1 and Nc2 clusters were dependent upon functional clr-2. The Nc1 cluster (65 genes) was comparably or more strongly expressed in the Pc2 strain under noninducing conditions. This cluster was highly enriched for genes encoding secreted CAZy proteins and included most major cellulase genes (Data S1). These data indicate that it is possible to induce cellulase gene expression in the absence of an inducer in N. crassa. Under no carbon source conditions, transcript abundances of CAZy genes in the Pc2 strain were comparable with those observed in the WT strain shifted to Avicel (Fig. 5B). However, when Pc2 was transferred to fresh sucrose media, CCR strongly reduced CAZy expression, although it was elevated over no carbon conditions and far above that measured in the WT on sucrose.

The Nc2 cluster (42 genes) had expression an order of magnitude lower than WT in the Aclr-2 mutant on Avi-cel, but still had significant induction over the WT on no carbon. They also showed some induction in Pc2 on no carbon, but most did not reach the same abundances as in the WT on Avicel. These data suggest that the genes in Nc2 require another cellulose-dependent factor for full induction. The Nc2 cluster included one highly expressed cellobiohydrolase gh6-3 (NCU07190), the major intracellular b-glucosidase gh3-1 (NCU00130), and the cellodextrin transporter cdt-1 (NCU00801).

Figure 5. Cellulase gene expression and activity by misexpression of clr-2 in N. crassa. (A) K-means clusters of genes (Nc1-4) induced under Avicel or no carbon conditions in WT, under Avicel conditions in a Dclr-2 mutant and under no carbon media conditions for a strain with constitutive expression of clr-2 (Pc2). Heat map displays log (FPKM) scaled from min expression (bright blue) to the maximal expression (bright yellow). (B) Total expression of genes encoding major CAZy classes of Pc2 on sucrose versus no carbon media, as compared to WT on sucrose, no carbon media, or Avicel. Note the similarity in CAZy expression class in WT on Avicel versus the Pc2 strain on media lacking a carbon source. A Aclr-2 strain on Avicel shows a low induction of genes encoding some hemicellulases, due to slight contamination of Avicel with hemicellulose (Znameroski et al. 2012). (C) Coomasie-stained SDS PAGE gel of culture supernatants from WT, Dclr-2 (A), and Pc2 strains shifted to Avicel (4 days), sucrose (2 days), or media lacking a carbon source (2 days). Secreted proteins labeled from molecular weights and intensity patterns are derived from (Tian et al. 2009; Phillips et al. 2011b; Znameroski et al. 2012). Note similarity of secreted protein profile of the Pc2 strain grown on sucrose or no carbon as compared to Avicel-exposed WT and Pc2 cultures. (D) A time course of CMCase activity of supernatants from WT, Dclr-2, and Pc2 cultures after shift from sucrose pregrown cultures (16 h) to either Avicel or sucrose.

Avicel No C

(A) WT Aclr-2 WT Pc2

Nc2 Nc3 Nc4



1e6 ■

Aclr-2 Pc2 Avi Suc

Pc2 No C

(C) Avicel Sucrose No Carbon

Gene NCU#

gh74-1 5955 ncw-1 5137

gh3-4 4952 gh6-2 9680 chb-1 7340 gh5-1 0762-gh7-1 5057' gh6-3 7190 gh43-6 7326 gh10-1 5924'

kDa 140

WT Avi WT Suc

Aclr-2 Avi Aclr-2 Suc

—*— Pc2 Avi --it- - Pc2 Suc

Hours after media shift

The Nc3 cluster (33 genes) was fully to partially dependent on clr-2 for induction under Avicel conditions, but remained uninduced by misexpression of clr-2 in Pc2. This cluster was dominated by hypothetical proteins that had low expression levels, but notably included one b-glucosidase gene gh3-4 (NCU07487). The Nc4 cluster

(53 genes) was clr-2 independent and was not induced by misexpression of clr-2 in Pc2. This cluster was dominated by xylanases and the xylose utilization pathway genes, reflecting induction of these genes in a clr-2-independent manner by low concentrations of hemicellulose retained in Avicel (Znameroski et al. 2012).

When supernatants taken from Pc2 cultures 24 h after a shift to sucrose were analyzed with SDS PAGE, a similar protein pattern was observed to that seen in WT and Pc2 cultures shifted to Avicel (Fig. 5C). The secreted proteins were fully active, as demonstrated by CMCase activity of the sucrose shifted Pc2 supernatants (Fig. 5D). The mis-expression of clr-2 complemented the cellulose growth defect and cellulase gene induction in the D clr-2 strain under Avicel conditions and in fact, showed elevated levels of CMCase activity.

Misexpression of clrB and clr-2 in A. nidulans

Our data indicated that it is possible to produce and secrete cellulases under noninducing conditions by heter-ologous regulation of the transcriptional regulator, CLR-2. To test whether misexpression of clr-2 homologs is sufficient for inducer-free cellulase production and secretion in other ascomycete fungi, we inserted the clrB coding sequences into the pyrG locus of the A. nidulans AclrB strain under the regulation of the constitutive gpdA promoter (PgB). A strain carrying an N-terminal GFP-tagged allele (GFP-PgB) showed nuclear GFP fluorescence on glucose liquid medium (Fig. 6A); clrB driven by its own promoter showed no fluorescence (Fig. 6A; GFP-B). The gpdA-regulated expression of clrB restored cellulase gene induction, growth, and enzyme activity to the AclrB mutant on Avicel (Fig. 6C, D). Similar to the N. crassa

Figure 6. Phenotypes associated with misexpression of clrB or clr-2 in A. nidulans. (A) Localization of GFP-tagged constructs in cells germinated in liquid glucose medium. GFP-labeled ClrB under native promoter (strain GFP-B) had no detectable fluorescence. GFP-labeled ClrB or CLR-2 driven by the gpdA promoter (strain GFP-PgB and GFP-Pg2) accumulated in nuclei, which were clearly distinguishable by their shape and prominent nucleoli. Arrowheads indicate nuclei. (B) WT and misexpression strains grown 3 days on 1% glucose or 1 % ethanol plates at 30°C. PgB and Pg2: constitutive expression of clrB and clr-2, respectively, by the gpdA promoter in AclrB background. PaB and Pa2: ethanol-inducible expression of clrB and clr-2, respectively, by the alcA promoter in AclrB background. (C) Transcript abundance of two major cellulases (cbhD and cdh) in A. nidulans WT versus strains with constitutive expression of clrB (PgB) or clr-2 (Pg2) when shifted to glucose [G], no carbon media [NC], or Avicel [A] for 6 h. Transcript abundance relative to actA was measured with realtime quantitative RT-PCR. (D) A time course of CMCase activity in WT, AclrB, and PgB strains following a shift to either Avicel or sucrose.


AN1273 (cbhD) AN7230 (cdh)

G | NC | A WT


AclrB PgB Pg2

(D (0 TO

—•—WTAvi WT Suc

—X— AclrB Avi - -X- - AclrB Suc —•— PgB Avi --0-- PgB Suc

24 48 72

Hours after media shift

clr-2 misexpressed strain, the A. nidulans PgB strain showed higher CMCase activity over the 96-hr time course as compared with WT. However, CMCase activity was not significantly induced when the PgB strain was grown for extended periods of time under sucrose conditions (Fig. 6D). Consistent with this result, mRNA abundance for two ClrB-dependent genes was several orders of magnitude below that of a WT culture shifted to Avicel when the PgB strain was shifted from sucrose to no carbon conditions (Fig. 6C), although AN7230 (CDH) transcript abundance was detectably higher in PgB strain than the WT under no carbon conditions. These data indicate that, in contrast to N. crassa, misexpression of clrB in A. nidulans was not sufficient to induce WT levels of cellulase gene expression and enzyme activity.

We then tested whether the introduction of clr-2 could complement the DclrB mutant for the induction of cellu-lolytic genes under Avicel conditions. As for clrB, the clr-2 coding sequence was placed under the control of the gpdA (Pg2) or alcA (Pa2) promoter. An N-terminal GFP-tagged Pg2 allele showed nuclear localization during growth on glucose in the DclrB mutant (Fig. 6A). However, clr-2 was unable to complement the DclrB mutant for the induction of cellulolytic genes under Avicel conditions. Induction of cellulase gene expression under nonin-ducing conditions was also not observed (Fig. 6C). In fact, the Pg2 (gpdA-clr-2) showed a strong growth defect under all conditions (Fig. 6B), whereas the strain with clr-2 under control of the ethanol-inducible alcA promoter (Pa2) was severely deficient for growth on inducing ethanol media. In contrast, an ethanol-inducible clrB strain (PaB) grew well in both conditions, although detec-tably slower than WT on ethanol.


In all filamentous fungi studied to date, expression of cellulolytic genes requires both relief from CCR and the presence of an inducer molecule, such as cellobiose or cellodextrins, or in T. reesei, cellobiose, sophorose, lactose, or xylose (Sternberg and Mandels 1979; Stricker et al. 2006, 2007; Hakkinen et al. 2012), or xylose in the Aspergilli (Gielkens et al. 1999; Andersen et al. 2008; Noguchi et al. 2009). Several independent lines of mutagenesis have produced strains with increased cellulase production and decreased CCR (Peterson and Nevalainen 2012; Liu et al. 2013; Porciuncula et al. 2013), but constitutive, robust production of cellulases without inducing molecules has remained elusive over 30 years of mutagenesis-based research. Our data show that it is possible to produce and secrete cellulases under noninducing conditions by misexpression of the transcriptional regulator, CLR-2, the first report of a transcription factor necessary

and sufficient for cellulase activity in any cellulolytic filamentous fungus. This observation suggests new opportunities for optimization of cellulase enzyme production in industrial strains without the need for cellulosic substrates or other inducing molecules. A genetic "master switch" for cellulase secretion may be particularly useful in the many species for which there are no known soluble cellu-lase-inducing molecules and for which limited genetic tools make extensive genetic engineering impractical.

Misexpression of clr-2 in N. crassa resulted in inducer-independent production of plant cell wall degrading enzymes. In A. nidulans, misexpression of clrB produced no detectable enzyme activity under noninducing conditions, although RT-PCR analyses revealed a measurable increase in transcript abundance for a cellobiose dehydrogenase (AN7230). We therefore infer that there is a fundamental difference in cellulase gene induction between Neurospora and Aspergillus species. Whereas CLR-2 is fully competent to drive transcription of its targets in noninducing conditions in N. crassa, ClrB requires other factors for any significant effect. These observations beg the question: are differences in mechanisms of CLR-2/ClrB induction indicative of an ancient divergence between Sordariomycete and Eurotiomycete fungi? Or are they reflective of the different lifestyles and preferred substrates of these two species? The DNA binding and dimerization domain of the N-terminus of CLR-2 and ClrB show several regions of sequence divergence, which are conserved broadly in Sordariomycete versus Euroti-omycete species. The inability of clr-2 to complement a deletion of clrB in A. nidulans and differences in CLR-2/ ClrB amino acid sequence suggests divergence in regulatory mechanisms for cellulolytic genes.

Until recently, studies on regulation of plant cell wall deconstruction in Aspergillus species focused predominantly on induction by hemicellulosic sugars via the tran-scriptional regulator, XlnR (van Peij et al. 1998; Gielkens et al. 1999; Delmas et al. 2012). A. nidulans is more proficient at saccharification of xylan and relatively less effective at degrading crystalline cellulose than N. crassa. This phenotypic distinction was consistent with both relative expression and diversity of CAZy families between species, with A. nidulans specifically inducing more xylanases, b-mannases, and pectate lyases in particular. Together these data suggest that A. nidulans and perhaps other Aspergillus species have evolved to primarily utilize amorphous polymers over crystalline cellulose. Canonical cellulases may therefore serve a more accessory role for hemicellulolytic activity by synergistic action on complex substrates. In contrast, N. crassa has apparently evolved to rely more heavily on breakdown of crystalline cellulose via signaling to CLR-2. This regulatory aspect is likely conserved among members of the Sordariomycetes, as,

similar to N. crassa (Sun et al. 2012), DxlnR mutants of Fusarium graminearum and F. oxysporum are unable to utilize hemicellulose, but are unaffected in cellulose decon-struction (Brunner et al. 2007; Calero-Nieto et al. 2007).

Clustering analysis of transcript abundance in an N. crassa strain with constitutive expression of clr-2 suggests two modes of induction by CLR-2, one in which it acts independently and one in which it requires another cellulose-responsive factor to achieve full induction. In T. reesei and Aspergilli, the transcriptional regulator XYR1/ XlnR, respectively, regulates expression of hemicellulase and cellulase genes (Stricker et al. 2006; Mach-Aigner et al. 2008; Noguchi et al. 2009). In T. reesei, a noncon-served transcriptional activator, ACEII (Aro et al. 2001) as well as the repressor ACEI (Aro et al. 2003) also affect cellulase gene expression. Recently, several additional transcription factors have been reported to play a role in regulation of plant cell wall degrading enzymes in asco-mycete fungi, including BglR (T. reesei), which may influence CCR through regulation of genes encoding b-glucosidase enzymes (Nitta et al. 2012), ClbR (A. aculeatus), which is involved in XlnR-independent cellobiose and cellulose induction of cbh1 (GH7) and endoglucanase (cmc2) (Kunitake et al. 2012), and McmA (A. nidulans) which affected induction of endoglucanases (eglA and eglB) and at least one cellobiohydrolase (cbhA) (Yamakawa et al. 2013). The interactions of these factors with each other and with XLR-1/XlnR and CLR-2/ClrB homologs deserve further investigation. An understanding of conservation of function across the phylogenetic spectrum may provide insight into fungal interaction with the environment and guide the selection and manipulation of fungal host species for industrial enzyme production.

Our comparative transcriptional analysis of clr-2/clrB mutants revealed a conserved and essential role for these transcription factors in response to cellulose. Strict conserved dependence on CLR-2/ClrB was limited to a relatively small group of orthologs, indicating a relatively simple cohort of essential genes for broad-spectrum cellulose degradation. The conservation of regulation of this gene set between two distantly related saprotrophic fungi suggests that these enzymes/proteins are key to cellulose deconstruction strategies. Recently, a transcriptional regulator (ManR) of beta-mannan utilization in Aspergillus oryzae was described (Ogawa et al. 2012). ManR is, in fact, the A. oryzae ortholog of ClrB and was recently shown to be essential for the regulation of cellulolytic genes (Ogawa et al. 2013). These results further confirm a conserved role for Clr-2/ClrB in regulation of synergistic ensemble of enzymes in response to plant cell wall poly-saccharides in diverse ascomycete fungi.

A large group of genes encoding CAZy proteins within the CLR-2/ClrB regulons showed low sequence conserva-

tion or very low expression in either N. crassa or A. nidulans. These observations are consistent with the large variability in numbers and types of genes encoding predicted plant cell wall degrading enzymes in the genomes of filamentous ascomycete species (Espagne et al. 2008; Berka et al. 2011; Hakkinen et al. 2012). These genes likely serve accessory functions in plant cell wall degradation that may be specific to a particular species' ecological niche. Interestingly, we also observed coregulation of secondary metabolism genes with cellulolytic genes and which were partially dependent upon functional ClrB. Further comparisons of gene regulation across a wider panel of fungal species with varied ecological niches and different preferred substrates may provide insights into the adaptive advantages conferred by proteins/enzymes encoded by these genes.

The polysaccharide monooxygenase enzyme class is an example of divergent regulation across these species. Our data in A. nidulans and published data on A. niger indicate that a single gene of the type-3 PMO subclass dominates expression in Aspergillus species exposed to cellulose (this study) or wheat straw (Delmas et al. 2012). In contrast, a spectrum of type-1, type-2, and type-3 PMOs are expressed in N. crassa on Avicel and on bagasse for the closely related thermophilic industrial species, M. thermo-phila (Gusakov 2011; Visser et al. 2011) and Thielavia terrestris (Berka et al. 2011). This divergent regulation of PMOs may hold clues to an as-yet-unappreciated functional difference in subclasses of these enzymes; a recent study identified distinct product chemistries from a type-1 and type-3 PMOs (Bey et al. 2013). Comparative analyses of enzyme cocktails in diverse filamentous fungi enabled by transcriptomic and proteomic approaches, which in some cases will be expedited by misexpression of CLR-2 homologs, will advance efforts to define tailored enzyme mixtures for maximal efficiency on different lig-nocellulosic feedstocks for biofuels and production of value-added chemicals.


This work was supported by a grant from Energy Biosciences Institute to N. L. G. and National Institutes of Health NRSA Trainee Grant #2 T32 GM 7127-36 A1 to S. T. C.

Conflict of Interest

None declared. References

Anders, S., and W. Huber. 2010. Differential expression analysis for sequence count data. Genome Biol. 11:R106

Andersen, M. R., W. Vongsangnak, G. Panagiotou, M. P. Salazar, L. Lehmann, and J. Nielsen. 2008. A trispecies Aspergillus microarray: comparative transcriptomics of three Aspergillus species. Proc. Natl. Acad. Sci. USA 105:43874392.

Aro, N., A. Saloheimo, M. IImen, and M. Penttila. 2001. ACEII, a novel transcriptional activator involved in regulation of cellulase and xylanase genes of Trichoderma reesei. J. Biol. Chem. 276:24309-24314.

Aro, N., M. IImen, A. Saloheimo, and M. Penttila. 2003. ACEI of Trichoderma reesei is a repressor of cellulase and xylanase expression. Appl. Environ. Microbiol. 69:56-65.

Aro, N., T. Pakula, and M. Penttila. 2005. Transcriptional regulation of plant cell wall degradation by filamentous fungi. FEMS Microbiol. Rev. 29:719-739.

Beeson, W. T., A. T. Iavarone, C. D. Hausmann, J. H. Cate, and M. A. Marletta. 2011. Extracellular aldonolactonase from Myceliophthora thermophila. Appl. Environ. Microbiol. 77:650-656.

Beeson, W. T., C. M. Phillips, J. H. D. Cate, and

M. A. Marletta. 2012. Oxidative cleavage of cellulose by fungal copper-dependent polysaccharide monooxygenases. J. Am. Chem. Soc. 134:890-892.

Berka, R. M., I. V. Grigoriev, R. Otillar, A. Salamov, J. Grimwood, I. Reid, et al. 2011. Comparative genomic analysis of the thermophilic biomass-degrading fungi Myceliophthora thermophila and Thielavia terrestris. Nat. Biotechnol. 29:922-927.

Bey, M., S. M. Zhou, L. Poidevin, B. Henrissat, P. M. Coutinho, J. G. Berrin, et al. 2013. Cello-oligosaccharide oxidation reveals differences between two lytic polysaccharide monooxygenases (family GH61) from Podospora anserina. Appl. Environ. Microbiol. 79:488-496.

Brunner, K., A. M. Lichtenauer, K. Kratochwill, M. Delic, and R. L. Mach. 2007. Xyr1 regulates xylanase but not cellulase formation in the head blight fungus Fusarium graminearum. Curr. Genet. 52:213-220.

Calero-Nieto, F., A. Di Pietro, M. I. G. Roncero, and C. Hera. 2007. Role of the transcriptional activator XInR of Fusarium oxysporum in regulation of xylanase genes and virulence. Mol. Plant Microbe Interact. 20:977-985.

Cantarel, B. L., P. M. Coutinho, C. Rancurel, T. Bernard, V. Lombard, and B. Henrissat. 2009. The Carbohydrate-Active EnZymes database (CAZy): an expert resource for glycogenomics. Nucleic Acids Res. 37:D233-D238.

Colot, H. V., G. Park, G. E. Turner, C. Ringelberg, C. M. Crew, L. Litvinkova, et al. 2006. A high-throughput gene knockout procedure for Neurospora reveals functions for multiple transcription factors. Proc. Natl. Acad. Sci. USA 103:1035210357.

Coradetti, S. T., J. P. Craig, Y. Xiong, T. Shock, C. G. Tian, and N. L. Glass. 2012. Conserved and essential transcription factors for cellulase gene expression in ascomycete fungi. Proc. Natl. Acad. Sci. USA 109:7397-7402.

Delmas, S., S. T. Pullan, S. Gaddipati, M. Kokolski, S. Malla, M. J. Blythe, et al. 2012. Uncovering the genome-wide transcriptional responses of the filamentous fungus Aspergillus niger to lignocellulose using RNA sequencing. PLoS Genet. 8:e1002875.

Du, J., S. Li, and H. Zhao. 2010. Discovery and

characterization of novel d-xylose-specific transporters from Neurospora crassa and Pichia stipitis. Mol. BioSyst. 6:21502156.

Elvin, M., J. J. Loros, J. C. Dunlap, and C. Heintzen. 2005. The PAS/LOV protein VIVID supports a rapidly dampened daytime oscillator that facilitates entrainment of the Neurospora circadian clock. Genes Dev. 19:2593-2605.

Espagne, E., O. Lespinet, F. Malagnac, C. Da Silva, O. Jaillon, B. M. Porcel, et al. 2008. The genome sequence of the model ascomycete fungus Podospora anserina. Genome Biol. 9:R77.

Floudas, D., M. Binder, R. Riley, K. Barry, R. A. Blanchette, B. Henrissat, et al. 2012. The Paleozoic origin of enzymatic lignin decomposition reconstructed from 31 fungal genomes. Science 336:1715-1719.

Frey, S. D., J. Six, and E. T. Elliott. 2003. Reciprocal transfer of carbon and nitrogen by decomposer fungi at the soil-litter interface. Soil Biol. Biochem. 35:1001-1004.

Galagan, J. E., S. E. Calvo, K. A. Borkovich, E. U. Selker, N. D. Read, D. Jaffe, et al. 2003. The genome sequence of the filamentous fungus Neurospora crassa. Nature 422:859-868.

Galagan, J. E., S. E. Calvo, C. Cuomo, L. J. Ma, J. R. Wortman, S. Batzoglou, et al. 2005. Sequencing of Aspergillus nidulans and comparative analysis with A. fumigatus and A. oryzae. Nature 438:1105-1115.

Galazka, J. M., C. G. Tian, W. T. Beeson, B. Martinez, N. L. Glass, and J. H. D. Cate. 2010. Cellodextrin transport in yeast for improved biofuel production. Science 330:84-86.

Gielkens, M. M., E. Dekkers, J. Visser, and L. H. de Graaff. 1999. Two cellobiohydrolase-encoding genes from Aspergillus niger require D-xylose and the xylanolytic transcriptional activator XlnR for their expression. Appl. Environ. Microbiol. 65:4340-4345.

Gusakov, A. V. 2011. Alternatives to Trichoderma reesei in biofuel production. Trends Biotechnol. 29:419-425.

Hakkinen, M., M. Arvas, M. Oja, N. Aro, M. Penttila, M. Saloheimo, et al. 2012. Re-annotation of the CAZy genes of Trichoderma reesei and transcription in the presence of lignocellulosic substrates. Microb. Cell Fact. 11:134.

Heimann, M., and M. Reichstein. 2008. Terrestrial ecosystem carbon dynamics and climate feedbacks. Nature 451:289-292.

Hieber, M., and M. O. Gessner. 2002. Contribution of stream detrivores, fungi, and bacteria to leaf breakdown based on biomass estimates. Ecology 83:1026-1038.

de Hoon, M. J., S. Imoto, J. Nolan, and S. Miyano. 2004. Open source clustering software. Bioinformatics 20:14531454.

Klich, M. A. 2002. Biogeography of Aspergillus species in soil and litter. Mycologia 94:21-27.

Kominkova, D., K. A. Kuehn, N. Busing, D. Steiner, and M. O. Gessner. 2000. Microbial biomass, growth, and respiration associated with submerged litter of Phragmites australis decomposing in a littoral reed stand of a large lake. Aquat. Microb. Ecol. 22:271-282.

Konno, N., K. Igarashi, N. Habu, M. Samejima, and A. Isogai. 2009. Cloning of the Trichoderma reesei cDNA encoding a glucuronan lyase belonging to a novel polysaccharide lyase family. Appl. Environ. Microbiol. 75:101-107.

Kunitake, E., S. Tani, J. I. Sumitani, and T. Kawaguchi. 2012. A novel transcriptional regulator, ClbR, controls the cellobiose- and cellulose-responsive induction of cellulase and xylanase genes regulated by two distinct signaling pathways in Aspergillus aculeatus. Appl. Microbiol. Biotechnol. 97:2017-2028.

Langmead, B., C. Trapnell, M. Pop, and S. L. Salzberg. 2009. Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 10: R25.

Li, X., W. T. Beeson, C. M. Phillips, M. A. Marletta, and J. H. Cate. 2012. Structural basis for substrate targeting and catalysis by fungal polysaccharide monooxygenases. Structure 20:1051-1061.

Liu, G., L. Zhang, Y. Qin, G. Zou, Z. Li, X. Yan, et al. 2013. Long-term strain improvements accumulate mutations in regulatory elements responsible for hyper-production of cellulolytic enzymes. Sci. Rep. 3:1569.

Mach, L., and S. Zeilinger. 2003. Regulation of gene expression in industrial fungi: Trichoderma. Appl. Microbiol. Biotechnol. 60:515-522.

Mach-Aigner, A. R., M. E. Pucher, M. G. Steiger, G. E. Bauer, and R. L. Mach. 2008. Transcriptional regulation of xyr1, encoding the main regulator of the xylanolytic and cellulolytic enzyme system in Hypocrea jecorina. Appl. Environ. Microbiol. 74:6554-6562.

Margeot, A., B. Hahn-Hagerdal, M. Edlund, R. Slade, and F. Monot. 2009. New improvements for lignocellulosic ethanol. Curr. Opin. Biotechnol. 20:372-380.

McCluskey, K. 2003. The fungal genetics stock center from molds to molecules. Adv. Appl. Microbiol. 52:245-262.

Nayak, T., E. Szewczyk, C. E. Oakley, A. Osmani, L. Ukil, S. L. Murray, et al. 2006. A versatile and efficient gene-targeting system for Aspergillus nidulans. Genetics 172:1557-1566.

Nitta, M., T. Furukawa, Y. Shida, K. Mori, S. Kuhara, Y. Morikawa, et al. 2012. A new Zn(II)(2)Cys(6)-type transcription factor BglR regulates beta-glucosidase expression in Trichoderma reesei. Fungal Genet. Biol. 49:388-397.

Noguchi, Y., M. Sano, K. Kanamaru, T. Ko, M. Takeuchi, M. Kato, et al. 2009. Genes regulated by AoXlnR, the xylanolytic and cellulolytic transcriptional regulator, in Aspergillus oryzae. Appl. Microbiol. Biotechnol. 85:141-154.

Ogawa, M., T. Kobayashi, and Y. Koyama. 2012. ManR, a novel Zn(II)2Cys6 transcriptional activator, controls the

beta-mannan utilization system in Aspergillus oryzae. Fungal Genet. Biol. 49:987-995.

Ogawa, M., T. Kobayashi, and Y. Koyama. 2013. ManR, a transcriptional regulator of the beta-mannan utilization system, controls the cellulose utilization system in Aspergillus oryzae. Biosci. Biotechnol. Biochem. 77:426-429.

van Peij, N. N. M. E., M. M. C. Gielkens, R. P. de Vries, J. Visser, and L. H. de Graaff. 1998. The transcriptional activator XlnR regulates both xylanolytic and endoglucanase gene expression in Aspergillus niger. Appl. Environ. Microbiol. 64:3615-3619.

Perkins, D. D., and B. C. Turner. 1988. Neurospora from natural populations: toward the population biology of a haploid eukaryote. Exp. Mycol. 12:91-131.

Peterson, R., and H. Nevalainen. 2012. Trichoderma reesei RUT-C30-thirty years of strain improvement. Microbiology 158:58-68.

Phillips, C. M., W. T. Beeson, J. H. Cate, and M. A. Marletta. 2011a. Cellobiose dehydrogenase and a copper-dependent polysaccharide monooxygenase potentiate cellulose degradation by Neurospora crassa. ACS Chem. Biol. 6:1399-1406.

Phillips, C. M., A. T. Iavarone, and M. A. Marletta. 2011b. Quantitative proteomic approach for cellulose degradation by Neurospora crassa. J. Proteome Res. 10:4177-4185.

Porciuncula, J., T. Furukawa, K. Mori, Y. Shida, H. Hirakawa, K. Tashiro, et al. 2013. Single nucleotide polymorphism analysis of a Trichoderma reesei hyper-cellulolytic mutant developed in Japan. Biosci. Biotechnol. Biochem. 77:534543.

Portnoy, T., A. Margeot, R. Linke, L. Atanasova, E. Fekete, E. Sandor, et al. 2011. The CRE1 carbon catabolite repressor of the fungus Trichoderma reesei: a master regulator of carbon assimilation. BMC Genomics 12:269.

Punt, P. J., M. A. Dingemanse, A. Kuyvenhoven, R. D. Soede, P. H. Pouwels, and C. A. van den Hondel. 1990. Functional elements in the promoter region of the Aspergillus nidulans gpdA gene encoding glyceraldehyde-3-phosphate dehydrogenase. Gene 93:101-109.

Quinlan, R. J., M. D. Sweeney, L. Lo Leggio, H. Otten, J. C. Poulsen, K. S. Johansen, et al. 2011. Insights into the oxidative degradation of cellulose by a copper metalloenzyme that exploits biomass components. Proc. Natl. Acad. Sci. USA 108:15079-15084.

Roberts, A., C. Trapnell, J. Donaghey, J. L. Rinn, and L. Pachter. 2011. Improving RNA-Seq expression estimates by correcting for fragment bias. Genome Biol. 12:R22.

Ruijter, G. J., and J. Visser. 1997. Carbon repression in Aspergilli. FEMS Microbiol. Lett. 151:103-114.

Sternberg, D., and G. R. Mandels. 1979. Induction of cellulolytic enzymes in Trichoderma reesei by sophorose. J. Bacteriol. 139:761-769.

Stricker, A. R., K. Grosstessner-Hain, E. Wurleitner, and

R. L. Mach. 2006. Xyr1 (xylanase regulator 1) regulates both

the hydrolytic enzyme system and D-xylose metabolism in Hypocrea jecorina. Eukaryot. Cell 5:2128-2137.

Stricker, A. R., M. G. Steiger, and R. L. Mach. 2007. Xyr1 receives the lactose induction signal and regulates lactose metabolism in Hypocrea jecorina. FEBS Lett. 581: 3915-3920.

Sun, J. P., and N. L. Glass. 2011. Identification of the CRE-1 cellulolytic regulon in Neurospora crassa. PLoS ONE 6:e25654.

Sun, J. P., C. G. Tian, S. Diamond, and N. L. Glass. 2012. Deciphering transcriptional regulatory mechanisms associated with hemicellulose degradation in Neurospora crassa. Eukaryot. Cell 11:482-493.

Szewczyk, E., T. Nayak, C. E. Oakley, H. Edgerton, Y. Xiong, N. Taheri-Talesh, et al. 2006. Fusion PCR and gene targeting in Aspergillus nidulans. Nat. Protoc. 1:3111-3120.

Tian, C., W. T. Beeson, A. T. Iavarone, J. Sun, M. A.

Marletta, J. H. Cate, et al. 2009. Systems analysis of plant cell wall degradation by the model filamentous fungus Neurospora crassa. Proc. Natl. Acad. Sci. USA 106:2215722162.

Updegraff, D. M. 1969. Semimicro determination of cellulose in biological materials. Anal. Biochem. 32:420-424.

Vishniac, W., and M. Santer. 1957. The thiobacilli. Bacteriol. Rev. 21:195-213.

Visser, H., V. Vivi, P.J. Punt, A.V. Gusakov, P.T. Olson, R. Joosten, et al. 2011. Development of a mature fungal technology and production platform for industrial enzymes based on a Myceliophthora thermophila isolate, previously

known as Chrysosporium lucknowense C1. Ind. Biotechnol. 7:214-223.

Vogel, H. 1956. A convenient growth medium for Neurospora

(medium N). Microb. Genet. Bull. 13:2-43. Waring, R. B., G. S. May, and N. R. Morris. 1989. Characterization of an inducible expression system in Aspergillus nidulans using alcA and tubulin-coding genes. Gene 79:119-130. Yamakawa, Y., Y. Endo, N. Li, M. Yoshizawa, M. Aoyama, A. Watanabe, et al. 2013. Regulation of cellulolytic genes by McmA, the SRF-MADS box protein in Aspergillus nidulans. Biochem. Biophys. Res. Commun. 431:777-782. Zhou, Q., J. Xu, Y. Kou, X. Lv, X. Zhang, G. Zhao, et al. 2012. Differential involvement of beta-glucosidases from Hypocrea jecorina in rapid induction of cellulase genes by cellulose and cellobiose. Eukaryot. Cell 11:1371-1381. Znameroski, E. A., S. T. Coradetti, C. M. Roche, J. C. Tsai, A. T. Iavarone, J. H. D. Cate, et al. 2012. Induction of lignocellulose-degrading enzymes in Neurospora crassa by cellodextrins. Proc. Natl. Acad. Sci. USA 109:6012-6017.

Supporting Information

Additional Supporting Information may be found in the online version of this article:

Data S1. Excel spreadsheet of expression profiling data from Neurospora crassa and Aspergillus nidulans.