- Open Access
Deletion of either the regulatory gene ara1 or metabolic gene xki1 in Trichoderma reesei leads to increased CAZyme gene expression on crude plant biomass
Biotechnology for Biofuels volume 12, Article number: 81 (2019)
Trichoderma reesei is one of the major producers of enzymes for the conversion of plant biomass to sustainable fuels and chemicals. Crude plant biomass can induce the production of CAZymes in T. reesei, but there is limited understanding of how the transcriptional response to crude plant biomass is regulated. In addition, it is unknown whether induction on untreated recalcitrant crude plant biomass (with a large diversity of inducers) can be sustained for longer. We investigated the transcriptomic response of T. reesei to the two industrial feedstocks, corn stover (CS) and soybean hulls (SBH), over time (4 h, 24 h and 48 h), and its regulatory basis using transcription factor deletion mutants (Δxyr1 and Δara1). We also investigated whether deletion of a xylulokinase gene (Δxki1) from the pentose catabolic pathway that converts potential inducers could lead to increased CAZyme gene expression.
By analyzing the transcriptomic responses using clustering as well as differential and cumulative expression of plant biomass degrading CAZymes, we found that corn stover induced a broader range and higher expression of CAZymes in T. reesei, while SBH induced more pectinolytic and mannanolytic transcripts. XYR1 was the major TF regulating CS utilization, likely due to the significant amount of d-xylose in this substrate. In contrast, ARA1 had a stronger effect on SBH utilization, which correlates with a higher abundance of l-arabinose in SBH that activates ARA1. Blocking pentose catabolism by deletion of xki1 led to higher expression of CAZyme encoding genes on both substrates at later time points. Surprisingly, this was also observed for Δara1 at later time points. Many of these genes were XYR1 regulated, suggesting that inducers for this regulator accumulated over time on both substrates.
Our data demonstrates the complexity of the regulatory system related to plant biomass degradation in T. reesei and the effect the feedstock composition has on this. Furthermore, this dataset provides leads to improve the efficiency of a T. reesei enzyme cocktail, such as by the choice of substrate or by deleting xki1 to obtain higher production of plant biomass degrading CAZymes.
Plant biomass is the most abundant renewable carbon source on Earth for conversion into biofuel and biochemicals by the biotechnology industry. It is composed of three major polysaccharides (cellulose, hemicellulose and pectin), and many different plant biomass degrading (PBD) enzymes are required for efficient degradation . Trichoderma reesei (Hypocrea jecorina) is a cellulolytic filamentous saprobic fungus that has been used in biotechnology for many decades, mainly for cellulase production . Major developments for industrial applications were reviewed previously , such as the improved-cellulase producer QM9414 strain or the hypersecreting RUT C30 strain (CCR derepressed, due to a partial truncation of CRE1) . The disaccharide lactose is the primary industrial inducer of T. reesei cellulase production, but induction by crude plant biomass is a promising alternative. However, a challenge remains to sustain induction when the limited inducers that are available have been consumed. Sustaining induction for longer time periods will lead to higher overall CAZyme yields as well as a more diverse array of CAZymes and reduce enzyme production costs.
While T. reesei has been suggested as a model to study plant biomass degradation , its strategy to degrade plant biomass differs from most other saprobes studied so far, as its genome encodes a narrow set of enzymes, some of which (e.g., several cellulases) are produced at high levels . Its molecular mechanisms for the production of plant biomass degrading enzymes and sugar catabolism have been studied [7,8,9,10], demonstrating that XYR1 is the major cellulolytic and xylanolytic regulator , but also involved in d-xylose and (partially) l-arabinose catabolism. A second regulator, ARA1, regulates l-arabinose and d-galactose releasing as well as catabolic enzymes in response to l-arabinose and d-galactose .
Carbon catabolism related to plant biomass conversion has been studied in many fungi and recently reviewed . Carbon catabolism in T. reesei is peculiar, as, more enzymes play a role in multiple catabolic pathways, compared to several other saprobes . For example, the T. reesei pentose catabolic pathway (PCP) and the d-galactose oxido-reductive pathway share three enzymes (Fig. 1), and each of these pathways are regulated by both XYR1 and ARA1 . When genes of carbon catabolic pathways are deleted, this can lead to the accumulation of metabolites, which can function as inducers. In Aspergillus niger, a xylulokinase mutant (where the last step of the PCP is blocked), resulted in accumulation of inducers, such as xylitol and l-arabitol . In T. reesei, xylitol and l-arabitol accumulation was observed in deletion strains (Δxyl1, Δlad1 and Δlxr3) of three earlier steps of the PCP . While there are no reports of the effect of a full deletion of the final step of the PCP, the xylulokinase (XKI1), its antisense inhibition increased xylitol production in T. reesei .
Transcriptomics is a sensitive tool to probe complex regulatory events, but only a few T. reesei transcriptomics studies have been performed using crude plant biomass [15,16,17], while others used polymers or mono- and disaccharides . In particular, only one transcriptomic study analyzed a regulatory mutant (Δxyr1) using crude plant biomass (wheat bran) , whereas no catabolic mutants have been analyzed by transcriptomics using crude plant biomass. This previous study, analyzing only a single time point, identified a set of genes regulated by XYR1 (including not only (hemi-)cellulolytic genes, but also genes encoding non-enzymatic cellulose active enzymes, sugar transporters and heat shock proteins) . Analysis across multiple time points is required to uncover the dynamic changes in gene expression patterns as the crude plant biomass is degraded by the fungus.
In this study, we analyzed the transcriptome of T. reesei during growth on the two industrial substrates soybean hulls (SBH) and corn stover (CS) over time, using two regulatory mutants (Δxyr1 and Δara1) and one metabolic mutant (Δxki1). These two substrates have different polysaccharide compositions [19, 20], allowing us to deeply explore how the regulatory system responds to a wide array of sugar inducers released from these polysaccharides. CS is richer in hemicellulose, particularly arabinoxylan, while SBH is richer in pectin, xyloglucan and mannan (Additional file 1). This study resulted in three main findings. T. reesei had higher and broader transcript levels of PBD CAZyme genes when cultured on CS. ARA1 had a larger role in the regulation of PBD transcripts on SBH compared to XYR1, which was the major TF regulating plant biomass degradation in CS. The block of pentose catabolism (by deletion of xki1 from the PCP) led to higher PBD CAZyme expression at later time points in the CS and SBH cultures.
The regulatory and catabolic mutants had severely reduced growth on pure mono- and polysaccharides compared to the reference strain, but not on crude plant biomass
Three T. reesei deletion mutants (Δxyr1, Δara1 and Δxki1) were phenotypically compared to the reference strain QM9414 by growth on various carbon sources, including mono- and disaccharides, polymers and crude plant biomass (Fig. 2). As reported previously [21, 22], deletion of xyr1 most severely affected growth on d-xylose, less severely on lactose and to an even lesser extent on l-arabinose, xylitol, arabinan and arabinoxylan (Fig. 2). Deletion of ara1 abolished growth on d-galactose and reduced growth on l-arabinose, l-arabitol, while growth on d-xylose, arabinan, arabinoxylan and lactose was not affected (Fig. 2). Deletion of the xylulokinase xki1 resulted in strongly reduced growth on d-xylose and to a lesser extent on l-arabinose and xylitol, while growth on l-arabitol was abolished (Fig. 2). In all three deletion strains, strong growth reduction was only observed on specific mono- and polysaccharides, but not on crude plant biomass (Fig. 2), perhaps reflecting the diversity of nutrients available in plant biomass and highlighting the complex regulatory network during growth on crude substrates.
The T. reesei reference strain expressed PBD CAZymes at higher levels on corn stover than on soybean hulls
CS or SBH cultures from transfer experiment were sampled after 4, 24 and 48 h for transcriptome analysis that focused on genes encoding PBD CAZymes, carbon catabolic enzymes and related TFs (Additional file 4). To investigate the adaptation to each substrate, we initially compared the PBD CAZyme transcriptome profiles by clustering all six conditions of the reference strain (Fig. 3). The 4 h and 24 h CS samples clearly separated from the other samples, while the 4 h SBH sample was also distant from the remaining samples (Fig. 3). Interestingly, the 24 h and 48 h SBH samples clustered with the 48 h CS sample (Fig. 3), and overall had less highly expressed genes than the other samples. This suggests that during growth on SBH the inducing compounds were more quickly removed from the cultures than on CS.
Deep transcriptomic analysis (Fig. 4), in terms of which PBDs were induced and the level of total expression, helped to elucidate the patterns found in the PBD CAZymes cluster analysis (Fig. 3). CS induced more as well as higher total expression of cellulolytic and xylanolytic genes (Fig. 4a, b). In contrast, SBH induced more as well as higher total expression of mannanolytic, amylolytic and pectinolytic genes at the initial stage (4 h) (Fig. 4). This indicates that T. reesei is able to sense the major inducers from each substrate, adapting the expression of PBD CAZyme encoding genes to the substrate composition.
CS induced more PBD CAZyme encoding genes compared to SBH (Fig. 3) and to a higher level of total expression at all three time points (Fig. 4). The peak of PBD CAZyme gene expression on CS was at 4 h where the total expression of xylanolytic genes was highest (such as xyn1/2/3/4, bxl1, aes1, agu1 and abf2) (Fig. 4b, Additional file 4), while cellulolytic gene expression was highest at 24 h (e.g., cbh1/2, egl1/2/3//5 and two LPMOs egl4 and cel61b) (Fig. 4b, Additional file 4). In general, in both substrates, the number of induced PBD CAZyme encoding genes and the total expression level decreased over time (Fig. 4), with a steeper decline over time in the total expression on SBH compared to CS (Fig. 4). The decrease over time led to a total level of PBD CAZyme gene expression at 48 h on both substrates that is comparable to the level in the d-fructose pre-cultures (Figs. 3, 4b) indicating that at 48 h little or no inducers were present in the cultures from both substrates. Considering that studies in A. niger [23, 24] and T. reesei  indicated that inducer concentrations below 1 mM already activate the regulatory systems, this suggests that in fact no inducers are present anymore.
Total expression of carbon catabolic genes in CS and SBH followed the PBD cellulolytic gene expression matches with CAZyme patterns where the expression decreased over time in both substrates, but for this gene group the total expression was comparable in both substrates at the same time point (Fig. 5). Similar to what was observed for the CAZyme genes, a more clear adaptation to substrate composition was observed at 4 h than at the later time points (Fig. 5). The total expression of genes involved in both the PCP and d-galactose oxido-reductive pathway (xyl1, lad1 and xdh1) was higher in CS, while in SBH the total expression of the l-rhamnose pathway was higher (Fig. 5b). Transcriptional regulator encoding genes appeared to be similarly induced in both substrates (Fig. 6), but small differences were observed that also correlated with the composition of the substrates. CS induced more highly xyr1 and ace3 (both (hemi-)cellulolytic activators [26, 27]), while SBH higher expressed rhr1 (ortholog of the A. niger rhamnose responsive regulator rhaR ) after 4 h, as well as xpp1 (xylanase repressor ). The two substrates demonstrated clear differences in their induction pattern and physiological response and this led us to initially analyze the effects of the three deletion mutants by each substrate separately and then compare these analyses.
XYR1 is the major TF regulating the degradation of corn stover, while ARA1 more strongly affects soybean hulls utilization
We initially analyzed the secretome profiles of the reference strain and what we considered phenotypically the most extreme mutant, Δxyr1, by SDS-PAGE gel analysis on later time points (24 h and 48 h), where we expected to see clear patterns. T. reesei reference strain secreted a different protein pattern in each substrate, where CS showed more intense bands especially around 25 kDa. According to our expectations, xyr1 deletion caused a severe secretome reduction in terms of bands intensity and range, in both substrates (Additional file 6).
Clustering analysis showed that in CS, the 4 h and 24 h samples of the reference, Δara1 and Δxki1 cluster as two related, time-dependent clusters, indicating that overall these strains behave very similar during growth on CS (Fig. 7). At 48 h, these strains still cluster together, but are now related to the 24 h and 48 h samples of Δxyr1, characterized by an overall reduction in gene expression compared to the reference strain at the earlier time points (Fig. 7). The 4 h sample of Δxyr1 is clearly distinct from the other samples, with also an overall low expression of the CAZyme genes, but with some genes that are still higher expressed than at later time points in this strain. The results, therefore, support a central role for XYR1 in degradation of CS.
A very different pattern was observed on SBH. Initially, there appears to be only a minor effect of xyr1 as at 4 h, the Δxyr1 sample clusters with the 4 h reference strain sample (Fig. 8). However, at later time points the Δxyr1 samples are again characterized by overall very low gene expression compared to the reference strain at the earlier time point. The 4 h samples of Δara1 and Δxki1 cluster together, but distant from the reference strain and Δxyr1 at this time point. However, they have some similarity to the later time points of Δxyr1, characterized by a low expression of part of the CAZyme genes (Fig. 8). Some genes that are lowly expressed in the Δara1 and Δxki1 strain at 4 h increase strongly in expression at the later time points, especially at 48 h, but this is not (Δxyr1) or much less (reference strain) the case for the other strains. Overall, ARA1 appears to have a stronger role in SBH degradation, especially at the early time points. Interestingly, the metabolic mutant always clustered with Δara1 at each time point on both substrates (Figs. 7, 8), which was unexpected, as the Δxki1 was expected to result in inducer accumulation and, therefore, upregulation of the ARA1 and XYR1 target genes, while Δara1 was expected to reduce expression of a subset of those genes.
More detailed analysis confirmed that Δxyr1 was the regulatory mutant more affected in CS, resulting in a lower total expression and number of PBD CAZymes in every time point (Fig. 9a, b). In contrast to CS, on SBH the xyr1 deletion had a smaller effect on the response in all of the time points compared to the other mutants, in terms of number of PBD CAZymes induced and their total expression level (Fig. 9c, d). In SBH the biggest reduction in gene expression for Δxyr1 was observed at 4 h, but only approximately half of the PBD CAZyme genes were affected compared to CS and the total expression level was similar to the reference (Fig. 9). The ara1 deletion had a much smaller effect on gene expression on CS, confirming the higher importance of XYR1 in CS utilization (Fig. 9a, b).
The number of PBD CAZymes affected in both of regulatory mutants after 4 h on CS was similar but the total expression level in Δara1 was still comparable to the reference (Fig. 9a, b). This was mainly due to xylanolytic genes, which remained expressed in Δara1, but were severely affected in Δxyr1. At 4 h in CS, carbon catabolism was also affected by both mutations. The PCP genes were lowly expressed in both regulatory mutants, but the d-galactose Leloir and oxido-reductive pathways were affected more by the ara1 deletion, while l-rhamnose and d-galacturonic pathways were affected only by the ara1 deletion (Fig. 10a, b).
Similar to CS, the initial response on SBH was also affected by both regulatory mutants, but the effect was larger for Δara1 than for Δxyr1 (Fig. 9c, d). In Δara1 induction of mannanolytic and pectinolytic genes were particularly reduced (Fig. 9c, d). In addition, genes of the PCP, both d-galactose pathways and the d-galacturonic acid pathway (only at 4 h) were severely reduced in Δara1, while the l-rhamnose pathway genes were not or lowly expressed in Δara1 (Fig. 10c, d). These pathways were not substantially affected in the xyr1 mutant on SBH. This indicates that Δara1 was not/less able to catabolize or release d-galactose, l-arabinose and l-rhamnose, confirming that ARA1 has a larger effect on SBH utilization than XYR1.
Surprisingly, in contrast to Δxyr1 and the initial response, at 24 h in CS and 24 h and 48 h in SBH Δara1 induced more PBD CAZymes and to a higher level compared to the reference (Fig. 9). The same phenomenon was observed also for the Δxki1 strain and will be described in the following section.
Deletion of xki1 or ara1 leads to higher expression of cellulolytic and xylanolytic genes in soybean hulls and corn stover
Clustering analysis (Figs. 7, 8) showed that Δxki1 and Δara1 samples always clustered together and by time point in both substrates, suggesting a similar response from each of the mutants, which was confirmed by transcriptomic analysis where PBD CAZyme genes (Fig. 9) and carbon catabolic genes (Fig. 10) were similarly expressed. In Δxki1 and Δara1, the initial responses (4 h) to both substrates was severely affected, while at later time points (24 h in CS, 24 h and 48 h in SBH) more PBD CAZyme genes were induced and at higher level compared to the reference (Fig. 9). Remarkably, Δxki1 appeared to be more extreme in its responses to both substrates compared to Δara1 (Fig. 9). The Δxki1 initial reduction in gene expression (4 h) to both substrates, but especially on CS, was more affected than that of Δara1, while during the PBD CAZyme gene expression peaks (24 h in CS, 24 h and 48 h in SBH) more PBD CAZyme genes were highly expressed compared to Δara1 (Fig. 9a, c). At these time points, and especially in SBH, genes of the PCP, d-galactose pathways and d-galacturonic acid pathway were also higher expressed in both strains (Fig. 10b, d). Many of the genes that were upregulated in one or both of the strains (Δxki1 and/or Δara1) and substrates (CS and/or SBH) are mainly regulated by XYR1 (Table 1).
In CS at 24 h (where the PBD CAZyme gene expression peaked) in both strains, mainly cellulolytic and xylanolytic genes, but also a few pectinolytic genes were more induced, while additionally in Δxki1 a few xyloglucanolytic genes were higher expressed (Fig. 9a, b). Many of these genes are described as XYR1 target genes [9, 22, 27, 30], including the major cellulolytic genes (e.g., bgl1, egl1/2/3/4/5 and cbh1/2), xylanolytic genes (e.g., xyn3/4, axe1 and the candidate β-xylosidase/α-l-arabinofuranosidase Trire2_3739), one pectinolytic gene (pgx1) and one mannanolytic gene (man1) (Table 1). Only in the Δxki1 strain, two arabinanolytic (e.g., abf2) gene and one PCP gene (lxr3) were higher expressed, which were also reported to be XYR1 regulated [9, 22, 30] (Table 1). Expression of xyr1 was also higher, while the cellulase repressor rce1  was lower expressed (Fig. 6).
In SBH at 48 h, Δxki1 and Δara1 had their highest PBD CAZyme gene expression, which included pectinolytic, amylolytic, cellulolytic and xylanolytic genes (Fig. 9). Similar to CS, xyr1 and ace3 were also higher expressed in Δxki1 and Δara1 (Fig. 6), and many of the genes upregulated in SBH at 48 h in Δxki1 and Δara1 have been described as XYR1 target genes [9, 22, 27, 30] (Table 1). These included cellulolytic (e.g., egl1/2/3/4/5 and cbh1/2), xylanolytic (e.g., xyn3/45, bxl1, axe1 and aes1), and mannanolytic (e.g., man1 and the candidate β-mannosidase Trire-2_62166) genes [8, 9, 18, 22, 27, 30] (Table 1). In addition to these, abf1, the candidate β-xylosidase/α-l-arabinofuranosidase Trire2_3739, bgl1 (Table 1) and two PCP genes, xyl1 (XYR1 regulated) and lxr3 were higher expressed in Δxki1, but not Δara1 .
In this study we evaluated the transcriptomic response of the T. reesei reference strain, two regulatory mutants and a metabolic mutant during growth on two plant biomass substrates, corn stover (CS, monocot) and soybean hulls (SBH, dicot). Our data showed that substrate composition strongly affected PBD CAZyme expression, resulting in higher induction of a broader set of CAZyme encoding genes in CS compared to SBH (Figs. 3, 4). This higher (hemi-)cellulolytic gene expression matches with the substrate composition (CS is richer in hemicellulose, especially arabinoxylan) (Additional file 1), as well as the more complete set of CAZymes in the T. reesei genome for CS degradation . In addition, PBD CAZyme and carbon catabolism related gene expression decreased over time earlier in SBH (Figs. 4, 5), suggesting that release of inducing compounds by T. reesei finished earlier on SBH. Indeed, T. reesei has only a few enzyme activities  for efficient degradation of SBH, such as low numbers of pectinases and α-xylosidases and a complete lack of endo-arabinanases and feruloyl esterases. This may have resulted in fewer inducers released from SBH and consequently in lower induction of a narrower set of PBD CAZyme encoding genes. d-xylose, which has been demonstrated to be a major inducer of the (hemi-)cellulolytic system in T. reesei , is mainly α-linked in xyloglucan in SBH, whereas it is β-linked in xylan in CS . In CS, the major β-xylosidase bxl1 was highly expressed at all three time points, while no β-xylosidase expression was found at any time point on SBH (Additional file 4). T. reesei has one putative α-xylosidase , which was expressed after 4 h (but not 24 h and 48 h) on SBH, possibly limiting the release of the α-linked d-xylose from SBH more so than the β-linked d-xylose in CS (Additional file 4). This was supported by a study, in which the addition of extra α-xylosidase activity to a T. reesei commercial enzyme cocktail improved significantly the amount of d-xylose released from pea or tamarind xyloglucan .
The data of this study provides leads to improve the production of a commercial T. reesei enzyme cocktail, such as by the choice of substrate on which the enzymes are produced and the time after which enzymes are harvest. CS appears a better substrate to obtain a (hemi-)cellulolytic cocktail, while SBH is better for a pectinolytic, amylolytic and mannanolytic cocktail (Fig. 4). In both substrates, the overall expression level was higher at the earliest time point (4 h), suggesting that high enzyme production will not be sustained over time unless the consumption of potential inducers can be impaired such as in the Δxki1 mutant. A similar pattern was observed in Podospora anserina using comparable methodology including the same substrates , where CS induced predominantly (hemi-)cellulases, while SBH induced more amylolytic and pectinolytic genes. However, in P. anserina, SBH was the broader and higher PBD CAZyme gene inducing substrate compared to CS. This indicates that the inducing effect of crude substrates can be species-specific, depending on the genome content and plant biomass degradation strategy. Nevertheless, commonalities can be found in the responses of fungi from diverse biotypes. Analysis of the T. reesei PBD CAZyme genes expressed in both substrates resulted in a core set of 35 shared enzyme activities (data not shown). Of these activities, 14 were in common with the 18 activities in the core set of P. anserina and saprobic basidiomycetes [34, 35]. These 14 activities included three cellulolytic (LPMO, CBH and EGL), one amylolytic (AGD), four xylanolytic (AXE, XLN, ABF, BXL), three mannanolytic (MAN, MND and LAC), two pectinolytic (LAC and ABF) and one xyloglucanolytic (XEG) gene. This core enzyme set could be considered as a general response of fungi from diverse biotypes to commonly found components of plant biomass.
We showed that particularly (hemi-)cellulolytic genes were more induced in CS, most likely due to the higher expression of the two (hemi-)cellulolytic regulators xyr1 and ace3 (Fig. 6). However, a higher expression of a TF does not necessarily lead to higher expression of its target genes, because they can be regulated also at post-transcriptional level, as has previously been shown for XYR1 and other TFs . However, our data demonstrates low expression for clr2 in all conditions, suggesting a different function in T. reesei for CLR2 compared to Neurospora crassa and several Aspergilli, where it has been described as a cellulolytic and mannanolytic regulator [36,37,38]. Overexpression of clr2 in T. reesei did not result in substantial enhancement in cellulase and xylanase activity . The orthologs of the A. niger d-galacturonic acid regulators gaaR and gaaX  were also poorly expressed in most of the conditions (Fig. 6), suggesting that the mechanism with which T. reesei responds to d-galacturonic acid may differ from Botrytis cinerea and A. niger [6, 8].
Our data showed that all mutations, both regulatory and catabolic, severely affected the initial response (4 h) to both substrates (Figs. 9, 10). This suggests an initial delay in the release and utilization of enough easily metabolized sugars/inducers at 4 h by the mutants, resulting in a lack of energy, lower co-factor regeneration (especially for Δxki1), such as NADH and NADPH that are necessary for the activity of many oxidoreductases of catabolic pathways, and carbon to synthesize the necessary proteins to degrade plant biomass. Lower PBD CAZyme gene expression was also observed in a study performed with comparable methodology in A. niger, where ΔxlnR and ΔxkiA mutants severely affected PBD expression in both CS and SBH at the early stage . Comparison with this A. niger study is particularly informative as similar conditions (with respect to time-points and substrates) and mutants were used.
Our study demonstrates that xyr1 is the major TF affecting CS utilization, where its deletion caused a massive reduction of PBD CAZyme gene expression at 4 h and 24 h, especially of cellulolytic and xylanolytic genes (Fig. 9). This matches with the substrate composition (Additional file 1) and the function described for this regulator, as indeed CS is richer in (hemi-)cellulose and XYR1 is the main (hemi-)cellulolytic activator [9, 22, 27]. This confirms a previous study, in which another (hemi-)cellulose-rich substrate (wheat bran) and a T. reesei Rut-C30 Δxyr1 mutant were used .
In contrast, at 4 h in SBH, substrate utilization was more affected by the ara1 deletion resulting in a more severe reduction of PBD CAZyme expression. This dependence of the early response to SBH on ARA1 is most likely due to the fact that ARA1 responds to l-arabinose and d-galactose  (inducers which SBH is richer in Additional file 1). During the later response (24 h and 48 h), other TFs indirectly compensated for this loss, such as the higher expression of the (hemi-)cellulolytic activators xyr1 and ace3 [8, 22, 26], or the lower expression of the cellulase repressor rce1  (Fig. 6). Supporting this role of these regulators, cellulolytic and xylanolytic genes were higher expressed in Δara1 at the later time points (Fig. 9).
Our study is the first which highlights the importance of TFs other than XYR1, in a pectin- and mannan rich substrate such as SBH for T. reesei. Most of the previous studies where xyr1 was deleted used substrates that did not contain pectin or mannan, such as lactose, cellulose or xylan-rich crude plant biomass [15, 18, 22, 27, 30, 41,42,43,44]. The use of SBH in our study not only showed that XYR1 was not the major regulator on this substrate, but also that XYR1 partially regulates a few pectinolytic and mannanolytic genes (Additional file 4). This suggests that the function of XYR1 is not limited to cellulolytic and xylanolytic genes , but is broader than what has so far been described [8, 9, 27, 30]. Another broader role for XYR1 was reported by Ma et al. , where XYR1 appeared to regulate not only (hemi-)cellulolytic genes, but also genes encoding non-enzymatic cellulose active enzymes, sugar transporters and heat shock proteins.
In A. niger, XlnR (xyr1 ortholog) and AraR (functional homolog of ara1) can compensate for each other’s loss, by inducing the target genes of the deleted regulator, most likely due to a similar binding motif . In contrast, T. reesei XYR1 and ARA1 are not able to compensate for each other loss, probably because they are not closely related and, therefore, also bind to distinct promoter sequences [8, 9]. XYR1 appeared to express its own target genes, mainly (hemi-)cellulolytic genes [9, 22, 27], to a higher level in the Δara1 strain, but not ARA1-target genes (Fig. 9).
The residual growth of Δxki1 on l-arabinose (which should result in a block of the PCP, Fig. 2), suggests the presence of another catabolic pathway in T. reesei to partially catabolize l-arabinose instead of the PCP. In contrast, the A. niger xylulokinase mutant cannot grow on l-arabinose , indicating a difference in the organization of these pathways between these two fungi. Blast analysis revealed that the T. reesei genome contains orthologs for the non-phosphorylative l-arabinose pathway from the bacterium Azospirillum brasiliense  (referred to as “alternative l-arabinose pathway” in our analysis). Whether this putative alternative l-arabinose pathway is responsible for the further catabolism of l-arabinose in Δxki1 strain (Fig. 10) requires additional studies.
In Δxki1, the putative block of the PCP resulted in higher PBD CAZyme expression at later time points on both substrates (24 h in CS and 48 h in SBH) (Fig. 9). Many of these genes were described as XYR1 regulated [9, 27, 30] (Table 1) and were also upregulated in Δara1. A similar inducing effect was also observed in A. niger ΔxkiA , where accumulation of inducers , such as xylitol and l-arabitol, resulted in more PBD CAZyme genes that were highly expressed compared to the reference strain at later time points. However, this was limited to genes acting on pectin or with an activity that could be involved in the degradation of several substrates. This inducer(s) accumulation could also be the explanation for our results with T. reesei, which resulted in higher expression of the (hemi-)cellulolytic regulator xyr1 (Fig. 6) and its target genes [9, 27, 30]. Xylitol and l-arabitol accumulation was already reported for other T. reesei PCP-knockout strains (Δxyl1, Δlad1, Δlxr3) . This inducer(s) accumulation (such as by xylitol and l-arabitol) is a possible explanation for the higher expression of PBD CAZymes observed also in the Δara1 strain. However, in this case, where a TF is missing, we cannot exclude the involvement of other regulatory mechanism(s) such as secondary/backup regulatory system(s). It was previously shown in A. niger that XlnR and AraR have an antagonistic effect on each other and that deletion of one, increases expression of the target genes of the other [47, 48]. Considering that growth on solid media, where sugars other than pentoses were available, was comparable to the reference strain (Fig. 2), deletion of xki1 could be used to improve production of T. reesei enzyme cocktails at industrial scale by limiting the catabolism of pentose inducers from a crude plant biomass substrate, potentially sustaining the induction of the enzyme encoding genes longer.
CS induces a broader and higher expression of PBD CAZyme encoding genes in T. reesei, while SBH could be used to induce an enzyme cocktail that is richer in pectinolytic and mannanolytic enzymes. XYR1 is the major TF affecting CS utilization, while ARA1 affects more SBH utilization. Blocking the PCP by deleting xki1 leads to higher expression of PBD CAZymes at later time points in the cultures, which could lead to a novel strategy to improve the enzyme cocktail production at industrial level.
Materials and methods
Strains, media, and growth conditions
Trichoderma reesei QM9414 (ATCC 26921)  was used as reference strain and compared to CBS 143327 (Δxyr1) , CBS143330 (Δara1)  and CBS143332 (Δxki11) (this study) in all experiments. All T. reesei plate cultures were incubated at 28 °C on PDA (Difco) for sporulation, or minimal medium (MM)  with 18 g/L Select agar (Invitrogen) during the transformation or growth profiling (in this case Na-citrate was removed). The growth profile was performed on MM with 25 mM d-glucose (Sigma), d-fructose (Sigma), d-xylose (Sigma), l-arabinose (Sigma), xylitol (Sigma), l-arabitol (Sigma), d-galactose (Sigma), lactose (Sigma), 1% arabinan (Megazyme), wheat arabinoxylan (Megazyme), apple pectin (Sigma), avicel (Fluka), 3% soybean hulls and corn stover in 9 cm Petri dishes. Duplicate plates were inoculated with 2 μL containing 1 × 103 spores, which were pre-germinated overnight in MM with 1% d-fructose and 0.1% peptone, and incubated in the dark for at least 5 days at 28 °C. Pre-germination facilitates replicable growth on C-sources where T. reesei spores germinate infrequently or do not germinate. Independent deletion strains were generated and tested for growth on a subset of C-sources to confirm the reliability of attributing the observed phenotypes to deleted gene (data not shown). We selected one strain to use in further studies and deposited these at the Westerdijk Fungal Biodiversity Institute collection, with strain number as indicated above.
A transfer experiment was performed for transcriptomics. 250 mL of complete medium (CM)  containing 2% d-fructose in 1 L Erlenmeyer flasks was inoculated with 2.5 × 108 fresh spores, harvested from a PDA plate, and incubated in a rotatory shaker at 28 °C for 20 h at 250 rpm. The mycelium was harvested by filtration, washed with liquid Mandels Andreotti medium (MA)  (without carbon source) and 2.5 g mycelium (wet weight) was transferred to 250 mL Erlenmeyer flasks containing 50 mL MA with 1% of soybean hulls or corn stover, and incubated in a rotatory shaker at 28 °C and 250 rpm. After pre-culturing and after 4 h, 24 h, and 48 h of incubation in CS or SBH, the mycelium was harvested by vacuum filtration, dried between tissue paper, directly frozen in liquid nitrogen and stored at − 45 °C . All experiments were performed in triplicates, with the exception of pre-cultures, which were performed in duplicates.
Molecular biology methods
The hygromycin BR cassette was amplified from the plasmid pLH1hph  and fused with 1 kb flanking regions up- and downstream of the xki1 gene by fusion-PCR and purified as described by Klaubauf et al. . This xki1 deletion cassette was used to transform spores of T. reesei QM9414 Δtku70  by electroporation as described by Schuster et al. , using a Bio-Rad Gene Pulser Electroporator System set at 1.8 kV, 800 Ω and 25 μF. DNA from transformants was screened by PCR for the absence of xki1 and the correct positioning of the insert as described by Klaubauf et al. . The absence of ectopic integrations was confirmed by Southern blot (Additional file 2) using DIG Easy Hyb kit (Roche) and Anti-Digoxigenin-AP, Fab fragments (Roche) with a probe designed to hybridize to part of the hygromycin resistance gene sequence and amplified with the PCR DIG Probe Synthesis Kit (Roche), according to the manufacturer protocols. Primers used for PCR reactions are listed in Additional file 3.
Total RNA was extracted from mycelium ground in a Tissue Lyser (QIAGEN) using TRIzol reagent (Invitrogen) according to the manufacturer’s instructions. RNA integrity and quantity were analyzed on a 1% agarose electrophoresis gel and with the RNA6000 Nano Assay, using the Agilent 2100 Bioanalyzer (Agilent Technologies) .
Culture filtrate samples (10 mL) were taken after 24 h and 48 h and centrifuged for 10 min, at ~ 10,000×g, 4 °C to separate the solid fraction from the supernatant and stored at − 20 °C. 150 µL of these culture filtrates from reference and Δxyr1 strains at 24 h and 48 h of cultivation were added to 50 µL of loading buffer (10% of 1 M Tris–HCl, pH 6.8; 42% Glycerol, 4% (w/v) SDS; 0.02% (w/v) bromophenol blue; 4% of 14.7 M Mercaptoethanol), boiled for 2 min to denature the proteins, cooled on ice for 2 min and centrifuged at ~ 10,000×g for 2 min to remove insoluble material. 20 µL was then loaded onto 12% (w/v) acrylamide SDS-PAGE gels and a molecular weight marker (Bio-Rad unstained marker) was used to identify the molecular mass of the protein bands. The gels were silver stained  and documented using the HP scanner 4400c.
RNA sequencing and read mapping
RNA samples (5–41 μg DNase-treated total RNA) were processed by Joint Genome Institute. RNA sequencing was performed using Illumina HiSeq 2500 (yield 1 TB of 1 × 101 bp). Raw fastq file reads were filtered and trimmed using the JGI QC pipeline. Using BBDuk [BBDuk: https://sourceforge.net/projects/bbmap/] raw reads were evaluated for artifact sequence by kmer matching (kmer = 25), allowing 1 mismatch and detected artifact was trimmed from the 3′ end of the reads. RNA spike-in reads, PhiX reads and reads containing any Ns were removed. Quality trimming was performed using the phred trimming method set at Q6. Reads under the length threshold were removed. Filtered reads from each library were aligned to the reference genome (https://genome.jgi.doe.gov/Trire2/Trire2.home.html) using HISAT version 0.1.4-beta . featureCounts  was used to generate the raw gene counts using gff3 annotations. On average 94% of the reads mapped to the genome. The RNA-seq data have been deposited at the Sequence Read Archive at NCBI with individual sample BioProject Accession numbers (PRJNA440083 to PRJNA440152 and PRJNA442529 to PRJNA442538.
RNA-seq data analysis
Raw gene counts were used to evaluate the level of correlation between biological replicates using Pearson’s correlation matrix (Additional file 5). DESeq 2 (version 1.10.0)  was used to determine which genes were differentially expressed (DE) between pairs of conditions. The parameters used to call a gene DE between conditions were adjusted p value ≤ 0.05, foldchange > 2.5 (log2foldchange > 1.32) and FPKM ≥ 18 in at least one condition. Genes with FPKM values < 18 in every condition were considered lowly expressed and ignored in the analysis.
PBD CAZyme (which had FPKM ≥ 18 in at least one of the conditions for a particular heatmap) or TF (all were clustered without regard to their minimum FPKM value) genes were hierarchically clustered using the heatmap.2 function (with default parameters: Euclidean distance, and complete linkage clustering method) from the gplots_3.0.1 package in R statistical language and environment 3.4.0. Log2 FPKM values were used for the color gradient of the heatmap and FPKM values < 1 were assigned to 1.
carbohydrate-active enzymes database
carbon catabolite repression
plant biomass degrading enzyme
pentose catabolic pathway
pentose phosphate pathway
acetyl xylan esterase
lytic polysaccharide monooxygenase
Makela MR, Donofrio N, de Vries RP. Plant biomass degradation by fungi. Fungal Genet Biol. 2014;72:2–9.
Bischof RH, Ramoni J, Seiboth B. Cellulases and beyond: the first 70 years of the enzyme producer Trichoderma reesei. Microb Cell Fact. 2016;15(1):106.
Druzhinina IS, Kubicek CP. Genetic engineering of Trichoderma reesei cellulases and their production. Microb Biotechnol. 2017;10(6):1485–99.
Peterson R, Nevalainen H. Trichoderma reesei RUT-C30–thirty years of strain improvement. Microbiology. 2012;158(Pt 1):58–68.
Kubicek CP. Systems biological approaches towards understanding cellulase production by Trichoderma reesei. J Biotechnol. 2013;163(2):133–42.
Martinez D, Berka RM, Henrissat B, Saloheimo M, Arvas M, Baker SE, Chapman J, Chertkov O, Coutinho PM, Cullen D, et al. Genome sequencing and analysis of the biomass-degrading fungus Trichoderma reesei (syn. Hypocrea jecorina). Nat Biotechnol. 2008;26(5):553–60.
Gupta VK, Steindorff AS, de Paula RG, Silva-Rocha R, Mach-Aigner AR, Mach RL, Silva RN. The post-genomic Era of Trichoderma reesei: what’s Next? Trends Biotechnol. 2016;34(12):970–82.
Benocci T, Aguilar-Pontes MV, Zhou M, Seiboth B, de Vries RP. Regulators of plant biomass degradation in ascomycetous fungi. Biotechnol Biofuels. 2017;10:152.
Benocci T, Aguilar-Pontes MV, Kun RS, Seiboth B, de Vries RP, Daly P. ARA1 regulates not only l-arabinose but also d-galactose catabolism in Trichoderma reesei. FEBS Lett. 2018;592(1):60–70.
Seiboth B, Metz B. Fungal arabinan and l-arabinose metabolism. Appl Microbiol Biotechnol. 2011;89(6):1665–73.
Khosravi C, Benocci T, Battaglia E, Benoit I, de Vries RP. Sugar catabolism in Aspergillus and other fungi related to the utilization of plant biomass. Adv Appl Microbiol. 2015;90:1–28.
Witteveen CFB, Busink R, Vondervoort PVD, Dijkema C, Swart K, Visser J. l-arabinose and d-xylose catabolism in Aspergillus niger. J Gen Microbiol. 1989;135:2163–71.
Herold S, Bischof R, Metz B, Seiboth B, Kubicek CP. Xylanase gene transcription in Trichoderma reesei is triggered by different inducers representing different hemicellulosic pentose polymers. Eukaryot Cell. 2013;12(3):390–8.
Hong Y, Dashtban M, Kepka G, Chen S, Qin W. Overexpression of d-xylose reductase (xyl1) gene and antisense inhibition of d-xylulokinase (xyiH) gene increase xylitol production in Trichoderma reesei. Biomed Res Int. 2014;2014:169705.
Bischof R, Fourtis L, Limbeck A, Gamauf C, Seiboth B, Kubicek CP. Comparative analysis of the Trichoderma reesei transcriptome during growth on the cellulase inducing substrates wheat straw and lactose. Biotechnol Biofuels. 2013;6(1):127.
Borin GP, Sanchez CC, de Santana ES, Zanini GK, Dos Santos RAC, de Oliveira Pontes A, de Souza AT, Dal’Mas R, Riano-Pachon DM, Goldman GH, et al. Comparative transcriptome analysis reveals different strategies for degradation of steam-exploded sugarcane bagasse by Aspergillus niger and Trichoderma reesei. BMC Genomics. 2017;18(1):501.
Ries L, Pullan ST, Delmas S, Malla S, Blythe MJ, Archer DB. Genome-wide transcriptional response of Trichoderma reesei to lignocellulose using RNA sequencing and comparison with. BMC Genomics. 2013;14:541.
Ma L, Chen L, Zhang L, Zou G, Liu R, Jiang Y, Zhou Z. RNA sequencing reveals Xyr1 as a transcription factor regulating gene expression beyond carbohydrate metabolism. Biomed Res Int. 2016;2016:4841756.
Buranov AU, Mazza G. Lignin in straw of herbaceous crops. Ind Crop Prod. 2008;28(3):237–59.
Mielenz JR, Bardsley JS, Wyman CE. Fermentation of soybean hulls to ethanol while preserving protein value. Bioresour Technol. 2009;100(14):3532–9.
Akel E, Metz B, Seiboth B, Kubicek CP. Molecular regulation of arabinan and l-arabinose metabolism in Hypocrea jecorina (Trichoderma reesei). Eukaryot Cell. 2009;8(12):1837–44.
Stricker AR, Grosstessner-Hain K, Wurleitner E, Mach RL. Xyr1 (xylanase regulator 1) regulates both the hydrolytic enzyme system and d-xylose metabolism in Hypocrea jecorina. Eukaryot Cell. 2006;5(12):2128–37.
Hasper AA, Visser J, de Graaff LH. The Aspergillus niger transcriptional activator XlnR, which is involved in the degradation of the polysaccharides xylan and cellulose, also regulates d-xylose reductase gene expression. Mol Microbiol. 2000;36:193–200.
Mach-Aigner AR, Omony J, Jovanovic B, van Boxtel AJ, de Graaff LH. d-xylose concentration-dependent hydrolase expression profiles and the function of CreA and XlnR in Aspergillus niger. Appl Environ Microbiol. 2012;78(9):3145–55.
Mach-Aigner AR, Pucher ME, Mach RL. d-xylose as a repressor or inducer of xylanase expression in Hypocrea jecorina (Trichoderma reesei). Appl Environ Microbiol. 2010;76(6):1770–6.
Hakkinen M, Valkonen MJ, Westerholm-Parvinen A, Aro N, Arvas M, Vitikainen M, Penttila M, Saloheimo M, Pakula TM. Screening of candidate regulators for cellulase and hemicellulase production in Trichoderma reesei and identification of a factor essential for cellulase production. Biotechnol Biofuels. 2014;7(1):14.
Mach-Aigner AR, Pucher ME, Steiger MG, Bauer GE, Preis SJ, Mach RL. Transcriptional regulation of xyr1, encoding the main regulator of the xylanolytic and cellulolytic enzyme system in Hypocrea jecorina. Appl Environ Microbiol. 2008;74(21):6554–62.
Gruben BS, Zhou M, Wiebenga A, Ballering J, Overkamp KM, Punt PJ, de Vries RP. Aspergillus niger RhaR, a regulator involved in l-rhamnose release and catabolism. Appl Microbiol Biotechnol. 2014;98(12):5531–40.
Derntl C, Kluger B, Bueschl C, Schuhmacher R, Mach RL, Mach-Aigner AR. Transcription factor Xpp1 is a switch between primary and secondary fungal metabolism. Proc Natl Acad Sci USA. 2017;114(4):E560–9.
Portnoy T, Margeot A, Seidl-Seiboth V, Le Crom S, Ben Chaabane F, Linke R, Seiboth B, Kubicek CP. Differential regulation of the cellulase transcription factors XYR1, ACE2, and ACE1 in Trichoderma reesei strains producing high and low levels of cellulase. Eukaryot Cell. 2011;10(2):262–71.
Cao Y, Zheng F, Wang L, Zhao G, Chen G, Zhang W, Liu W. Rce1, a novel transcriptional repressor, regulates cellulase gene expression by antagonizing the transactivator Xyr1 in Trichoderma reesei. Mol Microbiol. 2017;105(1):65–83.
Andersen MR, Giese M, de Vries RP, Nielsen J. Mapping the polysaccharide degradation potential of Aspergillus niger. BMC Genomics. 2012;13:313.
Jabbour D, Borrusch MS, Banerjee G, Walton JD. Enhancement of fermentable sugar yields by alpha-xylosidase supplementation of commercial cellulases. Biotechnol Biofuels. 2013;6(1):58.
Benocci T, Daly P, Aguilar-Pontes M, Lail K, Wang M, Lipzen A, Vivian N, Grigoriev I, de Vries R. Enzymatic adaptation of Podospora anserina to different plant biomass provides leads to optimized commercial enzyme cocktails. Biotechnol J. 2018 (in press).
Peng M, Aguilar-Pontes MV, Hainaut M, Henrissat B, Hilden K, Makela MR, de Vries RP. Comparative analysis of basidiomycete transcriptomes reveals a core set of expressed genes encoding plant biomass degrading enzymes. Fungal Genet Biol. 2017;112:40–6.
Coradetti ST, Craig JP, Xiong Y, Shock T, Tian C, Glass NL. Conserved and essential transcription factors for cellulase gene expression in ascomycete fungi. Proc Natl Acad Sci USA. 2012;109(19):7397–402.
Raulo R, Kokolski M, Archer DB. The roles of the zinc finger transcription factors XlnR, ClrA and ClrB in the breakdown of lignocellulose by Aspergillus niger. AMB Exp. 2016;6(1):5.
Ogawa M, Kobayashi T, Koyama Y. ManR, a transcriptional regulator of the beta-mannan utilization system, controls the cellulose utilization system in Aspergillus oryzae. Biosci Biotechnol Biochem. 2013;77(2):426–9.
Niu J, Alazi E, Reid ID, Arentshorst M, Punt PJ, Visser J, Tsang A, Ram AF. An evolutionarily conserved transcriptional activator-repressor module controls expression of genes for d-galacturonic acid utilization in Aspergillus niger. Genetics. 2017;205(1):169–83.
Khosravi C KJ, Battaglia E, Aguilar-Pontes MV, Lipzen A, Ng V, Grigoriev I, de Vries RP: Chapter 4. Transcriptome analysis of Aspergillus niger xlnR and xkiA mutants grown on corn stover and soybean hulls. PhD thesis. Utrecht, The Netherlands: Utrecht University; 2017.
Mello-de-Sousa TM, Rassinger A, Derntl C, Pocas-Fonseca MJ, Mach RL, Mach-Aigner AR. The relation between promoter chromatin status, Xyr1 and cellulase expression in Trichoderma reesei. Curr Genomics. 2016;17(2):145–52.
Lichius A, Seidl-Seiboth V, Seiboth B, Kubicek CP. Nucleo-cytoplasmic shuttling dynamics of the transcriptional regulators XYR1 and CRE1 under conditions of cellulase and xylanase gene expression in Trichoderma reesei. Mol Microbiol. 2014;94(5):1162–78.
Stricker AR, Steiger MG, Mach RL. Xyr1 receives the lactose induction signal and regulates lactose metabolism in Hypocrea jecorina. FEBS Lett. 2007;581(21):3915–20.
Dos Santos Castro L, de Paula RG, Antonieto AC, Persinoti GF, Silva-Rocha R, Silva RN. Understanding the Role of the Master Regulator XYR1 in Trichoderma reesei by Global Transcriptional Analysis. Front Microbiol. 2016;7:175.
Battaglia E, Visser L, Nijssen A, van Veluw GJ, Wosten HA, de Vries RP. Analysis of regulation of pentose utilisation in Aspergillus niger reveals evolutionary adaptations in Eurotiales. Stud Mycol. 2011;69(1):31–8.
Watanabe S, Kodaki T, Makino K. Cloning, expression, and characterization of bacterial l-arabinose 1-dehydrogenase involved in an alternative pathway of l-arabinose metabolism. J Biol Chem. 2006;281(5):2612–23.
Battaglia E, Visser L, Nijssen A, van Veluw J, Wösten HAB, de Vries RP. Analysis of regulation of pentose utilisation in Aspergillus niger reveals evolutionary adaptations in the Eurotiales. Stud Mycol. 2011;69:31–8.
de Groot MJL, van de Vondervoort PJI, de Vries RP, vanKuyk PA, Ruijter GJG, Visser J. Isolation and characterization of two specific regulatory Aspergillus niger mutants shows antagonistic regulation of arabinan and xylan metabolism. Microbiology. 2003;149:1183–91.
Montenecourt BS, Eveleigh DE. Preparation of mutants of Trichoderma reesei with enhanced cellulase production. Appl Environ Microbiol. 1977;34(6):777–82.
Penttila M, Nevalainen H, Ratto M, Salminen E, Knowles J. A versatile transformation system for the cellulolytic filamentous fungus Trichoderma reesei. Gene. 1987;61(2):155–64.
de Vries RP, Burgers K, van de Vondervoort PJ, Frisvad JC, Samson RA, Visser J. A new black Aspergillus species, A. vadensis, is a promising host for homologous and heterologous protein production. Appl Environ Microbiol. 2004;70(7):3954–9.
Mandels M, Andreotti RE. Problems and challenges in the cellulose to cellulase fermentation. Process Biochem. 1978;13:6.
Klaubauf S, Zhou M, Lebrun MH, de Vries RP, Battaglia E. A novel l-arabinose-responsive regulator discovered in the rice-blast fungus Pyricularia oryzae (Magnaporthe oryzae). FEBS Lett. 2016;590(4):550–4.
Hartl L, Kubicek CP, Seiboth B. Induction of the gal pathway and cellulase genes involves no transcriptional inducer function of the galactokinase in Hypocrea jecorina. J Biol Chem. 2007;282(25):18654–9.
Guangtao Z, Hartl L, Schuster A, Polak S, Schmoll M, Wang T, Seidl V, Seiboth B. Gene targeting in a nonhomologous end joining deficient Hypocrea jecorina. J Biotechnol. 2009;139(2):146–51.
Schuster A, Bruno KS, Collett JR, Baker SE, Seiboth B, Kubicek CP, Schmoll M. A versatile toolkit for high throughput functional genomics with Trichoderma reesei. Biotechnol Biofuels. 2012;5(1):1.
Chevallet M, Luche S, Rabilloud T. Silver staining of proteins in polyacrylamide gels. Nat Protoc. 2006;1(4):1852–8.
Kim D, Langmead B, Salzberg SL. HISAT: a fast spliced aligner with low memory requirements. Nat Methods. 2015;12(4):357–60.
Liao Y, Smyth GK, Shi W. featureCounts: an efficient general purpose program for assigning sequence reads to genomic features. Bioinformatics. 2014;30(7):923–30.
Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15(12):550.
Hakkinen M, Arvas M, Oja M, Aro N, Penttila M, Saloheimo M, Pakula TM. Re-annotation of the CAZy genes of Trichoderma reesei and transcription in the presence of lignocellulosic substrates. Microb Cell Fact. 2012;11:134.
TB and RJML carried out the experiments. TB analyzed the data and wrote the manuscript. MVAP performed part of the bioinformatics analysis. RSK generated the xki1 deletion strains. RPdV designed the study. RPdV and PD supervised the experiments and the manuscript. BS reviewed the manuscript and provided T. reesei QM9414 strains ATCC 26921 (reference), ∆tku70 and ∆xyr1. KL, MW, AL, VN and IVG performed RNA sequencing. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Availability of data and materials
The RNA-seq data have been deposited at the Sequence Read Archive at NCBI with individual sample BioProject Accession Numbers PRJNA440083 to PRJNA440152 and PRJNA442529 to PRJNA442538.
Consent for publication
Ethics approval and consent to participate
This study was supported by a Grant of the Applied Science Division of NWO, and the Technology Program of the Ministry of Economic Affairs 016.130.609 to RPdV. PD was supported by a Grant from the ALW division of NWO (824.15.023) to RPdV. BS was supported by the Austrian Science Fund project P24219. The work conducted by the U.S. Department of Energy Joint Genome Institute (JGI), was supported by the Office of Science of the U.S. Department of Energy under Contract No. DE-AC02-05CH11231.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Southern blot of Δxki1 strains. Positive gene deletion required bands of 6.4 kb and 10.8 kb for Δxki1. Both Δxki1 strains were correct.
Table with PCR primers used in this study.
Enzyme activity abbreviations and transcriptome dataset tables. Table with enzyme activity, their abbreviations and their predicted target substrate used in this study. The same color scheme for target substrates was used in the main text. A gene to be assigned as expressed more on a substrate (CS or SBH) requires a foldchange > 2.5, p ≤ 0.05 and at least 18 FPKM of expression in at least one condition. Genes with expression < 18 FPKM in each condition were excluded from subsequent analysis, because they were considered to be too poorly expressed.
Pearson correlation matrix of Trichoderma reesei transcriptomes. Raw gene counts were used to evaluate the level of correlation between biological replicates using Pearson’s correlation. Pearson correlation matrix were performed in R (v3.4.0) statistical language and environment, the core function from the stats base package and the corrplot (v 0.77) package were used for the analysis. One sample (reference strain on SBH at 48 h) was removed from the dataset because it correlated poorly with its replicates.
Analysis of the protein banding patterns from the three replicate culture supernatants of T. reesei reference (ref) and Δxyr1 strains cultured with either corn stover or soybean hulls for 24 h and 48 h. The same volume of culture supernatant was loaded for all samples.
About this article
Cite this article
Benocci, T., Aguilar-Pontes, M.V., Kun, R.S. et al. Deletion of either the regulatory gene ara1 or metabolic gene xki1 in Trichoderma reesei leads to increased CAZyme gene expression on crude plant biomass. Biotechnol Biofuels 12, 81 (2019). https://doi.org/10.1186/s13068-019-1422-y
- Plant biomass degradation
- Trichoderma reesei