- Open Access
Overproduction of native endo-β-1,4-glucanases leads to largely enhanced biomass saccharification and bioethanol production by specific modification of cellulose features in transgenic rice
© The Author(s) 2019
- Received: 30 July 2018
- Accepted: 29 December 2018
- Published: 9 January 2019
Genetic modification of plant cell walls has been implemented to reduce lignocellulosic recalcitrance for biofuel production. Plant glycoside hydrolase family 9 (GH9) comprises endo-β-1,4-glucanase in plants. Few studies have examined the roles of GH9 in cell wall modification. In this study, we independently overexpressed two genes from GH9B subclasses (OsGH9B1 and OsGH9B3) and examined cell wall features and biomass saccharification in transgenic rice plants.
Compared with the wild type (WT, Nipponbare), the OsGH9B1 and OsGH9B3 transgenic rice plants, respectively, contained much higher OsGH9B1 and OsGH9B3 protein levels and both proteins were observed in situ with nonspecific distribution in the plant cells. The transgenic lines exhibited significantly increased cellulase activity in vitro than the WT. The OsGH9B1 and OsGH9B3 transgenic plants showed a slight alteration in three wall polymer compositions (cellulose, hemicelluloses, and lignin), in their stem mechanical strength and biomass yield, but were significantly decreased in the cellulose degree of polymerization (DP) and lignocellulose crystalline index (CrI) by 21–22%. Notably, the crude cellulose substrates of the transgenic lines were more efficiently digested by cellobiohydrolase (CBHI) than those of the WT, indicating the significantly increased amounts of reducing ends of β-1,4-glucans in cellulose microfibrils. Finally, the engineered lines generated high sugar yields after mild alkali pretreatments and subsequent enzymatic hydrolysis, resulting in the high bioethanol yields obtained at 22.5% of dry matter.
Overproduction of OsGH9B1/B3 enzymes should have specific activity in the postmodification of cellulose microfibrils. The increased reducing ends of β-1,4-glucan chains for reduced cellulose DP and CrI positively affected biomass enzymatic saccharification. Our results demonstrate a potential strategy for genetic modification of cellulose microfibrils in bioenergy crops.
- Transgenic rice
- Cellulose modification
- Biomass saccharification
- Bioethanol production
- Chemical pretreatment
Rice is a staple food crop around the world, providing approximately 800 million metric tons of lignocellulose-based straw annually for potential production of biofuels, feeds and chemicals . Lignocellulosic ethanol is increasingly considered a partial replacement for fossil energy for the purposes of low carbon release and environmental care. The biochemical conversion of lignocellulose involves three major steps: initial physical and chemical pretreatments for wall polymer deconstruction, sequential enzymatic hydrolysis for sugar release, and final yeast fermentation for bioethanol production . Due to lignocellulose recalcitrance, however, the current biomass process for bioethanol production requires a strong pretreatment and expensive enzyme loading . Hence, genetic modification of plant cell walls has been raised as a promising solution to the recalcitrance in transgenic crops [4–6].
Lignocellulose recalcitrance is principally determined by the compositions, structures and interlinkages of wall polymers. Plant cell walls are composed mainly of cellulose, hemicelluloses and lignin with small amounts of pectin and wall proteins. As plant cell walls determine cell size and shape and provide mechanical support and protection against environmental stresses, genetic modification of plant cell walls may affect plant’s normal growth and mechanical strength . Slightly altering cell wall composition and structure and specially improving major wall polymer properties were proposed as feasible approaches for enhanced biomass saccharification and biofuel production .
As the most abundant biomass on the earth, cellulose provides the largest source of fermentable glucose for bioethanol production. Cellulose is composed of β-1,4-linked glucan chains that form crystalline microfibrils by intra- and intermolecular hydrogen bonds. The crystallinity index (CrI) was characterized by a comparison of the intensities of the X-rays scattered into the reflections representing the crystalline part and into the background representing the noncrystalline part of cellulosic materials . The cellulose CrI has been reported to affect biomass enzymatic saccharification negatively in various biomass residues [9–12]. In addition, the degree of polymerization (DP) of the β-1,4-linked glucans, another important cellulose feature, has also been shown to affect biomass enzymatic hydrolysis negatively [12–15]. It was reported that the conserved-site mutation of cellulose synthase 9 (OsCESA9) could reduce both cellulose DP and CrI in the rice Osfc16 mutant plant . The Osfc16 plant displays normal growth and development, while largely enhanced biomass enzymatic saccharification and bioethanol production were achieved. The results suggest that minor alteration of cellulose features may be efficient for cell wall modification that is beneficial for biomass conversion.
Endo-β-1,4-glucanases (EGases, EC126.96.36.199) have been found in both prokaryotic and eukaryotic organisms. Plant EGases belong to subgroup E2 of glycoside hydrolase family 9 (GH9) with three subclasses (A, B, C) [17, 18]. In plants, the EGases were proposed to distinctively cleave the internal β-1,4-glycosidic bonds between two glucose moieties in the center of a polysaccharide chain [17, 19]. It is hypothesized that the cellulase from the GH9 family participates primarily in repairing or arranging cellulose microfibrils during cellulose biosynthesis in plants . Among the three subclasses of GH9 family, GH9A is comprised of membrane anchored proteins, GH9B proteins are secreted with only one catalytic domain, and the GH9C class of proteins has a distinct C-terminal extended cellulose-binding domain [21, 22]. GH9A (KOR) has been characterized as an important member of the cellulose synthase complex for cellulose biosynthesis in Arabidopsis [23, 24]. Overexpression of the PtCel9A1(PtKOR) gene in Arabidopsis or overexpression of AtKOR in Populus both lead to an increase of noncrystalline cellulose level in transgenic plants [25, 26]. However, downregulation of the KOR gene significantly affects cellulose ultrastructure and plant growth in the poplar . OsGHB1, 3 and 16 were recently proposed to have enzymatic activity for reducing cellulose crystallinity in rice plants [27, 28], but the direct genetic and biochemical evidence about their detailed roles in cellulose modification are still lacking. This would necessitate exploring postsynthesis modification of cellulose microfibrils by genetic engineering of these endogenous cellulose degradation enzymes in plants.
In this study, we showed that overexpression of two genes from the glycoside hydrolase 9B family (OsGH9B1 and OsGH9B3) significantly increased reducing ends of β-1,4-glucan chains and reduced cellulose DP and CrI in transgenic rice plants. Moreover, the straw of both transgenic lines exhibited largely enhanced saccharification efficiency and increased bioethanol production after mild alkali pretreatment.
Phylogenetic analysis and expression profiling of OsGH9B1 and OsGH9B3
Selection of the transgenic rice plants overproducing OsGH9B1/B3 proteins with high cellulase activity
Largely enhanced biomass saccharification and bioethanol production in the OsGH9B1/B3 transgenic plants
Bioethanol production in rice
Ethanol production (% dry biomass)
rbcS::OsGH9B1 0.5% NaOH 50 °C for 2 h + 1% tween-80
rbcS::OsGH9B3 0.5% NaOH 50 °C for 2 h + 1% tween-80
1% H2SO4 121 °C for 15 min + ultrasound: 40 W 50 °C for 10 min
0.65% HNO3, 158.8 °C for 5.86 min
Torrefaction 220 °C for 40 min
1% maleic acid 190 °C for 3 min
Popping pretreatment (dry sample 20 °C/min to 220 °C, 1.96 MPa)
2% Lime 120 °C for 60 min + CO2 neutralization
Transgenic plant: 1% sodium hydroxide + 1% Tween-80
21% aqueous-ammonia 69 °C for 10 h + initial loading 3% glucan
Slightly affected plant growth and unaltered mechanical strength in transgenic plants
Small impact on cell wall contents and morphology in transgenic lines
Furthermore, this study determined the contents of three major cell wall polymers of the mature stem tissues in the transgenic rice plants. Compared with WT, the OsGH9B1 transgenic line #1-2 showed similar levels of all three wall polymers, whereas line #1-1 showed a moderate difference in the content of hemicelluloses. By comparison, the OsGH9B3 transgenic line #3-1 had a relatively lower lignin level than the WT by 8%, whereas the line #3-2 had three wall polymer contents similar to the WT (Fig. 6c). Taken together, overexpressions of OsGH9B1 and OsGH9B3 genes had little impact on wall polymer content and morphology in the transgenic plants, consistent with the observations of the normal mechanical strength detected in the transgenic plants (Fig. 6).
Remarkably reduced cellulose DP and CrI and increased CBHI enzymatic hydrolysis of cellulose substrate
Moreover, using GC/MS analysis, this study investigated the dynamic profiling of cellobiose releases (calculated as glucose releases) from crude cellulose of the mature stem tissues during cellobiohydrolase (CBHI; E.C. 188.8.131.52) hydrolysis. All OsGH9B1 and OsGH9B3 transgenic lines showed much higher glucose yields than those of the WT in three time points during CBHI hydrolysis (Fig. 7e). The glucose yields of CBHI hydrolysis were significantly and negatively correlated with both DP and CrI of crude cellulose (n = 15) (Fig. 7f). Since the CBHI enzyme has been known to specifically attack the reducing ends of β-1,4-glucan chains, the increased glucose yield is most likely due to the increased short β-1,4-glucan chains in the transgenic plants, which were accountable for the reduction of cellulose DP and CrI. More important, the glucose yields of CBHI hydrolysis were significantly and positively correlated with the cellulase activities detected in the stem of the transgenic pants with r value at − 0.707 (n = 15) (Fig. 7g). Therefore, the multiple results suggested that the OsGH9B1 and OsGH9B3 proteins should have cellulase activities for the modification of cellulose microfibrils in the transgenic plants.
Mechanism of the overproduced OsGH9B1 and OsGH9B3 for enhancing lignocellulose saccharification and ethanol production
Genetic modification of plant cell walls has been implicated in the largely enhanced lignocellulose enzymatic saccharification and biofuel production in transgenic crops. However, because plant cell walls have extremely complicated structures and diverse biological functions, large modifications of cell walls may affect plant growth and development. Hence, the selected transgenic crops should not only have largely increased biomass saccharification, but also need to maintain a normal plant growth and mechanical strength. Over the past years, attempts have been made to enhance lignocellulose enzymatic hydrolysis by altering hemicellulose features or reducing lignin contents [37, 38, 41–46], but most of the transgenic plants displayed defects in growth and strength or limited enhancement of biomass saccharification. This study has indicated that the minor modifications of cellulose microfibrils could have a large impact on the enhancement of biomass enzymatic hydrolysis with only slightly altered plant growth by overexpressing OsGH9B1/B3 genes in the transgenic rice crops, providing a powerful genetic engineering strategy for selection of bioenergy rice and other energy crops.
The cellulose DP and CrI are the key parameters that are negatively associated with lignocellulose enzymatic hydrolysis under various pretreatments in many biomass residues examined [9, 10, 12–15, 34, 35, 37–39]. Although the cellulose CrI value is in part associated with cellulose DP, it is also affected by the levels of wall polymers and their crosslinks [11, 40, 47, 48]. However, the finding that there was little change in the contents of three major wall polymers implied that reduction of cellulose CrI was due to the decreased DP in OsGH9B1/B3 transgenic lines in this study.
One of the advantages of this study is that we independently introduced two members of the OsGH9B gene family (OsGH9B1 and OsGH9B3) into rice plants. The transgenic lines exhibited similar alterations in cellulose properties, indicating the similar roles of OsGH9B1 and OsGH9B3 in postmodification of cellulose microfibrils. In Arabidopsis and Populus, several genes have been identified to be close to OsGH9B1 and OsGH9B3 based on phylogenetic analysis of the GH9 family in a previous study , yet their functions remain to be explored. It is of interest to test whether these members have similar cellulase activities specific for cellulose modification and for genetic improvement of biofuel plants in the future.
The Neighbor-Joining method was used for phylogenetic tree analysis , and the optimal tree was plotted with the sum of branch length at 4.47282155. The tree is drawn to scale, with branch lengths in the same units as those of the evolutionary distances used to infer the phylogenetic tree. The evolutionary distances were computed using the Poisson correction method  in the units of the number of amino acid substitutions per site. The phylogenetic analysis involves a total of 17 amino acid sequences, and all positions containing gaps and missing data were eliminated. Evolutionary analyses were conducted in MEGA6 .
Plasmid vector construction and transgenic line selection
The full-length cDNA of OsGH9B1 and OsGH9B3 were, respectively, amplified from young panicle of rice cultivar “Nipponbare” (a japonica variety) using primers as shown in Additional file 1: Table S1. OsGH9B1 and OsGH9B3 were separately inserted into the modified plant binary vector pCAMBIAI1300 driven by the rubisco small subunit (rbcS) promoter. Meanwhile, the eGFP gene was constructed to fuse with C-terminal of these genes. These two constructs were independently transferred into “Nipponbare” by Agrobacterium-mediated transformation with the “EHA105” strain. The homozygous transgenic lines were identified based on the hygromycin B screening for 3-4 generations, double checked by PCR analysis and verified by qRT-PCR and Western analysis as described below.
Total RNA isolation and qRT-PCR analysis
Total RNA was extracted from the second internodes of stem tissues at heading stage using the Trizol reagent (Invitrogen). cDNA was synthesized with the GoScript™ Reverse Transcription System (Promega, USA). Quantitative real time-PCR (qRT-PCR) was performed in triplicate using the SYBR Green PCR Master Mixture (ZF101, ZOMANBIO). A rice polyubiquitin gene (OsUBQ1) was used as the internal control. All primers used for qRT-PCR were listed in Additional file 1: Table S1.
Protein preparation and Western blot analysis
Total proteins were collected from the supernatants extracted from the second internodes of stem tissues at heading stage. The proteins were centrifuged at 100,000g for 1 h at 4 °C to collect the residues as the plasma membrane proteins as described by Li et al. . The supernatants were precipitated with acetone (3:1, v/v) at − 20 °C for 12 h to collect soluble proteins. The protein samples were loaded into 12% SDS-PAGE gel for protein separation, and the Western blot analysis was conducted as described by Li et al. . The commercial GFP antibody was used as the primary antibody reaction at 1:1000 dilutions and the affinity-purified phosphatase-labeled goat antirabbit IgG was applied as secondary antibody reaction at 1:5000. Protein bands were detected by the ECL Plus Western Blotting Detection, and scanned under a GeneGnome XRQ (Syngene Inc., Maryland, US).
GFP fluorescence observation
The protoplasts were obtained from the stem tissues of 2-week-old seedlings of rice as described by Yoo et al. . CLSM imaging via a Leica TCS SP8 confocal laser scanning system (Leica Microsystems, Wetzlar, Germany) was performed for GFP fluorescence observation.
Cellulase activity assay in vitro
The second internodes of rice stem tissues were ground into the powders by liquid nitrogen, and extracted with 100 mM sodium acetate trihydrate buffer (pH 5.5). After centrifugation at 12,000g for 10 min at 4 °C, the supernatants were collected for cellulase activity assay as described by Dai et al. . A total of 50 μL supernatant proteins were incubated with 50 μL 0.5 mM 4-methylumbelliferyl β-D-cellobioside (Sigma-Aldrich, USA) at 55 °C for 30 min and stopped by adding 30 μL 0.2 M sodium carbonate. The fluorescence intensity was recorded using a Spectrum Microplate Spectrophotometer (Tecan Infinite M200 PRO, Switzerland) at the excitation wavelength of 365 nm and emission wavelength of 480 nm. The protein concentration was determined by Bradford method  using BSA as the standard. All cellulase activity assays were independently conducted in triplicate.
Determination of the mechanical strength in the rice stem
The breaking and extension forces were detected in the stem tissues at the milk maturity stages of rice as described by [34, 35]. Totally 45, 43 and 27 individual plants of WT, transgenic lines OsGH9B1 and OsGH9B3 were, respectively, used for breaking forces examination. Total 38, 41 and 26 individual plants of WT, transgenic lines OsGH9B1 and OsGH9B3 were measured for extension forces, respectively.
Fluorescence microscopy and transmission electron microscopy analyses
The third leaf veins of three-leaved old seedlings were used for observation of cell wall morphology under fluorescence microscopy and transmission electron microscopy.
For fluorescence microscopic observation, the samples were fixed with 4% (w/v) paraformaldehyde, and dehydrated through an ethanol gradient (30%, 50%, 70%, 90% and 100%, each for 30 min), and then embedded in the paraplast plus. The sections (of 8 μm thickness) were cut using a microtome (RM2265 Leica Microsystems, Leica, Nussloch, Germany) and placed on lysine-treated slides which were dried for 2 days at 37 °C, and dewaxed with xylene and hydrated through an ethanol series (100–0%). The sections were stained with calcofluor white fluorochrome (Calcofluor White Stain; Fluka), and imaged using a microscope (Olympus BX-61, Olympus, Tokyo, Japan). For transmission electron microscopic observation, the samples were prepared as previously described by Fan et al. [34, 35]. The samples were postfixed in 2% (w/v) OsO4 for 1 h after extensively washing in the PBS buffer and embedded with Suprr Kit (Sigma-Aldrich, St. Louis, MO, USA). Sample sections were cut with an Ultracut E ultrami-crotome (Leica) and picked up on formvar-coated copper grids. After poststaining with uranyl acetate and lead citrate, the specimen was viewed under a Hitachi H7650 (Hitachi Ltd., Tokyo, Japan) transmission electron microscope.
Extraction of crude cell walls and cellulose samples
The homozygous transgenic rice plants and the wild type (Nipponbare) were grown in the experimental field of Huazhong Agricultural University, Wuhan, China. The mature stem tissues were dried, ground into powder through 40 mesh (0.425 mm × 0.425 mm) , and stored in a dry container. The powder samples were extracted with ddH2O at 25 °C for 2 h to remove soluble sugar, followed by chloroform: methanol (1:1) at 25 °C for 1 h and then methanol to remove lipids. The residues were then extracted with 70% (v/v) ethanol at 25 °C for 12 h, and washed two times with 70% (v/v) ethanol. The remaining residues were washed two times with acetone and dried under vacuum to obtain the final crude cell wall sample. The crude cell walls were further extracted with 4 M KOH (containing 1.0 mg/mL sodium borohydride) at 25 °C for 2 h to remove hemicellulose, and the remaining pellet was washed five times with ddH2O and extracted with 8% (w/v) sodium chlorate (containing 1.5% acetic acid, v/v) at 25 °C for 48 h to remove lignin. The remaining pellet was washed six to eight times with ddH2O and dried under vacuum to obtain the final crude cellulose sample.
Hemicellulose and cellulose extraction and determination
The crude cell wall samples from the above described extraction, were used for further extraction of hemicelluloses and cellulose fractions as described by Fan et al. [34, 35]. Total hexoses and pentoses released from 4 M KOH extraction and the pentoses released from 67% (v/v) H2SO4 hydrolysis were summed for determining the total hemicellulose content. Cellulose was estimated by calculating total hexoses from 67% (v/v) H2SO4 hydrolysis. The anthrone/H2SO4 method  and orcinol/HCl method  were applied for the hexoses and pentoses assay. d-glucose and d-xylose were prepared to plot standard curves, and the deduction from pentoses reading at 660 nm was carried out for calculation of final hexoses in order to eliminate the interference of pentose on hexose reading at 620 nm.
Total lignin was assayed using a two-step acid hydrolysis method according to the Laboratory Analytical Procedure of the National Renewable Energy Laboratory . The crude cell wall samples were hydrolyzed with 67% (v/v) H2SO4 at 25 °C for 90 min with a gentle shaking at 115 rpm, and subsequently diluted to 3.97% (w/w) with distilled water and heated at 115 °C for 60 min. The supernatant liquids were read at 205 nm for acid soluble lignin, and the remaining residues were placed in a muffle furnace at 575 °C ± 25 °C for 4 h for the acid insoluble lignin assay.
Detection of cellulose features (DP, CrI)
The crude cellulose DP assay was performed using viscosity method as previously described by Zhang et al. . Cellulose CrI was detected using X-ray diffraction (XRD) method (Rigaku-D/MAX instrument, Uitima III, Japan) as described by Segal et al. .
Crude cellulose hydrolysis by β-1,4-exoglucanase (cellobiohydrolase-CBHI)
CBHI enzyme hydrolysis assay was performed using crude cellulose samples. The crude cellulose samples (10 mg) were incubated with 0.5 U CBHI (E.C. 184.108.40.206; Megazyme, USA) at 50 °C for a time course of reactions at 30 min, 3 h, and 14 h. After centrifugation at 3000g, the supernatants were collected and treated with 2 M TFA at 120 °C for 1 h, and Myo-inositol (20 μg) was added as the internal standard. The supernatants were then dried under vacuum to remove TFA. Distilled water (200 μL) and freshly prepared solution of sodium borohydride (100 μL, 100 mg/mL in 6.5 M aqueous NH3) were added to each sample, incubated at 40 °C for 1 h, and the excess sodium borohydride was decomposed by adding acetic acid (200 μL). The sample was transferred into a 25-mL glass tube, and 1-methylimidazole (600 μL) and the acetic anhydride (4 mL) were added and mixed well to perform an acetylation reaction at 25 °C for 30 min. The excess acetic anhydride was decomposed by adding distilled water (10 mL). Dichloromethane (3 mL) was added, mixed gently, and left standing for phase separation. The collected lower phase was dehydrated by adding anhydrous sodium sulfate and analyzed using GC–MS (SHIMADZU GCMS-QP2010 Plus) as described by Li et al. .
Chemical pretreatments and biomass enzymatic saccharification
Alkali pretreatment: The crude cell wall samples were incubated with 6 mL 0.5% NaOH (w/v) and shaken at 150 rpm for 2 h at 50 °C. After centrifugation at 3000g for 5 min, the supernatants were collected for determination of hexoses and pentoses released from alkali pretreatment. The remaining pellets were subsequently washed five times with 10 mL of distilled water for sequential enzymatic hydrolysis.
Acid pretreatment: The crude cell wall samples were incubated with 6 mL of 0.5% H2SO4 (v/v) at 121 °C for 20 min in an autoclave (15 psi). The samples in tubes were then shaken at 150 rpm for 2 h at 50 °C. After centrifugation at 3000g for 5 min, the supernatants were collected for the determination of hexoses and pentoses released from the acid pretreatment, and the pellets were washed five times with 10 mL of distilled water for sequential enzymatic hydrolysis.
Enzymatic hydrolysis: The remaining residues obtained from alkali or acid pretreatment were washed with 6 mL of mixed-cellulase reaction buffer (0.2 M acetic acid–sodium acetate, pH 4.8), then incubated with 0.16% (w/v) mixed cellulases (Imperial Jade Biotechnology Co., Ltd. Ningxia 750002, China) with the final concentrations of cellulase at 10.60 FPU/g biomass, and xylanase at 6.72 U/g biomass. The measurement of mixed-cellulase activity was based on the filter paper assay according to the International Union of Pure and Applied Chemistry (IUPAC) guidelines, 1 FPU = 1 μmol/min of glucose formed during the hydrolysis reaction. The measurement of xylanase activity used 1% (w/v) xylan (Sigma-Aldrich Co. LLC, California, USA), as the substrate, 1 U = 1 μmol/min of xylose, formed during the hydrolysis reaction. The samples were shaken at 150 rpm at 50 °C with a time course hydrolysis for 12 h, 24 h, and 48 h. After centrifugation at 3000g for 10 min, the supernatants were collected for hexoses and pentoses assay.
Yeast fermentation and bioethanol measurement
The biomass powders were incubated with 6 mL 0.5% NaOH (w/v), shaken at 150 r/min for 2 h at 50 °C. After pretreatments, the biomass residues and supernatants were neutralized to pH 4.8 using appropriate amounts of H2SO4. Then, mixed cellulases were added to the final enzyme concentration at 1.6 g/L cosupplied with 1% Tween-80, and incubated at 150 rpm for 48 h at 50 °C. After enzymatic hydrolysis, the supernatants were collected for yeast fermentation. Yeast fermentation and ethanol measurement were performed as previously described by Jin et al.  and Zahoor et al.  by means of Saccharomyces cerevisiae (Angel yeast Co., Ltd., Yichang, China) and the dichromate oxidation method.
Data collection and statistical analysis
Biological triplicate samples were collected for each transgenic line selection, and chemical analysis was performed in technical triplicates. The SPSS statistical software was used for data analysis. Prior to statistical analysis, all data were analyzed by a Kolmogorov–Smirnov test to check for normal distribution of samples. Pearson correlation analysis was performed for correlation coefficients calculation, and Student’s t test was used for comparison analysis.
JH completed major experiment and wrote the manuscript. GL, XL, YL, and YW participated in the determination of cell wall composition and biomass digestibility analysis. YW and YC participated in transgenic plant selections. TX, GX, and FB analyzed the data. LW and LP designed the project, supervised the experiments, interpreted the data, and finalized the manuscript. All authors read and approved the final manuscript.
This work was supported in part by grants from the National Science Foundation of China (31670296; 31571721; 31171524; 31771775), the National 111 Project (B08032), and the Open Grant of the State Key Laboratory of Reproductive Regulation and Breeding of Grassland Livestock, School of Life Sciences, Inner Mongolia University to L. Peng.
The authors declare that they have no competing interests.
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- Domínguez-Escribà L, Porcar M. Rice straw management: the big waste. Biofuels Bioprod Bioref. 2009;4:154–9.View ArticleGoogle Scholar
- Lynd LR, Laser MS, Brandsby D, Dale BE, Davison B, Hamilton R, Himmel M, Keller M, McMillan JD, Sheehan J, Wyman CE. How biotech can transform biofuels. Nat Biotechnol. 2008;26:169–72.View ArticleGoogle Scholar
- Taherzadeh MJ, Karimi K. Pretreatment of lignocellulosic wastes to improve ethanol and biogas production: a review. Int J Mol Sci. 2008;9:1621–51.View ArticleGoogle Scholar
- Loqué D, Scheller HV, Pauly M. Engineering of plant cell walls for enhanced biofuel production. Curr Opin Plant Biol. 2015;25:151–61.View ArticleGoogle Scholar
- Vega-Sánchez ME, Ronald PC. Genetic and biotechnological approaches for biofuel crop improvement. Curr Opin Biotechnol. 2010;21:218–24.View ArticleGoogle Scholar
- Xie G, Peng L. Genetic engineering of energy crops: a strategy for biofuel production in China. J Integr Plant Biol. 2011;53:143–50.View ArticleGoogle Scholar
- Cosgrove DJ. Growth of the plant cell wall. Nat Rev Mol Cell Biol. 2005;6:850–61.View ArticleGoogle Scholar
- Thygesen A, Oddershede J, Lilholt H, Thomsen AB, Stahl K. On the determination of crystallinity and cellulose content in plant fibres. Cellulose. 2005;12:563–76.View ArticleGoogle Scholar
- Chang VS, Holtzapple MT. Fundamental factors affecting biomass enzymatic reactivity. Appl Biochem Biotechnol. 2000;84–86:5–37.View ArticleGoogle Scholar
- Laureano-Perez L, Teymouri F, Alizadeh H, Dale EB. Understanding factors that limit enzymatic hydrolysis of biomass characterization of pretreated corn stover. Appl Biochem Biotechnol. 2005;121–124:1081–99.View ArticleGoogle Scholar
- Xu N, Zhang W, Ren S, Liu F, Zhao C, Liao H, Xu Z, Huang J, Li Q, Tu Y, Yu B, Wang Y, Jiang J, Qin J, Peng L. Hemicelluloses negatively affect lignocellulose crystallinity for high biomass digestibility under NaOH and H2SO4 pretreatments in Miscanthus. Biotechnol Biofuels. 2012;5:58.View ArticleGoogle Scholar
- Zhang W, Yi Z, Huang J, Li F, Hao B, Li M, Hong S, Lv Y, Sun W, Ragauskas A, Hu F, Peng J, Peng L. Three lignocellulose features that distinctively affect biomass enzymatic digestibility under NaOH and H2SO4 pretreatments in Miscanthus. Bioresour Technol. 2013;130:30–7.View ArticleGoogle Scholar
- Pan X, Xie D, Yu RW, Saddler JN. The bioconversion of mountain pine beetle-killed lodgepole pine to fuel ethanol using the organosolv process. Biotechnol Bioeng. 2008;1:39–48.View ArticleGoogle Scholar
- Puri VP. Effect of crystallinity and degree of polymerization of cellulose on enzymatic saccharification. Biotechnol Bioeng. 1984;26:1219–22.View ArticleGoogle Scholar
- Zhang YH, Lynd LR. Toward an aggregated understanding of enzymatic hydrolysis of cellulose: non-complexed cellulase systems. Biotechnol Bioeng. 2004;88:797–824.View ArticleGoogle Scholar
- Li F, Xie G, Huang J, Zhang R, Li Y, Zhang M, Wang Y, Li A, Li X, Xia T, Qu C, Hu F, Ragauskas AJ, Peng L. OsCESA9 conserved-site mutation leads to largely enhanced plant lodging resistance and biomass enzymatic saccharification by reducing cellulose DP and crystallinity in rice. Plant Biotechnol J. 2017;15:1093–104.View ArticleGoogle Scholar
- Davison A, Blaxter M. Ancient origin of glycosyl hydrolase family 9 cellulase genes. Mol Biol Evol. 2005;22:1273–84.View ArticleGoogle Scholar
- Henrissat B. A classification of glycosyl hydrolases based on amino acid sequence similarities. Biochem J. 1991;280:309–16.View ArticleGoogle Scholar
- Libertini E, Li Y, McQueen-Mason SJ. Phylogenetic analysis of the plant endo-beta-1,4-glucanase gene family. J Mol Evol. 2004;58:506–15.View ArticleGoogle Scholar
- Hayashi T, Yoshida K, Park YW, Konishi T, Baba K. Cellulose metabolism in plants. Int Rev Cytol. 2005;247:1–34.View ArticleGoogle Scholar
- Lopez-Casado G, Urbanowicz BR, Damasceno CM, Rose JK. Plant glycosyl hydrolases and biofuels: a natural marriage. Curr Opin Plant Biol. 2008;11:329–37.View ArticleGoogle Scholar
- Robert S, Bichet A, Grandjean O, Kierzkowski D, Satiat-Jeunemaitre B, Pelletier S, Hauser MT, Höfte H, Vernhettes S. An Arabidopsis endo-1,4-beta-d-glucanase involved in cellulose synthesis undergoes regulated intracellular cycling. Plant Cell. 2005;17:3378–89.View ArticleGoogle Scholar
- Lei L, Zhang T, Strasser R, Lee CM, Gonneau M, Mach L, Vernhettes S, Kim SH, Cosgrove JD, Li S, Gu Y. The jiaoyao1 mutant is an allele of korrigan1 that abolishes endoglucanase activity and affects the organization of both cellulose microfibrils and microtubules in Arabidopsis. Plant Cell. 2014;26:2601–16.View ArticleGoogle Scholar
- Vain T, Crowell EF, Timpano H, Biot E, Desprez T, Mansoori N, Trindade LM, Pagant S, Robert S, Höfte H, Gonneau M, Vernhettes S. The Cellulase KORRIGAN is part of the cellulose synthase complex. Plant Physiol. 2014;165:1521–32.View ArticleGoogle Scholar
- Maloney VJ, Mansfield SD. Characterization and varied expression of a membrane-bound endo-beta-1,4-glucanase in hybrid poplar. Plant Biotechnol J. 2010;8:294–307.View ArticleGoogle Scholar
- Takahashi J, Rudsander UJ, Hedenstrom M, Banasiak A, Harholt J, Amelot N, Immerzeel P, Ryden P, Endo S, Ibatullin FM, Brumer H, del Campillo E, Master ER, Scheller HV, Sundberg B, Teeri TT, Mellerowicz EJ. KORRIGAN1 and its aspen homolog PttCel9A1 decrease cellulose crystallinity in Arabidopsis stems. Plant Cell Physiol. 2009;50:1099–115.View ArticleGoogle Scholar
- Huang J, Li Y, Wang Y, Chen Y, Liu M, Wang Y, Zhang R, Zhou S, Li J, Tu Y, Hao B, Peng L, Xia T. A precise and consistent assay for major wall polymer features that distinctively determine biomass saccharification in transgenic rice by near infrared spectroscopy. Biotechnol Biofuels. 2017;10:294.View ArticleGoogle Scholar
- Xie G, Yang B, Xu Z, Li F, Guo K, Zhang M, Wang L, Zou W, Wang Y, Peng L. Global identification of multiple OsGH9 family members and their involvement in cellulose crystallinity modification in rice. PLoS ONE. 2013;8:e50171.View ArticleGoogle Scholar
- Wang LQ, Guo K, Li Y, Tu YY, Hu HZ, Wang BR, Cui XC, Peng LC. Expression profiling and integrative analysis of the CESA/CSL superfamily in rice. BMC Plant Biol. 2010;10:282.View ArticleGoogle Scholar
- Dai Z, Hooker BS, Anderson DB, Thomas SR. Expression of Acidothermus cellulolyticus endoglucanase E1 in transgenic tobacco: biochemical characteristics and physiological effects. Transgenic Res. 2000;9:43–54.View ArticleGoogle Scholar
- Berry PM, Sterling M, Spink JH, Baker CJ, Sylvester-Bradley R, Mooney SJ, Tams AR, Ennos AR. Understanding and reducing lodging in cereals. Adv Agron. 2004;84:217–71.View ArticleGoogle Scholar
- Crook MJ, Ennos AR. Stem and root characteristics associated with lodging resistance in four winter wheat cultivars. J Agric Sci. 1994;123:167–74.View ArticleGoogle Scholar
- Islam MS, Peng S, Visperas RM, Ereful N, Bhuiya MSU, Julfiquar AW. Lodging-related morphological traits of hybrid rice in a tropical irrigated ecosystem. Field Crops Res. 2007;101:240–8.View ArticleGoogle Scholar
- Fan C, Feng S, Huang J, Wang Y, Wu L, Li X, Wang L, Tu Y, Xia T, Li J, Cai X, Peng L. AtCesA8 driven OsSUS3 expression leads to largely enhanced biomass saccharification and lodging resistance by distinctively altering lignocellulose features in rice. Biotechnol Biofuels. 2017;10:221.View ArticleGoogle Scholar
- Fan C, Li Y, Hu Z, Hu H, Wang G, Li A, Wang Y, Tu Y, Xia T, Peng L, Feng S. Ectopic expression of a novel OsExtensin-like gene consistently enhances plant lodging resistance by regulating cell elongation and cell wall thickening in rice. Plant Biotechnol J. 2017;16:254–63.View ArticleGoogle Scholar
- Jia J, Yu B, Wu L, Wang H, Wu Z, Li M, Huang P, Feng S, Chen P, Zheng Y, Peng L. Biomass enzymatic saccharification is determined by the non-KOH-extractable wall polymer features that predominately affect cellulose crystallinity in corn. PLoS ONE. 2014;9:e108449.View ArticleGoogle Scholar
- Li M, Feng S, Wu L, Li Y, Fan C, Zhang R, Zou W, Tu Y, Jing HC, Li S, Peng L. Sugar-rich sweet sorghum is distinctively affected by wall polymer features for biomass digestibility and ethanol fermentation in bagasse. Bioresour Technol. 2014;167:14–23.View ArticleGoogle Scholar
- Li Q, Song J, Peng S, Wang JP, Qu G-Z, Sederoff RR, Chiang VL. Plant biotechnology for lignocellulosic biofuel production. Plant Biotechnol J. 2014;12:1174–92.View ArticleGoogle Scholar
- Pei Y, Li Y, Zhang Y, Yu C, Fu T, Zou J, Tu Y, Peng L, Chen P. G-lignin and hemicellulosic monosaccharides distinctively affect biomass digestibility in rapeseed. Bioresour Technol. 2016;203:325–33.View ArticleGoogle Scholar
- Wu Z, Zhang M, Wang L, Tu Y, Zhang J, Xie G, Zhou W, Li F, Guo K, Li Q, Gao C, Peng L. Biomass digestibility is predominantly affected by three factors of wall polymer features distinctive in wheat accessions and rice mutants. Biotechnol Biofuels. 2013;6:183.View ArticleGoogle Scholar
- Eudes A, Liang Y, Mitra P, Loqué D. Lignin bioengineering. Curr Opin Biotechnol. 2014;26:189–98.View ArticleGoogle Scholar
- Linger JG, Vardon DR, Guarnieri MT, Karp EM, Hunsinger GB, Franden MA, Johnson CW, Chupka G, Strathmann TJ, Pienkos PT, Beckham GT. Lignin valorization through integrated biological funneling and chemical catalysis. Proc Natl Acad Sci USA. 2014;111:12013–8.View ArticleGoogle Scholar
- Liu C-J, Cai Y, Zhang X, Gou M, Yang H. Tailoring lignin biosynthesis for efficient and sustainable biofuel production. Plant Biotechnol J. 2014;12:1154–62.View ArticleGoogle Scholar
- Poovaiah CR, Nageswara-Rao M, Soneji JR, Baxter HL, Stewart CN Jr. Altered lignin biosynthesis using biotechnology to improve lignocellulosic biofuel feedstocks. Plant Biotechnol J. 2014;12:1163–73.View ArticleGoogle Scholar
- Ragauskas AJ, Beckham GT, Biddy MJ, Chandra R, Chen F, Davis MF, Davison BH, Dixon RA, Gilna P, Keller M, Langan P, Naskar AK, Saddler JN, Tschaplinski TJ, Tuskan GA, Wyman CE. Lignin valorization: improving lignin processing in the biorefinery. Science. 2014;344:1246843.View ArticleGoogle Scholar
- Yang F, Mitra P, Zhang L, Prak L, Verhertbruggen Y, Kim JS, Sun L, Zheng K, Tang K, Auer M, Scheller HV, Loqué D. Engineering secondary cell wall deposition in plants. Plant Biotechnol J. 2013;11:325–35.View ArticleGoogle Scholar
- Li F, Ren S, Zhang W, Xu Z, Xie G, Chen Y, Tu Y, Li Q, Zhou S, Li Y, Tu F, Liu L, Wang Y, Jiang J, Qin J, Li S, Li Q, Jing HC, Zhou F, Gutterson N, Peng L. Arabinose substitution degree in xylan positively affects lignocellulose enzymatic digestibility after various NaOH/H2SO4 pretreatments in Miscanthus. Bioresour Technol. 2013;130:629–37.View ArticleGoogle Scholar
- Wang Y, Huang J, Li Y, Xiong K, Wang Y, Li F, Liu M, Wu Z, Tu Y, Peng L. Ammonium oxalate-extractable uronic acids positively affect biomass enzymatic digestibility by reducing lignocellulose crystallinity in Miscanthus. Bioresour Technol. 2015;196:391–8.View ArticleGoogle Scholar
- Du Q, Wang L, Yang X, Gong C, Zhang D. Populus endo-β-1,4-glucanases gene family: genomic organization, phylogenetic analysis, expression profiles and association mapping. Planta. 2015;241:1417–34.View ArticleGoogle Scholar
- Saitou N, Nei M. The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol. 1987;4:406–25.PubMedPubMed CentralGoogle Scholar
- Zuckerkandl E, Pauling L. Evolutionary divergence and convergence in proteins. In: Bryson V, Vogel HJ, editors. Evolving Genes and Proteins. New York: Academic Press; 1965. p. 97–166.View ArticleGoogle Scholar
- Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. MEGA6: Molecular evolutionary genetics analysis version 6.0. Mol Biol Evol. 2013;30:2725–9.View ArticleGoogle Scholar
- Yoo SD, Cho YH, Sheen J. Arabidopsis mesophyll protoplasts: a versatile cell system for transient gene expression analysis. Nat Protoc. 2007;2:1565–72.View ArticleGoogle Scholar
- Bradford MM. A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem. 1976;72:248–54.View ArticleGoogle Scholar
- Fry SC. The growing plant cell wall: chemical and metabolic analysis. London: Longman; 1988.Google Scholar
- Dische Z. Color reactions of carbohydrates. In: Whistler RL, Wolfrom ML, editors. Methods in carbohydrate chemistry. New York: Academic Press; 1962. p. 477–512.Google Scholar
- Sluiter A, Hames B, Ruiz R, Scarlata C, Sluiter J, Templeton D, Crocker D. Determination of structural carbohydrates and lignin in biomass. Tech. Rep. NREL/TP-510-42618, NREL, Golden, Co. 2008.Google Scholar
- Segal L, Creely JJ, Martin AE, Conrad CM. An empirical method for estimating the degree of crystallinity of native cellulose using the X-ray diffractometer. Text Res J. 1959;29:786–94.View ArticleGoogle Scholar
- Jin W, Chen L, Hu M, Sun D, Li A, Li Y, Zhen H, Zhou S, Tu Y, Xia T, Wang Y, Xie G, Li Y, Bai B, Peng L. Tween-80 is effective for enhancing steam-exploded biomass enzymatic saccharification and ethanol production by specifically lessening cellulase absorption with lignin in common reed. Appl Energy. 2016;175:82–90.View ArticleGoogle Scholar
- Zahoor, Tu Y, Wang L, Xia T, Sun D, Zhou S, Wang Y, Li Y, Zhang H, Zhang T, Madadi M, Peng L. Mild chemical pretreatments are sufficient for complete saccharification of steam-exploded residues and high ethanol production in desirable wheat accessions. Bioresour Technol. 2017;243:319–26.View ArticleGoogle Scholar
- Belal EB. Bioethanol production from rice straw residues. Braz J Microbiol. 2013;44:225–34.View ArticleGoogle Scholar
- Kim I, Lee B, Park JY, Choi SA, Han JI. Effect of nitric acid on pretreatment and fermentation for enhancing ethanol production of rice straw. Carbohydr Polym. 2014;99:563–7.View ArticleGoogle Scholar
- Sheikh MMI, Kim CH, Park HJ, Kim SH, Kim GC, Lee JY, Sim SW, Kim JW. Effect of torrefaction for the pretreatment of rice straw for ethanol production. J Sci Food Agric. 2013;93:3198–204.View ArticleGoogle Scholar
- Jung YH, Park HM, Kim KH. Whole slurry saccharification and fermentation of maleic acid-pretreated rice straw for ethanol production. Bioprocess Biosyst Eng. 2015;38:1639–44.View ArticleGoogle Scholar
- Wi SG, Choi IS, Kim KH, Kim HM, Bae HJ. Bioethanol production from rice straw by popping pretreatment. Biotechnol Biofuels. 2013;6:166.View ArticleGoogle Scholar
- Park J, Shiroma R, Al-Haq MI, Zhang Y, Ike M, Arai-Sanoh Y, Ida A, Kondo M, Tokuyasu K. A novel lime pretreatment for subsequent bioethanol production from rice straw—Calcium capturing by carbonation (CaCCO) process. Bioresour Technol. 2010;101:6805–11.View ArticleGoogle Scholar
- Li Y, Liu P, Huang J, Zhang R, Hu Z, Feng S, Wang Y, Wang L, Xia T, Peng L. Mild chemical pretreatments are sufficient for bioethanol production in transgenic rice straws overproducing glucosidase. Green Chem. 2018. https://doi.org/10.1039/c8gc00694f.View ArticleGoogle Scholar
- Ko JK, Bak JS, Jung MW, Lee HJ, Choi IG, Kim TH, Kim KH. Ethanol production from rice straw using optimized aqueous-ammonia soaking pretreatment and simultaneous saccharification and fermentation processes. Bioresour Technol. 2009;100:4374–80.View ArticleGoogle Scholar