Dissecting cellobiose metabolic pathway and its application in biorefinery through consolidated bioprocessing in Myceliophthora thermophila
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.
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.
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.
KeywordsMyceliophthora thermophila Cellulose Cellobiose Malic acid Metabolic engineering Thermothelomyces thermophilus
CRISPR associated protein 9
clustered regularly interspaced short palindromic repeats
polymerase chain reaction
quantitative real time polymerase chain reaction
reductive tricarboxylic acid
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 . 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) . 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 . 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 . 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.
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 , 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.
Disruption of Mtcpp dramatically affects malate production in M. thermophila
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) . Rapid substrate supply was recognized as one strategy to maintain a high flux of reaction . Moreover, fast uptake of substrate is a prerequisite for efficient cell factory production of biochemicals . Cellobiose transporter gene cdt-1 from N. crassa has been systematically characterized and used for improving uptake of cellobiose . 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.
Elevation of metabolic flux of phosphorolytic pathway is propitious to efficient production of malic acid from cellobiose
Malate production further improved by simultaneous engineering of two cellobiose catabolism pathways
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).
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 . 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 . 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 . 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 . 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 . 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 . 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 .
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 . 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 . 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.
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 . 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 . Briefly, using M. thermophila genome sequence and the target gene as inputs, the sgRNACas9 tool  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 , 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  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 . 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.
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 . 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 , 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 . 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.
We thank all members of the Tian laboratory for their critical comments.
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.
This work was supported by funding from National Key Program of Research and Development (2018YFA0900500), National Natural Science Foundation of China (NSFC31601013, 31670042, 31972879).
Ethics approval and consent to participate
Consent for publication
The authors declare that they have no competing interests.
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