Skip to main content

Advertisement

Dissecting cellobiose metabolic pathway and its application in biorefinery through consolidated bioprocessing in Myceliophthora thermophila

Article metrics

Abstract

Background

Lignocellulosic biomass has long been recognized as a potential sustainable source for industrial applications. The costs associated with conversion of plant biomass to fermentable sugar represent a significant barrier to the production of cost-competitive biochemicals. Consolidated bioprocessing (CBP) is considered a potential breakthrough for achieving cost-efficient production of biomass-based fuels and commodity chemicals. During the degradation of cellulose, cellobiose (major end-product of cellulase activity) is catabolized by hydrolytic and phosphorolytic pathways in cellulolytic organisms. However, the details of the two intracellular cellobiose metabolism pathways in cellulolytic fungi remain to be uncovered.

Results

Using the engineered malic acid production fungal strain JG207, we demonstrated that the hydrolytic pathway by β-glucosidase and the phosphorolytic pathway by phosphorylase are both used for intracellular cellobiose metabolism in Myceliophthora thermophila, and the yield of malic acid can benefit from the energy advantages of phosphorolytic cleavage. There were obvious differences in regulation of the two cellobiose catabolic pathways depending on whether M. thermophila JG207 was grown on cellobiose or Avicel. Disruption of Mtcpp in strain JG207 led to decreased production of malic acid under cellobiose conditions, while expression levels of all three intracellular β-glucosidase genes were significantly up-regulated to rescue the impairment of the phosphorolytic pathway under Avicel conditions. When the flux of the hydrolytic pathway was reduced, we found that β-glucosidase encoded by bgl1 was the dominant enzyme in the hydrolytic pathway and deletion of bgl1 resulted in significant enhancement of protein secretion but reduction of malate production. Combining comprehensive manipulation of both cellobiose utilization pathways and enhancement of cellobiose uptake by overexpression of a cellobiose transporter, the final strain JG412Δbgl2Δbgl3 produced up to 101.2 g/L and 77.4 g/L malic acid from cellobiose and Avicel, respectively, which corresponded to respective yields of 1.35 g/g and 1.03 g/g, representing significant improvement over the starting strain JG207.

Conclusions

This is the first report of detailed investigation of intracellular cellobiose catabolism in cellulolytic fungus M. thermophila. These results provide insights that can be applied to industrial fungi for production of biofuels and biochemicals from cellobiose and cellulose.

Background

Lignocellulosic biomass has long been recognized as a potential sustainable source for many industrial applications, including the biosynthesis of biofuels and commodity chemicals. Once established, these processes would make important contributions to rural development and enhanced sustainability of agricultural landscapes. The processes of microbial conversion of plant cell walls include cellulolytic enzyme production, saccharification of plant biomass, and synthesis of the desired products [1, 2]. The costs involved in conversion of insoluble plant lignocellulose into fermentable sugar remain a significant barrier to commercialization. Economic analysis has revealed that consolidated bioprocessing (CBP), which implies incorporating cellulase secretion and the biochemical biosynthetic pathway into a single cell, will enjoy the benefit of cost-efficient production of biomass-based fuels and commodity chemicals [3, 4]. Recently, cellulolytic organisms, such as Trichoderma, Neurospora, Clostridium, and Myceliophthora have been considered as the CBP strain candidates for producing biochemicals directly from plant cell walls [5,6,7,8].

When cellulolytic organisms grow on plant cell wall, extracellular endo-/exo-glucanases synergistically depolymerize cellulose with cellobiose as the major product [9]. After being imported into the cell by a cellodextrin transporter, cellobiose is mainly cleaved through two pathways; namely, the hydrolytic pathway and the phosphorolytic pathway. In the hydrolytic pathway, β-glucosidase converts cellobiose to two molecules of glucose, which can be further metabolized through glycolysis, while the phosphorolytic pathway uses cellobiose phosphorylase to cleave intracellular cellobiose with inorganic phosphate (Pi) to produce one glucose molecule and one glucose-1-phosphate molecule. Glucose-1-phosphate is then catalyzed to glucose-6-phosphate by phosphoglucomutase, without the need for ATP. Thus, the phosphorolytic pathway requires one ATP for each molecule of cellobiose to be metabolized by glycolysis, while two ATP molecules are consumed for phosphorylation of glucose generated by hydrolysis of cellobiose to form glucose-6-phosphate in the first step of glycolysis [10, 11]. In organisms, the energy advantages of phosphorolytic cleavage would provide extra ATP for microbial growth, cellulase synthesis, and even production of biochemicals from plant cellulose. The phosphorolytic pathway together with cellobiose transport have been incorporated into Saccharomyces cerevisiae for improved ethanol production from cellobiose [12, 13]. There is increasing evidence that a relative dominance of phosphorolytic cleavage over hydrolytic intracellular cleavage of cellobiose is widespread in cellulolytic anaerobic bacteria; for example, in Ruminococcus albus, Prevotella ruminicola, and Clostridium thermocellum [10, 14, 15]. Nevertheless, the detail of the two intracellular cellobiose utilization pathways in aerobic cellulolytic fungi remains to be investigated.

The thermophilic filamentous fungus Myceliophthora thermophila (Synonym: Thermothelomyces thermophilus) is able to secret a large amount of hydrolytic enzymes and grow robustly on cellulosic materials, making it exceptionally attractive for biorefinery application [16, 17]. Myceliophthora thermophila has been developed into a mature system for carbohydrate hydrolase production at industrial level (C1 strain) [18]. The multiple characteristics mentioned above and the capability to assimilate all sugar released from plant biomass qualify this fungus as the promising CBP strain candidate [19]. Recently, we incorporated the export system of malic acid and elevated metabolic flux of the reductive tricarboxylic acid (rTCA) pathway in M. thermophila. The resultant strain was able to produce malic acid by direct conversion of hemicellulose and cellulose [7]. Of four native synthetic pathways to malic acid, the rTCA pathway is considered the most simple and efficient. The process starts with the carboxylation of pyruvate (from glycolysis) to oxaloacetate and then subsequent reduction to l-malic acid [20, 21]. Theoretically, the pathway can fix 1 mol CO2/1 mol malate and processes the highest theoretical yield of 2 mol/mol glucose with redox balance. However, the energy balance for malic acid synthesis via the rTCA pathway is barely even, because modest ATP needs to support both microbial growth and cellulase synthesis. Therefore, the yield of malic acid should benefit from increased intracellular ATP concentration. In this study, using the previously engineered malic acid production strain JG207 of M. thermophila, we investigated the behaviors of the phosphorolytic and hydrolytic cellobiose catabolic pathways for application to malic acid production from cellobiose and Avicel. Through combined engineering of the two cellobiose utilization pathways and enhanced cellobiose uptake, malic acid production by M. thermophila showed significant improvement when grown on cellobiose or Avicel. These results provide novel insights that can be applied to industrial fungi engineering for the production of bio-based fuels and chemicals from plant biomass.

Results

Investigation of intracellular cellobiose metabolic pathway in M. thermophila

In cellulolytic filamentous fungi, the cleavage of intracellular cellobiose into glucose is mainly catalyzed via the hydrolytic pathway [22, 23]. Myceliophthora thermophila genome encodes at least eight genes encoding predicted β-glucosidase enzymes, including four secreted β-glucosidases and four intracellular enzymes. However, a previous systems-level transcriptomic study indicated that only three intracellular members (bgl1, Mycth_115968; bgl2, Mycth_38200; and bgl3, Mycth_62925) showed significant increased transcription levels during growth on Avicel or plant biomass [17, 24]. Although three secreted β-glucosidases were identified by mass spectrometry in the supernatant of M. thermophila culture grown on plant biomass [25], their expression levels were extremely low [17, 24]. Based on transcriptomic data, we hypothesized that the three intracellular β-glucosidase genes (bgl1, bgl2, and bgl3) might be the most relevant enzymes in the cellobiose hydrolytic pathway of M. thermophila.

In the cellobiose phosphorolytic pathway, there is only one predicted cellobiose phosphorylase encoding by gene Mycth_2308030 (named as Mtcpp here) in the M. thermophila genome, which was classified into Glycoside Hydrolase family 94 (GH94). Previously, one malate-producing strain JG207 of M. thermophila, which exhibited fast utilization of variable carbon sources including cellobiose and Avicel, was constructed through overexpressing malate transporter gene (mae) and pyruvate carboxylase gene (pyc) in the wild-type M. thermophila [7]. The transcriptional level of Mtcpp was found to be significantly increased in strain JG207 under cellobiose or Avicel conditions, compared with that in the wild-type M. thermophila strain via RT-qPCR analysis (Fig. 1b). This suggested the predicted MtCPP is of physiological relevance and might play a crucial role in the efficient metabolism of intracellular cellobiose. Based on these data, we predicted that both cellobiose cleavage pathways exist and are involved in intracellular cellobiose catabolism in M. thermophila (Fig. 1a).

Fig. 1
figure1

Intracellular metabolic pathway of cellobiose. a Overview of intracellular cellobiose cleavage. b Transcriptional levels of Mtcpp in malate-producing strain Myceliophthora thermophila JG207 grown on cellobiose and Avicel for 2 days. CPP cellobiose phosphorylase, BG β-glucosidase, CDT cellodextrin transporter, HXK hexose kinase

Disruption of Mtcpp dramatically affects malate production in M. thermophila

To assess the role of the phosphorolytic pathway on intracellular cellobiose utilization when M. thermophila is grown on cellobiose and cellulose, we created the cellobiose phosphorylase gene (Mtcpp) deletion strain on the background of the JG207 strain. The Mtcpp gene in the M. thermophila JG207 strain was disrupted via homologous replacement with a neo-inclusive cassette mediated by the CRISPR/Cas9 system [26]. The correct recombination events in the resultant mutants were confirmed by PCR analysis (Additional file 2: Figure S1). When grown on 75 g/L cellobiose, the resultant JG207ΔMtcpp strain produced 55.2 g/L malic acid, representing a 30.7% decrease in the malate titer when compared with the parental JG207 strain (79.7 g/L) (Fig. 2a). In contrast, protein secretion, extracellular β-glucosidase activity and biomass of the JG207ΔMtcpp strain were higher than in the parent strain; protein concentration, β-glucosidase activity and biomass were increased by 19.3%, 36.7% and 15%, respectively (Fig. 2c, d and Additional file 3: Figure S1). A previous report indicated that cellobiose and its derivatives can function as an inducer of lignocellulolytic enzyme gene expression in cellulolytic fungi [23]. The increased protein secretion might result from reduced efficiency of intracellular cellobiose degradation generated by the deletion of Mtcpp. Although a significantly increased transcriptional level of bgl2 was detected via RT-qPCR analysis (Fig. 2b), the deficiency of cellobiose utilization in disruption of Mtcpp was not rescued by an alternative cellobiose hydrolysis pathway enhanced by up-regulating β-glucosidase. This clearly suggests that the phosphorolytic pathway is the dominant pathway for cellobiose utilization in this thermophilic fungus when grown on cellobiose.

Fig. 2
figure2

Phenotypes of the strain JG207ΔMtcpp on cellobiose in shaking flask. a Profiles of malic acid production. b Transcriptional levels of intracellular β-glucosidase genes (bgl1, bgl2, and bgl3) in strain JG207ΔMtcpp grown on cellobiose for 2 days. The protein concentration (c) and activity of β-glucosidase (d) in the supernatant of JG207ΔMtcpp culture after 4 days on cellobiose. The values and error bars represent means and standard deviations of independent triplicate experiments, respectively

When grown on Avicel, surprisingly, no significant change was observed on production of malic acid by the JG207ΔMtcpp strain when compared with that of the JG207 parent strain (Fig. 3a). In addition, the biomass, protein secretion and enzyme activities of JG207ΔMtcpp culture were similar to those of strain JG207 (Fig. 3c, d and Additional file 3: Figure S1). Deletion of Mtcpp resulted in significantly elevated transcriptional levels of all three intracellular β-glucosidase genes, which might rescue the impairment of the disrupted phosphorolytic pathway on cellobiose metabolism (Fig. 3c). These results indicated that: (1) different regulation patterns of intracellular cellobiose degradation may emerge depending on whether M. thermophila is grown on cellobiose or cellulose, (2) the hydrolysis pathway of cellobiose might play a bigger role when M. thermophila is grown on Avicel.

Fig. 3
figure3

Physiological characterization of the strain carrying the deletion of Mtcpp on Avicel in shaking flask. a Time-course of malic acid production. b Transcriptional levels of intracellular β-glucosidase genes (bgl1, bgl2, and bgl3) in strain JG207ΔMtcpp grown on Avicel for 2 days. The protein concentration (c) and activity of β-glucosidase (d) in the supernatant of JG207ΔMtcpp culture after 4 days on Avicel. The values and error bars represent means and standard deviations of independent triplicate experiments, respectively

Enhanced cellobiose uptake facilitates faster cellobiose fermentation and malate production

Despite the energy advantage of the phosphorolytic pathway, the rate of cellobiose phosphorolysis was limited by the unfavorable energetics of the reaction (ΔG° = + 3.6 kJ mol−1) [27]. Rapid substrate supply was recognized as one strategy to maintain a high flux of reaction [28]. Moreover, fast uptake of substrate is a prerequisite for efficient cell factory production of biochemicals [25]. Cellobiose transporter gene cdt-1 from N. crassa has been systematically characterized and used for improving uptake of cellobiose [29]. Therefore, for more efficient uptake of cellobiose into the host, the genes cdt-1 was fused to the strong constitutive promoter of eif (encoding elongation initial factor) and incorporated into the M. thermophila JG207 strain. After confirmation of the presence of the transgene by PCR analysis (Additional file 2: Figure S1), the physiological characterizations of resultant strain JG207cdt was conducted when grown on cellobiose and cellulose.

When compared with the parent strain JG207, the uptake rate of cellobiose was improved by 51% in strain JG207cdt with 6 copies of cdt-1 in its genome (Fig. 4a and Additional file 4: Figure S1). When grown on cellobiose and Avicel for 4 days, strain JG207cdt produced 64.3 g/L and 55.8 g/L malic acid, representing 17% and 14% increases in the malate titer (55.0 g/L on cellobiose and 49.1 g/L on Avicel), respectively. After 7 days of culture, malic acid titers were 84.4 g/L and 69.7 g/L on cellobiose and Avicel, respectively, corresponding to yields of 1.13 g/g and 0.93 g/g, respectively (Fig. 4b, c). These results indicate that enhancement of cellobiose uptake led to increased production of biochemicals from plant biomass. Subsequently, transcriptional levels of the genes involved in intracellular cellobiose degradation were analyzed when substrate uptake was elevated. When compared with the parent strain JG207, the genes bgl1 and bgl2 encoding β-glucosidase exhibited significantly increased expression levels in strain JG207cdt under cellobiose conditions (Fig. 4d), while the transcription levels of all three intracellular β-glucosidase genes and cellobiose phosphorylase gene Mtcpp were significantly improved in strain JG207cdt when grown on Avicel (Fig. 4e). These results clearly show that to improve the performance of the cell as a factory for producing bio-based chemicals under both cellobiose and cellulose conditions, engineering the two intracellular cellobiose metabolic pathways simultaneously would be a good strategy.

Fig. 4
figure4

The acceleration of cellobiose uptake. a Cellobiose transport rate of the mycelia from the strain JG207cdt overexpressing cellobiose transporter gene cdt-1 from Neurospora crassa. Titers of malic acid in the culture of JG207cdt were determined when grown on cellobiose (b) and Avicel (c) after 4 days and 8 days in shaking flash. d, e Transcriptional levels of intracellular β-glucosidase genes and cellobiose phosphorylase gene in strain JG207cdt when grown on cellobiose and Avicel for 2 days

Elevation of metabolic flux of phosphorolytic pathway is propitious to efficient production of malic acid from cellobiose

Given the results above, overexpression of phosphorolytic enzyme-encoding gene was performed to improve the cell factory chemical production ability through enhancement of phosphorolytic pathway efficiency. In previous report, the gene Ctcpp from themophilic bacterium C. thermocellum has been characterized and functionally overexpressed in S. cerevisiae to improve ethanol production from cellobiose [28]. Therefore, companied with the cdt-1-overexpressing cassette, each of two cellobiose phosphorylase genes Mtcpp and Ctcpp behind strong constitutive promoter of eif were introduced into strain JG207 to generate the JG412 and JG413 strains, respectively. RT-qPCR analysis indicated that 4 copies of Ctcpp and 5 copies of Mtcpp were integrated into the genomes of the strains JG412 and JG413, repectively (Additional file 4: Figure S1). As expected, the activities of phosphorylase were increased by 15% and 27% in strains JG412 and JG413, respectively, when compared with the parental strain (Fig. 5a). These data suggest that the Ctcpp gene from anaerobic bacteria can be functionally expressed in thermophilic filamentous fungi. When grown on cellobiose, the JG412 and JG413 strains consistently produced 92.4 g/L and 88.84 g/L, respectively, 9.5% and 5.2% more than that produced by strain JG207cdt overexpressing cellobiose transporter gene cdt-1 (Fig. 5b). This indicates that the yield of malic acid can benefit from the energy advantages of phosphorolytic cleavage of cellobiose. However, as shown in Fig. 5c, extra overexpressing cellobiose phosphorylase gene had no effect on malate production under Avicel conditions, which is consistent with the hypothesis above that the hydrolytic pathway plays the major role for cellobiose utilization under cellulose conditions.

Fig. 5
figure5

Elevation of metabolic flux of phosphorolytic pathway by overexpressing cellobiose phosphorylase gene. Each of cellobiose phosphorylase genes (Ctcpp or Mtcpp) was co-incorporated with cellobiose transporter gene cdt-1 into M. thermophila JG207 to generate strains JG412 and JG413, respectively. a The activity of cellobiose phosphorylase in strain JG412 and JG413 relative to strain JG207cdt after 2 days of shaken-flask culture on cellobiose. Fermentation profiles of engineered M. thermophila with cellobiose phosphorylases on cellobiose (b) and Avicel (c) in shaking flask. Values are the mean of two independent fermentations and error bars represent the standard deviation

Malate production further improved by simultaneous engineering of two cellobiose catabolism pathways

To further tune the fungal cell factory to produce malic acid from cellobiose and cellulose, we sought to simultaneously engineer the two cellobiose catabolic pathways. Importantly, we knew there is only one phosphorylase gene in this thermophilic fungus, whereas there are three β-glucosidase genes that might be involved in the cellobiose hydrolytic pathway. In cellulolytic filamentous fungi, the expression levels of genes encoding β-glucosidase were much higher than those of phosphorylase genes when responding to cellobiose and even plant biomass [17, 23, 30], while deletion of all three main β-glucosidase genes led to defective cellobiose utilization [22, 31]. To further investigate the effect of β-glucosidase gene disruption in M. thermophila on production of malic acid from cellobiose and Avicel, seven mutant strains, including single, double, and triple mutant strains carrying different combinations of glucosidase gene deletion sets on the background of strain JG412, were constructed and tested. When grown on cellobiose or Avicel, four mutant strains (JG412Δbgl1, JG412Δbgl1Δbgl2, JG412Δbgl1Δbgl3, and JG412Δbgl1Δbgl2Δbgl3) with the deletion of bgl1 showed significantly decreased the titer of malic acid. In particular, strain JG412Δbgl1Δbgl2Δbgl3 produced the lowest malate titers (58.6 g/L and 52.0 g/L, corresponding to 6.1 g/g biomass and 3.9 g/g biomass), which were 34% and 23% less than parental strain JG412 (69.3 g/L and 92.4 g/L, corresponding to 13.7 g/g biomass and 7.5 g/g biomass) on cellobiose and Avicel, respectively (Fig. 6a, e), although final biomass was improved by 42.5% and 48.2% on cellobiose and Avicel, respectively. Two individual β-glucosidase deletion strains (JG412Δbgl2 and JG412Δbgl3) produced similar titers of malic acid and biomass compared with strain JG412. Only strain JG412Δbgl2Δbgl3 exhibited similar biomass production but gave an increased titer of malic acid when grown on cellobiose and Avicel. After growth on cellobiose and Avicel for 8 days, titers of malic acid reached 101.2 g/L and 77.4 g/L (corresponding to 14.6 g/g biomass and 8.0 g/g biomass, respectively), with respective yields of 1.35 g/g and 1.03 g/g (Fig. 6a, b and d, f). These results clearly suggest that the ability of the fungal cell factory to produce biochemicals can be further improved by fine regulation of two cellobiose metabolic pathways, combined with elevated uptake of substrate.

Fig. 6
figure6

Effect of the distinct combination of intracellular β-glucosidase gene deletion sets on production of malic acid. Physiological characterizations of the strains JG412Δbgl2Δbgl3 and JG412Δbgl1Δbgl2Δbgl3 were determined when grown on cellobiose (ac) and Avicel (df) in shaking flask. a, e Time-course of malate production. b, f Dry weights of mycelia in the culture of these strains grown on cellobiose and Avicel for 8 days. c, g Protein concentration in the supernatant after 4 days of culture. d, h Assay of ATP concentration in strains grown on cellobiose and Avicel for 2 days, respectively

In N. crassa and Penicillium decumbens, deletion of all main β-glucosidase genes that provide the bulk of glucose-generating activity from cellobiose led to impaired cellobiose degradation and enhancement of protein secretion [23, 32]. When assessing secreted protein of the mutant strains in response to cellobiose or Avicel, we found that four mutant strains (JG412Δbgl1, JG412Δbgl1Δbgl2, JG412Δbgl1Δbgl3, and JG412Δbgl1Δbgl2Δbgl3) displayed significantly increased protein secretion. The highest level of secreted protein was achieved in the culture of strain JG412Δbgl1Δbgl2Δbgl3 when grown on cellobiose and Avicel. These data indicated that β-glucosidase encoded by bgl1 was the dominant enzyme in converting cellobiose to glucose. The highest-level malate producer JG412Δbgl2Δbgl3 secreted a slightly elevated protein when grown on cellobiose and Avicel, whereas mutant strains JG412Δbgl2 and JG412Δbgl3 secreted protein at levels similar to parent strain JG412 (Fig. 6c, g).

Based on the fact that protein synthesis and secretion consume ATP, which is the cofactor of malate dehydrogenase catalyzing the conversion of oxaloacetate to malate, we hypothesized that decreased malate production might result from lower intracellular ATP concentration in mutant strain JG412Δbgl1Δbgl2Δbgl3. Therefore, assays of intracellular ATP were performed for the mutants. As shown in Fig. 6, the intracellular ATP concentrations of strain JG412Δbgl1Δbgl2Δbgl3 were decreased by 87% and 77% relative to parental strain JG412 when grown on cellobiose and Avicel, respectively (Fig. 6d, h).

Discussion

Cellulosic plant biomass has many desirable features as a potential energy source, but is difficult to efficiently convert into biofuels and commodity chemicals. The approach of CBP represents a promising technology for achieving this conversion in a cost-efficient manner [4]. To achieve low-cost production of bioethanol and biochemicals from cellulose via CBP, there is a real need for improved understanding of the mechanisms relating to intracellular cellobiose, which is the major end product of cellulase.

Previous works have reported that two pathways, the hydrolytic and phosphorolytic pathways, are used to efficiently degrade intracellular cellobiose in cellulolytic organisms. The hydrolytic pathway based on β-glucosidase is relatively widespread and is found in cellulolytic bacteria and filamentous fungi [11]. With bioenergy advantages, the phosphorolytic pathway seems to be limited almost entirely to bacteria and all published examples of cellobiose degradation are from bacteria, especially anaerobic bacteria [10, 33, 34]. The benefits of phosphorolytic cleavage of cellobiose can partly compensate for ATP consumption in supporting microbial growth and cellulase synthesis [11]. In contrast to cellulolytic anaerobic bacteria, cellular respiration in aerobic filamentous fungi can provide sufficient ATP for maintaining cell growth and cellulase production at the expense of NADH generated through catabolism of the carbon source. To date, few reports have emerged on the cellobiose degradation via phosphorylase in filamentous fungi. However, when developed as the CBP host, the energy advantages of phosphorolytic cleavage of cellobiose providing extra ATP in filamentous fungi would be beneficial in treatment of plant biomass. In this study, we found that enhancement of cellobiose catabolic flux led to improved expression levels of phosphorylase gene in M. thermophila when grown on cellobiose and Avicel, suggesting that the phosphorolytic pathway worked together with β-glucosidase to catalyze the degradation of cellobiose.

In filamentous fungi, systematic transcriptomic profiles of cellulase genes presented a large divergence in response to cellulose and its hydrolysate cellobiose [23]. Herein, disruption of the phosphorolytic pathway resulted in significantly decreased production of malic acid when M. thermophila JG207ΔMtcpp was grown on cellobiose. However, the reduction in malic acid production in strain JG207ΔMtcpp was not significantly different from that observed in the parent strain JG207 in cellulose condition. Transcriptional levels of all three intracellular β-glucosidase genes were significantly elevated to rescue the impairment of the disrupted phosphorolytic pathway on cellobiose metabolism under Avicel conditions. Enhancement of phosphorolytic cleavage by overexpression of the cellobiose phosphorylase gene also led to distinct fluctuations in the production of malic acid in response to cellobiose and Avicel. These trends revealed that in M. thermophila, the hydrolytic pathway plays the major role under cellulose conditions, whereas the phosphorolytic pathway contributed more in terms of intracellular cellobiose cleavage under cellobiose conditions.

The ability of a sugar transporter to dominate sugar input into cell factories that link extracellular biomass utilization and intracellular metabolic pathways is considered a critical factor for efficient biosynthesis of desired product in CBP [25, 29]. Engineering a sugar transporter to reduce released sugar was beneficial to relieving inhibition of fungal cellulases by their hydrolysis, for instance cellobiose and cellodextrin [35]. Moreover, the phosphorolysis reaction is unfavorably energetic and high substrate concentration is necessary to maintain an efficient flux of the reaction. In S. cerevisiae, cellobiose fermentation by the phosphorolytic pathway was greatly improved by using cellodextrin transporter with elevated rates of cellobiose transport [28]. When grown on cellulose, overexpression of cellobiose transporter gene cdt-1 from N. crassa simultaneously enhanced the metabolic flux of the hydrolytic and phosphorolytic pathways. However, when under cellobiose conditions, only β-glucosidase genes showed significantly increased transcriptional levels when uptake of cellobiose was improved. Even so, increased production of malic acid and protein secretion in culture supernatants of the strain overexpressing cdt-1 were detected when grown on cellobiose and Avicel, which is consistent with the previous report that a precise regulation network adjusts cellulase secretion and lignocellulose degradation according to intracellular metabolic efficiency in M. thermophila [7].

Previous works reported that cellobiose or a modified version of cellobiose function as an inducer of lignocellulolytic gene expression and when responding to cellobiose or Avicel, the deletion of the main β-glucosidase genes led to efficient induction of cellulase gene expression in filamentous fungi, such as N. crassa, Trichoderma reesei, and P. decumbens [23, 32, 36]. When these mutant strains with divergent combinations of glucosidase gene deletion sets were cultivated on cellobiose or cellulose, we found that the mutants with deletion of the main β-glucosidase gene bgl1 showed significantly increased protein secretion, which was distinguished from the phenomenon in N. crassa [23]. These data indicated that β-glucosidase encoded by bgl1 was the dominant intracellular enzyme catalyzing the conversion of cellobiose to glucose. Of note, secreted protein in the culture of strain JG412Δbgl1Δbgl2Δbgl3 was approximately fivefold that observed in parent strain JG412. However, the strategies for constructing CBP-enabling microbes are not the same as those for the development of fungal hyper-producers of cellulolytic enzymes [37]. When converting plant biomass into biochemicals by CBP-enabling microbes, the balance of cellulase secretion for lignocellulose degradation and rapid carbon utilization in the cell is required for elevated yield of the target product. Excessive secretion of protein would increase ATP consumption, which would compromise synthesis of the target product. Only strain JG207Δbgl2Δbgl3 showed a slightly improved protein secretion and a significantly increased titer of malic acid when grown on cellobiose and Avicel. Further fine tuning of the hydrolytic and phosphorolytic pathways of intracellular cellobiose degradation through improved balance of energy considerations and protein secretion is the next step to improving the performance of M. thermophila as a cell factory.

Conclusions

In this study, we demonstrated that both cellobiose cleavage pathways are used for intracellular cellobiose cleavage in M. thermophila. The bioenergetic advantages of phosphorolytic cleavage of cellobiose are propitious to efficient production of malic acid by this fungal CBP system. Myceliophthora thermophila displayed divergent regulation patterns of intracellular cellobiose catabolic pathways when grown on cellobiose and cellulose. The hydrolytic pathway plays a major role under cellulose conditions whereas the phosphorolytic pathway contributed more in terms of intracellular cellobiose metabolism under cellobiose conditions. After engineering the two cellobiose metabolic pathways simultaneously, production of malic acid by final strain JG412Δbgl2Δbgl3 showed significant improvement, producing up to 101.2 g/L and 77.4 g/L malic acid from cellobiose and Avicel, respectively.

Materials and methods

Strains and culture conditions

Myceliophthora thermophila JG207 was constructed previously, by overexpressing malate transporter gene and pyruvate carboxylase gene in M. thermophila ATCC42464 [7]. The JG207 strain and its derivates were grown on 1 × Vogel’s minimal medium supplemented with 2% glucose (MM medium) at 35 °C to obtain conidia, and antibiotic was added when needed for transformant screening.

Escherichia coli DH5α was used for vector construction and propagation. Strains were cultivated in Luria–Bertani (LB) medium with 100 µg/mL ampicillin for plasmid selection.

Vector construction for genetic engineering

For the construction of target genes overexpressing plasmids, cellobiose transporter gene (cdt-1, NCU00801) amplified from Neurospora crassa genomic DNA was ligated between SpeI/BamHI of pAN52-PgpdA-bar plasmid carrying the bar selectable marker to form cdt-1 overexpressing plasmid PgpdA-cdt1-bar, using the NEB Gibson assembly kit. The strong constitutive promoter of eif (Mycth_2297659) was employed to efficiently overexpress cellobiose phosphorylase genes. The polymerase chain reaction (PCR) fragment of cellobiose phosphorylase gene (Mtcpp, Mycth_2308030) from M. thermophila genome was amplified using paired primers (Additional file 1). Ctcpp (GenBank No. AB013109) from Clostridium thermocellum was codon-optimized on the basis of N. crassa codon frequency (http://www.kazusa.or.jp/codon/) and artificially synthesized. Terminator Tcbh of cbh1 (MYCTH_109566) was amplified from M. thermophila genome. With the aid of the NEB Gibson assembly kit, the amplicons were ligated between BglII/BamHI of pAN52-PgpdA-bar plasmid to generate the corresponding plasmids Peif-Mtcpp-bar and Peif-Ctcpp-bar.

The construction of sgRNA expression plasmids was performed as described previously [26]. Briefly, using M. thermophila genome sequence and the target gene as inputs, the sgRNACas9 tool [38] was used to identify specific sgRNAs target sites in Mtcpp (Mycth_2308030), bgl1 (Mycth_115968), bgl2 (Mycth_62925), and bgl3 (Mycth_ 8200). The oligos with low off-target probability was selected and protospacer sequences are presented in Additional file 1. Myceliophthora thermophila U6 promoter and a target-directed sgRNA fragment were amplified from U6p-sgRNA plasmid [26], assembled by overlapping PCR, and cloned into a pJET1.2/blunt cloning vector, forming the plasmids U6-Mtcpp -sgRNA, U6-bgl1-sgRNA, U6-bgl2-sgRNA, and U6-bgl3-sgRNA.

The vector carrying donor DNA was constructed to perform genomic modification. The 5’- and 3’-flanking fragments of Mtcpp, bgl1, bgl2, and bgl3 were amplified from the M. thermophila genome. These fragments and selectable marker cassettes PtrpC-neo from plasmid p0380-neo [39] were assembled using the NEB Gibson assembly kit and cloned into pPK2BarGFPD and digested with SpeI/EcoRV to generate the donor DNA sequences donor-Mtcpp-neo, donor-bgl1-neo, donor-bgl2-neo, and donor-bgl3-neo.

All vectors were constructed using E. coli DH5α and the target genes cloned into shuttle vectors were sequenced to verify the authenticity of the plasmid construction.

Transformation of Myceliophthora protoplasts

Polyethylene glycol-mediated transformation of M. thermophila protoplasts was performed as described previously [40]. For gene overexpression, 10 µg of linearized plasmid was transformed into M. thermophila protoplasts as needed. A plate supplemented with 100 μg mL−1 phosphinothricin was used for transformant selection.

For Mtccp deletion, the mixture of PCR amplicons of Ptef1-Cas9-TtprC cassette, U6p-Mtcpp-sgRNA cassette, and donor-Mtcpp-neo cassette was co-transformed into M. thermophlia JG207 protoplasts.

For multiple gene replacement involving β-glucosidase genes (bgl1, bgl2, and bgl3), sgRNA and donor expression cassettes were mixed with cas9-expression PCR cassette and co-transformed into JG412 strain. The putative transformants were selected with 100 μg/L G418, followed by sequential identification via PCR.

All primer sequences used in this study are listed in Additional file 1.

Shake flask cultivation

To evaluate the capabilities of malic acid production, batch cultivation was performed in 50 mL of medium inoculated with mature spores to a final concentration of 2.5 × 105 spores/mL in a 250-mL Erlenmeyer flask. The culture was incubated at 45 °C with shaking at 150 rpm in a rotary shaker. Samples (1 mL) were taken at different intervals. Each liter of the cultivation medium contained 75 g of carbon source (cellobiose or Avicel), 0.15 g of KH2PO4, 0.15 g of K2HPO4, 0.1 g of MgSO4·7H2O, 0.1 g of CaCl2·2H2O, 8 g of Bacto peptone, 1 mL of biotin (0.1 g/L), and 1 mL of trace element of Vogel’s salt, and was sterilized by autoclaving. Subsequently, sterilized CaCO3 was added as neutralizing agent to a final concentration of 80 g/L to keep the pH at approximately 6.0.

For intracellular ATP assays and RNA extraction cellobiose or Avicel, the strains were incubated in 50 mL of medium with a final concentration of 40 g/L CaCO3 in 250-mL Erlenmeyer flasks at 150 rpm in an orbital shaker for 2 days.

Metabolite analysis

Prior to organic acid detection in culture broth, 1 mL of 2 M sulfuric acid was added into 1 mL of well-mixed sample in a 15-mL tube and the mixture was incubated at 80 °C for 30 min. The mixture was vortexed at intervals to resolve the dicarboxylic acid adequately. Then, 2 mL of distilled water was added and an aliquot was used for metabolite analysis after mixing. Organic acid was monitored by high-performance liquid chromatography (HPLC) equipped with a Waters 2489 UV detector and an Aminex HPX-87H column (Bio-Rad) at 35 °C. The mobile phase was 5 mM H2SO4 with a constant flow rate of 0.5 mL/min. Data analysis was performed using the Waters e2695 separation module.

Assay of mycelium dry weight in culture

Quantification of cell mass was performed after 8 days culture, using a previously described method [41]. Briefly, 2 M HCl was added to a sample of known volume to solubilize undissolved CaCO3. The treated broth was centrifuged and washed twice with sterilized water, dried and weighed (w1 = cellulose + mycelium). The residual Avicel (w2 = cellulose) could be measured after solubilizing fungal biomass from the culture with a mixture of acetic acid and nitrate reagent [42], and then the mycelium dry weight could be calculated by subtracting w2 from w1.

Protein and enzyme activity assay

The assay of secreted protein and enzyme activities in the supernatants of the culture after 4 days on Avicel or cellobiose. Total secreted protein in supernatants was determined using a Bio-Rad protein assay (Bio-Rad) with bovine serum albumin as the standard at 595 nm. Endoglucanase activities of cell cultures were determined by Remazol brilliant Blue R-conjugated CMC purchased from Megazyme. β-Glucosidase activity was assayed with 1.0 mg/mL p-nitrophenyl β-d-glucopyranoside (Sigma-Aldrich) as the substrate in 50 mM citrate buffer (pH 4.8) at 50 °C. Sodium carbonate (1 M) was used to terminate the enzymatic reaction after 10 min and the released p-nitrophenol (pNP) was measured at 420 nm. One unit (U) of β-glucosidase activity was defined as the number of micromoles of pNP released per minute by the enzyme in 1 mL of culture supernatant.

Cellobiose consumption assays in M. thermophila

After 18 h of growth in 100 mL of 1 × Vogel’s salts plus 2% (w/v) glucose at 45 °C, the mycelia were then washed three times in 1 × Vogel’s salts without added carbon and then transferred to Vogel’s salts containing 0.5% (w/v) cellobiose for induction. After an additional 4 h, the mycelia were washed again as above and resuspended in the uptake buffer (1 × Vogel’s salts plus 10 mM cellobiose and 10 μg/mL cycloheximide) for 20 min. The amount of sugar remaining in the supernatant was then determined. After the consumption assay, the fungal biomass was blotted dry and completely dried overnight at 105 °C to determine the dry weight for data normalization.

Quantitative real time-PCR analysis

For the assay of relative transcription levels of targe genes, sample preparation and RNA extraction were performed using the method described previously [7]. Quantitative PCR was carried out with SYBR Green Realtime PCR Master Mix (Toyobo, Osaka, Japan) using a CFX96 real-time PCR detection system (Bio-Rad). The PCR reaction mixture (with three replicates) included 75 ng of template RNA, 0.4 μL of each primer (10 μM), 10 μL of RNA-direct SYBR® Green Realtime PCR Master Mix, and 8.2 μL of H2O. Negative controls contained an equal volume of water instead of RNA. Actin gene (MYCTH_2314852) was used as an internal control. The relative transcript level of each gene was calculated by the 2−ΔΔCt method.

For copy number assay of genes ectopically inserted into M. thermophila genome, fungal genomic DNA was extracted from transformants as described previously and used as the template for RT-qPCR. Quantitative PCR was carried out with SYBR Green Realtime PCR Master Mix (Toyobo, Osaka, Japan) with a CFX96 real-time PCR detection system (Bio-Rad), according to the manufacturer’s instructions. The oligonucleotides of the primers for each gene were optimized to obtain amplification efficiency between 95 and 105% and only one melting temperature on the melting curve.

The primers used for RT-qPCR are listed in Additional file 1.

Measurement of intracellular ATP levels and cellobiose phosphorylase activity

A 50-mL sample of mycelial medium was poured into a Buchner funnel fitted with four pieces of gauze. The residue was washed with distilled water until most CaCO3 was removed, and then immediately homogenized in liquid nitrogen and stored at − 80 °C. A prechilled mortar and pestle were used for frozen mycelia disruption. The resulting paste was transferred into l mL of phosphate-buffered saline (pH 7.4). After centrifugation for 10 min at 4 °C, clear supernatant was used for protein quantitation and further assay.

The intracellular ATP concentration was determined using the ATP Quantification kit (Sigma-Aldrich) according to the manufacturer’s instructions and normalized to the protein concentration in the extract.

The measurement of cellobiose phosphorylase activity was performed at 45 °C in an assay mixture (100 μL) consisting of 50 mM phosphate buffer (pH 7.4) and 10 mM cellobiose for 10 min. The reaction was stopped completely by adding 50 μL of Tris–HCl buffer (4 M, pH 7.0). Glucose-1-phophate concentrations were determined continuously using the glucose-1-phophate Assay Kit (Sigma-Aldrich) according to the provided protocol. One unit of cellobiose phosphorylase activity was defined as the amount of cellobiose phosphorylase releasing 1 μmol of glucose-1-phophate from cellobiose per minute.

Statistical significance tests

A one-tailed homoscedastic (equal variance) t test was employed for all statistical significance tests, unless otherwise noted. n.s represented p-value > 0.05; * represented p-value < 0.05; ** represented p-value < 0.01 and *** represented p-value < 0.001.

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its additional files.

Abbreviations

ATP:

adenosine triphosphate

Avicel:

microcrystalline cellulose

BG:

β-glucosidase

Cas9:

CRISPR associated protein 9

CBP:

consolidated bioprocessing

CDT:

cellodextrin transporter

CPP:

cellobiose phosphorylase

CRISPR:

clustered regularly interspaced short palindromic repeats

HXK:

hexose kinase

PCR:

polymerase chain reaction

RT-qPCR:

quantitative real time polymerase chain reaction

rTCA:

reductive tricarboxylic acid

References

  1. 1.

    Lynd LR, van Zyl WH, McBride JE, Laser M. Consolidated bioprocessing of cellulosic biomass: an update. Curr Opin Biotechnol. 2005;16(5):577–83.

  2. 2.

    den Haan R, van Rensburg E, Rose SH, Gorgens JF, van Zyl WH. Progress and challenges in the engineering of non-cellulolytic microorganisms for consolidated bioprocessing. Curr Opin Biotechnol. 2015;33:32–8.

  3. 3.

    Althuri A, Gujjala LKS, Banerjee R. Partially consolidated bioprocessing of mixed lignocellulosic feedstocks for ethanol production. Bioresour Technol. 2017;245(Pt A):530–9.

  4. 4.

    Himmel ME, Ding SY, Johnson DK, Adney WS, Nimlos MR, Brady JW, Foust TD. Biomass recalcitrance: engineering plants and enzymes for biofuels production. Science. 2007;315(5813):804–7.

  5. 5.

    Gusakov AV. Alternatives to Trichoderma reesei in biofuel production. Trends Biotechnol. 2011;29(9):419–25.

  6. 6.

    Olson DG, McBride JE, Shaw AJ, Lynd LR. Recent progress in consolidated bioprocessing. Curr Opin Biotechnol. 2012;23(3):396–405.

  7. 7.

    Li J, Lin L, Sun T, Xu J, Ji J, Liu Q, Tian C. Direct production of commodity chemicals from lignocellulose using Myceliophthora thermophila. Metab Eng. 2019. https://doi.org/10.1016/j.ymben.2019.05.007.

  8. 8.

    Zhao C, Chen S, Fang H. Consolidated bioprocessing of lignocellulosic biomass to itaconic acid by metabolically engineering Neurospora crassa. Appl Microbiol Biotechnol. 2018;102(22):9577–84.

  9. 9.

    Lynd LR, Weimer PJ, van Zyl WH, Pretorius IS. Microbial cellulose utilization: fundamentals and biotechnology. Microbiol Mol Biol Rev. 2002;66(3):506.

  10. 10.

    Zhang YHP, Lynd LR. Kinetics and relative importance of phosphorolytic and hydrolytic cleavage of cellodextrins and cellobiose in cell extracts of Clostridium thermocellum. Appl Environ Microb. 2004;70(3):1563–9.

  11. 11.

    Zhang YH, Lynd LR. Cellulose utilization by Clostridium thermocellum: bioenergetics and hydrolysis product assimilation. Proc Natl Acad Sci USA. 2005;102(20):7321–5.

  12. 12.

    Chomvong K, Kordic V, Li X, Bauer S, Gillespie AE, Ha SJ, Oh EJ, Galazka JM, Jin YS, Cate JH. Overcoming inefficient cellobiose fermentation by cellobiose phosphorylase in the presence of xylose. Biotechnol Biofuels. 2014;7:85.

  13. 13.

    Sadie CJ, Rose SH, den Haan R, van Zyl WH. Co-expression of a cellobiose phosphorylase and lactose permease enables intracellular cellobiose utilisation by Saccharomyces cerevisiae. Appl Microbiol Biotechnol. 2011;90(4):1373–80.

  14. 14.

    Lou JR, Dawson KA, Strobel HJ. Cellobiose and cellodextrin metabolism by the ruminal bacterium Ruminococcus albus. Curr Microbiol. 1997;35(4):221–7.

  15. 15.

    Lou J, Dawson KA, Strobel HJ. Role of phosphorolytic cleavage in cellobiose and cellodextrin metabolism by the ruminal bacterium Prevotella ruminicola. Appl Environ Microb. 1996;62(5):1770–3.

  16. 16.

    Singh B. Myceliophthora thermophila syn. Sporotrichum thermophile: a thermophilic mould of biotechnological potential. Crit Rev Biotechnol. 2016;36(1):59–69.

  17. 17.

    Berka RM, Grigoriev IV, Otillar R, Salamov A, Grimwood J, Reid I, Ishmael N, John T, Darmond C, Moisan MC, et al. Comparative genomic analysis of the thermophilic biomass-degrading fungi Myceliophthora thermophila and Thielavia terrestris. Nat Biotechnol. 2011;29(10):922–7.

  18. 18.

    Visser H, Joosten V, Punt PJ, Gusakov AV, Olson PT, Joosten R, Bartels J, Visser J, Sinitsyn AP, Emalfarb MA, et al. Development of a mature fungal technology and production platform for industrial enzymes based on a Myceliophthora thermophila isolate, previously known as Chrysosporium lucknowense C1. Ind Biotechnol. 2011;7(3):10.

  19. 19.

    Gu S, Li J, Chen B, Sun T, Liu Q, Xiao D, Tian C. Metabolic engineering of the thermophilic filamentous fungus Myceliophthora thermophila to produce fumaric acid. Biotechnol Biofuels. 2018;11(1):323.

  20. 20.

    Zelle RM, de Hulster E, van Winden WA, de Waard P, Dijkema C, Winkler AA, Geertman JM, van Dijken JP, Pronk JT, van Maris AJ. Malic acid production by Saccharomyces cerevisiae: engineering of pyruvate carboxylation, oxaloacetate reduction, and malate export. Appl Environ Microbiol. 2008;74(9):2766–77.

  21. 21.

    Brown SH, Bashkirova L, Berka R, Chandler T, Doty T, McCall K, McCulloch M, McFarland S, Thompson S, Yaver D, Berry A. Metabolic engineering of Aspergillus oryzae NRRL 3488 for increased production of l-malic acid. Appl Microbiol Biotechnol. 2013;97(20):8903–12.

  22. 22.

    Cai PL, Wang B, Ji JX, Jiang YS, Wan L, Tian CG, Ma YH. The putative cellodextrin transporter-like protein clp1 is involved in cellulase induction in Neurospora crassa. J Biol Chem. 2015;290(2):788–96.

  23. 23.

    Znameroski EA, Coradetti ST, Roche CM, Tsai JC, Iavarone AT, Cate JH, Glass NL. Induction of lignocellulose-degrading enzymes in Neurospora crassa by cellodextrins. Proc Natl Acad Sci USA. 2012;109(16):6012–7.

  24. 24.

    Xu G, Li J, Liu Q, Sun W, Jiang M, Tian C. Transcriptional analysis of Myceliophthora thermophila on soluble starch and role of regulator AmyR on polysaccharide degradation. Bioresour Technol. 2018;265:558–62.

  25. 25.

    Hara KY, Kobayashi J, Yamada R, Sasaki D, Kuriya Y, Hirono-Hara Y, Ishii J, Araki M, Kondo A. Transporter engineering in biomass utilization by yeast. FEMS Yeast Res. 2017. https://doi.org/10.1093/femsyr/fox061.

  26. 26.

    Liu Q, Gao R, Li J, Lin L, Zhao J, Sun W, Tian C. Development of a genome-editing CRISPR/Cas9 system in thermophilic fungal Myceliophthora species and its application to hyper-cellulase production strain engineering. Biotechnol Biofuels. 2017;10:1.

  27. 27.

    Alexander JK. Purification and specificity of cellobiose phosphorylase from Clostridium thermocellum. J Biol Chem. 1968;243(11):2899–904.

  28. 28.

    Ha SJ, Galazka JM, Joong OhE, Kordic V, Kim H, Jin YS, Cate JH. Energetic benefits and rapid cellobiose fermentation by Saccharomyces cerevisiae expressing cellobiose phosphorylase and mutant cellodextrin transporters. Metab Eng. 2013;15:134–43.

  29. 29.

    Galazka JM, Tian C, Beeson WT, Martinez B, Glass NL, Cate JH. Cellodextrin transport in yeast for improved biofuel production. Science. 2010;330(6000):84–6.

  30. 30.

    Liu Q, Li J, Gao R, Li J, Ma G, Tian C. CLR-4, a novel conserved transcription factor for cellulase gene expression in ascomycete fungi. Mol Microbiol. 2019;111(2):373–94.

  31. 31.

    Hildebrand A, Szewczyk E, Lin H, Kasuga T, Fan Z. Engineering Neurospora crassa for improved cellobiose and cellobionate production. Appl Environ Microbiol. 2015;81(2):597–603.

  32. 32.

    Chen M, Qin Y, Cao Q, Liu G, Li J, Li Z, Zhao J, Qu Y. Promotion of extracellular lignocellulolytic enzymes production by restraining the intracellular beta-glucosidase in Penicillium decumbens. Bioresour Technol. 2013;137:33–40.

  33. 33.

    Kim SK, Himmel ME, Bomble YJ, Westpheling J. Expression of a cellobiose phosphorylase from Thermotoga maritima in Caldicellulosiruptor bescii improves the phosphorolytic pathway and results in a dramatic increase in cellulolytic activity. Appl Environ Microbiol. 2018;84(3):e02348.

  34. 34.

    Liu N, Fosses A, Kampik C, Parsiegla G, Denis Y, Vita N, Fierobe HP, Perret S. In vitro and in vivo exploration of the cellobiose and cellodextrin phosphorylases panel in Ruminiclostridium cellulolyticum: implication for cellulose catabolism. Biotechnol Biofuels. 2019;12:208.

  35. 35.

    Voutilainen SP, Puranen T, Siika-Aho M, Lappalainen A, Alapuranen M, Kallio J, Hooman S, Viikari L, Vehmaanpera J, Koivula A. Cloning, expression, and characterization of novel thermostable family 7 cellobiohydrolases. Biotechnol Bioeng. 2008;101(3):515–28.

  36. 36.

    Zhou Q, Xu J, Kou Y, Lv X, Zhang X, Zhao G, Zhang W, Chen G, Liu W. Differential involvement of beta-glucosidases from Hypocrea jecorina in rapid induction of cellulase genes by cellulose and cellobiose. Eukaryot Cell. 2012;11(11):1371–81.

  37. 37.

    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.

  38. 38.

    Xie S, Shen B, Zhang C, Huang X, Zhang Y. sgRNAcas9: a software package for designing CRISPR sgRNA and evaluating potential off-target cleavage sites. PLoS ONE. 2014;9(6):e100448.

  39. 39.

    Xu J, Li J, Lin L, Liu Q, Sun W, Huang B, Tian C. Development of genetic tools for Myceliophthora thermophila. BMC Biotechnol. 2015;15:35.

  40. 40.

    Yang F, Gong Y, Liu G, Zhao S, Wang J. Enhancing cellulase production in thermophilic fungus Myceliophthora thermophila ATCC42464 by RNA interference of cre1 gene expression. J Microbiol Biotechnol. 2015;25(7):1101–7.

  41. 41.

    Wang B, Cai P, Sun W, Li J, Tian C, Ma Y. A transcriptomic analysis of Neurospora crassa using five major crop residues and the novel role of the sporulation regulator rca-1 in lignocellulase production. Biotechnol Biofuels. 2015;8:21.

  42. 42.

    Updegraff DM. Semimicro determination of cellulose in biological materials. Anal Biochem. 1969;32(3):420–4.

Download references

Acknowledgements

We thank all members of the Tian laboratory for their critical comments.

Funding

This work was supported by funding from National Key Program of Research and Development (2018YFA0900500), National Natural Science Foundation of China (NSFC31601013, 31670042, 31972879).

Author information

JL and CT designed the experiments. JL, SG, ZZ, BC, QL, TS, and WS performed metabolic engineering experiments. JL and CT analyzed the data and wrote the manuscript. All authors read and approved the final manuscript.

Correspondence to Chaoguang Tian.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Li, J., Gu, S., Zhao, Z. et al. Dissecting cellobiose metabolic pathway and its application in biorefinery through consolidated bioprocessing in Myceliophthora thermophila. Fungal Biol Biotechnol 6, 21 (2019) doi:10.1186/s40694-019-0083-8

Download citation

Keywords

  • Myceliophthora thermophila
  • Cellulose
  • Cellobiose
  • Malic acid
  • Metabolic engineering
  • Thermothelomyces thermophilus