Patent Application
20130248128
The present invention relates generally to a process for treating lignocellulosic biomass by decomposing the lignin in the lignocellulosic biomass.
Lignocellulosic biomass is plant biomass that includes cellulose, hemicellulose, and lignin. Cellulose and hemicellulose are carbohydrate polymers that are tightly bound to the lignin. Lignocellulosic biomass can be grouped into four main categories: (1) agricultural residues; (2) energy crops; (3) wood residues, including sawmill and paper mill discards; and (4) municipal paper waste. Lignocellulosic biomass represents a potentially sustainable source of fuel and commodity chemicals, offers economic advantages over corn starch for the production of biofuels, and could contribute to carbon sequestration without impacting food crop prices. Lignocellulosic biomass could satisfy the energy needs for transportation and electricity generation, while contributing to carbon sequestration and limiting the accumulation of greenhouse gases in the atmosphere.
Potential feedstocks of lignocellulosic biomass are abundant and include crops (e.g. corn and sugarcane), agricultural wastes, forest products (e.g. wood), grasses, and algae. Among the feedstocks, wood has been widely used for the production of paper, as a construction material, and as a solid fuel. Wood is composed mainly of cellulose, hemicellulose, and lignin. Lignin includes an amorphous network of crosslinked phenylpropanoid units.
The conversion of lignocellulosic biomass into liquid fuels and/or other commodity chemicals typically includes the following steps: (1) pretreatment; (2) hydrolysis of cellulose and hemicellulose into fermentable sugars; and (3) fermentation of the sugars into the liquid fuels (e.g. ethanol) and other commodity chemicals. The pretreatment is energy-intensive but necessary due to the complex structure of the plant cell wall and the chemical resistance of lignin, which limits the access of enzymes to cellulose. An ideal pretreatment should break the lignocellulosic complex, increase the active surface area, and decrease the cellulosic crystallinity while limiting the generation of inhibitory by-products and minimizing hazardous wastes and wastewater.
A major bottleneck in the large-scale conversion of biomass to biofuels is the pretreatment delignification process that provides enzymes access to cellulose, the main source of fermentable sugars. Most current pretreatments, such as ammonia fiber explosion, alkaline hydrolysis, and acid hydrolysis, require high temperatures that increase the operation costs and generate toxic byproducts. The pretreatment is also the most expensive step in the conversion of lignocellulosic biomass to ethanol. Less expensive pretreatments that are environmentally friendly are desirable.
Various treatments have been investigated for removing the lignin, which would improve the yield of fermentable sugars for the production of biofuels. Most of these treatments are energy-intensive and/or generate toxic byproducts that affect their economic viability. A “green” pretreatment strategy was reported to replicate and optimize the enzymatic activity of natural white rot fungi such as Phanerochaete chrysosporium, which degrade biomass completely, including the lignin. The reactivity of the manganese-dependent peroxidase enzyme produced from P. chrysosporium was studied with lignin model compounds. The enzyme requires MnII and H2O2 to degrade lignin. The reaction is proposed to involve the oxidation of MnII to MnIII, a known one-electron oxidant. Stoichiometric Mn(OAc)3 was shown to oxidize guaiacyl and syringyl lignin models at a pH ranging from 2.5 to 4.1 at room temperature. The use of Mn(OAc)3 as a catalyst for the delignification of wood with H2 O2 has not been reported.
Studies involving the use of transition metal catalysts and H2O2 for the oxidative delignification of wood have been reported. A study related to the ability of several metalloporphyrins based on Fe, Co, Zn and Mn to oxidize lignin models has been reported. This work has been limited by the complex nature of these metalloporphyrins and their costly synthesis, as well as difficulties associated with catalyst recovery. Several other Mn and Fe complexes of synthetic macrocyclic ligands, including [(TACN)Mn(μ-O)3Mn(TACN)](PF6)2 (TACN=1,4,7-trimethyl-1,4,7-triazacyclo-nonane) and polypyridyl ligands, were shown to catalyze the delignification of wood using hydrogen peroxide. Methyl-trioxorhenium was reported to catalyze the oxidation of lignin model compounds and lignin. Although promising activity was observed at 60° C. using [(TACN)Mn(μ-O)3Mn(TACN)](PF6)2, the expensive synthetic ligands have limited the application of this type of catalyst.
A combination of Co(OAc)2 and Mn(OAc)2 was reported to catalyze the aerobic auto-oxidation of lignin in acetic acid solution at 140-220° C. In ionic liquid solution, Mn(NO3)2 and CoCl2 were found to catalyze the oxidation of various lignin and lignin models in air, but this also requires elevated temperatures (80-100° C.) and/or high pressures (83 atm).
A simpler process for delignification of lignocellulosic biomass may improve the economic viability of oxidative delignification.
To achieve the foregoing and other objects, and in accordance with the purposes of the present invention, as embodied and broadly described herein, the present invention provides a process for treating lignocellulosic biomass. The process involves dissolving manganese (III) acetate into water to form a first aqueous solution, combining an aqueous solution of hydrogen peroxide with the first aqueous solution to form a second aqueous, said second aqueous solution comprising a pH of less than about 6, providing lignocellulosic biomass that includes lignin, and combining the second aqueous solution with the lignocellulosic biomass under conditions suitable for the decomposition of the lignin, thereby treating the lignocellulosic biomass.
The invention relates to a process for the treatment of lignocellulosic biomass by delignification of the biomass. The process is inexpensive, simple, and effective under ambient conditions. The process may be applied to any biomass that contains lignin. When the process is applied to wood, for example, the result is delignification of the wood. The process may be used for the delignification of grasses such as but not limited to switchgrass, The process may be used for the delignification of non-food agricultural waste material, such as but not limited to wood (e.g. wood chips), plant residues, corn stover, grain husks, etc. In short, the process can be used for the delignification of substrates that contain lignin. It should be understood that the invention is not limited use with any particular type of types of lignin (organosolv lignin, kraft lignin, etc.). In an embodiment, manganese (III) acetate (Mn(OAc)3) catalyzes the delignification of wood at room temperature in aqueous solution using hydrogen peroxide. In another embodiment, manganese (II) acetate in an acetate buffered solution also catalyzes the delignification of lignocellulosic biomass using hydrogen peroxide. In other embodiments, manganese (II) triflate (i.e. trifluoromethanesulfonate) or manganese trifluoroacetate are expected to also catalyze the delignification of lignocellulosic biomass using hydrogen peroxide. The process can be performed at ambient temperature and also at elevated temperatures that do not exceed the decomposition temperature of hydrogen peroxide, which is about 150° C. Temperatures of 145° C., 140° C., 135° C., 130° C., 125° C., 120° C., 110° C., 105° C., 100° C., 95° C., 90° C., 85° C., 80° C., 75° C., 70° C., 65° C., 60° C., 55° C., 50° C., 45° C., 40° C., 35° C., 30° C., 25° C., ambient temperature, and temperatures in between any of these values, are all suitable for the process. Reaction times for the decomposition of the lignin of a week or less (e.g. 6 days, 5 days, 4 days, 3 days, 2 days, 1 day, less than 1 day, and all times in between) are suitable reaction times, as well as times greater than one week. Also within the scope of the invention are concentrations of hydrogen peroxide in the hydrogen peroxide solution of about 30% or less. Concentrations of the manganese containing solution up to about 2 Molar are also within the scope of this invention.
An initial assessment was made using different manganese-containing materials for carrying out the delignification of wood. Multiple poplar wood sections of comparable sizes (50 μm thickness) were immersed in H2O2 solutions (2.2 M) containing the complexes (50 mM). Several manganese-containing materials were tested, including Mn(OAc)3, Mn(acac)3 (acac=acetylacetonate), MnO2, Mn(pic)3 (Hpic=picolinic acid), Mn(pic)(dipic)(H2O) (Hdipic=dipicolinic acid), NMe4[Mn(opba)(H2O)2] (opba=o-phenylenebis(oxamate)) and Mn(malt)3 (malt=maltol). The reaction mixtures were monitored by optical microscopy. Only the solution containing Mn(OAc)3 caused visible degradation of the lignocellulosic matrix of poplar at room temperature within a few days. For the other complexes, the poplar section kept its integrity even after seven days, and the samples remained unchanged microscopically. Control experiments under identical conditions with hydrogen peroxide only (2.2 M) and hydrogen peroxide (2.2 M) with an acetate buffer (150 mM) showed no visible changes to the wood structure. No visible changes were observed using a variety of other transition-metal-containing salts including FeCl2, CuCl, Cu(OAc)2, MnSO4, NaVO3, or Co(OAc)2, under otherwise identical conditions.
The visible changes occurring to the wood structure upon exposure to the solution containing Mn(OAc)3 and hydrogen peroxide were then investigated in more detail. When immersed without any vigorous agitation, the poplar section broke down in smaller fragments in the presence of Mn(OAc)3 after two days at room temperature. The poplar fragments grew visibly smaller, and after five days, the poplar section turned into a fine solid residue at the bottom of the vial. With only mild manual agitation, the poplar section became fragmented in less than one day. The pH of the Mn(OAc)3 solution was originally less than about 6. A pH from about 3.0 to about 5.5 may be used. In an embodiment, the pH was 4.6 before the introduction of the sample and remained so after seven days. When monitored by optical microscopy, the lignin-rich middle lamella between cells and the cell corners became darker and wider. After a one-day treatment and mild manual agitation, the poplar section was cleaved along the ray parenchyma cells, the middle lamella, and vessels. Rows of poplar cells, as well as individual cells, became free from large fragments and laid on their side on the Petri dish. In some areas, loose material from the wood decomposition covered entirely the underlying wood structure. Some bubbling was also observed, particularly around cells damaged by mechanical action (cutting and manipulation during sample preparation), and along the ray parenchyma cells. The wood fragments became smaller and after 3 days, only a few large fragments with more than several hundred cells remained. Isolated cells and short rows of cells were then commonly seen. Although the middle lamella between cells became looser and wider, the cellulose-rich cell walls remained relatively intact, even after five days. However after seven days, even individual cells were visibly degraded. At this time, the sample was left to dry in air and microscopic images revealed a seemingly amorphous film covering the bottom of the Petri dish.
To characterize the Chemical degradation, Raman images were collected from the poplar section before and after a one-day catalytic treatment. Two representative cells were selected from two different areas on the sample. For a sample that was left to dry overnight, the middle lamellae and cell corners appeared to widen. This result following drying was consistently reproduced in multiple experiments. Raman images of cellulose and lignin were obtained by integrating over the wave number ranges of 1070-1170 cm−1 and 1590-1640 cm−1, respectively. These spectral ranges included the 1096, 1121, 1152 cm−1 bands from cellulose, and the 1602 and 1620 cm−1 bands from lignin. Due to a weak signal-to-ratio for lignin, a linear background was subtracted from the integrated data. An overall decrease in the cellulose and lignin Raman signal was observed after the one-day treatment. This decrease was not attributable to a smaller sample thickness because the laser penetration depth was smaller than 6 micrometers (μm) and all cells lying on their side had a thickness of about 50 μm after a three-day treatment. The Raman signal decrease indicates a loss of material, particularly in the case of lignin, where the signal was barely above the noise level after treatment. For the cellulose, the signal decrease could indicate a loss of material or a decrease in the crystallinity.
The catalytic degradation was pronounced along the lignin-rich middle lamellae. Prior to the treatment, the cellulose was mostly concentrated in the secondary cell wall, while the lignin was concentrated along the middle lamellae and in the cell corners. After treatment, the cellulose signal was strongest in the secondary cell wall layers closest to the lumens, while it remained strong close to the middle lamellae. No lignin was detected in the widened middle lamellae, while only traces remained in the secondary cell wall layers closest to the middle lamellae. These results confirmed a delignification and the loosening of the lignocellulosic matrix, which led to the fragmentation of the sample.
Raman spectra collected from areas that included multiple poplar cells further confirmed the delignification process. In the dry wood spectrum, the cellulose and lignin bands were clearly visible in the spectral ranges 1070-1170 cm−1 and 1590-1640 cm−1, respectively. The bands located between 1270 and 1380 cm−1 have previously been assigned to various stretching vibrations in cellulose and lignin. The Raman spectrum collected from the solid residue that remained upon evaporation of the catalyst solution exhibited a strong band at around 940 cm−1, which was assigned to acetate anion. After treatment of the wood with Mn(OAc)3/H2O2, Raman spectra were collected from the remaining solid residues. Raman spectra of the amorphous film indicated the presence of manganese acetate and cellulose. The Raman spectrum from dried poplar fragments similar to those shown in FIGS. 2e and 2h still exhibited strong cellulose bands at 1096 and 1121 cm−1 with limited broadening, while the lignin bands at 1602 and 1620 cm−1 were absent. The bands located between 1270 and 1380 cm−1 became also absent. The Raman spectra show that the delignified wood product is very pure in cellulose with little detectable lignin.
To assess the pretreatment effect on biomass conversion, poplar sawdust pretreated with Mn(OAc)3 (50 mM) and hydrogen peroxide (2.2 M) for 2, 4 and 7 days was subjected to enzymatic hydrolysis for 24 hours at 55° C. Poplar sawdust exposed for the same durations to water only were also prepared as controls. The glucose concentration in the broth resulting from enzymatic hydrolysis was then determined by a LC/MS analysis, Before the enzymatic treatment of the wood, the excess solution containing hydrogen peroxide and Mn was removed and the solid residue was immersed in 10 mL of deionized water for 24 hours. All samples, including controls, were then rinsed five times with deionized water. The rinsing was necessary because similar control experiments conducted on sawdust exposed to H2O2 (2.2 M) only resulted in lower glucose yields compared to the controls exposed only to water. These results suggested that the excess hydrogen peroxide and/or Mn inhibited the enzymatic activity involved in cellulose hydrolysis.
LS/MS data showed a small increase in glucose yield for the controls only exposed to water with increasing exposure time. This can be partially explained by the overall expansion of wood cells in water, which is known to widen pits in the cell wall and improve the access of enzymes. For the rinsed pretreated samples, the glucose yield was consistently higher than the controls, showing an improvement ranging from 20% to 40%. The improved glucose yield observed after a two-day treatment means that longer pretreatments of several days are unnecessary for this treatment to have a positive effect on biomass conversion. For the treated samples, the aqueous solutions removed from the samples during rinsing contained an unknown amount of white insoluble solid residue that was excluded from enzymatic hydrolysis, In contrast, the solutions removed from the controls were clear. Optical microscopy and Raman spectroscopy showed that this solid residue was mostly constituted of individual delignified wood cells and amorphous cellulose. This material loss may have reduced the amount of delignified wood and cellulose available for hydrolysis. The improved yields mentioned above therefore underestimate the pretreatment effect on biomass conversion.
Upon dissolving Mn(OAc)3 in water, a dark brown precipitate formed immediately, presumably due to the well-known disproportionation of Mn(OAc)3 in the absence of excess acetic acid. Slow addition of hydrogen peroxide to the mixture resulted in initial bubbling accompanied by dissolution of the solid, forming a clear, colorless solution of pH 4.6. The absence of color suggests that MnII is the dominant species in solution. Both MnIII and MnIV have been reported to be reduced to MnII by H2O2 under acidic conditions. Consistent with this idea, a solution of MnII(OAc)2 (50 mM), acetic acid (HOAc) (100 mM), and H2O2 (2.2 M) showed similar catalytic activity to the original solution prepared from MnIII(OAc)3 (50 mM) and H2O2 (2.2 M). Furthermore, identical UV-vis spectra were obtained from an aqueous solution prepared from MnIII (OAc)3 and H2O2 (2 equiv) and an aqueous solution prepared from MnII(OAc)2, (1 equiv), and H2O2 (1.5 equiv).
The pH of the solution was found to affect the catalytic activity. For example, an unbuffered solution of MnII(OAc)2 and H2O2 at a pH of about 6.0 underwent rapid, vigorous bubbling due to catalytic disproportionation of the hydrogen peroxide. A similar reaction was observed upon raising the pH of the solution prepared from MnIII(OAc)3 and H2O2 above pH of approximately 6 by addition of sodium carbonate or sodium phosphonate buffer. This catalase-type reactivity of manganese is well-known and resulted in complete consumption of the H2O2 within several hours at room temperature, preventing the delignification activity. In contrast, the H2O2 was consumed much more slowly in a solution of MnIII(OAc)3 (50 mM) at pH 4.6, diminishing from an initial concentration of 2.2 M to approximately 1.1 M only after 7 days.
Detailed studies of the pH dependence of the catalytic reaction were complicated by the finding that the catalytic reaction was affected by the presence of other types of ions in solution. For instance, carrying out the reaction with added NaCl (0.2, 1, and 2M) resulted in slower fragmentation of the wood. Likewise, increasing the concentration of acetate buffer (to 0.2, 0.5, 1, and 2 M) also resulted in a qualitative decrease in the observed fragmentation rate. No delignification was observed using Mn(OAc)3 and H2O2 in NaH2PO4 buffers (0.5 M, pH˜1.6 M or 2.5 M). As discussed above, rapid disproportionation was observed upon addition of H2O2 to a solution of Mn(OAc)3 in Na2HPO4 buffer (0.5 M, pH˜6.5) or Na2CO3 buffer (0.5 M, pH of about 9.9).
There are a variety of possible mechanisms for the manganese-catalyzed reaction. Previous studies of the oxidation of phenolic arylglycerol β-aryl ether lignin dimers by Mn-peroxidases proposed both single electron transfer and hydrogen atom abstraction pathways. Detailed studies suggest that hydride transfer, electron transfer, and hydrogen atom transfer pathways are all possible in the reactions of high-valent Mn-oxo dimers. Hydrogen atom abstraction was also proposed for oxidations of alkyl aromatics by Mn(IV) and Mn(V) oxo porphyrins. A number of other mechanisms have been invoked for Mn-based oxidations, including oxo-transfer from a high-valent Mn complex, which is commonly proposed in olefin epoxidation and other oxidation reactions. Notably, MnII salts were recently found to catalyze the epoxidation of olefins in acetonitrile/water solution using peroxyacetic acid as the oxidant. Alternatively, a radical mechanism could be involved for the wood oxidation. Sawyer and others have found that several Mn complexes, including Mn(salen), catalyze oxygenated Fenton-type chemistry, activating O2 in the presence of tBuOOH to oxidize hydrocarbons via radical intermediates. Consistent with this idea, recent work involving the treatment of spruce wood with several iron salts under acidic conditions has shown that Fenton-type chemistry can degrade the lignocellulose matrix, producing fragments high in cellulose. However, a combination of MnCl2 and 2,3-dihydroxybenzoic acid was found to be ineffective at inducing delignification under the reaction conditions. Due to the variety of pathways known for Mn-based oxidations and the complex nature of the wood substrate, the mechanisms of oxidation are under investigation.
More details related to the experimental procedures are described below. Unless specified otherwise, all manipulations were carried out under air at ambient temperature. All chemicals were obtained from FISHER SCIENTIFIC and used as received. UV-Vis spectra were obtained on an AGILENT UV-Vis spectrometer 8743. Complexes Mn(pic)3 (Hpic=picolinic acid), Mn(pic)(dipic)(H2O) (Hdipic=dipicolinic acid), NMe4[Mn(opba)(H2O)2] (opba=o-phenylenebis(oxamate)) and Mn(malt)3 (malt=maltol) were prepared according to published procedures. Transverse sections of poplar wood (Populus tremuloides) of 50 μm thickness were prepared using a sliding microtome. The sections were dried in an oven for 4 hours between glass slides at 60° C. to prevent curling. pH measurements were recorded using an IQ150 pH meter (IQ Scientific Instruments, Carlsbad, Calif.).
Oxidation of wood using transition metal salts. In a small glass vial, an appropriate amount of a metal salt (FeCl2, CuCl, Cu(OAc)2, Mn(OAc)3, MnSO4, NaVO3, Fe(OAc)2, or Co(OAc)2) corresponding to 0.10 mmol of the salt was dissolved in deionized water (1.5 mL). Hydrogen peroxide (0.5 mL of a 30% aqueous solution, 4.4 mmol) was added dropwise, resulting in vigorous bubbling in some cases. A 5×8 mm2 poplar section was then immersed in the vial, and the reaction was monitored by a time-lapse series of photographs collected over a period of seven days.
Determination of hydrogen peroxide concentration in transition metal salt solutions. Hydrogen peroxide concentrations were determined by a previously published procedure involving spectrophotometric titration with an aqueous solution of ammonium heptamolybdate (see: Chai, X.-S.; Hou, Q. X.; Luo, Q.; Zhu, J. Y. Anal. Chim. Acta 2004, 507, 281-284, incorporated by reference). A stock solution was prepared by dissolving (NH4)6Mo7O24.4H2O (0.10 g, 0.081 mmol) in 250 mL of a 0.5 M solution of H2SO4. In a small glass vial, the appropriate metal acetate salt (Cu(OAc)2, Mn(OAc)3, Mn(OAc)2, Fe(OAc)2, or Co(OAc)2, 0.10 mmol) was dissolved in deionized water (1.5 mL). Hydrogen peroxide (0.5 mL of a 30% aqueous solutions, 4.4 mmol) was added dropwise. After 10-15 minutes, the initial concentration of H2O2 was measured by spectrophotometric titration after mixing 4 microliters (μL) of the sample with 1 mL of a solution of (NH4)6Mo7O24.4H2O in a quartz cuvette. The H2O2 concentration of the as-produced sample and the sample diluted ten times was provided by their absorbance at 350 nm. Calibration was performed with H2O2 solutions of concentrations 0%, 0.3%, 0.6%, 0.9% and 1.2%. The concentrations of H2O2 in each vial were determined again by titration once every 24 hours for 7 days.
Oxidation of wood with Mn(OAc)3. In a small glass vial, Min(OAc)3 (27 mg, 0.10 mmol) was suspended in deionized water (1.5 mL). A dark brown precipitate formed immediately. Upon dropwise addition of H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol), slight bubbling was observed and the brown solid dissolved, forming a clear, colorless solution of pH 4.6. A 5×8 mm2 poplar section was immersed in a vial containing 2 mL of this catalyst solution and a time-lapse series of photographs was collected over a period of seven days. For high-resolution images, another 4×8 mm2 section was kept immersed in 2 mL of catalyst solution contained in a polystyrene Petri dish for seven days. The Petri dish was regularly filled with the catalyst solution to compensate for evaporation and keep the solution volume constant. Just before imaging, the Petri dish was partially drained to reduce foaming and keep the sample close to the low working-distance objective. Optical images were collected in transmission with a ZEISS AXIOVERT 200M (Göttingen, Germany) inverted microscope using a 63× oil objective (NA 1.25). After the imaging session, the Petri dish was refilled with the catalyst solution.
Effect of Mn(OAc)3/H2O2 pretreatment on glucose yield from cellulose treatment. In a glass vial, Mn(OAc)3 (402 mg, 1.5 mmol) was suspended in deionized water (11.25 mL). Dropwise addition of H2O2 (3.75 mL of a 30% aqueous solution, 33.0 mmol) resulted in initial bubbling, forming a clear, colorless solution. To assess the efficiency of the pretreatment on the glucose yield after enzymatic hydrolysis, 500 mg of poplar sawdust (20-30 mesh) was placed in each of six glass test tubes. Three of the six samples were immersed for 2, 4, or 7 days in 5 mL of the Mn(OAc)3/H2O2 solution prepared as described above, while the other three were immersed in 5 mL of deionized water (control) for the same durations. After the treatment, the supernatant solution was removed from the pretreated sample by pipette and the solid residue was immersed in 10 mL of water for 24 h to remove the remaining H2O2 and catalyst. Each sample was then rinsed five times with 5 mL of deionized water before enzymatic hydrolysis. At each rinsing, the excess water was extracted with a pipette.
Enzymatic cellulose hydrolysis. Cellulases (Celluclast 1.5 L from Trichoderma reesei) and cellobiases (NOVEZYME 188 from Aspergillus niger) were obtained from NOVOZYMES (Franklinton, N.C.). The weight ratios of Celluclast 1.5 L and NOVOZYME 188 to wood were 1% and 0.05%, respectively. The enzyme mixture of cellulases and cellobiases was prepared in 0.05 M sodium acetate buffer at pH 4.8. Five mL of enzyme solution was added to the nine sawdust samples (500 mg each). The enzymatic hydrolysis took place in a water bath maintained at 55° C. for 24 h. After hydrolysis, the broth was filtered using 0.2 μm Spartan-3 filters with Teflon membranes (SCHLEICHER & SCHUELL BIOSCIENCE, Keene, N.H.) before liquid chromatography/mass spectrometry (LC/MS) analysis.
Raman microscopy. Raman spectra and images were collected with the 776 nm laser line of a tunable Ti:Sapphire laser (Mira 900-P, Coherent, Palo Alto, Calif.) coupled with a 532 nm solid state laser (MILLENIA VIIIs, SPECTRA-PHYSICS, Mountain View, Calif.). The laser beam was focused to a line using a plano-convex BK 7 150 mm focal length cylindrical lens (CKX150AR.16, Newport Corp., Irvine, Calif.) and redirected to an inverted microscope (CARL ZEISS AXIOVERT 200, Göttingen, Germany) by a Raman edge dichroic (z785rdc, CHROMA TECHNOLOGY, Rockingham, Vt.), At the sample, the laser line is about 1 μm wide and 100 μm long, with a total power of 80 mW at the sample. The sample was illuminated and the Raman signal was collected in a backscattering geometry through the same C-apochromat 63× water immersion objective (NA 1.2, CARL ZEISS). The Raman signal was focused onto the entrance of a HOLOSPEC f/2.2 spectrograph (KAISER OPTICAL SYSTEMS Ann Arbor, Mich.) and filtered with a Holographic Super-Notch-Plus Filter (HSPF-785.0AR-2.0, KAISER OPTICAL SYSTEMS, Ann Arbor, Mich.). The signal was then dispersed with a holographic grating (HSG-785-LF, KAISER) and imaged with a liquid nitrogen-cooled CCD camera (LN/CCD-1024E, PRINCETON INSTRUMENTS, Trenton, N.J.). The spectrometer was calibrated spectrally with 4-acetamidophenol, and spatially using a USAF-1951 resolution test target. The CCD images were corrected for CCD bias voltage, spherical aberrations, and the non-uniform power along the focused laser line. Raman images were acquired line by line by moving the sample by 0.5 μm steps with an exposure time of 2 min for each line. Raman spectra were obtained by integrating CCD images spatially over the area of interest. The exposure time for spectra is 30 s. Bright-field images were collected from an InfinityX-32 camera (LUMENERA CORP., Ottawa, Canada) through the same objective.
Liquid chromatography/mass spectrometry analysis (LC/MS). For quantitation of glucose, 400 μL aliquots of each sample were diluted with a 10 mM (13C6 1,2,3,4,5,6,6-d7, M+13) isotope enriched glucose standard solution in water such that the final concentration was 0.750 mM, 3 mM, and 6 mM in enriched glucose. A Thermo Scientific LTQ XL 2D linear quadrupole ion trap mass spectrometer interfaced with an electrospray ionization source and equipped with a Surveyor LC system was used. Separations were performed using a GLYCOSEP R HPLC column (4.6 mm×150 mm) (PROZYME, California, USA). The injection volume was 10 μL. A 5 min linear gradient (acetonitrile 5-10%, 0.1% formic acid in water 88-83%, methanol 7%) was used at a flow rate of 500 μL/min. Retention times for both glucose and isotope enriched glucose were 2.9-3.4 min. After 5 min, the gradient changed to 83% acetonitrile to wash the column for 2 min, followed by a 3 mm hold at original concentrations to re-equilibrate the column. Blank water runs were performed between each sample to ensure complete washing of the column. The mass spectrometer was operated in positive, single ion mode. The total ion count for the M+1 peaks of glucose (m/z 181) and the isotope enriched glucose (m/z 194) were compared for each dilution concentration of each sample. The ratio of the two peaks, the known concentration of the isotope enriched glucose, and volume corrections were used to calculate the concentration of native glucose. The peak ratios were also compared using negative ion mode and found to be consistent across samples.
Oxidation of wood with added NaCl. Mn(OAc)3 (27 mg, 0.10 mmol) was added to each of 3 vials. NaCl (0.024 g, 0.41 mmol) was added to the first vial. To the second vial, NaCl (0.116 g, 2.0 mmol) was added. NaCl (0.232 g, 4.0 mmol) was also added to the third vial. Deionized water (1.5 mL) and H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) were then added to each of the three vials. A 5×8 mm2 poplar section was then immersed in each vial and a time-lapse series of photographs was collected over a period of seven days. Fragmentation of the wood piece was observed in each vial, but the fragmentation occurred more slowly with increasing concentration of NaCl, with the third vial (2 M NaCl) breaking into a few fragments only after several days at room temperature.
Oxidation of wood with added acetate buffer. Mn(OAc)3 (27 mg, 0.10 mmol) was added to each of 5 vials, suspended in deionized water (1 mL), and H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) was added. Acetic acid was then added to vial 2 (23 μL, 0.37 mmol), vial 3 (57 μL, 0.91 mmol), vial 4 (114 μL, 1.81 mmol), and vial 5 (228 μL, 3.62 mmol). The pH was recorded in each vial, and then adjusted to ca. 4.6 by addition of a 5 M NaOH solution (30-320 μL, 0.15-1.6 mmol). A final volume of 2 mL was then obtained by addition of deionized water. A 5×8 mm2 poplar section was then immersed in each vial and a time-lapse series of photographs was collected over a period of seven days. The degree of fragmentation decreased with increasing concentration of acetate buffer, with the sample immersed in 2 M acetate buffer remaining intact even after seven days.
Oxidation of wood in Na2CO3 buffer. In a small vial, Mn(OAc)3 (27 mg, 0.10 mmol) and Na2CO3 (106 mg, 1.0 mmol) were dissolved in deionized water (1.5 mL), forming a suspension of pH 9.9. Dropwise addition of H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) resulted in violent bubbling, which subsided after 10-15 minutes. At this time, the pH of the solution was recorded to be 9.6. A 5×8 mm2 poplar section was then immersed in the vial and the reaction monitored over a period of seven days. No fragmentation of the wood was observed.
Oxidation of wood in NaH2PO4 buffer, pH=1.6. In a small vial, Mn(OAc)3 (27 mg, 0.10 mmol) and H3PO4 (0.84 mL, of a 1.2 M aqueous solution, 1.0 mmol) were combined with aqueous NaOH (35 μL of a 5 M aqueous solution, 0.18 mmol). The final volume was adjusted to 1.5 mL by addition of deionized water, and then H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) was added. At this time, the pH of the solution was found to be 1.6. A 5×8 mm2 poplar section was then immersed in the vial and the reaction monitored over a period of seven days. No fragmentation of the wood was observed.
Oxidation of wood in NaH2PO4 buffer, pH=2.5. In a small vial, Mn(OAc)3 (27 mg, 0.10 mmol) and H3PO4 (0.84 mL of a 1.2 M aqueous solution, 1.0 mmol) were combined with aqueous NaOH (134 μL of a 5 M aqueous solution, 0.67 mmol). The final volume was adjusted to 1.5 mL by addition of deionized water, and then H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) was added. At this time, the pH of the solution was found to be 2.5. A 5×8 mm2 poplar section was then immersed in the vial and the reaction monitored over a period of seven days. No fragmentation of the wood was observed.
Oxidation of wood in Na2HPO4 buffer, pH=6.5. In a small vial, Mn(OAc)3 (27 mg, 0.10 mmol) and H3PO4 (0.84 mL of a 1.2 M aqueous solution, 1.0 mmol) were combined with aqueous NaOH (280 μL of a 5 M aqueous solution, 1.4 mmol). The final volume was adjusted to 1.5 mL by addition of deionized water, and then H2O2 (0.5 mL of a 30% aqueous solution, 4.4 mmol) was added, resulting in significant bubbling. At this time, the pH of the solution was found to be 6.5. A 5×8 mm2 poplar section was then immersed in the vial and the reaction monitored over a period of seven days. No fragmentation of the wood was observed.
In conclusion, an aqueous solution of manganese acetate an hydrogen peroxide showed a remarkable activity for the delignification of wood at room temperature. The mild, inexpensive process may be used to facilitate biofuel production by efficient removal of lignin.
Although the present invention has been described with reference to specific details, it is not intended that such details should be regarded as limitations upon the scope of the invention, except as and to the extent that they are included in the accompanying claims. For example, instead of manganese (III) acetate, manganese (II) acetate in an acetate buffered solution has also been shown to decompose lignin from lignocellulosic biomass. Manganese trifluoroacetate and manganese triflate (i.e. trifluorosulfonate) are also expected to decompose lignin from lignocellulosic biomass. Reaction times of a week or less for the decomposition of the lignin are within the scope of this invention.
This invention was made with government support under Contract No. DE-AC52-06NA25396 awarded by the U.S. Department of Energy. The government has certain rights in the invention.
