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Organosolv pretreatment of sorghum bagasse using a low concentration of hydrophobic solvents such as 1-butanol or 1-pentanol

Biotechnology for Biofuels volume 9, Article number: 27 (2016) Cite this article

Abstract

Background

The primary components of lignocellulosic biomass such as sorghum bagasse are cellulose, hemicellulose, and lignin. Each component can be utilized as a sustainable resource for producing biofuels and bio-based products. However, due to their complicated structures, fractionation of lignocellulosic biomass components is required. Organosolv pretreatment is an attractive method for this purpose. However, as organosolv pretreatment uses high concentrations of organic solvents (>50 %), decreasing the concentration necessary for fractionation would help reduce processing costs. In this study, we sought to identify organic solvents capable of efficiently fractionating sorghum bagasse components at low concentrations.

Results

Five alcohols (ethanol, 1-propanol, 2-propanol, 1-butanol, and 1-pentanol) were used for organosolv pretreatment of sorghum bagasse at a concentration of 12.5 %. Sulfuric acid (1 %) was used as a catalyst. With 1-butanol and 1-pentanol, three fractions (black liquor, liquid fraction containing xylose, and cellulose-enriched solid fraction) were obtained after pretreatment. Two-dimensional nuclear magnetic resonance analysis revealed that the lignin aromatic components of raw sorghum bagasse were concentrated in the black liquor fraction, although the major lignin side-chain (β-O-4 linkage) was lost. Pretreatment with 1-butanol or 1-pentanol effectively removed p-coumarate, some guaiacyl, and syringyl. Compared with using no solvent, pretreatment with 1-butanol or 1-pentanol resulted in two-fold greater ethanol production from the solid fraction by Saccharomyces cerevisiae.

Conclusions

Our results revealed that a low concentration (12.5 %) of a highly hydrophobic solvent such as 1-butanol or 1-pentanol can be used to separate the black liquor from the solid and liquid fractions. The efficient delignification and visible separation of the lignin-rich fraction possible with this method simplify the fractionation of sorghum bagasse.

Background

The depletion of fossil fuels and environmental pollution associated with fossil fuel use have increased interest in the utilization of biomass as a feedstock for the production of biofuels and bio-based chemicals [1, 2]. Starch-rich biomass is one of the main feedstocks used for these purposes; however, this results in direct competition with global food supplies. Lignocellulosic biomass is a promising alternative feedstock because it is abundant, inexpensive, and renewable. Sorghum (Sorghum bicolor L. Moench), which is a highly productive C4 photosynthetic plant, can be used to produce lignocellulosic fractions. Sorghum is also attractive because it uses water efficiently and is drought tolerant [3]. The lignocellulosic fraction produced from sorghum is typically referred to as sorghum bagasse.

The primary components of sorghum bagasse are cellulose, hemicellulose, and lignin [4], each of which can be valorized. For example, cellulose and hemicellulose are used as carbohydrate sources for fermentation, whereas cellulose pulp is used for paper, and lignin is a renewable source of aromatics [5–7]. The fractionation of sorghum bagasse into its primary components can be carried out in a biorefinery [5, 8]. However, because cellulose is highly crystalline in nature, exhibits complex chemical cross-linking between components, and is recalcitrant to hydrolysis due to the sheathing by hemicellulose and lignin, the fractionation of sorghum bagasse requires appropriate pretreatment [9, 10]. Organosolv pretreatment is a practical methodology for fractionating sorghum bagasse because it facilitates the isolation of high-quality lignin and high-purity cellulose [2, 11, 12]. Organosolv pretreatment involves the use of high-concentration (30–70 %) organic or aqueous organic solvents at temperatures of 100–200 °C, with or without the addition of catalysts [13]. Thus, organosolv pretreatment is expensive and necessitates the recovery of the organic solvents used. Decreasing the concentration of organic solvent necessary for effective pretreatment would thus reduce the cost of fractionation.

As indicated above, organosolv pretreatment has the advantage of enabling the isolation of lignin [2]. The composition of plant cell walls can be characterized by two-dimensional 1H-13C heteronuclear single-quantum coherence nuclear magnetic resonance (2D 1H-13C HSQC NMR) spectroscopy [14, 15]. Thus, 2D-NMR spectroscopy can be used to elucidate the fate of lignin during organosolv pretreatment of sorghum bagasse.

The aim of the present study was to investigate the fractionation effectiveness of five different organic solvents (ethanol, 1-propanol, 2-propanol, 1-butanol, and 1-pentanol) at a relatively low concentration (12.5 %) in organosolv pretreatment of sorghum bagasse. Sulfuric acid was used as the catalyst. The detailed structures of the lignin products obtained in the black liquor and solid fraction of samples pretreated with 1-butanol or 1-pentanol were characterized using 2D 1H-13C HSQC NMR spectroscopy.

Results and discussion

The influence of solvent type on organosolv fractionation of sorghum bagasse

Sorghum bagasse was fractionated into three primary components important in biorefinery processes: cellulose, hemicellulose, and lignin. In this study, fractionation was evaluated by comparing pretreatment using five different organic solvents (ethanol, 1-propanol, 2-propanol, 1-butanol, and 1-pentanol) at a low concentration (12.5 %). Pretreatment with no addition of solvent was used as a control.

After treatment at 180 °C for 45 min, samples were centrifuged (Fig. 1). Interestingly, three fractions (solid, liquid, and black liquor) were obtained with 1-butanol or 1-pentanol as the solvent, but only two fractions (solid and liquid) were obtained using ethanol, 1-propanol, or 2-propanol as the solvent and when no solvent was used (control). These results suggest that differences in the physiochemical properties of the solvents affect fractionation. The greater hydrophobicity of 1-butanol and 1-pentanol (partition coefficients: logP ow = 0.88 and 1.51, respectively) compared with ethanol, 1-propanol, and 2-propanol (logP ow = −0.31, 0.25, and 0.05, respectively) resulted in clearer fractionation when using the former solvents. The control condition was equal to dilute acid pretreatment [16]. Thus, hydrophobic 1-butanol and 1-pentanol separated the black liquor fraction from the acid solution even at the low concentration of 12.5 %.

Fig. 1
figure1

Organosolv pretreatment of sorghum bagasse using 12.5 % solvent concentration. Ethanol, 1-propanol, 2-propanol, 1-butanol, and 1-pentanol were used as the solvent. No addition of solvent was the control. Using ethanol, 1-propanol, and 2-propanol as the solvent and no solvent (control), a solid fraction and a liquid fraction were obtained. Using 1-butanol and 1-pentanol as the solvent, a black liquor fraction was obtained in addition to solid and liquid fractions

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Cellulose-enriched solid fraction

To clarify the effect of solvent type on raw sorghum bagasse, the solid fraction obtained after pretreatment was characterized. Compared with the control, the dry weight of the solid fraction decreased when 1-butanol or 1-pentanol was used as the solvent, but ethanol, 1-propanol, and 2-propanol had no effect on solid fraction dry weight (Fig. 2a). Cellulose is reportedly enriched in the solid fraction of samples pretreated using acid [9], and an increase in the cellulose content in all solid fractions was observed compared with the raw biomass (Fig. 2b). In particular, the cellulose content was higher in the solid fraction when 1-butanol or 1-pentanol was used as the solvent (59.1 and 62.2 %, respectively) compared with ethanol, 1-propanol, 2-propanol, or no solvent (control) (51.6–55.6 %). Cellulose recovery in the solid fraction ranged from 84.4 to 91.1 % when ethanol, 1-propanol, 2-propanol, or 1-butanol was used as the solvent and when no solvent was used (control) (Additional file 1). Cellulose recovery in the solid fraction was 71.9 % when 1-pentanol was used as the solvent. Similar to the trend with dry weight (Fig. 2a), the acid-insoluble lignin content was lower in the solid fraction when 1-butanol or 1-pentanol was used as the solvent compared with other solvents (Fig. 2b). Accordingly, the greatest increase in glucose yield compared with the control was observed with 1-butanol or 1-pentanol as the solvent, but increased glucose yield was also observed with ethanol, 1-propanol, and 2-propanol (Fig. 2c).

Fig. 2
figure2

Properties of the solid fraction obtained after organosolv pretreatment. a Weight of the solid fraction obtained after pretreatment. b Carbohydrate and lignin composition of the solid fraction. c Glucose yield from the solid fraction. Organosolv pretreatment of sorghum bagasse was carried out using ethanol, 1-propanol, 2-propanol, 1-butanol, and 1-pentanol as the solvent and no solvent (control)

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Lignin removal, as calculated using the equation [(lignin in bagasse)—(lignin in solid fraction)]/(lignin in bagasse), was higher when 1-butanol or 1-pentanol was used as the solvent (64.7–74.3 %), compared with the use of no solvent, ethanol, 1-propanol, or 2-propanol (44.1–49.7 %) (Fig. 2a, b). Lignin, which is degraded by sulfuric acid, is reportedly liberated from the cell wall and forms droplets that attach to cellulose molecules [17]. Hydrophobic alcohols would dissolve these lignin droplets and prevent their attachment to cellulose. The removal of lignin from cellulose reportedly increases the accessibility to hydrolytic enzymes and reduces the degree of irreversible adsorption of the enzyme to lignin [18]. Thus, organosolv pretreatment using 1-butanol or 1-pentanol efficiently removes acid-insoluble lignin, resulting in enhanced enzymatic hydrolysis of cellulose.

Liquid fraction containing hemicellulose-derived sugars

It was expected that hemicellulose-derived sugars, mainly xylose, would be contained in the liquid fraction [2]. The amount of xylose contained in the liquid fraction of samples pretreated with ethanol, 1-propanol, 2-propanol, 1-butanol, 1-pentanol, or with no solvent (control) was similar (Fig. 3a). The xylose recovery in the liquid fraction was higher (90.6–97.4 %) when using ethanol, 1-propanol, 1-pentanol, or no solvent, compared with 2-propanol and 1-butanol (85.5 and 79.2 %, respectively), as calculated using the following equation: (xylose amount in liquid fraction)/[(total xylose)—(xylose amount in solid fraction)]. The reason for the decreased xylose recovery when using 2-propanol or 1-butanol as the solvent is unclear.

Fig. 3
figure3

Composition of the liquid fraction. a Glucose and xylose. b Furfural and 5-HMF. c Acetic acid and formic acid. The amount (g) of each component obtained from 6 g of raw biomass is shown

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Compared with the control, the amount of glucose in the liquid fraction was lower in the solvent-pretreated samples (Fig. 3a). Furfural and 5-hydroxymethylfurfural (5-HMF) were contained in the liquid fraction (Fig. 3b). The harsh conditions of pretreatment resulted in the production of similar amounts of acetic and formic acids in the liquid fraction (Fig. 3c). In addition, solvents were blended in the liquid fraction (data not shown). The presence of acetic and formic acids, furfural, 5-HMF, and the pretreatment solvent would inhibit subsequent fermentation. These fermentation inhibitors could be removed, and the xylose and glucose in the liquid fraction could be concentrated, by subsequent application of membrane separation nanofiltration [19, 20].

Lignin contained in the black liquor fraction

A black liquor fraction was obtained when 12.5 % 1-butanol or 1-pentanol was used as the solvent (Fig. 1). Lignin was precipitated from the black liquor fraction by dilution with water [2]. Lignin recovery, as calculated using the equation (lignin in black liquor)/[(lignin in raw biomass)—(lignin in solid fraction)], was 12.5 and 25.6 % using 1-butanol or 1-pentanol as the solvent, respectively, corresponding to 8.1 and 19.1 % lignin content in the raw sorghum bagasse, respectively (Fig. 4). The lignin recovery in the present study was similar to that of a previous study, which reported 5.1–17.2 % lignin recovery from wheat straw pretreated with 50–60 % ethanol at 190–210 °C [5]. However, our lignin recovery was lower than that from rye straw pretreated at 190 °C for 3 h at a 1.3 % acid concentration (35 %) [21]. Therefore, process optimization of lignin recovery with respect to solvent concentration, temperature, time, and acid concentration will be necessary in the future. It is also possible that low lignin recovery was due to the loss of water-soluble products from lignin degradation [21].

Fig. 4
figure4

Yield of lignin in black liquor. Lignin recovery was calculated as follows: (lignin in black liquor)/[(lignin in raw biomass)—(lignin in solid fraction)]

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Next, the composition and structure of the lignins in the black liquor fraction were analyzed using 2D 1H-13C HSQC NMR [15]. The syringyl, guaiacyl, and p-hydroxyphenyl lignin units are important aromatic elements of the plant cell wall [22]. Strong signals related to these lignin components (regions of interest [ROIs] 7–13) were detected in the black liquor, compared with raw sorghum bagasse (Fig. 5 and Additional file 2). Other strong signals related to aromatic components, such as p-coumarate (ROIs 1–6) and ferulate (ROIs 15 and 16), were detected in the black liquor. The only aromatic region signal that was weaker in the black liquor was that related to cinnamyl alcohol (ROI 14). Accordingly, signals related to methoxyl (ROIs 17 and 18) groups were stronger, as methoxyl groups are found in the side chains of syringyl, guaiacyl, and ferulate [23].

Fig. 5
figure5

Peaks of raw sorghum bagasse and black liquor. Left portion of figure shows NMR peaks of raw biomass. Middle and right portions of figure show NMR peaks of black liquor obtained after organosolv pretreatment of sorghum bagasse using 1-butanol or 1-pentanol as the solvent, respectively

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In contrast, the signal related to a major interunit structure, β–O–4 (ROI 24), was weaker in the black liquor than in raw sorghum bagasse. This was probably due to partial cleavage of the thermally labile β–O–4 unit in raw sorghum bagasse under heat treatment [24, 25]. Another signal (ROI 25) related to the β–O–4 unit was stronger in the black liquor, but the reason for this difference is unclear. Signals related to other minor interunit structures in raw sorghum bagasse were either stronger or weaker in the black liquor. These results suggest that most of the lignin aromatic components were concentrated in the black liquor in samples pretreated using 1-butanol or 1-pentanol as the solvent; however, the major linkage structure was lost.

Which lignin constituent is most affected by 1-butanol or 1-pentanol was also investigated by comparing 2D NMR signals of solid fractions obtained by pretreatment with no solvent (control), 1-butanol, or 1-pentanol (Fig. 6 and Additional file 3). Compared with the solid fraction obtained using no solvent (control), signals related to p-coumarate (ROIs 2–6) were weaker in solid fractions obtained using 1-butanol or 1-pentanol as the solvent. In addition, the signals related to guaiacyl (ROI 10), syringyl (ROIs 11 and 12), and minor β–O–4 interunits (ROIs 21–23, 26, and 27) in solid fractions obtained using 1-butanol or 1-pentanol as the solvent were weaker compared with the control. Accordingly, because the guaiacyl, syringyl, and β–O–4 units contain a methoxyl side chain, methoxyl-related signals (ROIs 17 and 18) were weaker in solid fractions obtained using 1-butanol or 1-pentanol [23]. The removal of p-coumarate, syringyl, and guaiacyl from the solid fraction using 1-butanol or 1-pentanol corresponded with the results of increased aromatic lignin regions in the black liquor fraction and decreased acid-insoluble content in the solid fraction.

Fig. 6
figure6

Peak of solid fractions. Left, middle, and right portions of figure show NMR peaks of the solid fractions obtained by organosolv pretreatment of sorghum bagasse using no solvent (control) and 1-butanol and 1-pentanol as the solvent, respectively

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Ethanol fermentation using the solid fraction

The solid fraction obtained after organosolv pretreatment can be utilized as a sugar source for microbial fermentation. The solid fractions obtained after organosolv pretreatment using 1-butanol or 1-pentanol as the solvent were subjected to simultaneous saccharification and fermentation by S. cerevisiae. Ethanol production using each of these solid fractions was compared with that obtained with control solid fraction (Fig. 7). As expected, the ethanol production rates obtained with solid fractions of samples pretreated with 1-butanol or 1-pentanol (2.6 and 2.8 g/L/h, respectively) were about 1.6 times higher in the first 9 h than those obtained with the solid fraction of samples pretreated with no solvent (1.6 g/L/h). After 96 h of fermentation, ethanol production from the 1-butanol and 1-pentanol solid fractions was about twice that of the control, reaching 43.1 and 47.2 g/L, respectively. In addition, the theoretical ethanol yield from the 1-butanol and 1-pentanol solid fractions was 59.6 and 62.1 %, respectively, compared with 32.4 % for the control. As suggested previously [26], organosolv delignification and the resultant supply of readily hydrolyzable cellulose substrates results in an increase in the concentration of microbial fermentation products.

Fig. 7
figure7

Simultaneous saccharification and fermentation of solid fractions by Saccharomyces cerevisiae. Solid fractions were obtained by organosolv pretreatment of sorghum bagasse using 1-butanol (closed square) and 1-pentanol (closed triangle) as the solvent and no solvent (closed circle). Ethanol fermentation was initiated from 200 g/L of solid fraction

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Conclusions

Sorghum bagasse was fractionated by organosolv pretreatment using various solvents at a low concentration of 12.5 %. The catalyst for the reaction was 1 % sulfuric acid, and the reaction was carried out at 180 °C for 45 min. Pretreatment with the highly hydrophobic solvents 1-butanol and 1-pentanol produced three visible fractions (i.e., a cellulose-enriched solid fraction, a liquid fraction containing hemicellulose-derived xylose, and a black liquor fraction containing lignin). However, only two fractions were produced upon pretreatment with ethanol, 1-propanol, or 2-propanol (i.e., a solid fraction containing cellulose and a liquid fraction containing xylose), and recovery of lignin was difficult. 2D NMR spectroscopy revealed that the black liquor fraction contained lignin aromatic components, such as guaiacyl, syringyl, p-hydroxyphenyl, p-coumarate, and ferulate. The aliphatic β–O–4 unit of lignin was absent in the black liquor fraction. Pretreatment with 1-butanol or 1-pentanol effectively removed p-coumarate, syringyl, and some of the guaiacyl from raw sorghum bagasse. The 1-butanol or 1-pentanol should be recovered after pretreatment and recycled using separation technologies such as pervaporation [27, 28]. We demonstrated here the effective organosolv pretreatment of sorghum bagasse using a low concentration of hydrophobic solvent (1-butanol or 1-pentanol).

Methods

Plant materials

The hybrid sorghum cultivar Tentaka [29] was grown in 2013 at an experimental field in Okinawa, Japan. Whole plants were harvested at the heading stage and then fully dried in a greenhouse. After removal of the panicles, the culms were ground into a fine powder using a blender (WB-1; TGK, Hachioji, Japan) fitted with a 2-mm screen.

Organosolv pretreatment

Organosolv pretreatment was performed using a laboratory-scale thermostirrer (HHE-19G-U; Koike Precision Instruments, Kanagawa, Japan) having a total volume of 100 mL. Sorghum bagasse powder (6 g) was suspended in 80 mL of aqueous solution. The aqueous solution included 70 mL of 1 % sulfuric acid and 10 mL of solvent (ethanol, 1-propanol, 2-propanol, 1-butanol, or 1-pentanol). An aqueous solution consisting of 80 mL of 1 % sulfuric acid was used as the control. Next, the mixture was treated at 180 °C for 45 min, with agitation at 200 rpm. The optimal temperature and agitation speed for pretreatment were determined according to a previous report [30]. After pretreatment, the mixture was centrifuged at 3500 rpm for 10 min for fractionation. Solid and liquid fractions were obtained under the control condition and with ethanol, 1-propanol, or 2-propanol (Fig. 1). When using 1-butanol or 1-pentanol as the solvent, the supernatant including the liquid and black liquor fractions was recovered and again centrifuged at 3500 rpm for 10 min in order to separate the fractions. The upper phase contained the black liquor fraction, and the lower phase contained the liquid fraction. The solid fraction was washed with deionized water, neutralized to pH 7.0, then dried; the dry weight was measured using an electronic balance (XS105DU; Mettler Toledo, Greifensee, Switzerland). Lignin was separated from the black liquor fraction by precipitation upon dilution with 80 mL of water. The compositions of cellulose, hemicellulose, acid-insoluble lignin, acid-soluble lignin, and ash were determined according to the National Renewable Energy Laboratory method [31].

Sugar analysis

Sugar analysis was performed as described previously [30]. The liquid fraction was neutralized to pH 5.0 by the addition of calcium hydroxide. An aliquot of sample (1.5 μL) was mixed with 1.5 μL of 0.1 % (w/w) Ribitol as internal standard, and then the mixture was dried in a vacuum concentrator (7810010; Labconco, Kansas City, MO, USA). The dried residue was dissolved in 100 μL of 20 mg/mL of methoxyamine hydrochloride in pyridine and incubated at 30 °C for 90 min, after which 50 μL of N-methyl-N-trimethylsilyltrifluoroacetamide was added and the sample was incubated at 37 °C for 30 min. A 10 μL aliquot of the solution was subjected to gas chromatography-mass spectrometry (GC–MS) (GCMS-2010plus; Shimadzu, Kyoto, Japan) under the following conditions: column, Agilent CP-Sil 8CB-MS (30 m × 0.25 mm); carrier gas, helium; injection temperature, 230 °C; oven temperature, 80 °C at t = 0–2 min, then increased to 330 °C at 15 °C/min.

Byproduct analysis

Byproduct analysis was performed as described previously [30]. Acetone (900 μL) was added to 100 µL of liquid fraction and mixed thoroughly. The sample was then centrifuged at 21,880×g and room temperature for 10 min. The supernatant (10 µL) was subjected to GC–MS analysis (GC-MS-2010plus; Shimadzu). 5-HMF and furfural were analyzed under the following conditions: column, Agilent CP-Sil 8CB-MS (30 m × 0.25 mm); carrier gas, helium; injection temperature, 250 °C; oven temperature, 50 °C at t = 0–5 min, then increased to 280 °C at 20 °C/min. Acetic acid and formic acid were analyzed under the following conditions: column, Agilent DB-FFAP (60 m × 0.25 mm); carrier gas, helium; injection temperature, 250 °C; oven temperature, 100 °C at t = 0 to 5 min, then increased to 230 °C at 10 °C/min.

Enzymatic saccharification

Enzymatic saccharification of the solid fraction (10 % dry weight) was performed by adding 0.3 M citrate buffer (pH 4.8) and cellulase (Celic CTec2, Novozyme, Bagsvaerd, Denmark) at a concentration of 6.6 filter paper units (FPU)/g-dry biomass. Tetracycline (40 μg/mL) and cycloheximide (30 μg/mL) were added to prevent microbial growth. The reaction mixture was incubated at 50 °C in a chemi station (PPS-2000, Tokyo Rikakikai, Tokyo, Japan) with agitation at 120 rpm for 72 h. Enzymatic saccharification was stopped by rapid chilling on ice, followed by centrifugation at 21,880×g for 10 min at 4 °C. The sugars in the supernatant were analyzed as described above.

Composition analysis

Compositional analysis was performed according to the National Renewable Energy Laboratory (NREL) method [31]. Obtained sugar was analyzed as described above. The amount of acid-soluble lignin was determined by measuring the optical density (OD) at 240 nm.

Solution 2D NMR spectroscopy

Sample preparation for solubilized lignocelluloses was similar to previously reported methods [32, 33]. Briefly, the dried sample was further ground using a Pulverisette 5 ball mill (Fritsch GmbH, Idar-Oberstein, Germany). The ball-milled powder (30 mg) was mixed with 600 µL of dimethyl sulfoxide (DMSO)-d6:pyridine-d5 (4:1), heated at 50 °C for 30 min in a Thermomixer Comfort (Eppendorf AG, Hamburg, Germany), then centrifuged at 20,380×g for 5 min. The supernatant was transferred to 5-mm ϕ NMR tubes and subjected to NMR analysis. NMR spectra were recorded on an Avance III HD-600 (Bruker, Billerica, MA, USA) equipped with a 5-mm TXI-cryoprobe operated at 600 MHz for 1H- and 125 MHz for 13C-NMR. The temperature of all NMR samples was maintained at 319 K. The chemical shifts were referenced to the methyl group of DMSO-d6 at 13C = 40.03 ppm and 1H = 2.582 ppm.

Two-dimensional 1H-13C heteronuclear single-quantum spectra were collected using echo/antiecho gradient selection (the hsqcetgp pulse program in the Bruker library). Forty-eight regions of interest (ROIs) were compared with previously assigned chemical shifts [23, 34]. ROI details are described in Additional file 4.

Liquefaction and ethanol fermentation

Liquefaction of the solid fraction was performed in a 50 mL polypropylene tube (Corning Inc., NY, USA) set in a Thermo Block Rotator SN-06BN heat block (Nissin, Tokyo, Japan), as described previously [35]. The tube was closed with a silicone plug (As One, Osaka, Japan), into which a hole was made using a disposable needle (φ = 0.6 mm) (Termo Corp., Tokyo, Japan). In the tube, the solid fraction (final weight 200 g/L) was mixed with medium containing 50 mM citric acid buffer (pH 5.0) and 6.6 FPU/g-biomass of commercial cellulase (Cellic CTec2; Novozymes Inc., Bagsvaerd, Denmark) and axially rotated at 35 rpm at 50 °C for 2 h.

Saccharomyces cerevisiae strain BY4741 (genotype: MATa his3∆1 leu2∆0 met15∆0 ura3∆0) [36] was purchased from the American Type Culture Collection (ATCC) as ATCC No. 404002. The cells were aerobically propagated for 24 h at 30 °C and 150 rpm in 5 mL of YPD medium [10 g/L yeast extract [Becton, Dickinson and Company, Tokyo, Japan], 20/g L polypeptone (Wako Pure Chemical Industries, Ltd., Osaka, Japan), and 20 g/L glucose], and then cultivated for 24 h in 500 mL of YPD medium. The cells were collected by centrifugation at 3000×g for 10 min at 4 °C and washed twice with distilled water. Ethanol fermentation was initiated by the addition of yeast extract (final concentration 10 g/L), peptone (final concentration 20 g/L), and S. cerevisiae cells (50 g-wet cells/L, corresponding to 10 g-dry cells/L) after 2 h of liquefaction of the solid fraction. Ethanol fermentation was conducted by axial agitation at 35 rpm and 35 °C for 48 h. Theoretical ethanol yield (%) was calculated as the percent of 0.511 g-ethanol/g-sugar of consumed glucose as follows:

$${\text{Ethanol}}\,{\text{yield}}\,{ = }\,\frac{{{\text{Ethanol}}\,{\text{produced}}\,\left( {\text{g}} \right)}}{{{\text{Glucan}}\,{\text{in}}\,{\text{solid}}\,{\text{fraction}}\left( {\text{g}} \right)}}\,$$

Abbreviations

2D 1H-13C HSQC NMR:

two-dimensional 1H-13C heteronuclear single-quantum coherence nuclear magnetic resonance

ROI:

region of interest

5-HMF:

5-hydroxymethylfurfural

GC–MS:

gas chromatography-mass spectrometry

FPU:

filter paper units

References

  1. 1.

    Tanaka T, Kondo A. Cell surface engineering of industrial microorganisms for biorefining applications. Biotechnol Adv. 2015;33:1403–11.

    Article  CAS  Google Scholar 

  2. 2.

    Zhao X, Cheng K, Liu D. Organosolv pretreatment of lignocellulosic biomass for enzymatic hydrolysis. Appl Microbiol Biotechnol. 2009;82:815–27.

    Article  CAS  Google Scholar 

  3. 3.

    Rooney WL, Blumenthal J, Bean B, Mullet JE. Designing sorghum as a dedicated bioenergy feedstock. Biofuels Bioprod Bioref. 2007;1:147–57.

    Article  CAS  Google Scholar 

  4. 4.

    Kim M, Day DF. Composition of sugar cane, energy cane, and sweet sorghum suitable for ethanol production at Louisiana sugar mills. J Ind Microbiol Biotechnol. 2011;38:803–7.

    Article  CAS  Google Scholar 

  5. 5.

    Wildschut J, Smit AT, Reith JH, Huijgen WJ. Ethanol-based organosolv fractionation of wheat straw for the production of lignin and enzymatically digestible cellulose. Bioresour Technol. 2013;135:58–66.

    Article  CAS  Google Scholar 

  6. 6.

    Zakzeski J, Bruijnincx PCA, Jongerius AL, Weckhuysen BM. The catalytic valorization of lignin for the production of renewable chemicals. Chem Rev. 2010;110:3552–99.

    Article  CAS  Google Scholar 

  7. 7.

    Huber GW, Iborra S, Corma A. Synthesis of transportation fuels from biomass: chemistry, catalysts, and engineering. Chem Rev. 2006;106:4044–98.

    Article  CAS  Google Scholar 

  8. 8.

    Lan W, Liu CF, Sun RC. Fractionation of bagasse into cellulose, hemicellulose, and lignin with ionic liquid treatment followed by alkaline extraction. J Agric Food Chem. 2011;59:8691–701.

    Article  CAS  Google Scholar 

  9. 9.

    Mosier N, Wyman C, Dale B, Elander R, Lee YY, Holtzapple M, Ladisch M. Feature of promising technologies for pretreatment of lignocellulosic biomass. Bioresour Technol. 2005;96:673–86.

    Article  CAS  Google Scholar 

  10. 10.

    Sun Y, Cheng J. Hydrolysis of lignocellulosic materials for ethanol production: a review. Bioresour Technol. 2002;83:1–11.

    Article  CAS  Google Scholar 

  11. 11.

    Huijgen WJJ, Smit AT, de Wild PJ, den Uil H. Fractionation of wheat straw by prehydrolysis, organosolv delignification and enzymatic hydrolysis for production of sugars and lignin. Bioresour Technol. 2012;114:389–98.

    Article  CAS  Google Scholar 

  12. 12.

    Zhang K, Pei Z, Wang D. Organic solvent pretreatment of lignocellulosic biomass for biofuels and biochemicals: a review. Bioresour Technol. 2016;199:21–33.

    Article  CAS  Google Scholar 

  13. 13.

    Taherzaden M, Karimi K. Pretreatment of lignocellulosic wastes to improve ethanol and biogas production: a review. Int J Mol Sci. 2008;9:1621–51.

    Article  Google Scholar 

  14. 14.

    Tsuji Y, Vanholme R, Tobimatsu Y, Ishikawa Y, Foster CE, Kamimura N, et al. Introduction of chemically labile substructures into Arabidopsis lignin through the use of LigD, the Cα-dehydrogenase from Sphingobium sp. strain SYK-6. Plant Biotechnol J. 2015;13:821–32.

    Article  CAS  Google Scholar 

  15. 15.

    Mansfield SD, Kim H, Lu F, Ralph J. Whole plant cell wall characterization using solution-state 2D NMR. Nat Protoc. 2012;7:1579–89.

    Article  CAS  Google Scholar 

  16. 16.

    Teramura H, Sasaki K, Oshima T, Aikawa S, Matsuda F, Okamoto M, et al. Changes in lignin and polysaccharide components in 13 cultivars of rice straw following dilute acid pretreatment as studied by solution-state 2D 1H-13C NMR. PLoS One. 2015;10:e0128417.

    Article  Google Scholar 

  17. 17.

    Selig MJ, Viamajala S, Decker SR, Tucker MP, Himmel ME, Vinzant TB. Deposition of lignin droplets produced during dilute acid pretreatment of maize stems retards enzymatic hydrolysis of cellulose. Biotechnol Prog. 2007;23:1333–9.

    Article  CAS  Google Scholar 

  18. 18.

    Alvira P, Tomás-Pejó E, Ballesteros M, Negro MJ. Pretreatment technologies for an efficient bioethanol production process based on enzymatic hydrolysis: a review. Bioresour Technol. 2010;101:4851–61.

    Article  CAS  Google Scholar 

  19. 19.

    Weng YH, Wei HJ, Tsai TY, Lin TH, Wei TY, Guo GL, et al. Separation of furans and carboxylic acids from sugars in dilute acid rice straw hydrolysates by nanofiltration. Bioresour Technol. 2010;101:4889–94.

    Article  CAS  Google Scholar 

  20. 20.

    He Y, Bagley DM, Leung KT, Liss SN, Liao BQ. Recent advances in membrane technologies for biorefining and bioenergy production. Biotechnol Adv. 2012;30:817–58.

    Article  CAS  Google Scholar 

  21. 21.

    Perez-Cantu L, Schreiber A, Schütt F, Saake B, Kirsch C, Smirnova I. Comparison of pretreatment methods for rye straw in the second generation biorefinery: effect on cellulase, hemicellulase and lignin recovery. Bioresour Technol. 2013;142:428–35.

    Article  CAS  Google Scholar 

  22. 22.

    Chylla RA, Van Acker R, Kim H, Azapira A, Mukerjee P, Markley JL, et al. Plant cell wall profiling by fast maximum likelihood reconstruction (FMLR) and region-of-interest (ROI) segmentation of solution-state 2D 1H-13C NMR spectra. Biotechnol Biofuels. 2013;6:45.

    Article  CAS  Google Scholar 

  23. 23.

    Kim H, Ralph J. Solution-state 2D NMR of ball-milled plant cell wall gels in DMSO-d6/pyridine-d5. Org Biomol Chem. 2010;8:576–91.

    Article  CAS  Google Scholar 

  24. 24.

    Kim JY, Hwang H, Oh S, Kim YS, Kim UJ, Choi JW. Investigation of structural modification and thermal characteristics of lignin after heat treatment. Int J Biol Macromol. 2014;66:57–65.

    Article  CAS  Google Scholar 

  25. 25.

    Trajano HL, Engle NL, Foston M, Ragauskas AJ, Tschaplinski TJ, Wyman CE. The fate of lignin during hydrothermal pretreatment. Biotechnol Biofuels. 2013;6:110.

    Article  CAS  Google Scholar 

  26. 26.

    Pan X, Gilkes N, Kadla J, Pye K, Saka S, Gregg D, et al. Bioconversion of hybrid poplar to ethanol and co-products using an organosolv fractionation process: optimization of process yield. Biotechnol Bioeng. 2006;94:851–61.

    Article  CAS  Google Scholar 

  27. 27.

    Xue C, Du GQ, Chen LJ, Ren JG, Sun JX, Bai FW, et al. A carbon nanotube filled polydimethylsiloxane hybrid membrane for enhanced butanol recovery. Sci Rep. 2014;4:5925.

    CAS  Google Scholar 

  28. 28.

    Negishi H, Sakaki K, Ikegami T. Silicalite pervaporation membrane exhibiting a separation factor of over 400 for butanol. Chem Lett. 2010;39:1312–4.

    Article  CAS  Google Scholar 

  29. 29.

    Venuto B, Kindiger B. Forage and biomass feedstock production from hybrid forage sorghum and sorghum-sudangrass hybrids. Jpn Soc Grassl Sci. 2008;54:189–96.

    Article  Google Scholar 

  30. 30.

    Matsuda F, Yamasaki M, Hasunuma T, Ogino C, Kondo A. Variation in biomass properties among rice diverse cultivars. Biosci Biotechnol Biochem. 2011;75:1603–5.

    Article  CAS  Google Scholar 

  31. 31.

    Sluiter A, Hames B, Ruiz R, Scarlata C, Sluiter J, Templeton D, et al. Determination of structural carbohydrates and lignin in biomass. Golden: Natl Renew Energy Lab; 2011.

    Google Scholar 

  32. 32.

    Meng X, Foston M, Leisen J, DeMartini J, Wyman CE, Ragauskas AJ. Determination of porosity of lignocellulosic biomass before and after pretreatment by using Simons’ stain and NMR techniques. Bioresour Technol. 2013;144:467–76.

    Article  CAS  Google Scholar 

  33. 33.

    Komatsu T, Kikuchi J. Comprehensive signal assignment of 13C-labeled lignocellulose using multidimensional solution NMR and 13C chemical shift comparison with solid-state NMR. Anal Chem. 2013;85:8857–65.

    Article  CAS  Google Scholar 

  34. 34.

    Okushita K, Komatsu T, Chikayama E, Kikuchi J. Statistical approach for solid-state NMR spectra of cellulose derived from a series of variable parameters. Polym J. 2012;44:895–900.

    Article  CAS  Google Scholar 

  35. 35.

    Matano Y, Hasunuma T, Kondo A. Display of cellulases on the cell surface of Saccharomyces cerevisiae for high yield ethanol production from high-solid lignocellulosic biomass. Bioresour Technol. 2012;108:128–33.

    Article  CAS  Google Scholar 

  36. 36.

    Brachmann CB, Davies A, Cost GJ, Caputo E, Li J, Hieter P, et al. Designer deletion strains derived from Saccharomyces cerevisiae S288C: a useful set of strains and plasmids for PCR-mediated gene disruption and other applications. Yeast. 1998;14:115–32.

    Article  CAS  Google Scholar 

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Authors’ contributions

HT, KS, and AK designed this study and drafted the manuscript. HT, TO, and HK-a performed the biomass pretreatment and compositional analysis. MO, TS-h, FM, and JK carried out the NMR analysis and interpreted the NMR results. HK-a and CO analyzed sugars and byproducts. KH, TS-a, and HK-i prepared the sorghum bagasse and helped to revise the manuscript. TO and FM performed enzymatic saccharification. KS and AK performed ethanol fermentation. MO, TS-h, and JK revised the manuscript. All authors read and approved the final manuscript.

Acknowledgements

This work was supported in part by Grants-in-Aid from the NC-CARP project of the Ministry of Education, Culture, Sports, Science and Technology, Japan, and by the Special Coordination Fund for the Promotion of Science and Technology, Creation of Innovation Centers for Advanced Interdisciplinary Research Areas (Innovative Bioproduction Kobe), MEXT, Japan.

Competing interests

The authors declare that they have no competing interests.

Author information

Affiliations

  1. Department of Chemical Science and Engineering, Graduate School of Engineering, Kobe University, 1-1 Rokkodaicho, Nada-ku, Hyogo, Kobe, 657-8501, Japan

    Hiroshi Teramura, Tomoko Oshima, Hideo Kawaguchi, Chiaki Ogino & Akihiko Kondo

  2. Organization of Advanced Science and Technology, Kobe University, 1-1 Rokkodaicho, Nada-ku, Hyogo, Kobe, 657-8501, Japan

    Kengo Sasaki

  3. Department of Bioinformatic Engineering, Graduate School of Information Science and Technology, Osaka University, 1-5 Yamadaoka, Osaka, Suita, 565-0871, Japan

    Fumio Matsuda

  4. RIKEN Center for Sustainable Resource Science, 1-7-22 Suehiro-cho, Tsurumi-ku, Kanagawa, Yokohama, 230-0045, Japan

    Fumio Matsuda, Mami Okamoto, Tomokazu Shirai, Jun Kikuchi & Akihiko Kondo

  5. Bioscience and Biotechnology Center, Nagoya University, 1 Furo-cho, Chikusa-ku, Nagoya, 464-8601, Japan

    Ko Hirano, Takashi Sazuka & Hidemi Kitano

  6. Graduate School of Medical Life Science, Yokohama City University, 1-7-29 Suehirocho, Tsurumi-ku, Yokohama, 230-0045, Japan

    Jun Kikuchi

  7. Graduate School of Bioagricultural Sciences and School of Agricultural Sciences, Nagoya University, 1 Furo-cho, Chikusa-ku, Nagoya, 464-8601, Japan

    Jun Kikuchi

Authors
  1. Hiroshi Teramura
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  2. Kengo Sasaki
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  3. Tomoko Oshima
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  4. Fumio Matsuda
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  5. Mami Okamoto
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  7. Hideo Kawaguchi
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  8. Chiaki Ogino
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  9. Ko Hirano
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  13. Akihiko Kondo
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Corresponding author

Correspondence to Akihiko Kondo.

Additional files

Additional file 1.

Mass balance of glucose, xylose and lignin. Black bar, lined bar, gray bar, open bar and dotted bar indicated recovery in solid fraction, liquid fraction, liquid fraction byproduct, black liquor and unknown. (A) Mass balance of glucose. Liquid fraction byproduct and black liquor mean 5-HMF. (B) Mass balance of xylose. Liquid fraction byproduct and black liquor mean furfural. (C) Mass balance of lignin.

Additional file 2.

Peak intensities obtained by 2D NMR analysis of raw sorghum bagasse and black liquor. Black liquor was obtained after organosolv pretreatment of sorghum bagasse using 1-butanol or 1-pentanol as the solvent. Blue bar indicates peak intensity of raw sorghum bagasse. Orange and green bars indicate peak intensities of the solid fraction obtained using 1-butanol and 1-pentanol as the solvent, respectively.

Additional file 3.

Peak intensities obtained by 2D NMR analysis of solid fractions. The solid fractions were obtained by organosolv pretreatment of sorghum bagasse using 1-butanol and 1-pentanol as the solvent and no solvent (control). Red, orange, and blue bars indicate solid fraction pretreated with no solvent, 1-butanol, and 1-pentanol, respectively.

Additional file 4.

Annotation of each 2D 1H-13C HSQC NMR spectrum peak.

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Teramura, H., Sasaki, K., Oshima, T. et al. Organosolv pretreatment of sorghum bagasse using a low concentration of hydrophobic solvents such as 1-butanol or 1-pentanol. Biotechnol Biofuels 9, 27 (2016). https://doi.org/10.1186/s13068-016-0427-z

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Keywords

  • Sorghum bagasse
  • Organosolv pretreatment
  • Fractionation
  • 1-butanol
  • 1-pentanol
  • Lignin

Biotechnology for Biofuels

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