- Open Access
Enhanced cellulase production by decreasing intercellular pH through H+-ATPase gene deletion in Trichoderma reesei RUT-C30
Biotechnology for Biofuels volume 12, Article number: 195 (2019)
Cellulolytic enzymes produced by Trichoderma reesei are widely used for the industrial production of biofuels and chemicals from lignocellulose. We speculated that intracellular pH during the fermentation process can affect cellulase induction.
In this study, two H+-ATPase genes, tre76238 and tre78757, were first identified in T. reesei. Deletion of tre76238 and tre78757 in T. reesei RUT-C30 confirmed that tre76238 has a major function in maintaining intracellular pH, whereas tre78757 has a minor function. The tre76238 deletion strain Δ76238 displayed a high level of cellulase production using cellulase-repressive glucose as a sole carbon source, along with intracellular acid accumulation and growth retardation. Our results indicated that intracellular acid accumulation in Δ76238 stimulated a significant increase in the cytosolic Ca2+ levels. Ca2+ channels were shown to be necessary for cellulase production using glucose as the carbon source in Δ76238. Delayed Δ76238 growth could be reversed by optimizing the medium’s nitrogen sources to produce ammonia for intracellular acid neutralization in the early phase. This may be useful for scale-up of cellulase production using glucose as the carbon source.
This study provides a new perspective for significant alterations in the cellulase expression pattern of T. reesei Δ76238, indicating a new mechanism for cellulase regulation under conditions of low intracellular pH.
As the most abundant and renewable resource in nature, lignocellulosic biomass has been widely used to produce biofuels and bioproducts, which have received increased focus for further research . Biological conversion of lignocellulosic biomass into fermentable sugars by cellulosic enzyme usage is an environment-friendly and promising approach. However, the production cost of a large amount of biomass-degrading enzymes is still a significant challenge for commercial biofuel production [2,3,4]. The filamentous fungus Trichoderma reesei is an important producer for most cellulolytic enzymes used in biomass conversion today . The cellulases produced in T. reesei mainly comprise two cellobiohydrolases (CBHI and CBHII), two endoglucanases (EGI and EGII), and β-glucosidase I (BGLI) [6, 7].
A complex regulatory network is needed for the accurate regulation of cellulase gene expression . Several transcription factors for cellulase gene expression have been characterized in T. reesei, including the main transactivator of cellulase and hemicellulase expression, XYR1 , as well as the carbon catabolite repressor, CRE1 . In T. reesei, CREI is known to repress the transcription of several cellulase genes such as the CBHI-encoding gene cbh1 and the main transactivator XYRI [11,12,13,14], in the presence of d-glucose. XYR1 is considered the essential activator controlling the major cellulase and hemicellulase gene expression . Many cellulase high-producing T. reesei mutants have been obtained by classical mutagenesis for several decades. The moderately overproducing strain QM9414 (ATCC 26921) and the T. reesei hyperproducing strain RUT-C30 (ATCC 56765) are the most widely used T. reesei strains in academic research [6, 16].
The productivity and efficiency of cellulolytic enzymes produced by T. reesei is significantly affected by culture pH [17, 18]. Earlier reports have shown that a lower pH during the fermentation process might favor efficient cellulase production [7, 18], whereas a higher pH is essential for xylanase production . The best cellulase production was obtained at a lower pH (4.0 minimum) by Bailey et al. . Some reports have suggested that optimizing pH in fermentation broth can improve and maintain industrial cellulase production in T. reesei [17, 20, 21]. However, studies based on regulating and maintaining pH for cellulase production in T. reesei were only done by changing the extracellular pH in fermentation broth [7, 18,19,20,21]. Extracellular acids may be transported into the cells, affecting the intracellular pH homeostasis and stimulating the upstream (hemi-) cellulase regulation pathway, though this is unclear [22, 23]. The effect of directly changing intracellular pH on cellulase production in T. reesei has also aroused great interest.
Carbon source consumption during T. reesei growth is sometimes accompanied by acid production . Aside from the acid in the cultural environment, intracellular pH homeostasis is also achieved by multiple regulation of molecules via pumps and exchangers . The fungal plasma membrane H+-ATPase is the primary proton pump that exports cellular protons, using ATP as an energy source [23, 25] and plays a key role in intracellular pH homeostasis . Plasma membrane H+-ATPases have been functionally characterized in Saccharomyces cerevisiae, Schizosaccharomyces pombe, and Neurospora crassa [26,27,28]. The major plasma membrane H+-ATPases are encoded by the gene pma1 in S. cerevisiae and S. pombe. pma2, the isogene of pma1, is not required for growth . The pmal mutants of S. cerevisiae were apparently defective at maintaining internal pH, and some mutants were unable to grow either at a low pH or in the presence of a weak acid . Therefore, deleting H+-ATPases is a feasible approach for efficiently reducing the intracellular pH.
In this study, plasma membrane H+-ATPase genes tre76238 and tre78757, which have a great effect on intracellular pH homeostasis, were identified in T. reesei for the first time. Deletion of the gene tre76238 in T. reesei RUT-C30 resulted in significant cellulase production using glucose as the sole carbon source. We further researched the underlying mechanism of significant alterations in the cellulase expression pattern of Δ76238. The medium was also optimized for accelerating Δ76238 growth in the early phase. These findings provide a new strategy for enhanced cellulase production by regulating intracellular pH homeostasis. Our research indicates a new mechanism for cellulase regulation in low intracellular pH conditions, which warrants further research.
H+-ATPase isogenes tre76238 and tre78757 were identified in Trichoderma reesei
Fungal plasma membrane H+-ATPases play an important role in intracellular pH homeostasis . Two plasma membrane H+-ATPase isogenes, tre76238 and tre78757, were identified by a BLAST search of the genome sequence of Trichoderma reesei (https://genome.jgi.doe.gov/Trire_Chr/Trire_Chr.home.html  or https://genome.jgi.doe.gov/TrireRUTC30_1/TrireRUTC30_1.home.html ) for homologs of the H+-ATPase genes pma1 and pma2 from Saccharomyces cerevisiae .
The open reading frame of tre76238 is 2949 bp (CDS Sequence), encoding a 982-amino acid protein TRE76238 with three conserved domains based on comparison to the yeast Pma1 structure . One is a cation ATPase N-terminus (smart00831: residues 74–134). The second conserved domain is an E1-E2 ATPase domain (pfam00122: residues 142–410). The third conserved domain is a P-type ATPase domain (residues 643–701). The open reading frame of tre78757 is 2772 bp (CDS Sequence). The putative protein TRE78757 contains 923 amino acids, and also has three conserved domains similar to TRE76238. The structure of TRE76238 and TRE78757 proteins was generated using the Phyre2 server . The highest confidence models were based on the Neurospora model , and are shown in Additional file 1: Fig. S1.
Through the phylogenetic analysis shown in Fig. 1, we found that TRE76238 protein and its putative orthologs formed a cluster separate from the TRE78757 orthologs. TRE78757 protein is more closely related to the functionally characterized plasma membrane H+-ATPases of Saccharomyces cerevisiae, Neurospora crassa, and Schizosaccharomyces pombe . We predicted that the cluster containing TRE76238 may be specific to some filamentous fungi.
Deletion of tre76238 in T. reesei RUT-C30 showed growth retardation
This study aimed to examine the effect of reducing intracellular pH on cellulase production by blocking proton transport outside T. reesei cells. The genes tre76238 and tre78757 were deleted in hyper-cellulolytic T. reesei RUT-C30 to form the deletion mutants Δ76238 and Δ78757, respectively. Δ76238 and Δ78757 strains were separately cultivated in 100 mL MA medium with 2% (w/v) Avicel, 2% (w/v) lactose, or 2% (w/v) glucose as the sole carbon source, followed by measurement of the biomass dry weight (Fig. 2).
Knockout of tre78757 in T. reesei RUT-C30 had no significant effect on growth in glucose, lactose, and Avicel (Fig. 2) containing cultures. However, Δ76238 strain growth was significantly decreased (Fig. 2a, b) and formed a mycelium pellet during fermentation when cultured in glucose and lactose (see Additional file 1: Fig. S2). T. reesei RUT-C30 biomass accumulation reached a maximum after 48 h of culture. Slow biomass accumulation occurred at the early fermentation phase in Δ76238, which reached its highest level after 96 h using glucose as the carbon source (Fig. 2a). Δ76238 biomass accumulation was also severely delayed using lactose as the carbon source in the early fermentation phase (Fig. 2b). Δ76238 growth in Avicel was similar to that of T. reesei RUT-C30, but was only slightly retarded at the early fermentation phase (Fig. 2c). The results indicated that tre76238 deletion markedly impaired the growth of T. reesei RUT-C30 with glucose or lactose as the carbon source; however, this impairment could be partially eliminated using Avicel as the sole carbon source (Fig. 2c).
We tried to delete tre78757 in the Δ76238 strain to form a double deletion strain. A homokaryotic transformant of the tre78757 gene could not be obtained upon deleting it in the Δ76238 strain, suggesting that the function of plasma membrane H+-ATPase is essential for T. reesei RUT-C30. Double deletion of tre76238 and tre78757 is lethal for T. reesei RUT-C30. The H+-ATPase gene tre76238 is more important for growth than tre78757 in T. reesei RUT-C30.
The most significant difference in Δ76238 growth was found in the glucose condition, followed by lactose, and the least difference was found with Avicel. Therefore, cellulase repressor-glucose and inducer-lactose was used for further research.
Deletion of gene tre76238 impairs the ability to transport protons out of cells
To address whether tre76238 is necessary for intracellular pH homeostasis, the external pH and intracellular pH of the tre76238 deletion strain Δ76238 was measured using a pH electrode and fluorescent pH probe BCECF-AM (pKa: 6.98, working range is 6.0–8.0), respectively . Using the fluorescent pH probe BCECF-AM, greater green fluorescence intensity of mycelium represented lower proton concentration and higher pH . Green fluorescence was nearly undetected when intracellular pH was less than 6 .
The external pH of Δ76238 using glucose or lactose as the carbon source is shown in Fig. 3a, b. The external pH of Δ76238 was higher than that of T. reesei RUT-C30 using glucose or lactose as the carbon source (Fig. 3a, b). As shown in Fig. 3c for intracellular pH, only a few tiny green fluorescent particles were distributed in the hyphae of the mutant Δ76238 (Fig. 3c) in glucose and lactose conditions, compared with those in the parental strain T. reesei RUT-C30. This indicated that most hyphae of Δ76238 were acidic (pH < 6.0), except a few sub-organelles maintaining a pH greater than 6.0. However, whole hyphae of T. reesei RUT-C30 exhibited continuous green fluorescence. The intracellular pH of Δ76238 was apparently lower than that of T. reesei RUT-C30, showing that proton accumulation occurs in the cytosol of the mutant Δ76238 due to tre76238 deletion. Therefore, knockout of the H+-ATPase gene tre76238 had a great influence on the intracellular pH in T. reesei RUT-C30.
No significant differences in the external and intracellular pH were observed between Δ78757 and parental strains of T. reesei RUT-C30 using glucose or lactose as the carbon source (Additional file 1: Fig. S3A–D).
We further characterized the overall biological activity of T. reesei Δ76238 by measuring mitochondrial activity. The mitochondria of Δ76238 and T. reesei RUT-C30 were characterized by labeling with MitoTracker® Red CMXRos. Red fluorescence was almost undetected in the mutant Δ76238, whereas the hyphae of T. reesei RUT-C30 showed marked red fluorescence with glucose as the carbon source (Fig. 3d). No significant differences in mitochondrial activity were observed between Δ78757 and the parental strain T. reesei RUT-C30 using glucose or lactose as the carbon source (Additional file 1: Fig. S3E). The results indicated that aerobic metabolism in Δ76238 is very weak. The results also demonstrated that decreased mitochondrial activity was the reason for Δ76238 growth retardation.
Monosaccharide (glucose) and lactose metabolism easily produces acids through glycolysis compared with Avicel . Deleting tre76238 in T. reesei RUT-C30 destroyed the cellular ability to extrude protons from the cells and a large amount of acid produced by glucose metabolism could not be discharged, thus affecting growth. However, as a long-acting carbon source, Avicel was slowly hydrolyzed into glucose, thus accumulating less acid. This could be extruded slowly by TRE78757. Δ76238 growth could be restored by adding an appropriate amount of aqueous ammonia (see Additional file 1: Fig. S4), indicating that the growth delay occurred because of proton accumulation.
tre76238 deletion in T. reesei RUT-C30 led to high levels of cellulase production using the repressive carbon source glucose
We further measured the cellulase activities of Δ76238, as the intracellular pH of Δ76238 was obviously changed. Surprisingly, Δ76238 exhibited significantly increased cellulase production compared with the parental strain T. reesei RUT-C30 using glucose or lactose as the carbon source. As shown in Fig. 4a, b, Δ76238 exhibited high levels of FPase and PNPCase activity (both about 0.8 U/mL) after 5 days of cultivation. Meanwhile, T. reesei RUT-C30 had nearly no FPase and PNPCase activity using glucose as the carbon source. Using lactose as the carbon source, Δ76238 demonstrated two times higher FPase and PNPCase activity (both about 0.8 U/mL after 5 days of cultivation) than that of T. reesei RUT-C30 (Fig. 4c, d). When Δ76238 was cultivated in Avicel, FPase and PNPCase reached 1.2 U/mL, similar to that of T. reesei RUT-C30 (Additional file 1: Fig. S5). It is remarkable that tre76238 deletion resulted in continuous accumulation of cellulase in T. reesei RUT-C30 using glucose as the carbon source.
However, the Δ78757 strain exhibited no significant difference in cellulase production compared with T. reesei RUT-C30 in glucose, lactose, and Avicel (Additional file 1: Fig. S6). This was consistent with the lack of growth rate differences, accumulation of intracellular acid, and difference in mitochondrial activity detected between Δ78757 and T. reesei RUT-C30.
To further confirm the effects on enhancing cellulase production, the expression levels of the four main T. reesei cellulase genes, cbh1 (cellobiohydrolase I), cbh2 (cellobiohydrolase II), egl1 (endoglucanase I), and egl2 (endoglucanase II), were analyzed by real-time quantitative PCR (qPCR) (Fig. 5). In the Δ76238 strain, the expression levels of four cellulase genes (cbh1, cbh2, egl1, and egl2) were significantly increased compared to those in T. reesei RUT-C30 using glucose as the carbon source. These results were consistent with the enhanced cellulase production in Δ76238.
In addition, the expression levels of cbh1, cbh2, egl1, and egl2 in Δ76238 were significantly increased compared with those in T. reesei RUT-C30 using lactose as the carbon source (Additional file 1: Fig. S7).
The transcriptional activator xyr1 is an essential activator controlling the expression of the major cellulase genes . The xyr1 expression level was measured by qPCR (Fig. 5e). Interestingly, xyr1 continuously maintained a high expression level from 72 to 120 h in Δ76238 using glucose as the carbon source, indicating that the Δ76238 had a different xyr1 expression pattern compared with that of T. reesei RUT-C30. From 96 to 120 h, the xyr1 transcription level in Δ76238 was much higher than that in T. reesei RUT-C30. The possible reasons may involve significantly different expression patterns of cellulase genes and the main transcription factor xyr1 in Δ76238.
Ca2+channels are essential for cellulase production in Δ76238 using glucose as the carbon source
Aside from H+-ATPase, proton exchangers are also associated with proton and ion homeostasis, such as the Ca2+/H+ exchanger . A“H+-gated pathway” demonstrated that pH variations allow Ca2+ transportation via the Ca2+/H+ exchanger . We speculated that acid accumulation in Δ76238 hindered the growth of the strain. Ca2+/H+ exchange may also have played an important role in transporting protons out of the Δ76238 cells, along with transporting Ca2+ into the cytoplasm, to cause a Ca2+ burst in Δ76238 cells. Moreover, an appropriate Ca2+ concentration markedly stimulated the Ca2+ signal transduction pathway , which activated Crz1 (calcineurin-responsive zinc finger transcription factor 1) to induce cellulase expression in T. reesei [41, 42].
We, therefore, investigated the cytosolic Ca2+ level in Δ76238 with glucose as the sole carbon source. We used the Fluo-3/AM fluorescent dye , in which the green fluorescence intensity represents the relative amounts of free cytosolic Ca2+ . As shown in Fig. 6a, a stronger green fluorescence intensity was observed in Δ76238 compared with that in the parental strain T. reesei RUT-C30 at 96 h and 120 h, demonstrating that the level of cytosolic Ca2+ in Δ76238 was significantly increased compared to that in T. reesei RUT-C30.
Cytosolic Ca2+ is one of the secondary messengers that induces calcium signaling to trigger the downstream pathway . Our previous work involving Mn2+ elicitation and DMF induction showed that an increased cytosolic Ca2+ concentration can trigger calcium signal transduction pathways and induce cellulase expression in T. reesei [41, 42]. Cellulase production stimulated by low intracellular pH may be similar to that of Mn2+ and DMF stimulation . To test our hypothesis, the expression levels of the final calcium signaling gene crz1 (encoding Crz1) were quantitatively determined by qPCR. With glucose as the sole carbon source, the transcription level of crz1 in Δ76238 was markedly increased in Δ76238 compared with that in the parental strain T. reesei RUT-C30 (Fig. 6b). This demonstrated that the increased level of cytosolic Ca2+ is one reason for increased cellulase production in Δ76238.
To address whether the cytosolic Ca2+ burst in Δ76238 mediates enhanced cellulase production when glucose is the sole carbon source, we used LaCl3, a plasma membrane Ca2+ channel blocker, to prevent influx of external Ca2+ . We found that conidia of Δ76238 cannot germinate at 1 mM LaCl3 and above (Fig. 7a), whereas the parental strain RUT-C30 can grow well at 5 mM LaCl3. As shown in Fig. 7b, when glucose was the sole carbon source, cellulase production per g biomass of Δ76238 was obviously reduced, as LaCl3 concentration increased. Only a small amount of green fluorescence was observed in Δ76238 treated with 0.5 mM LaCl3 when glucose was the sole carbon source (Fig. 7c). These results confirmed that calcium signaling plays a dominant role in cellulase and biomass production in Δ76238.
Optimizing the medium promotes the growth of Δ76238 for cellulase production in a jar fermenter
Δ76238 showed significantly increased cellulase production under low-cost carbon source glucose conditions. However, the low growth rate due to intracellular acid accumulation using glucose as the carbon source, hindered its application. Δ76238 growth could be restored by adding appropriate amounts of aqueous ammonia (Additional file 1: Fig. S4). Proton accumulation suppressed Δ76238 growth in the early phase. Therefore, we hope to promote its growth rate by optimizing the medium in the first conidia germination stage. A simple optimization strategy is to use a nitrogen-rich medium as the seed medium, followed by transferring the culture to the fermentation medium using glucose as the sole carbon source, to produce cellulase in a jar fermenter.
We initially attempted to choose yeast extract, tryptone, and wheat bran as candidates for extra nitrogen sources, at different concentrations (5 g/L to 20 g/L) added in MA medium. Figure 8a shows that addition of 5 g/L to 10 g/L yeast extract was the best choice for promoting Δ76238 biomass production, and increased the biomass by 45% more than when there was no extra nitrogen addition after 72-h cultivation.
As shown in Fig. 8c of the flow chart, when cultivated in 100 mL MA medium containing 5 g/L extra yeast extract for 72 h, the Δ76238 biomass was collected by filtering and was transferred to a 3 L jar fermenter. This had a final working volume of 1 L MA medium, containing 2% (w/v) glucose as the sole carbon source for cellulase production. The FPase and PNPCase activities of Δ76238 had reached high levels on the 2nd day (Fig. 8b). Therefore, Δ76238 may be feasible for amplifying fermentation (Fig. 8c).
In this study, we investigated the influence of intracellular pH on cellulase production by T. reesei. Plasma membrane H+-ATPase from fungi is a proton pump that plays a key role in intracellular pH regulation [23, 28, 35]. In this study, two H+-ATPase genes, tre76238 and tre78757, were researched in T. reesei. Our results initially demonstrated that the H+-ATPase gene tre76238 is involved in cellulase induction in T. reesei, and that cellulase can be produced in the repressive carbon source glucose culture conditions. This extends our knowledge of cellulase regulation.
The hypersecreting mutant T. reesei RUT-C30 was selected as the parental strain for H+-ATPase gene knockout due to its defective carbon catabolite repression phenotype (mutated cre1). Carbon catabolite repression (CCR) in T. reesei is the means by which cells manage the priority use of glucose over more complex molecules such as cellulose. Although T. reesei RUT-C30 carries a truncated form of CREI and has a general loss of CREI-mediated carbon catabolite repression, T. reesei RUT-C30 produces very low levels of cellulases with glucose as the sole carbon source . The mutant Δ76238 was constructed by deletion of tre76238 in T. reesei RUT-C30. Δ76238 showed retardation in strain growth and significant cellulase production, with glucose as the sole carbon source, compared with the parental strain T. reesei RUT-C30. Deletion of tre76238 in mutant Δ76238 was re-complemented by transforming the wild-type tre76238 into its genome. The resulting complementation strain R76238 was obtained and demonstrated the restoration of growth and enzyme activities to levels similar to those of the starting strain T. reesei RUT-C30 (Additional file 1: Fig. S8). This demonstrated that gene knockout of tre76238 contributed to growth retardation and improved cellulase production in Δ76238 using glucose as the carbon source.
We also deleted tre76238 in the wild-type strain T. reesei QM6a and another mutant, T. reesei QM9414, which is closest to the wild-type strain. However, no cellulase production phenotype was detected under conditions of glucose as the sole carbon source except growth delay (Additional file 1: Fig. S9). The intact cre1 in both T. reesei QM6a and QM9414 might be the main reason for the lack of a cellulase production phenotype using glucose as the carbon source, which requires further study.
The growth rate of deletion strains showed that tre76238 plays a major role and tre78757 plays a minor role as plasma membrane H+-ATPases in T. reesei. The tre78757 gene, a functionally interchangeable isogene of tre76238, is dispensable for growth and is an additional function for tre76238. When tre76238 was deleted from T. reesei, tre78757 functioned as a plasma membrane H+-ATPase in T. reesei. Similarly, of the two H+-ATPase isogenes pma1 and pma2 in S. cerevisiae, pma1 is essential for growth, whereas pma2 is dispensable . Therefore, according to the gene functions, the H+-ATPase genes tre76238 and tre78757 were separately named for pma1 and pma2 in T. reesei.
We explored the reasons for significant cellulase production in Δ76238 using glucose as the carbon source. First, we analyzed the transcriptional levels of the main factor xyr1. xyr1 transcription in T. reesei RUT-C30 can occur under conditions of glucose as a cellulase-repressive carbon source due to the lack of cre1 . Stricker et al.  reported that the transcription level of xyr1 in T. reesei RUT-C30 in these glucose conditions gradually decreased with time, whereas the transcription level of xyr1 under conditions of lactose as a cellulase-inducing carbon source was continuous. Meanwhile, xyr1 was continuously transcribed in Δ76238 under conditions of glucose as a repressive carbon source (Fig. 5), which is quite different from that in the parental strain T. reesei RUT-C30.
Second, we analyzed the concentration of cytosolic Ca2+. Zhai et al.  reported that Ca2+ is transported in Arabidopsis cells, mainly through a Ca2+/H+ exchange system driven by the proton-motive force from plasma membrane H+-ATPase. As reported by Inesi et al. , H+ concentration reduction by conditions of high pH prevented Ca2+/H+ exchange. Deleting the H+-ATPase gene tre76238 in T. reesei impaired the transportation of protons out of cells, and significantly increased the concentration of intracellular protons (Fig. 3). Significantly increased intracellular Ca2+ levels were found in Δ76238 (Fig. 6). Chen et al.  reported that a cytosolic Ca2+ burst can markedly stimulate T. reesei cellulase production. The increased Ca2+ level was demonstrated to be necessary for increasing cellulase production in Δ76238. Δ76238 showed no cytosolic Ca2+ burst and could not produce cellulase using glucose as the carbon source after the Ca2+ channel blocker LaCl3 was added (Fig. 7). Plasma membrane Ca2+ channels can also affect the intracellular pH [38, 39]. High LaCl3 concentrations (> 1 mM) completely hindered the growth of Δ76238 (Fig. 7a). Therefore, calcium signaling was demonstrated to play a dominant role in Δ76238 cellulase and biomass production.
These results imply a mechanistic model of cellulase production in Δ76238 using glucose as the carbon source (Fig. 9). In Δ76238, it was difficult for intracellular protons to be exported from cells due to the defective function of H+-ATPase gene tre76238. Instead, Ca2+ channels, such as Ca2+/H+ exchangers , play an important role in transporting protons out of Δ76238 and balancing the intracellular pH. Intracellular acid accumulation in Δ76238 produced a proton gradient, and large pH variations allowed Ca2+ transportation by the Ca2+/H+ exchanger . This led to a cytosolic Ca2+ burst that activated the calcium signal transduction pathway, inducing cellulase production in T. reesei (Fig. 6). We, therefore, carried out a BLAST search of the Trichoderma reesei (https://genome.jgi.doe.gov/pages/blast-query.jsf?db=Trire2) genome sequence for genetic matches to the Ca2+/H+ exchanger genes from some organisms, including Saccharomyces cerevisiae  and Escherichia coli . Seven putative Ca2+/H+ exchanger genes (tre79599, tre55595, tre79398, tre56744, tre82544, tre62835, and tre68169) were identified in T. reesei; however, understanding their functions in Ca2+ transportation warrants further study. Moreover, knockout of these Ca2+/H+ exchanger genes may also change the intracellular pH in T. reesei, as occurs in mammalian cells .
Intracellular acid accumulation totally changed the intracellular environment, making cellulase production with glucose as a repressive carbon source, a more complicated process. Other reasons for enhancing Δ76238 cellulase production using glucose still need to be further researched, and may be meaningful for improving industrial cellulase production using T. reesei. Earlier studies have shown that many T. reesei intracellular β-glucosidases catalyze transglycosylation, glycosylating glucose to generate sophorose , which is the most effective soluble inducer for cellulase production . Proton accumulation in Δ76238 might activate the intracellular transglycosylation reaction to form the tiny cellulase inducer sophorose, thus inducing cellulase production in Δ76238.
Our study demonstrated that Δ76238 growth can be accelerated in the early phase, and cellulase production can be stable after transfer to a scale-up culture in new medium. Therefore, Δ76238 has the potential for industrial cellulase production using glucose as a low-cost carbon source. Depending on the results of this study, we predicted whether establishment of a controlled switch for tre76238 transcription downregulation in T. reesei RUT-C30 would allow normal growth during the early phase of fermentation with the switch turned on. The strain can then produce a large amount of cellulase during the late phase of fermentation with the switch turned off. This kind of smart T. reesei strain may have potential for industrial application.
In summary, this study reports a H+-ATPase gene deletion strain Δ76238 with greatly enhanced cellulase production in addition to intracellular acid accumulation and growth retardation using cellulase-repressive glucose as the sole carbon source (Fig. 9). Our results indicate that intracellular acid accumulation in Δ76238 stimulated a significant increase in the levels of cytosolic Ca2+. It also triggered Ca2+-CRZ1 signaling to induce cellulase gene transcription using glucose as the carbon source. Ca2+channels were demonstrated to be necessary for cellulase production using glucose as the carbon source in Δ76238. Δ76238 growth delay could be reversed by optimizing the medium’s nitrogen sources to produce ammonia. This allowed neutralization of intracellular acid in the early phase, which may be used for scale-up cellulase production using glucose as the carbon source. This study provides a new perspective for greatly altering the cellulase expression pattern in T. reesei Δ76238, and demonstrates a new mechanism for cellulase regulation in conditions of low intracellular pH.
Strains and culture conditions
The T. reesei hosts used in this research include QM9414 (ATCC 26921) and RUT-C30 (ATCC 56765). Spore suspensions were prepared by cultivating the fungus on potato-dextrose plates, after which the spores were harvested, suspended in a buffer containing 0.8% NaCl, 0.025% Tween 20 and 20% glycerol, and stored at − 80 °C.
To analyze enzyme production, conidia (final concentration 106/mL) of T. reesei strains were grown at 28 °C, in 100 mL of MA medium containing 2% (w/v) Avicel (PH-101, Sigma-Aldrich), 2% (w/v) lactose, or 2% (w/v) glucose as the sole carbon source . Mycelia were collected at different time intervals and kept frozen at − 80 °C for RNA extraction. The supernatant was used for enzyme assays.
Biomass concentration assay
For biomass analysis, the mycelium from lactose and glucose was harvested using pre-weighed glass microfiber filters (Cat. No. 1822-055, Whatman, Kent, UK) at appropriate time intervals, washed with water, dried at 65 °C for one day, and analyzed. The biomass dry weight from Avicel was measured as described by Zhang et al. . Each experiment was performed in three biological replicates.
Vector construction and transformation
Trichoderma reesei RUT-C30 lacking tku70  was used as the recipient for all targeted gene knockouts. Deletion cassettes for selected genes were constructed by ligating 0.9 to 1 kb 5′- and 3′-flanks of each gene to the hygromycin-resistant plasmid LML2.1 . As shown in Additional file 1: Fig. S10, the upstream fragment was ligated to the PacI- and XbaI-linearized LML2.1 using the ClonExpress™ II One Step Cloning Kit (Vazyme, Nanjing, China). Subsequently, the downstream fragment was inserted into the SwaI site to form the deletion cassettes. The re-complementation cassettes of the genes were constructed by ligating whole gene sequences (including the 1.5 kb promoter, gene coding sequence, and 1 kb terminator) to LML2.1. Re-complementation cassettes were transformed into the corresponding gene knockout mutants as described previously .
Deletion cassettes were transformed into T. reesei by Agrobacterium-mediated transformation . Re-complementation cassettes were transformed into the corresponding gene knockout mutants by Agrobacterium-mediated transformation . The hygromycin-resistant cassette can be self-excised by xylose-induced Cre recombinase , if necessary. The putative gene disruption mutants generated by double crossover were verified by diagnostic PCR using the primers XX-CF and XX-CR (XX represents the gene name). The fragments generated from the genome of transformants by PCR, using the primers XX-CF and XX-CR, were sequenced to verify the correct transformants. The primers used in this study are shown in Additional file 1: Table S1.
Bio-informatics analysis and phylogenetic analysis
Protein sequences were obtained from the Joint Genome Institute of Department of Energy (USDOE-JGI) website (http://genome.jgipsf.org/Trire2/). Homologs of T. reesei proteins were identified using BLASTP (http://blast.ncbi.nlm.nih.gov/), with an E value < 10−5 applied as a cutoff. Putative transmembrane regions were predicted by the TMHMM program v.2.0 (http://www.cbs.dtu.dk/services/TMHMM-2.0/). Protein modeling was performed using the PHYRE2 server . Alignments of multiple protein sequences were performed using MUSCLE . Phylogenetic analysis of protein was carried out in MEGA6 using the neighbor-joining method with 1000 bootstrap replicates.
Cellulase production in a jar fermenter
For promoting the growth of T. reesei strains using glucose as the sole carbon source, MA medium was optimized by separately adding different nitrogen sources (5 g/L or 10 g/L yeast extract, 5 g/L or 10 g/L tryptone, 10 g/L or 20 g/L wheat bran). After determining the best nitrogen source for growth, T. reesei strains were cultured in 100 mL optimized MA medium in the early phase (3 days), adding 5 g/L yeast extract. The strains were washed and transferred into a 3 L jar fermenter (Baoxing BIO-ENGINEERING EQUIPMENT, shanghai, China) with a final working volume of 1 L MA medium, containing 2% (w/v) glucose with 10% inoculation for the late phase of cellulase production. The supernatant was used for enzyme assays.
RNA isolation and real-time quantitative PCR (RT-qPCR)
The levels of gene-specific mRNA were assessed using RT-qPCR as per our previous study . In brief, total RNA was carefully extracted from frozen mycelia using a FastRNA Pro Red Kit (MPbio, Irvine, CA, USA) as per the manufacturer’s instructions. Total RNA (500 ng) was reverse-transcribed and cDNA was synthesized using the PrimeScript RT Reagent Kit with gDNA eraser (TaKaRa, Japan), according to the manufacturer’s instructions. qPCR was performed using an ABI StepOne thermocycler (Applied Biosystems, Foster City, CA, USA) and the TransStart TipTop Green qPCR SuperMix (TransGen, Shanghai, China) with 200 nM of forward and reverse primers (Additional file 1: Table S1). Thermal cycling was conducted under the following conditions: an initial denaturation step at 95 °C, followed by 40 amplification cycles of 5 s at 94 °C and 60 s at 64 °C. For transcription analysis, an SYBR green assay with reference to the sar1 gene was performed . Melt curves were obtained after each RT-qPCR run to confirm the specificity of amplification and the absence of primer dimers.
Enzyme activity assays
Filter paper hydrolase (FPase) activity, representing total extracellular cellulase activity, was determined using the 3, 5-dinitrosalicylic acid method .
Cellobiohydrolase activity (pNPCase) was determined using 5 mM p-nitrophenol-d-cellobioside (Sigma-Aldrich) as a substrate in 50 mM sodium acetate buffer at pH 5.0 . The release of p-nitrophenol was assessed by measuring absorbance at 405 nm. One unit of enzymatic activity was defined as 1 μmol of p-nitrophenol released from the substrate per minute.
Intracellular pH was detected using the fluorescent pH probe BCECF-AM (pKa: 6.98, working range is 6.0–8.0) . Living cell green fluorescence was measured using an S Plan Fluor ELWD 40×, 0.45 numerical aperture (NA) objective and a digital sight camera on an Eclipse Ti inverted Nikon, using a FITC filter with excitation filters from 420 nm to 490 nm, 10 nm intervals, and an emission filter of 535 nm.
Mitochondrial activity was detected using MitoTracker® Red CMXRos, using a Texas Red filter with excitation filters from 500 nm to 620 nm, 10 nm intervals, and an emission filter of 670 nm. The fluorescence was resolved from background fluorescence using the CareStream Multispectral program.
Fluo-3/AM (Sigma) was used to assess the level of cytoplasmic Ca2+ in T. reesei according to the manufacturer’s protocol. Fluo-3/AM (50 μM final concentration) was loaded into cells by incubation at 37 °C for 30 min, and the cells were then washed thrice with phosphate-buffered saline. Images of Ca2+ green fluorescence were obtained using an S Plan Fluor ELWD 40x, 0.45 numerical aperture (NA) objective and a digital sight camera on an Eclipse Ti inverted Nikon or Nikon A1R confocal microscope, comprising an FITC filter (420–490 nm band-pass excitation filter, and emission filter of 535 nm). The intensity of green fluorescence was quantified using NIS-Elements F package software. To eliminate the contribution of background fluorescence, cells without Fluo-3 AM labeling were also imaged under identical conditions.
All experiments were carried out at least three times with identical or similar results. The error values indicate the standard deviation (SD) from the mean of triplicates. Statistical significance was calculated using Student’s t test analysis with a significance of p < 0.05.
Availability of data and materials
All data generated or analyzed during this study are included in this published article and its additional files.
calcineurin-responsive zinc finger transcription factor 1
filter paper hydrolase activity, representing total extracellular cellulase activity
Ulaganathan K, Goud BS, Reddy MM, Kumar VP, Balsingh J, Radhakrishna S. Proteins for breaking barriers in lignocellulosic bioethanol production. Curr Protein Pept Sci. 2015;16:100–34.
Lynd LRWP, van Zylu WH, Pretorius IS. Microbial cellulose utilization: fundamentals and biotechnology. Microbiol Mol Biol Rev. 2002;1:739.
Tisch D, Kubicek CP, Schmoll M. New insights into the mechanism of light modulated signaling by heterotrimeric G-proteins: ENVOY acts on gna1 and gna3 and adjusts cAMP levels in Trichoderma reesei (Hypocrea jecorina). Fungal Genet Biol. 2011;48:631–40.
Zhao S, Yan YS, He QP, Yang L, Yin X, Li CX, Mao LC, Liao LS, Huang JQ, Xie SB, et al. Comparative genomic, transcriptomic and secretomic profiling of Penicillium oxalicum HP7-1 and its cellulase and xylanase hyper-producing mutant EU2106, and identification of two novel regulatory genes of cellulase and xylanase gene expression. Biotechnol Biofuels. 2016;9:203.
Xu Q, Singh A, Himmel ME. Perspectives and new directions for the production of bioethanol using consolidated bioprocessing of lignocellulose. Curr Opin Biotechnol. 2009;20:364–71.
Peterson R, Nevalainen H. Trichoderma reesei RUT-C30–thirty years of strain improvement. Microbiology. 2012;158:58–68.
Hakkinen M, Sivasiddarthan D, Aro N, Saloheimo M, Pakula TM. The effects of extracellular pH and of the transcriptional regulator PACI on the transcriptome of Trichoderma reesei. Microb Cell Fact. 2015;14:63.
Bischof RH, Ramoni J, Seiboth B. Cellulases and beyond: the first 70 years of the enzyme producer Trichoderma reesei. Microb Cell Fact. 2016;15:106.
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;5:2128–37.
Ilmén MTC, Penttilä M. The glucose repressor gene cre1 of Trichoderma: isolation and expression of a full-length and a truncated mutant form. Mol Gen Genet MGG. 1996;1:451–60.
Mello-De-Sousa TM, Gorsche R, Rassinger A. A truncated form of the Carbon catabolite repressor 1 increases cellulase production inTrichoderma reesei. Biotechnol Biofuels. 2014;7:129.
Portnoy T, Margeot A, Linke R. The CRE1 carbon catabolite repressor of the fungus Trichoderma reesei: a master regulator of carbon assimilation. BMC Genomics. 2011;12:269.
Nakari-Setala T, Paloheimo M, Kallio J, Vehmaanpera J, Penttila M, Saloheimo M. Genetic modification of carbon catabolite repression in Trichoderma reesei for improved protein production. Appl Environ Microbiol. 2009;75:4853–60.
Strauss J, Mach RL, Zeilinger S, Hartler G, Stöfer G, Wolschek M. CRE1, the carbon catabolite repressor protein from Trichoderma reesei. FEBS Lett. 1995;376:103–7.
Furukawa T, Shida Y, Kitagami N, Mori K, Kato M, Kobayashi T, Okada H, Ogasawara W, Morikawa Y. Identification of specific binding sites for XYR1, a transcriptional activator of cellulolytic and xylanolytic genes in Trichoderma reesei. Fungal Genet Biol. 2009;46:564–74.
Le Crom S, Schackwitz W, Pennacchio L, Magnuson JK, Culley DE, Collett JR, Martin J, Druzhinina IS, Mathis H, Monot F, et al. Tracking the roots of cellulase hyperproduction by the fungus Trichoderma reesei using massively parallel DNA sequencing. Proc Natl Acad Sci USA. 2009;106:16151–6.
Knapp JS, Legg M. The effect of different cellulosic growth substrates and pH on the production of cellulolytic enzymes by Trichoderma reesei. J Appl Microbiol. 1986;61:11.
Adav SS, Ravindran A, Chao LT, Tan L, Singh S, Sze SK. Proteomic analysis of pH and strains dependent protein secretion of Trichoderma reesei. J Proteome Res. 2011;10:4579–96.
Bailey MJ, Buchert J, Viikari L. Effect of Ph on production of xylanase by Trichoderma reesei on xylan-based and cellulose based media. Appl Microbiol Biotechnol. 1993;40:224–9.
Xiong H, von Weymarn N, Leisola M, Turunen O. Influence of pH on the production of xylanases by Trichoderma reesei Rut C-30. Process Biochem. 2004;39:731–6.
Li C, Yang Z, Zhang RH, Zhang D, Chen S, Ma L. Effect of pH on cellulase production and morphology of Trichoderma reesei and the application in cellulosic material hydrolysis. J Biotechnol. 2013;168:470–7.
Valkonen M, Penttila M, Bencina M. Intracellular pH responses in the industrially important fungus Trichoderma reesei. Fungal Genet Biol. 2014;70:86–93.
Portillo F. Regulation of plasma membrane H + -ATPase in fungi and plants. Biochim Biophys Acta. 2000;1469:31–42. https://doi.org/10.1016/S0304-4157(99)00011-8.
Casey JR, Grinstein S, Orlowski J. Sensors and regulators of intracellular pH. Nat Rev Mol Cell Biol. 2010;11:50–61.
Serrano R. Structure and function of proton translocating ATPase in plasma membranes of plants and fungi. Biochim Biophys Acta. 1988;1:1–28.
Remy E, Meyer M, Blaise F, Chabirand M, Wolff N, Balesdent MH, Rouxel T. The Lmpma1 gene of Leptosphaeria maculans encodes a plasma membrane H+ -ATPase isoform essential for pathogenicity towards oilseed rape. Fungal Genet Biol. 2008;45:1122–34.
Serrano R, et al. Yeast plasma membrane ATPase is essential for growth and has homology with (Na|[plus]| |[plus]| K|[plus]|), K|[plus]|- and Ca2|[plus]|-ATPases. Nature. 1986;319:689–93.
Ghislain M, Goffeau A. The pma1 and pma2 H+ -ATPases from Schizosaccharomyces pombe are functionally interchangeable. J Biol Chem. 1991;266:18276–9.
Mccusker JHPDS, Haber JE. Pleiotropic plasma membrane ATPase mutations of Saccharomyces cerevisiae. Mol Cell Biol. 1987;7:4082–8.
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;26:553–60.
Jourdier E, Baudry L, Poggi-Parodi D, Vicq Y, Koszul R, Margeot A, Marbouty M, Bidard F. Proximity ligation scaffolding and comparison of two Trichoderma reesei strains genomes. Biotechnol Biofuels. 2017;10:151.
Fernandes AR, Sa-Correia I. Transcription patterns of PMA1 and PMA2 genes and activity of plasma membrane H+ -ATPase in Saccharomyces cerevisiae during diauxic growth and stationary phase. Yeast. 2003;20:207–19.
Kane PM. Proton transport and pH control in Fungi. In: Advances in experimental medicine and biology. 2016. p. 33–68.
Bennett-Lovsey RM, Herbert AD, Sternberg MJ, Kelley LA. Exploring the extremes of sequence/structure space with ensemble fold recognition in the program Phyre. Proteins. 2008;70:611–25.
Kuhlbrandt WZ, Dietrich J. Structure, mechanism, and regulation of the neurospora plasma membrane H-ATPase. Science. 2002;297(5587):1692–6.
Rochon P, Jourdain M, Mangalaboyi J, Fourrier F, Soulie-Begu S, Buys B, Dehlin G, Lesage JC, Chambrin MC, Mordon S. Evaluation of BCECF fluorescence ratio imaging to properly measure gastric intramucosal pH variations in vivo. J Biomed Opt. 2007;12:064014.
Franck P, Petitipain N, Cherlet M. Measurement of intracellular pH in cultured cells by flow cytometry with BCECF-AM. J Biotechnol. 1996;46:187–95.
Inesi G, Tadini-Buoninsegni F. Ca(2+)/H (+) exchange, lumenal Ca(2+) release and Ca (2+)/ATP coupling ratios in the sarcoplasmic reticulum ATPase. J Cell Commun Signal. 2014;8:5–11.
Lewis D, Pilankatta R, Inesi G, Bartolommei G, Moncelli MR, Tadini-Buoninsegni F. Distinctive features of catalytic and transport mechanisms in mammalian sarco-endoplasmic reticulum Ca2+ ATPase (SERCA) and Cu+ (ATP7A/B) ATPases. J Biol Chem. 2012;287:32717–27.
Chen L, Zou G, Wang J, Wang J, Liu R, Jiang Y, Zhao G, Zhou Z. Characterization of the Ca(2+)—responsive signaling pathway in regulating the expression and secretion of cellulases in Trichoderma reesei Rut-C30. Mol Microbiol. 2016;100:560–75.
Chen Y, Shen Y, Wang W, Wei D. Mn(2 +) modulates the expression of cellulase genes in Trichoderma reesei Rut-C30 via calcium signaling. Biotechnol Biofuels. 2018;11:54.
Chen Y, Wu C, Shen Y, Ma Y, Wei D, Wang W. N, N-dimethylformamide induces cellulase production in the filamentous fungus Trichoderma reesei. Biotechnol Biofuels. 2019;12:36.
Takahashi ACP, Lechleiter JD, Herman B. Measurement of intracellular calcium. Physiol Rev. 1999;79:1089–125.
Thewes S. Calcineurin-Crz1 signaling in lower eukaryotes. Eukaryot Cell. 2014;13:694–705.
Lang RJ, Hashitani H, Tonta MA, Suzuki H, Parkington HC. Role of Ca2+ entry and Ca2+ stores in atypical smooth muscle cell autorhythmicity in the mouse renal pelvis. Br J Pharmacol. 2007;152:1248–59.
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. https://doi.org/10.1111/mmi.12824.
Stricker AR, Steiger MG, Mach RL. Xyr1 receives the lactose induction signal and regulates lactose metabolism in Hypocrea jecorina. FEBS Lett. 2007;581:3915–20.
Zhai J, Xu H, Cong X, Deng Y, Xia Z, Huang X, Hao G, Jiang X. Ca2+/H+ exchange in the plasma membrane of Arabidopsis thaliana leaves. Acta Physiol Plant. 2012;35:161–73.
Cunningham KW, Fink GR. Calcineurin inhibits VCX1-dependent H+/Ca2+ exchange and induces Ca2+ ATPases in Saccharomyces cerevisiae. Mol Cell Biol. 1996;16:2226–37.
Ivey DM, Guffanti AA, Zemsky J. Cloning and characterization of a putative Ca2+/H+ antiporter gene from Escherichia coli upon functional complementation of Na+/H+ antiporter-deficient strains by the overexpressed gene. J Biol Chem. 1993;268:11296–303.
Guo B, Sato N, Biely P, Amano Y, Nozaki K. Comparison of catalytic properties of multiple beta-glucosidases of Trichoderma reesei. Appl Microbiol Biotechnol. 2016;100:4959–68.
Li Y, Liu C, Bai F, Zhao X. Overproduction of cellulase by Trichoderma reesei RUT C30 through batch-feeding of synthesized low-cost sugar mixture. Bioresour Technol. 2016;216:503–10.
Zhang J, Zhang G, Wang W, Wang W, Wei D. Enhanced cellulase production in Trichoderma reesei RUT C30 via constitution of minimal transcriptional activators. Microb Cell Fact. 2018;17:75.
Zhang L, Zhao X, Zhang G, Zhang J, Wang X, Zhang S, Wang W, Wei D. Light-inducible genetic engineering and control of non-homologous end-joining in industrial eukaryotic microorganisms: LML 3.0 and OFN 1.0. Sci Rep. 2016;6:20761.
Lv D, Wang W, Wei D. Construction of two vectors for gene expression in Trichoderma reesei. Plasmid. 2012;67:67–71.
Edgar RC. MUSCLE: a multiple sequence alignment method with reduced time and space complexity. BMC Bioinform. 2004;5:113.
Steiger MG, Mach RL, Mach-Aigner AR. An accurate normalization strategy for RT-qPCR in Hypocrea jecorina (Trichoderma reesei). J Biotechnol. 2010;145:30–7.
Tk G. Measurement of cellulase activities. Pure Appl Chem. 1987;59:257–68.
This research was supported by the Open Funding Project of the State Key Laboratory of Bioreactor Engineering and the Fundamental Research Funds for the Central Universities (No. 222201714053).
Ethics approval and consent to participate
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.