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Cellulosic hydrocarbons production by engineering dual synthesis pathways in Corynebacterium glutamicum

Biotechnology for Biofuels and Bioproducts volume 15, Article number: 29 (2022) Cite this article

Abstract

Background

Lignocellulose provides the only practical carbohydrates feedstock for sustainable bioproduction of hydrocarbons as future alternative of fossil fuels. Production of hydrocarbons from lignocellulose is achieved by a biorefinery process chain including pretreatment to breakdown the crystalline structure for cellulase-catalyzed hydrolysis, detoxification of inhibitory compounds generated during pretreatment, enzymatic hydrolysis to fermentable monosaccharide sugars, and fermentation to hydrocarbon products. The major barriers on fermentative production of hydrocarbons from lignocellulose include two aspects: one is the inherent stress of pretreatment-derived inhibitors on microbial cells, the other is the toxicity of hydrocarbons to cell membranes. The microbial cell factory should be tolerant to both inhibitor stress and hydrocarbons toxicity.

Results

Corynebacterium glutamicum was selected as the starting strain of hydrocarbons synthesis since it is well adapted to lignocellulose hydrolysate environment. The dual hydrocarbon synthesis pathways were constructed in an industrial C. glutamicum S9114 strain. The first pathway was the regular one in microalgae composed of fatty acyl-acyl carrier protein (fatty acyl-ACP) reductase (AAR) and aldehyde deformylating oxygenase (ADO) with fatty acyl-ACP as precursor. The second pathway was the direct decarboxylation of free fatty acid by fatty acid decarboxylase (OleT) using the rich fatty acids from the disruption of the transcriptional regulator fasR gene. The transmembrane transportation of hydrocarbon products was avoided by secretively expressing the fatty acid decarboxylase (OleT) to the extracellular space. The hydrocarbons generation from glucose reached 29.2 mg/L, in which the direct decarboxylation pathway contributed more than 70% of the total hydrocarbons generation, and the AAR–ADO pathway contributed the rest 30%.

Conclusion

The dual hydrocarbon synthesis pathways (OleT and AAR–ADO pathways) were constructed in the inhibitors tolerant C. glutamicum S9114 strain for hydrocarbon production using lignocellulose feedstock as the starting feedstock. When corn stover was used for hydrocarbons production after dry acid pretreatment and biodetoxification, the hydrocarbons generation reached 16.0 mg/L. This study provided a new strategy for hydrocarbons synthesis using microbial cell factory suitable for lignocellulose feedstock.

Background

Current hydrocarbon fuels are dominantly produced from petroleum refining [1, 2]. The coming carbon-neutral economy requires the production of future aviation fuel and diesel in a sustainable way from renewable resources. Among all potential feedstocks, lignocellulose provides the only practical carbohydrates option for bioproduction of biofuels by its abundance and availability [3, 4].

Various microorganisms had been tested and engineered as microbial cell factories for hydrocarbons synthesis [5, 6]. The most acknowledged pathway is the decarbonylation of fatty acyl-ACP to fatty aldehydes by fatty acyl-ACP reductase (AAR) or the reduction of fatty acid by fatty acid reductase (FAR) [1, 7], then the fatty aldehydes are converted to hydrocarbons by aldehyde deformylating oxygenase (ADO) or aldehyde decarbonylase (ADS) [8, 9]. An alternative pathway is the direct decarboxylation of free fatty acids to terminal alkenes by fatty acid decarboxylase OleT [10], nonheme iron oxidase UndA [11], or fatty acid desaturase UndB [12] when abundant free fatty acids are available.

Pretreatment generally leads to the partial degradation of hemicellulose (mainly xylan) to furfural and cellulose to 5-hydroxymethyl furfural (HMF), and lignin to various phenolic compounds, along with other weak organic acids [13]. Biodetoxification fungus completely removes the most toxic inhibitors of furfural and HMF, as well as most of acetic acid and phenolics such as p-hydroxybenzaldehyde, vanillin, syringaldehyde, etc. However, the residual phenolics and acetic acid are not removed as completely as furfural and HMF because the extensive biodetoxification leads to the loss of xylose sugars. These residual inhibitors still show observable inhibitions to the cell growth and hydrocarbons synthesis metabolism of microorganisms such as Escherichia coli and most of the hydrocarbon synthesis strains. Furthermore, lipophilic hydrocarbons are toxic to cells due to the interference on cell membranes. The accumulation of hydrocarbons inside the cell increases the permeability and fluidity of the cell membrane and interferes with the function of membrane proteins, which in turn affects energy transfer and the stability of the cell membrane [14]. Previous studies showed that the microorganism C. glutamicum was unusually adaptive to lignocellulose hydrolysate environment by its strong tolerance to residual inhibitors of biodetoxifications and well utilization of rich vitamin B components in lignocellulose [15,16,17,18,19,20]. In this study, C. glutamicum was selected as the potential microbial cell factory [16, 18].

One of the uniqueness of C. glutamicum is that considerable free fatty acids are generated by C. glutamicum including oleic acid (C18:1), followed by palmitic acid (C16:0), and minor palmitoleic acid (C16:1) and stearic acid (C18:0) by the multi-enzyme complex fatty acid synthases (FASs) (one FAS-I modular and three FAS-II modules NCgl0281, NCgl0283 and NCgl0527) [21, 22]. The free fatty acids are accumulated and well maintained in extracellular space of C. glutamicum due to lack of β-oxidation pathway for fatty acid degradation, and lack of phosphatidic acid phosphatase (PAP) and diacylglycerol acyltransferase (DGAT) to triacylglyceride (microbial lipid) [23]. These advantages further suggest that C. glutamicum might be a favorable candidate of biorefinery hydrocarbons fermentation strains, though the cell membrane toxicity by hydrocarbons still exists.

We engineered an industrial C. glutamicum strain by constructing the dual hydrocarbon synthesis pathways in this study. One pathway was the regular algal pathway by fatty acyl-ACP reductase (AAR) and aldehyde deformylating oxygenase (ADO) with fatty acyl-CoA as precursor; the other pathway was the direct decarboxylation of fatty acid by fatty acids decarboxylase (OleT). The toxicity of the intracellularly generated hydrocarbons by transmembrane transportation was lessened by the secretive expression of OleT guided by a signal peptide. To increase the fatty acids substrate supply, the transcriptional regulator fasR gene was disrupted to increase C16 and C18 fatty acids as the additional substrate supply [24]. The resulting engineered C. glutamicum was applied for hydrocarbons fermentation using corn stover as feedstock for hydrocarbons production. This study provided a new strategy of metabolic engineering for hydrocarbons production using lignocellulose feedstock.

Results

Construction of AAR–ADO hydrocarbon synthesis pathway in C. glutamicum

To construct the first AAR–ADO pathway from the fatty acyl-ACP substrate for hydrocarbons synthesis, the fragments of the lipoyl-ACP reductase gene aar (synpcc7942_1594) and the fatty aldehyde decarbonylase gene ado (synpcc7942_1593) from Synechococcus elongatus PCC7942 were synthesized and the expression plasmids were constructed; then the plasmid were introduced to C. glutamicum S9114 (Fig. 1a, Box I). The two genes aar (synpcc7942_1594) and ado (synpcc7942_1593) were expressed under the control of promoter H36 with different alignments (C. glutamicum ZW1, ZW2, and ZW3 in Table 1). The gene combination of ado and aar with the consensus SD sequence aar-rbs-ado (ZW2) showed the optimal hydrocarbon generation among the gene alignments. Then this gene fragment aar-rbs-ado was integrated into the location of the TetR-type transcriptional regulator fasR to generate a recombinant C. glutamicum HW4. Figure 1b shows that the typical alkene components C21H44, C23H48, C28H58, C29H60 and C30H62, among other hydrocarbon components, were detected in the fermentation broth of C. glutamicum HW4, indicating that the stable AAR–ADO hydrocarbon synthesis pathway had been established in genome scale.

Fig. 1
figure 1figure 1

Hydrocarbons synthesis pathway in Corynebacterium glutamicum and construction of AAR–ADO pathway. a Overall hydrocarbons synthesis pathway in C. glutamicum S9114; black lines represent native pathways. Red lines represent overexpressing heterologous genes. Red cross represents the deletion of the gene. ACP acyl carrier protein, AAR acyl-ACP reductase, ADH aldehyde reductase, ADO aldehyde deformylating oxygenase, ACC acetyl CoA carboxylase, FAS fatty acid synthase, FAT fatty acyl-ACP thioesterase, ACS fatty acyl-CoA synthetase, sGDH glucose dehydrogenase, FDH1 formic acid dehydrogenase, AasS fatty acyl-ACP synthetase, OleT fatty acid decarboxylase. b GC–MS chromatogram of hydrocarbons production in C. glutamicum S9114 (control) and HW4 (with AAR–ADO pathway). Shake-flask fermentation, 30 °C, 200 rpm, pH 7.0 maintained by adding 5 M NaOH. Abundance represented the response intensity of chromatogram peaks. C. glutamicum S9114 generated no hydrocarbons thus the peaks (black line) were not visible on the chromatogram; c metabolic modifications of C. glutamicum for hydrocarbons production chart. Fermentation parameters were similar to b

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Table 1 Strains and plasmids used
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The fasR disruption by the aar-rbs-ado cluster also led to the excessive generation of C16 and C18 fatty acids. The fatty acids generation by the parental C. glutamicum S9114 was about ~ 10 mg/L fermentation broth by GC–MS detection with dodecane as the standard. The disruption of fasR in C. glutamicum HW4 resulted in the fatty acid generation up to 103 mg/L, approximately one order of magnitude greater than that by the parental strain (Fig. 1c).

To increase the hydrocarbons production of C. glutamicum HW4, a systematic metabolic engineering was performed (Fig. 1a) including (i) separately overexpressing aar and ado in plasmids pH36mob to increase the copy numbers (Fig. 1a, Box I); (ii) expression of NADPH reductase genes pntAB, udhA and sgdh to increase the NADPH supply (Fig. 1a, Box II); (iii) expression of fatty acyl-ACP synthase AasS from Vibrio harveyi B392 to convert free fatty acids to fatty acyl-ACP (Fig. 1a, Box III) [25], and (iv) expression of formic acid dehydrogenase FDH1 from S. cerevisiae S288C to degrade the byproduct formic acid (Fig. 1a, Box IV). However, these efforts showed no improvements or even negative results (Fig. 1d), except that the enhancement of NADPH supply by overexpression of udhA and sgdh genes (encoding UdhA and sGDH, respectively) with ~ 8% increase of hydrocarbons production.

Constructing the fatty acid decarboxylation pathway in C. glutamicum and the secretive expression

To increase the hydrocarbons production by C. glutamicum, the second pathway was constructed by direct decarboxylation of free fatty acid. Free fatty acids accumulation is the unique phenomenon of C. glutamicum because of the lack of lack of β-oxidation pathway for fatty acid degradation, as well as the lack of phosphatidic acid phosphatase (PAP) and diacylglycerol acyltransferase (DGAT) to produce triacylglyceride (microbial lipid) [21]. The direct decarboxylation pathway of free fatty acids was constructed by overexpression of the oleT gene encoding the fatty acid decarboxylase OleT (Fig. 1a, Box V). Two fatty acid decarboxylase genes, oleTJE from Jeotgalicoccus sp. ATCC 8456 and oleTMC from Macrococcus caseolyticus WP_041635889.1 [10, 26], were selected, synthesized, and heterologously expressed in C. glutamicum S9114. The di-alkenes of C12H22 and C14H26, as well as the mono-alkenes of C15H30 and C17H34, were produced by the overexpression of the two oleT genes (Fig. 2). The greater hydrocarbons generation of oleTMC expression indicates OleTMC was more adaptive for fatty acid decarboxylation in C. glutamicum S9114.

Fig. 2
figure 2

GC–MS result of hydrocarbon production via different fatty acid decarboxylases in C. glutamicum S9114. Shake-flask fermentation at 30 °C, 200 rpm, pH 7.0 maintained by adding 5 M NaOH

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To avoid the cell membrane damage by the transmembrane transportation of hydrocarbons, the extracellular decarboxylation of fatty acids into hydrocarbons were designed by the secretive expression of OleT (Fig. 3a). Two secretory pathways were tested, one was the Sec pathway to secret the unfolded proteins by the peptide Ncgl1289 from C. glutamicum ATCC13032 [27], the other was the Tat pathway to secret the folded proteins by cgR_0494 from C. glutamicum S9114 [28,29,30]. Each of the signal peptide genes was ligated with oleTJE and oleTMC by overlap PCR, then inserted into the expression plasmids and introduced to C. glutamicum S9114 to obtain four recombinants, S9114-pH36-NsoleTJE, S9114-pH36-RsoleTJE, S9114-pH36-NsoleTMC and S9114-pH36-RsoleTMC. Both the SDS-PAGE and the Western blotting did not show the clear protein bands due to the high fatty acids content for protein extraction in the fermentation broth. Figure 3b shows that the secretive expression of OleT significantly improved the hydrocarbons generation. Among the hydrocarbons produced, the secretive expression of OleTMC by the Sec pathway (S9114-pH36-NsoleTMC) showed approximately fourfolds greater hydrocarbons (9.6 mg/L) than the intracellular expression (S9114-pH36-OleTMC, 2.4 mg/L), and approximately 36% more hydrocarbons than the secretive expression of OleTMC by the Tat pathway (S9114-pH36-RsoleTMC, 7.1 mg/L). The results suggest that the cell damage was partially relieved by the secretion of decarboxylase and considerable hydrocarbons were generated in the extracellular space.

Fig. 3
figure 3

Secretive expression of fatty acid decarboxylase and hydrocarbon synthesis in C. glutamicum S9114. a Illustration of concept; b hydrocarbons production. oleTJE, oleTMC represent C. glutamicum S9114 with the overexpression of corresponding genes; NsoleTJE, NsoleTMC represent C. glutamicum S9114 with the secretive expression of oleTJE/MC through Sec pathway; RsoleTJE, RsoleTMC represent C. glutamicum S9114 with the secretive expression of oleTJE/MC through Tat pathway. Shake-flask fermentation, 30 °C, 200 rpm, pH 7.0 maintained by adding 5 M NaOH

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Cell surface display of the OleT expression was also tried by expressing the anchor proteins NCgl1221, NCgl1337, PorB and PorC from C. glutamicum S9114. Unfortunately, the results show no observable improvement or even suppression by the surface display expression of OleT under the control of the promotor Eftu and H36 (Fig. 4).

Fig. 4
figure 4

Hydrocarbons production of displaying fatty acid decarboxylase OleTMC on the cell surface under the control of H36 promote and Eftu promoter. Control represents C. glutamicum S9114 with the overexpression of oleTMC. Fermentations were carried out in shake flask, 30 °C, 200 rpm, pH 7.0 maintained by adding 5 M NaOH

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Dual pathways construction for hydrocarbons synthesis in C. glutamicum

The two secretive overexpression of OleTMC by the Sec secretive pathway and the Tat secretive pathway were expressed in C. glutamicum HW4 (carrying the AAR–ADO pathway in genome scale) to give the two recombinants C. glutamicum recombinants, HW5 and HW6, respectively (Fig. 5a).

Fig. 5
figure 5

Hydrocarbons production by dual synthesis pathways in C. glutamicum. a Secretive expression of fatty acid decarboxylase OleTMC in C. glutamicum HW4. b Hydrocarbons production by dual synthesis pathways in C. glutamicum. HW5 indicates C. glutamicum HW4 with the secretive expression of oleTMC through Sec pathway and HW6 indicates C. glutamicum HW4 with the secretive expression of oleTMC through Tat pathway. Fermentation was carried out in shake flask, 30 °C, 200 rpm. pH was maintained at 7.0 by adding 5 M NaOH. c Improved hydrocarbons production by optimizing the culture conditions. Fermentation was carried out in a 1-L fermentor. The medium was mentioned in “Materials and methods”. The basic fermentation conditions were 30 °C, pH 7 and 600 rpm. When one of the fermentation parameters was changed for optimization, the others remained the same

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Figure 5b shows that both the recombinants C. glutamicum HW5 and HW6 significantly enhanced the generation of both the di-alkenes (C12H22 and C14H26) and the mono-alkenes (C15H30 and C17H34). The hydrocarbons generation by OleT pathway in C. glutamicum HW5 (Sec secretive pathway) (10.1 mg/L) were 1.9 times greater than the control (without the secretive expression HW4-pH36-OleTMC, 3.5 mg/L), and 13% higher than that of C. glutamicum HW6 (Tat secretive pathway, 8.9 mg/L). The total hydrocarbons production by the dual pathways of AAR–ADO and the OleTMC in C. glutamicum HW5 reached 16.0 mg/L.

The optimal fermentation parameters of C. glutamicum HW5 with the dual hydrocarbons synthesis pathways were examined in bioreactors with automatic pH control and dissolved oxygen input using glucose as carbon resource (Fig. 5c). The results show that the hydrocarbons production was not affected by NADPH addition, and 30 °C and pH 7.0 were suitable for cell growth and hydrocarbons production; the hydrocarbons generation increased with increasing oxygen transfer rate by varying the stirring rate. At the proper fermentation conditions (30 °C, pH 7.0 and 750 rpm), totally 29.2 mg/L of hydrocarbons were produced, including 14.5 mg/L of di-alkenes and 7.3 mg/L of mono-alkenes by C. glutamicum HW5.

Corn stover was used as carbohydrates feedstock for hydrocarbon production by C. glutamicum HW5 (Fig. 6a). Corn stover hydrolysate was prepared by enzymatically hydrolyzing 15% (w/w) of the dry acid pretreated and biodetoxified corn stover with the addition of 5 g/L (NH4)2SO4, 1 g/L KH2PO4, 1 g/L K2HPO4 and 0.25 g/L MgSO4. The total hydrocarbons production by the dual pathways in C. glutamicum HW5 reached 10.8 mg/L, in which the OleTMC pathway generated 7.8 mg/L and the AAR–ADO pathway generated 3.0 mg/L of hydrocarbons.

Fig. 6
figure 6

Hydrocarbons fermentation by C. glutamicum HW5 using corn stover hydrolysate. Fermentation was carried out in a 3-L fermentor, 30 °C, 600 rpm and 1.4 vvm of aeration. pH was maintained at 7.0 by adding 5 M NaOH and 2 M H2SO4. Corn stover hydrolysate was prepared by hydrolyzing the biodetoxified corn stover

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The hydrocarbons generated from the two pathways shared different carbon chain lengths. The carbon number of hydrocarbons from the OleT pathway was less than 20 and the retention time on GC–MS chromatograph was between 7–8 min. The carbon number from the AAR–ADO pathway was greater than 20 and the retention time on GC–MS was greater than 10 min (Fig. 6b). The hydrocarbons generation could be translated to 0.205 mg hydrocarbons/g cellulose in corn stover.

Hydrocarbons production from biomass has been the focus of metabolic engineering and various microorganisms had been engineered as microbial cell factories for hydrocarbons synthesis. This study used C. glutamicum as the hydrocarbons producing strain by its two inherent properties: inhibitors tolerance and free fatty acid generation. The dual hydrocarbons synthesis pathways were constructed and 10.8 mg/L of hydrocarbons was generated when corn stover was used, in which the OleT pathway contributed more than 70% of the total generation of hydrocarbons. The high residual fatty acids level indicated a further upgrading potential of hydrocarbons production by further metabolic engineering.

One of the uncertainties of hydrocarbons production is the less accurate calculation of hydrocarbons content based on the peak areas of hydrocarbons generation of GC–MS chromatogram due to the high and irregular fatty acids peaks on the baseline of GC–MS chromatogram. Due to the high boiling point of fatty acid and non-volatility, the accuracy of hydrocarbons measurement was negatively affected. Highly possible, the hydrocarbons contents were under-estimated because of the merge of hydrocarbons peaks with fatty acids peaks. We tried to measure the fatty acid content using GC–MS and eliminate the fatty acid content from hydrocarbon components for an accurate measurement. However, the high boiling points of fatty acids led to the incomplete volatilization of fatty acids and carbon residues accumulation in GC column (thus damaged the column). We also tried the esterification of the fatty acids in the samples, but this procedure caused a heavy loss of hydrocarbons and the accuracy of hydrocarbon measurement was even worse. A more accurate analysis method is under investigation to determine hydrocarbons contents with the existence of high free fatty acids in the fermentation broth.

Conclusion

The dual hydrocarbon synthesis pathways (OleT and AAR–ADO pathways) were constructed in the inhibitors tolerant C. glutamicum S9114 strain for hydrocarbon production using lignocellulose feedstock as the starting feedstock. The first one is the regular AAR–ADO pathway and the second is the fatty acid decarboxylation pathway from fatty acids by taking advantage of free fatty acid generation of C. glutamicum. The fatty acid decarboxylation pathway was further enhanced significantly by secretive expression of fatty acid decarboxylase OleT and performed the extracellular catalysis by secreted OleT enzyme. The hydrocarbons generation from glucose reached 29.2 mg/L, in which the direct decarboxylation pathway contributed more than 70% of the total hydrocarbons generation, and the AAR–ADO pathway contributed the rest 30%. When corn stover was used for hydrocarbons production after dry acid pretreatment and biodetoxification, the hydrocarbons generation reached 16.0 mg/L. This study provided a new strategy for hydrocarbons synthesis using microbial cell factory suitable for lignocellulose feedstock. The high residual fatty acids level indicated a further upgrading potential of hydrocarbons production by further metabolic engineering.

Discussion

Although the major inhibitors (furfural, 5-hydroxymethylfurfural, acetic acid) generated during pretreatment were removed by biodetoxification, the residual phenolic compounds still showed considerable stress on fermentation strains. In this study, we selected a high robust C. glutamicum as microbial cell factory for synthesis of hydrocarbons and the hydrocarbon products were successfully synthesized by the engineered C. glutamicum using corn stover feedstock after dry biorefinery processing. To improve the low hydrocarbons synthesis efficiency of C. glutamicum, two hydrocarbon synthesis pathways were constructed, the first hydrocarbon synthesis pathway of AAR–ADO originates from cyanobacteria, and the second fatty acid decarboxylation pathway utilizes the unique and rich free fatty acid substrates.

Due to the knockout of the fasR gene, the engineered C. glutamicum accumulated considerably high fatty acids in the extracellular environment. We expressed the fatty acid decarboxylase and secreted the enzyme into the extracellular space (fermentation broth) to conduct the fatty acid decarboxylation reaction in extracellular way. This method avoided the accumulation of hydrocarbons inside the cells and the lessened the toxicity on membrane integrity, resulting in a threefold higher production of hydrocarbons than that of the control strain. We also were found there was still high level of free fatty acids in the fermentation broth after the decarboxylation, suggesting that the fatty acid decarboxylase activity was not enough to convert the fatty acids to the hydrocarbons completely. The further improvement on catalytic efficiency of fatty acid decarboxylase is required. The major contribution of this study is the dual pathways of hydrocarbons synthesis with great potentials for future engineering of microbial cell factory with strong lignocellulose derived inhibitors tolerance.

Materials and methods

Strains and media

Strains and plasmids used in this study are listed in Table 1.

Escherichia coli BL21 was used for plasmid construction and cultured in LB medium. C. glutamicum S9114 was used as the starting strain and the genome sequence referred in NCBI with the access number NZ_AFYA01000018. C. glutamicum was cultured in CM2B medium (yeast extract 10 g/L, peptone 10 g/L, NaCl 10 g/L). The CGXII-NL medium for hydrocarbons fermentation contained 60 g/L glucose, 1.0 g/L (NH4)2SO4, 2.5 g/L urea, 1.0 g/L KH2PO4, 1.0 g/L K2HPO4, 42 g/L MOPS, 0.25 g/L MgSO4, 0.01 g/L CaCl2, 0.01 g/L FeSO4·7H2O, 0.01 g/L MnSO4·H2O, 0.001 g/L ZnSO4·7H2O, 0.0002 g/L CuSO4·5H2O, 0.00002 g/L NiCl2·6H2O, 0.0002 g/L biotin, 0.0005 g/L thiamin, 0.03 g/L PCA. 50 μg/mL of kanamycin was added into the media if needed.

Plasmids and recombinants construction

The primers used for plasmids construction are shown in Additional file 1: Table S1. The fragments of aar, ado, sgdh, aasS, fdh1, oleTJE and oleTMC genes were synthesized by Shanghai Generay Biotech, Shanghai, China. The pntAB and udhA genes were amplified from E. coli BL21 genome. These fragments were then constructed into the expression vectors pH36mob and pEftumob separately by digestion-ligation or in-fusion cloning. The fragments of aar-ado, ado-rbs-aar and ado-TacM-aar were obtained by overlapping the corresponding fragments and then inserted into the expression vector pH36mob, resulting in several plasmids pH36-aar-ado, pH36-ado-rbs-aar, and pH36-ado-TacM-aar.

The signal peptide sequences of Ncgl1289 and cgR_0949 were amplified from C. glutamicum ATCC 13032 and C. glutamicum S9114. Then the signal peptide sequences of Ncgl1289 and the fragment of oleTJE gene were overlapped together and inserted into pH36mob, resulting pH36-NsoleTJE. Plasmids pH36-NsoleTMC, pH36-RsoleTJE and pH36-RsoleTMC were obtained in the same way. Plasmids were constructed similarly by fusing membrane protein sequences of Ncgl1337, Ncgl1221, porB, and porC in front of oleTMC for expression of oleTMC on the cell surface under the control of the promotor Eftu and H36. All the above overexpression plasmids were verified via sequencing analysis and then transformed into C. glutamicum by electroporation. The recombinant strains grown on plates with kanamycin resistance were verified by colony PCR.

The up- and down-fragments of fasR gene were cloned from C. glutamicum S9114, and then inserted into pK18mobsacb. The fragment aar-rbs-ado was inserted between the up- and down-fragments of fasR gene, resulting in the pK18-ΔfasR-aar-rbs-ado plasmid. This plasmid was verified by sequencing analysis and transformed into C. glutamicum by electroporation. The correct recombinant mutant was isolated through two rounds of homologous recombination and verified by colony PCR [31].

Lignocellulose feedstock and biorefinery processing

Corn stover was harvested from Nanyang, Henan, China, in fall 2020. The raw biomass was air dried and milled, and then pretreated using the dry acid pretreatment method [32, 33]. Acid pretreatment was operated according to the protocols in [34,35,36,37,38]. A 20-L helical ribbon impeller-driven reactor was fed with 1200 g of corn stover (dry base) and 500–600 g of sulfuric acid solution to the dry solid weight to the acid liquid weight of 2:1. The corn stover and acid solution were co-currently fed into the reactor and stirred for 3 min at 50 rpm. The hot steam was then jetted into the reactor and maintained at 175 °C for 5 min. The pretreated corn stover solids were discharged from the bottom outlet port of the reactor without free wastewater generation, then briefly milled to move the extra-long fibers. The acid catalyst usage was adjusted according to the method previously described [39].

The solid-state biodetoxification was conducted in a 15-L bioreactor. The spore suspension of Amorphotheca resinae ZN1 was inoculated to the freshly pretreated corn stover solids and cultured at 30 °C for 48 h. Then the seed was inoculated into pretreated corn stover solids at 10% (w/w) mass ratio, and incubated at 30 °C for 36–48 h with the aeration rate of 1 vvm (air volume per culture volume per min). The brief stirring was conducted at 50 rpm every 12 h [33, 40]. The corn stover hydrolysate (CSH) was prepared by hydrolyzing the biodetoxified corn stover [16]. The duration of all fermentations was 72 h. All fermentations were carried out in triplicate, and the error bars were indicated by the standard derivations of three biological replicates.

Hydrocarbon fermentation

The seed culture was prepared as described in our previous study [16]. The shake-flask fermentation was conducted by inoculating the seed culture at 5% (v/v) inoculum ratio in 250-mL shake flasks containing 30 mL CGXII medium at 30 °C, 200 rpm. The pH was maintained at 7.0 by adding 5 M NaOH.

The bioreactor fermentation was conducted in a 1-L fermenter at 30 °C, 600 rpm and 1.4 vvm aeration, pH 7.0 by adding 2 M H2SO4 and 5 M NaOH automatically. The seed culture was inoculated into 600 mL of the fermentation medium at 10% (v/v) inoculum ratio. The cellulosic hydrocarbons fermentation was carried out in a 3-L fermenter containing 800 mL 15% (w/w) solids content corn stover hydrolysate. The other fermentation conditions were the same as mentioned above.

Hydrocarbon extraction and quantification

Hydrocarbons were extracted from 60 mL fermentation broth using 30 mL the mixture of methanol and chloroform (the ratio of methanol/chloroform was 2:1) for 24 h and then centrifuged at 10,000 rpm for 10 min. The solvent layer on the bottom of the mixture was rotary-evaporated to remove the solvent and the hydrocarbons obtained were re-dissolved by adding 1 mL of chloroform to obtain the samples for hydrocarbons measurement.

Samples were analyzed by Agilent 6890 GC–MS (Agilent Technologies, Santa Clara, CA, USA) with HP-5-MS column. The initial temperature was 50 °C and maintained for 2 min, then ramped up to 80 °C at a rate of 15 °C/min and held at 80 °C for 3 min, after that the temperature was ramped up to 280 °C at a rate of 15 °C/min and held at 280 °C for 8 min. The flow rate of the carrier gas helium was 1 mL/min. NIST MS SEARCH 2.0 library was used for qualitative analysis, and the matching degree of samples and standard products reached more than 95%. The internal calibration was 100 mg/L dodecane (C12H26) and the concentration of the hydrocarbons was calculated according to the ratio of the chromatographic peak area.

Availability of data and materials

All data generated or analyzed during this study are included in this article. If additional information is needed, please contact the corresponding author.

References

  1. Schirmer A, Rude MA, Li X, Popova E, Cardayre SD. Microbial biosynthesis of alkanes. Science. 2010;329(5991):559–62.

    CAS  Article  Google Scholar 

  2. Kissin YV. Chemical mechanisms of catalytic cracking over solid acidic catalysts: alkanes and alkenes. Catal Rev. 2001;43(1–2):85–146.

    CAS  Article  Google Scholar 

  3. Ahamed A, Ahring BK. Production of hydrocarbon compounds by endophytic fungi Gliocladium species grown on cellulose. Bioresour Technol. 2011;102(20):9718–22.

    CAS  Article  Google Scholar 

  4. Gianoulis TA, Griffin MA, Spakowicz DJ, Dunican BF, Strobel SA. Genomic analysis of the hydrocarbon-producing, cellulolytic, endophytic fungus Ascocoryne sarcoides. PLos Genet. 2012;8(3): e1002558.

    CAS  Article  Google Scholar 

  5. Howard RW, Blomquist GJ. Ecological, behavioral, and biochemical aspects of insect hydrocarbons. Annu Rev Entomol. 2005;50:371–93.

    CAS  Article  Google Scholar 

  6. Kang MK, Nielsen J. Biobased production of alkanes and alkenes through metabolic engineering of microorganisms. J Ind Microbiol Biotechnol. 2017;44(4–5):613–22.

    CAS  Article  Google Scholar 

  7. Howard TP, Middelhaufe S, Moore K, Edner C, Kolak DM, Taylor GN, Parker DA, Lee R, Smirnoff N, Aves SJ. Synthesis of customized petroleum-replica fuel molecules by targeted modification of free fatty acid pools in Escherichia coli. Proc Natl Acad Sci USA. 2013;110(19):7636–41.

    CAS  Article  Google Scholar 

  8. Li N, Chang WC, Warui DM, Booker SJ, Krebs C, Bollinger JM. Evidence for only oxygenative cleavage of aldehydes to Alk(a/e)nes and formate by cyanobacterial aldehyde decarbonylases. Biochemistry. 2012;51(40):7908–16.

    CAS  Article  Google Scholar 

  9. Marsh E, Waugh MW. Aldehyde decarbonylases: enigmatic enzymes of hydrocarbon biosynthesis. ACS Catal. 2013;3(11):2515–21.

    CAS  Article  Google Scholar 

  10. Rude MA, Baron TS, Brubaker S, Alibhai M, Cardayre SD, Schirmer A. Terminal olefin (1-alkene) biosynthesis by a novel P450 fatty acid decarboxylase from Jeotgalicoccus species. Appl Environ Microbiol. 2011;77(5):1718–27.

    CAS  Article  Google Scholar 

  11. Rui Z, Li X, Zhu XJ, Liu J, Domigan B, Barr I, Cate JHD, Zhang WJ. Microbial biosynthesis of medium-chain 1-alkenes by a nonheme iron oxidase. Proc Natl Acad Sci USA. 2014;111(51):18237–42.

    CAS  Article  Google Scholar 

  12. Rui Z, Harris NC, Zhu XJ, Huang W, Zhang WJ. Discovery of a family of desaturase-like enzymes for 1-alkene biosynthesis. ACS Catal. 2015;5(12):7091–4.

    CAS  Article  Google Scholar 

  13. Yi X, Gao QQ, Zhang L, Wang X, Bao J. Heterozygous diploid structure of Amorphotheca resinae ZN1 contributes efficient biodetoxification on solid pretreated corn stover. Biotechnol Biofuels. 2019;12:126.

    Article  Google Scholar 

  14. Sikkema J, de Bont JA, Poolman B. Mechanisms of membrane toxicity of hydrocarbons. Microbiol Rev. 1995;59(2):201–22.

    CAS  Article  Google Scholar 

  15. Becker J, Rohles CM, Wittmann C. Metabolically engineered Corynebacterium glutamicum for bio-based production of chemicals, fuels, materials, and healthcare products. Metab Eng. 2018;50:122–41.

    CAS  Article  Google Scholar 

  16. Wen JB, Xiao Y, Liu T, Gao QQ, Bao J. Rich biotin content in lignocellulose biomass plays the key role in determining cellulosic glutamic acid accumulation by Corynebacterium glutamicum. Biotechnol Biofuels. 2018;11:132.

    Article  Google Scholar 

  17. Wang X, Khushk I, Xiao Y, Gao QQ, Bao J. Tolerance improvement of Corynebacterium glutamicum on lignocellulose derived inhibitors by adaptive evolution. Appl Microbiol Biotechnol. 2018;102(1):377–88.

    CAS  Article  Google Scholar 

  18. Wen JB, Bao J. Engineering Corynebacterium glutamicum triggers glutamic acid accumulation in biotin-rich corn stover hydrolysate. Biotechnol Biofuels. 2019;12:86.

    Article  Google Scholar 

  19. Jin C, Huang Z, Bao J. High-titer glutamic acid production from lignocellulose using an engineered Corynebacterium glutamicum with simultaneous co-utilization of xylose and glucose. ACS Sustain Chem Eng. 2020;8(16):6315–22.

    CAS  Article  Google Scholar 

  20. Jin C, Bao J. Lysine production by dry biorefining of wheat straw and cofermentation of Corynebacterium glutamicum. J Agric Food Chem. 2021;69(6):1900–6.

    CAS  Article  Google Scholar 

  21. Radmacher E, Alderwick LJ, Besra GS, Brown AK, Gibson KJC, Sahm H, Eggeling L. Two functional FAS-I type fatty acid synthases in Corynebacterium glutamicum. Microbiology. 2005;151(7):2421–7.

    CAS  Article  Google Scholar 

  22. Akcuraa M, Turanb V, Koktenc K, Kaplan M. Fatty acid and some micro element compositions of cluster bean (Cyamopsis tetragonoloba) genotype seeds growing under Mediterranean climate. Ind Crops Prod. 2019;128:140–6.

    Article  Google Scholar 

  23. Plassmeier J, Li YY, Rueckert C, Sinskey AJ. Metabolic engineering Corynebacterium glutamicum to produce triacylglycerols. Metab Eng. 2016;33:86–97.

    CAS  Article  Google Scholar 

  24. Takeno S, Takasaki M, Urabayashi A, Mimura A, Muramatsu T, Mitsuhashi S, Ikeda M. Development of fatty acid-producing Corynebacterium glutamicum strains. Appl Environ Microbiol. 2013;79:21.

    Article  Google Scholar 

  25. Jiang Y, Chan CH, Cronan JE. The soluble acyl-acyl carrier protein synthetase of Vibrio harveyi B392 is a member of the medium chain acyl-coa synthetase family. Biochemistry. 2006;45(33):10008–19.

    CAS  Article  Google Scholar 

  26. Lee JW, Niraula NP, Trinh CT. Harnessing a P450 fatty acid decarboxylase from Macrococcus caseolyticus for microbial biosynthesis of odd chain terminal alkenes. Metab Eng Commun. 2018;7: e00076.

    Article  Google Scholar 

  27. Yim SS, Choi JW, Lee RJ, Lee YJ, Lee SH, Kim SY, Jeong KJ. Development of a new platform for secretory production of recombinant proteins in Corynebacterium glutamicum. Biotechnol Bioeng. 2016;113(1):163–72.

    CAS  Article  Google Scholar 

  28. Liu X, Wei Z, Zhao Z, Dai X, Bai Z. Protein secretion in Corynebacterium glutamicum. Crit Rev Biotechnol. 2016;37(4):541–51.

    Article  Google Scholar 

  29. Zhang L, Jia H, Xu D. Construction of a novel twin-arginine translocation (Tat)-dependent type expression vector for secretory production of heterologous proteins in Corynebacterium glutamicum. Plasmid. 2015;82:50–5.

    CAS  Article  Google Scholar 

  30. Wen JB, Bao J. Improved fermentative γ-aminobutyric acid production by secretory expression of glutamate decarboxylase by Corynebacterium glutamicum. J Biotechnol. 2021;331:19–25.

    CAS  Article  Google Scholar 

  31. Schaefer A, Tauch A, Jaeger W, Kalinowski J, Thierbach G, Puehler A. Small mobilizable multi-purpose cloning vectors derived from the Escherichia coli plasmids pK18 and pK19: selection of defined deletions in the chromosome of Corynebacterium glutamicum. Gene. 1994;145(1):69–73.

    CAS  Article  Google Scholar 

  32. Zhang J, Wang XF, Chu D, He YQ, Bao J. Dry pretreatment of lignocellulose with extremely low steam and water usage or bioethanol production. Bioresour Technol. 2011;102(6):4480–8.

    CAS  Article  Google Scholar 

  33. He YQ, Zhang J, Bao J. Acceleration of biodetoxification on dilute acid pretreated lignocellulose feedstock by aeration and the consequent ethanol fermentation evaluation. Biotechnol Biofuels. 2016;9:19.

    Article  Google Scholar 

  34. He YQ, Fang ZH, Zhang J, Li XL, Bao J. De-ashing treatment of corn stover improves the efficiencies of enzymatic hydrolysis and consequent ethanol fermentation. Bioresour Technol. 2014;169:552–8.

    CAS  Article  Google Scholar 

  35. He YQ, Zhang J, Bao J. Dry dilute acid pretreatment by co-currently feeding of corn stover feedstock and dilute acid solution without impregnation. Bioresour Technol. 2014;158:360–4.

    CAS  Article  Google Scholar 

  36. Liu G, Zhang Q, Li HG, Qurishi AS, Zhang J, Bao XM, Bao J. Dry biorefining maximizes the potentials of simultaneous saccharification and co-fermentation for cellulosic ethanol production. Biotechnol Bioeng. 2018;115:60–9.

    CAS  Article  Google Scholar 

  37. Zhang J, Wang XS, Chu DQ, He YQ, Bao J. Dry pretreatment of lignocellulose with extremely low steam and water usage for bioethanol production. Bioresour Technol. 2011;102:4480–8.

    CAS  Article  Google Scholar 

  38. Zhang B, Ahemed F, Zhan BR, Bao J. Transformation of lignocellulose to starch-like carbohydrates by organic acid-catalyzed pretreatment and biological detoxification. Biotechnol Bioeng. 2021;118(10):4105–18.

    CAS  Article  Google Scholar 

  39. Han XS, Bao J. General method to correct the fluctuation of acid based pretreatment efficiency of lignocellulose for highly efficient bioconversion. ACS Sustain Chem Eng. 2018;6:4212–9.

    CAS  Article  Google Scholar 

  40. Yi X, Gao QQ, Zhang L, Wang X, He YQ, Hu FX, Zhang J, Zou G, Yang SH, Zhou ZH, Bao J. Heterozygous diploid structure of Amorphotheca resinae ZN1 contributes efficient biodetoxification on solid pretreated corn stover. Biotechnol Biofuels. 2019;12:126.

    Article  Google Scholar 

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Acknowledgements

The authors are grateful to the National Natural Science Foundation of China for funding this research.

Funding

This research was supported by the National Natural Science Foundation of China (21978083, 31961133006).

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Author notes

  1. Ying-Ying Xu, Ke-Jun Hua and Zhen Huang equally contributed to this work

Authors and Affiliations

  1. State Key Laboratory of Bioreactor Engineering, East China University of Science and Technology, 130 Meilong Road, Shanghai, 200237, China

    Ying-Ying Xu, Ke-Jun Hua, Zhen Huang, Ping-Ping Zhou, Jing-Bai Wen, Ci Jin & Jie Bao

  2. College of Food and Biology Engineering, Henan University of Animal Husbandry and Economy, 6 Longzihu North Road, Zhengzhou, 450046, Henan, China

    Ping-Ping Zhou

  3. School of Chemical and Biological Engineering, Yichun University, 576 Xuefu Road, Yichun, 336000, Jiangxi, China

    Jing-Bai Wen

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  1. Ying-Ying Xu
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Contributions

YYX, KJH and ZH conducted the metabolic engineering, hydrocarbons fermentation and GC–MS analysis. PPZ conducted the screening of relevant genes. JBW provided secretive expression suggestions. CJ provided genetic manipulation and revision suggestion. JB conceived the research and experiment. YYX, KJH and JB wrote the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Jie Bao.

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Supplementary Information

Additional file 1: Table S1.

Primers used in this study.

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Xu, YY., Hua, KJ., Huang, Z. et al. Cellulosic hydrocarbons production by engineering dual synthesis pathways in Corynebacterium glutamicum. Biotechnol Biofuels 15, 29 (2022). https://doi.org/10.1186/s13068-022-02129-7

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  • DOI: https://doi.org/10.1186/s13068-022-02129-7

Keywords

  • Hydrocarbons
  • Lignocellulose
  • Corynebacterium glutamicum
  • Dual synthesis pathways
  • Fatty acid decarboxylase OleT
  • Secretive expression

Biotechnology for Biofuels and Bioproducts

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