- Open Access
Yield-determining factors in high-solids enzymatic hydrolysis of lignocellulose
© Kristensen et al.; licensee BioMed Central Ltd. 2009
Received: 12 November 2008
Accepted: 08 June 2009
Published: 08 June 2009
Working at high solids (substrate) concentrations is advantageous in enzymatic conversion of lignocellulosic biomass as it increases product concentrations and plant productivity while lowering energy and water input. However, for a number of lignocellulosic substrates it has been shown that at increasing substrate concentration, the corresponding yield decreases in a fashion which can not be explained by current models and knowledge of enzyme-substrate interactions. This decrease in yield is undesirable as it offsets the advantages of working at high solids levels. The cause of the 'solids effect' has so far remained unknown.
The decreasing conversion at increasing solids concentrations was found to be a generic or intrinsic effect, describing a linear correlation from 5 to 30% initial total solids content (w/w). Insufficient mixing has previously been shown not to be involved in the effect. Hydrolysis experiments with filter paper showed that neither lignin content nor hemicellulose-derived inhibitors appear to be responsible for the decrease in yields. Product inhibition by glucose and in particular cellobiose (and ethanol in simultaneous saccharification and fermentation) at the increased concentrations at high solids loading plays a role but could not completely account for the decreasing conversion. Adsorption of cellulases was found to decrease at increasing solids concentrations. There was a strong correlation between the decreasing adsorption and conversion, indicating that the inhibition of cellulase adsorption to cellulose is causing the decrease in yield.
Inhibition of enzyme adsorption by hydrolysis products appear to be the main cause of the decreasing yields at increasing substrate concentrations in the enzymatic decomposition of cellulosic biomass. In order to facilitate high conversions at high solids concentrations, understanding of the mechanisms involved in high-solids product inhibition and adsorption inhibition must be improved.
Climate changes and shortage of fossil fuels have sparked a growing demand for liquid biofuels which in turn has increased the amount of research into the production of lignocellulose-derived bioethanol [1, 2]. However, being an insoluble and highly heterogeneous substrate, lignocellulosic materials pose several challenges in conversion to fermentable sugars. In addition to understanding complex enzyme system kinetics, these biomass-related challenges include recalcitrance to hydrolysis  and mixing difficulties . Water content in the hydrolysis slurry is directly correlated to rheology, that is, viscosity and shear rate during mixing , important for the interaction between lignocellulose and cell wall-degrading enzymes. Thus, water is not only critical in hydrolysis being a substrate and a prerequisite for enzyme function, but is also crucial for enzyme transport mechanisms throughout hydrolysis as well as mass transfer of intermediates and end-products . Maintaining high substrate concentrations throughout the conversion process from biomass to ethanol is important for the energy balance and economic viability of bioethanol production.
High-solids enzymatic hydrolysis can be defined as taking place at solids levels where initially there are no significant amounts of free liquid water present . By increasing the solids loading, the resulting sugar concentration and consequently ethanol concentration increase, having significant effects on processing costs, in particular distillation [8–10]. Furthermore, lower water content allows for a larger system capacity, less energy for heating and cooling of the slurry and less waste water . Model-based estimations have shown significant reductions of operating costs of simultaneous saccharification and fermentation (SSF) of pretreated softwood when the initial solids concentration was increased . Unfortunately, there are also disadvantages to increasing the substrate concentration. Concentrations of end products and inhibitors will increase, causing enzymes and fermenting organisms to not function optimally. Also, high-solids loadings can cause insufficient mixing, or mixing can be too energy-consuming in conventional stirred-tank reactors as the viscosity of slurries increases abruptly at increasing solids loadings, in particular over 20% solids [11, 12].
In situ native cellulase systems have been reported to function at solids levels as high as 76% (all concentrations are given as total solids on a w/w basis) , indicating that enzymatic hydrolysis may be limited by the laboratory or industrial process set-up. Twelve to fifteen per cent total solids is often considered the upper limit at which pretreated biomass can be mixed and hydrolysed in conventional stirred-tank reactors [7, 14, 15]. However, at the laboratory scale, enzymatic hydrolysis at up to 32% total solids has been reported [12, 16]. A number of studies have utilised fed-batch operations in order to increase the final solids loading [7, 11, 17, 18]. We have previously described a gravimetric mixing reactor design that allows batch enzymatic liquefaction and hydrolysis of pretreated wheat straw at up to 40% solids concentration . This is a significant increase from what has previously been possible, and thus significantly increases the techno-economic potential of the whole process. The gravimetric mixing principle has been up-scaled and used in a pilot plant for several years [19, 20].
Some groups have suggested that the mechanism behind the decreasing conversion is product inhibition [12, 16, 25] or inhibition by other compounds such as sugar-derived inhibitors (furfural and hydroxymethylfurfural (HMF))  and lignin . Others have suggested it may be explained by mass transfer limitations or other effects related to the increased content of insoluble solids, such as non-productive adsorption of enzymes [14, 28]. However, the specific mechanism(s) responsible for the decreasing hydrolytic efficiency are still uncertain [4, 29].
It should be noted that inhibition primarily affects the hydrolysis rate and not the maximum conversion or yield, given sufficient time. With limited reaction times and not fully converted, the conversion will correspond to the inhibition, that is, the conversion being a measure of the 'accumulated' inhibition. Working with initial reaction velocities in high-solids hydrolysis involves great difficulties due to the non-liquid properties of the substrate. For that reason, degree of conversion has been used to estimate the increased inhibition that appears to take place at elevated solids contents.
In this paper the possible mechanisms behind the solids effect have been divided into the following four categories: Compositional and substrate effects; product inhibition; water concentration; and cellulase adsorption. These four topics will be introduced below.
Compositional and substrate effects
The heterogeneity and structure of lignocellulosic biomass means that high viscosity prevents efficient mixing at high solids concentrations when performed in conventional stirred-tank reactors [14, 28, 30]. The viscosity of lignocellulosic slurries increases sharply over a certain threshold (typically around 20% solids) but, despite the extreme difference in viscosity between, for example, 5% and 40% solids loading, the conversion of lignocellulosics as a function of solids appears to be linear (Figure 1). Although mixing of substrate and enzymes is crucial for an efficient liquefaction, our previous findings showed that it does not appear that lack of mixing is the cause of the decreasing conversion, at least not at the solids levels documented . This is in accordance with the recent findings of Hodge and co-workers who concluded that possible mass transfer limitations caused by insoluble solids were not apparent at below 20% insoluble solids content . At very high solids levels (above 20 to 30% dry matter), a mass transfer limitation may be involved in the lower yield, but the linearity of the solids effect over a large range of conditions with a number of substrates (wheat and barley straw [4, 12, 14], corn stover , softwood [22, 24], hardwood [16, 23] and an industrial ethanol fermentation residue (vinasse) ) indicates that a single factor may be responsible for the effect (all the way from, for example, 5% to 40% dry matter).
In order to be able to establish that the solids effect is not caused by lignin adsorption or lignin-derived inhibitors (phenolics), experiments for this paper were carried out with filter paper. Filter paper has the advantage of containing no lignin yet still retains the secondary cell wall structure, as opposed to Sigmacell and Avicel, for example.
End-product inhibition plays an important role in enzymatic hydrolysis as glucose, cellobiose and ethanol have demonstrated their ability to significantly inhibit endoglucanases, cellobiohydrolases and β-glucosidase [31, 32]. However, working with an insoluble substrate and kinetics that do not follow the Michaelis-Menten model, the exact type of inhibition is difficult to determine . The decrease in hydrolysis rate over time has been attributed to inhibition by the accumulated end products . Others conclude that when hydrolysing natural, lignocellulosic substrates, cellulases are more resistant to product inhibition than with amorphous reference materials and that the early stage decrease in hydrolysis rate is not caused by product inhibition [35, 36]. In high-solids enzymatic hydrolysis of pretreated corn stover, Hodge and co-workers recently found that increased sugar concentrations were the primary cause of performance inhibition . Based on the above, we have investigated the inhibitory effect of increased sugar concentration in connection with high-solids enzymatic hydrolysis.
Working with a system with low water content may directly affect enzyme performance. Not only is water a substrate for the hydrolysis but it is also the solvent that allows the function of enzymes, contact between enzymes and substrate and transport of products . We have previously investigated the role of water in enzymatic hydrolysis . In this study, we wanted to investigate if the solids effect was related to a lower concentration of water in relation to solids. As mentioned, hydrolysis is possible at very high solids concentrations but the rate of reaction may be impaired under such conditions .
We have investigated the role of water concentration by replacing various amounts of the water in enzymatic hydrolysis with oleyl alcohol, an inert oil that does not directly affect the function of the enzymes [38, 39].
Cellulose accessibility and degree of adsorption of cellulases are well known as controlling factors for conversion rates and yields [40, 41]. It has long been known that certain hydrolysis products are able to inhibit cellulase adsorption . It has, however, recently been shown that glucose and especially cellobiose strongly inhibit cellulase adsorption in a linear fashion . This adsorption inhibition can be seen as a sub-class of product inhibition where the catalytic site may not necessarily be involved. In order to investigate whether adsorption (or lack thereof) could possibly be involved in the observed solids effect, the adsorption of enzyme was measured in hydrolysis of filter paper at different solids contents.
Results and discussion
Compositional and substrate effects
The filter paper used in the experiments for the present paper contained approximately 15% hemicellulose in the form of 14% mannan and 1% arabinan. However, experiments with hydrolysis of Whatman filter paper (98% cellulose) (not shown) and hydrolysis of α-cellulose also displayed the same trend at increasing solids loadings . As regarding lignin, the fact that a hemicellulose-free substrate exhibits the same trend at increasing solids contents indicates that hemicellulose-derived sugars/inhibitors are not the cause of the solids effect either.
It is worth noting that it is not only the concentration of the inhibitor that is important but the inhibitor-to-enzyme ratio should also be considered. Depending on the difference in concentrations of substrate and enzymes and thus their collision rate, the inhibitor-to-enzyme level can determine the degree of inhibition. Xiao and co-workers showed that in hydrolysis of a cellobiose solution, addition of 20, 50 and 100 g/l of glucose to 2, 5 and 10% cellobiose (w/v) resulted in β-glucosidase inhibition of 53, 51 and 48%, respectively. The almost identical degree of inhibition at different sugar concentrations shows that the inhibitor-to-enzyme ratio is essential in product inhibition . Based on this, it does not appear likely that inhibition of β-glucosidase is the main cause of the solids effect. However, indirectly the cellobiohydrolases are even stronger inhibited by glucose. The high glucose concentration inhibits β-glucosidase, which in turn leads to an accumulation of cellobiose, which acts as a particularly strong inhibitor of cellobiohydrolases .
Surprisingly, cellobiose concentrations in our experiments have generally been low. Normally, even at high solids concentrations and 80% conversion, less than 10% of the converted material is found as cellobiose (data not shown). For comparison, during experiments with lower proportions of β-glucosidase, inhibition caused cellobiose proportions of over 35% of the converted material while still retaining a certain degree of hydrolysis (data not shown).
SSF is normally used to offset the well-known effects of glucose and cellobiose inhibition but interestingly the solids effect has also been observed under those conditions [12, 17, 19]. Ethanol is also known to act as an inhibitor of cellulases (although less severe an inhibitor than cellobiose) [31, 45], indicating that other factors may influence the conversion under these conditions.
In conclusion, product inhibition at increased solids concentrations was found to be a significant and potentially determining factor for the solids effect. However, the linearity over a large range of solids contents of our experiments does not fit with the current models for product inhibition.
Oleyl alcohol has previously been shown to exhibit partitioning behaviour towards water and sugars  and our experiments showed no detrimental effects on enzyme performance (data not shown). Therefore, it was possible to use oleyl alcohol to replace water in order to investigate the water-to-enzyme/solids ratio while keeping the viscosity similar. The reasoning behind these experiments is that by substituting part of the water, it is possible to run a hydrolysis with an altered water-to-enzyme ratio but with a more-or-less constant viscosity of the slurry. If a lack of water is causing the solids effect, then the hydrolysis conversion where a certain amount of the water has been replaced should be lower, presumably at the level of the corresponding solids level (taking only the aqueous phase in consideration).
However, the sugar concentration is not the only parameter that has been changed. Oleyl alcohol may act as a mixing agent, fully or partially replacing the effect of water in assisting mass transfer, even if neither enzymes nor sugars can be solubilised in oleyl alcohol. As previously discussed, the interconnection of factors affecting the yield is characteristic of lignocellulose hydrolysis, complicating the identification of limiting factors.
There is no doubt that water plays a number of important roles in enzymatic hydrolysis, and that these roles become even more crucial in systems with no free water. As cellulases can only break down cellulose when adsorbed onto the material, efficient mass transfer of enzymes is likely to increase conversion. Also, diffusion of released sugars away from the catalytic sites will theoretically prevent local product inhibition. Mechanical stirring may also directly change the size distribution of larger particles. Unfortunately, our understanding of these mechanistic interactions is limited and also depends on the cell wall structure of the substrate. It is likely that such factors affect the degree of conversion at very high solids loadings, essentially causing a drop-off in yield over a certain solids loading. However, as already discussed, the observed solids effect is also seen at loadings as low as 2 to 5% solids and thus mass transfer at neither the macroscopic nor the molecular level appears be responsible for the solids effect.
Related to the diffusion of enzymes is the phenomenon of substrate inhibition, which has previously been described in connection with hydrolysis of cellulose . At increased substrate concentrations, with a fixed enzyme loading, the lateral (two-dimensional) diffusion of bound enzymes is believed to be restricted, thus inhibiting the synergy between exo and endo-enzymes . However, this form of synergistic inhibition relates to a fixed enzyme load where the amount of substrate is increased, that is, a decreasing enzyme-substrate ratio as opposed to a constant ratio as used in our and other's experiments. Therefore, this phenomenon is not likely to be involved in the solids effect. Traditionally, substrate inhibition is explained as a situation where two molecules of substrate bind to the enzyme simultaneously, thereby blocking activity. However, this mechanism is not likely to be applicable to the hydrolysis of cellulose due to its insoluble nature .
In conclusion, water itself as a substrate or diffusing agent in enzymatic hydrolysis does not appear to be the limiting factor responsible for the solids effect, nor is substrate inhibition involved.
Based on an experiment with a fixed cellobiose concentration, Kumar and Wyman argue that binding inhibition can be reversed using high substrate concentrations . However, working with a fixed inhibitor concentration over a range of solids concentrations does not reflect the actual conditions since high solids loadings will invariably lead to higher product concentrations. At any degree of conversion, the ratio between substrate and inhibitor (product) in hydrolysis will be constant no matter the initial solids concentration. Xiao and co-workers also observed reduced impact of products on inhibition at higher solids loadings, but again it was measured against a constant inhibitor concentration . Based on our experiments we do not believe that increased solids concentrations can reverse binding inhibition, rather the opposite.
It can be argued that the phenomenon described above is a variant of product inhibition. In both competitive and non-competitive inhibition the catalytic site is affected, which is not necessarily the case with inhibition of adsorption. Although β-glucosidase does not bind to the substrate and thus is not affected in this way, the binding inhibition of endoglucanases and cellobiohydrolases can possibly explain the low cellobiose levels under conditions where hydrolysis is inhibited.
It is not known to what extent inhibition of adsorption is responsible for the solids effect, or if it can be partially avoided through SSF. It has previously been shown that adsorption inhibition could not explain the decrease in cellulase activity . In an attempt to learn more about the nature of the inhibition, we used the data of the experiment in Figure 2 to investigate the relationship between the rate of reaction and glucose concentration. We found no direct relationship (data not shown), possibly due to the fact that different proportions of the substrate remained, that is, when 50% of the substrate has been converted, the remainder is more difficult to hydrolyse.
It is likely that the cellulose binding domains (CBD) of the cellulases are affected by glucose and cellobiose. Binding of cellulases and clarification of the role of CBDs is an important topic in cellulosic biomass conversion, and has been the topic of numerous studies. Being able to alter the CBD to make it less susceptible to a high concentration of products may contribute to making high yields at high solids concentrations a reality.
The extent of enzymatic conversion of cellulosic biomass was investigated at varying solids concentrations. The conversion decreased at increasing solids concentration in a linear fashion, an effect that appears to be a generic or intrinsic feature of lignocellulose conversion. This decrease partially offsets the significant advantages of working at high solids concentrations. The solids effect did not appear to be caused by lignin content or hemicellulose-derived inhibitors. Lack of mixing of the insoluble substrate did not appear to be causing the effect either.
The increased concentration of glucose and cellobiose at high solids concentration are likely to cause product inhibition even when the enzyme-to-inhibitor ratio is constant. However, the solids effect has also been observed in SSF where much less sugar is present.
It was found that at increasing solids concentrations, the proportion of adsorbed cellulase decreased. There was a statistically significant correlation between this adsorption inhibition and the decreasing yields at increasing substrate concentrations. Thus, the solids effect may well be explained by inhibition of the binding of the cellulases. The exact extent and mechanism of the adsorption inhibition is still unknown. It is possible that improvement of cellulase CBDs may lead to enzymes that are more resistant to high sugar concentrations and thus higher conversions at high solids concentrations, significantly improving the viability of lignocellulosic biomass conversion.
The composition of filter paper (AGF 725, 140 g/m2 from Frisenette ApS, Knebel, Denmark) was analysed using two-step acid hydrolysis according to the procedure published by NREL . Dry matter content was determined using a Sartorius MA 30 moisture analyser at 105°C. The released sugars were quantified by high performance liquid chromatography (HPLC) as described below. The filter paper was found to consist of 80.6% glucan, 0.42% Klason lignin, 14.4% mannan, 1.0% arabinan, and 0.24% ash.
The hydrolyses were performed using an enzyme mixture of Celluclast 1.5 L and Novozym 188 (weight ratio 5:1, both from Novozymes A/S, Bagsværd, Denmark) with a filter paper activity of 75 FPU per gram of dry matter (DM), as measured by the filter paper assay . Enzyme loadings of 5 to 20 FPU per gram of DM and a hydrolysis times from 24 to 84 h were used. Hydrolysis temperature was 50 ± 1°C. Initial total solids content ranged from 5 to 35% (w/w) and pH was kept constant by adding sodium citrate buffer (pH 4.80, 50 mM final concentration).
Hydrolysis experiments were performed at one of two scales. The 'large' scale hydrolyses were done in a horizontal, five-chambered liquefaction reactor where each chamber is 20 cm wide and 60 cm in diameter as described in . In this reactor, a total reaction mass (solids and liquids) of 5 kg was used. The rotational speed was approximately 6 rpm.
The 'small' scale hydrolysis was performed in 100 ml plastic bottles (total reaction mass 50 g), also at 5 to 25% solids content (w/w); buffer concentration and enzyme loadings as described above. The bottles were placed in a heated, horizontally placed drum, rotating at 60 rpm. The 80 cm diameter drum was equipped with two inside paddles that lifted and dropped the plastic bottles during rotation, mimicking the gravimetric mixing described in [4, 20]. All small-scale experiments were performed in either duplicate or triplicate.
Samples for HPLC sugar analysis were boiled for 10 min to terminate the reaction. Whole slurry was sampled after vigorous shaking to ensure a representable mixture of solids and liquid. Samples were then diluted five to tenfold with eluent before insoluble material was removed by centrifugation at 4,200 × g for 10 min. The dilution factor was determined by measuring the weight of the sample before and after dilution. When working at high insoluble solids concentrations there is an increasing difference between the concentration in the liquid phase and the overall concentration of a component . The dilution step minimises the measurement error introduced by the content of insoluble material, which would otherwise result in an overestimation when calculating the conversion, as discussed in .
The content of monosaccharides in the hydrolysed samples (D-glucose, D-xylose, L-arabinose and D-cellobiose) was quantified on a Dionex Summit HPLC system equipped with a Shimadzu RI-detector. The separation was performed in a Phenomenex Rezex RHM column at 80°C with 5 mM H2SO4 as eluent at a flow rate of 0.6 ml min-1. Samples were filtered through a 0.45 μm filter and diluted with eluent before analysis on HPLC.
Before hydrolysis, various amounts of D-glucose (Sigma-Aldrich, Brøndby, Denmark) were added to the substrate. Conditions were as described above.
Water replacement experiments
Hydrolysis was run at 'large' scale, as described above, with 20% solids content (w/w) and an enzyme loading of 10 FPU (g DM)-1. Twenty-five per cent (w/w) of the initial aqueous phase was substituted with oleyl alcohol. It was found that neither the enzyme nor the released sugars was present in the oleyl alcohol. Sugar concentration was measured in the aqueous phase only.
For cellulase adsorption studies, samples were kept on ice after hydrolysis instead of boiling, in order to prevent any desorption of enzyme from the solids. Rather than estimating the adsorption indirectly with a colorimetric method, total nitrogen content of the biomass was determined on an elemental analyser coupled to an isotope ratio mass spectrometer (ANCA SL & 20–20, Europa Scientific, Crewe, UK). This method of measuring enzyme adsorption has recently been described by Kumar and Wyman . As the cellulase mixture of Celluclast 1.5 L and Novozym 188 contains a proportion of non-binding enzymes, enzyme adsorption will never reach 100% of the added amount. To be able to subtract the nitrogen content of the liquid of the spun-down samples, the nitrogen content of the aqueous phase was measured with the Kjeldahl method.
The project is financially supported by the Danish Research Agency contract 2104-05-0008.
- Gray KA, Zhao L, Emptage M: Bioethanol. Curr Opin Chem Biol 2006, 10: 141-146. 10.1016/j.cbpa.2006.02.035View ArticleGoogle Scholar
- Jørgensen H, Kristensen JB, Felby C: Enzymatic conversion of lignocellulose into fermentable sugars: challenges and opportunities. Biofpr 2007, 1: 119-134.Google Scholar
- Himmel ME, Ding SY, Johnson DK, Adney WS, Nimlos MR, Brady JW, Foust TD: Biomass recalcitrance: Engineering plants and enzymes for biofuels production. Science 2007, 315: 804-807. 10.1126/science.1137016View ArticleGoogle Scholar
- Jørgensen H, Vibe-Pedersen J, Larsen J, Felby C: Liquefaction of lignocellulose at high solids concentrations. Biotechnol Bioeng 2007, 96: 862-870. 10.1002/bbb.4View ArticleGoogle Scholar
- Pimenova NV, Hanley AR: Effect of corn stover concentration on rheological characteristics. Appl Biochem Biotechnol 2004, 113–16: 347-360. 10.1385/ABAB:114:1-3:347View ArticleGoogle Scholar
- Felby C, Thygesen LG, Kristensen JB, Jørgensen H, Elder T: Cellulose-water interactions during enzymatic hydrolysis as studied by time domain NMR. Cellulose 2008, 15: 703-710. 10.1007/s10570-008-9222-8View ArticleGoogle Scholar
- Hodge DB, Karim MN, Schell DJ, McMillan JD: Model-Based Fed-Batch for High-Solids Enzymatic Cellulose Hydrolysis. Appl Biochem Biotechnol 2009, 152: 88-107. 10.1007/s12010-008-8217-0View ArticleGoogle Scholar
- Wingren A, Galbe M, Zacchi G: Techno-economic evaluation of producing ethanol from softwood: Comparison of SSF and SHF and identification of bottlenecks. Biotechnol Prog 2003, 19: 1109-1117. 10.1021/bp0340180View ArticleGoogle Scholar
- Katzen R, Madson PW, Moon GD: Alcohol destillation – the fundamentals. In The Alcohol Textbook. Edited by: Jacques KA, Lyons TP, Kelsall DR. Nottingham: Nottingham University Press; 1999:103-125.Google Scholar
- Zacchi G, Axelsson A: Economic-Evaluation of Preconcentration in Production of Ethanol from Dilute Sugar Solutions. Biotechnol Bioeng 1989, 34: 223-233. 10.1002/bit.260340211View ArticleGoogle Scholar
- Fan ZL, South C, Lyford K, Munsie J, van Walsum P, Lynd LR: Conversion of paper sludge to ethanol in a semicontinuous solids-fed reactor. Bioprocess Biosyst Eng 2003, 26: 93-101. 10.1007/s00449-003-0337-xView ArticleGoogle Scholar
- Mohagheghi A, Tucker M, Grohmann K, Wyman C: High Solids Simultaneous Saccharification and Fermentation of Pretreated Wheat Straw to Ethanol. Appl Biochem Biotechnol 1992, 33: 67-81. 10.1007/BF02950778View ArticleGoogle Scholar
- Mandels M, Reese ET: Inhibition of Cellulases. Annu Rev Phytopathol 1965, 3: 85-102. 10.1146/annurev.py.03.090165.000505View ArticleGoogle Scholar
- Rosgaard L, Andric P, Dam-Johansen K, Pedersen S, Meyer AS: Effects of substrate loading on enzymatic hydrolysis and viscosity of pretreated barley straw. Appl Biochem Biotechnol 2007, 143: 27-40. 10.1007/s12010-007-0028-1View ArticleGoogle Scholar
- Tolan JS: Iogen's process for producing ethanol from cellulosic biomass. Clean Technol Environ Policy 2002, 3: 339-345. 10.1007/s10098-001-0131-xView ArticleGoogle Scholar
- Cara C, Moya M, Ballesteros I, Negro MJ, Gonzalez A, Ruiz E: Influence of solid loading on enzymatic hydrolysis of steam exploded or liquid hot water pretreated olive tree biomass. Process Biochem 2007, 42: 1003-1009. 10.1016/j.procbio.2007.03.012View ArticleGoogle Scholar
- Varga E, Klinke HB, Reczey K, Thomsen AB: High solid simultaneous saccharification and fermentation of wet oxidized corn stover to ethanol. Biotechnol Bioeng 2004, 88: 567-574. 10.1002/bit.20222View ArticleGoogle Scholar
- Ballesteros M, Oliva JM, Manzanares P, Negro MJ, Ballesteros I: Ethanol production from paper material using a simultaneous saccharification and fermentation system in a fed-batch basis. World J Microbiol Biotechnol 2002, 18: 559-561. 10.1023/A:1016378326762View ArticleGoogle Scholar
- Thomsen MH, Thygesen A, Jørgensen H, Larsen J, Christensen BH, Thomsen AB: Preliminary results on optimisation of pilot scale pre-treatment of wheat straw used in co-production of bioethanol and electricity. Appl Biochem Biotechnol 2006, 129–132: 448-460.Google Scholar
- Larsen J, Petersen MØ, Thirup L, Li HW, Iversen FK: The IBUS process – Lignocellulosic Bioethanol Close to a Commercial Reality. Chem Eng Technol 2008, 31: 765-772. 10.1002/ceat.200800048View ArticleGoogle Scholar
- Ingesson H, Zacchi G, Yang B, Esteghlalian AR, Saddler JN: The effect of shaking regime on the rate and extent of enzymatic hydrolysis of cellulose. J Biotechnol 2001, 88: 177-182. 10.1016/S0168-1656(01)00273-5View ArticleGoogle Scholar
- Lu YP, Yang B, Gregg D, Saddler JN, Mansfield SD: Cellulase adsorption and an evaluation of enzyme recycle during hydrolysis of steam-exploded softwood residues. Appl Biochem Biotechnol 2002, 98: 641-654. 10.1385/ABAB:98-100:1-9:641View ArticleGoogle Scholar
- Schwald W, Breuil C, Brownell HH, Chan M, Saddler JN: Assessment of Pretreatment Conditions to Obtain Fast Complete Hydrolysis on High Substrate Concentrations. Appl Biochem Biotechnol 1989, 20–1: 29-44. 10.1007/BF02936471View ArticleGoogle Scholar
- Tengborg C, Galbe M, Zacchi G: Influence of enzyme loading and physical parameters on the enzymatic hydrolysis of steam-pretreated softwood. Biotechnol Prog 2001, 17: 110-117.View ArticleGoogle Scholar
- Hodge DB, Karim MN, Schell DJ, McMillan JD: Soluble and insoluble solids contributions to high-solids enzymatic hydrolysis of lignocellulose. Bioresour Technol 2008, 99: 8940-8948. 10.1016/j.biortech.2008.05.015View ArticleGoogle Scholar
- Panagiotou G, Olsson L: Effect of compounds released during pretreatment of wheat straw on microbial growth and enzymatic hydrolysis rates. Biotechnol Bioeng 2007, 96: 250-258. 10.1002/bit.21100View ArticleGoogle Scholar
- Pan XJ: Role of functional groups in lignin inhibition of enzymatic hydrolysis of cellulose to glucose. J Biobased Mater Bioenergy 2008, 2: 25-32. 10.1166/jbmb.2008.005View ArticleGoogle Scholar
- Sørensen I, Pedersen S, Meyer AS: Optimization of reaction conditions for enzymatic viscosity reduction and hydrolysis of wheat arabinoxylan in an industrial ethanol fermentation residue. Biotechnol Prog 2006, 22: 505-513. 10.1021/bp050396oView ArticleGoogle Scholar
- Rosgaard L, Pedersen S, Cherry JR, Harris P, Meyer AS: Efficiency of new fungal cellulase systems in boosting enzymatic degradation of barley straw lignocellulose. Biotechnol Prog 2006, 22: 493-498. 10.1021/bp050361oView ArticleGoogle Scholar
- Georgieva TI, Hou XR, Hilstrom T, Ahring BK: Enzymatic hydrolysis and ethanol fermentation of high dry matter wet-exploded wheat straw at low enzyme loading. Appl Biochem Biotechnol 2008, 148: 35-44. 10.1007/s12010-007-8085-zView ArticleGoogle Scholar
- Bezerra RMF, Dias AA: Enzymatic kinetic of cellulose hydrolysis – Inhibition by ethanol and cellobiose. Appl Biochem Biotechnol 2005, 126: 49-59. 10.1007/s12010-005-0005-5View ArticleGoogle Scholar
- Xiao ZZ, Zhang X, Gregg DJ, Saddler JN: Effects of sugar inhibition on cellulases and beta-glucosidase during enzymatic hydrolysis of softwood substrates. Appl Biochem Biotechnol 2004, 113–16: 1115-1126. 10.1385/ABAB:115:1-3:1115View ArticleGoogle Scholar
- Gruno M, Valjamae P, Pettersson G, Johansson G: Inhibition of the Trichoderma reesei cellulases by cellobiose is strongly dependent on the nature of the substrate. Biotechnol Bioeng 2004, 86: 503-511. 10.1002/bit.10838View ArticleGoogle Scholar
- Holtzapple M, Cognata M, Shu Y, Hendrickson C: Inhibition of Trichoderma-Reesei Cellulase by Sugars and Solvents. Biotechnol Bioeng 1990, 36: 275-287. 10.1002/bit.260360310View ArticleGoogle Scholar
- Zhang S, Wolfgang DE, Wilson DB: Substrate heterogeneity causes the nonlinear kinetics of insoluble cellulose hydrolysis. Biotechnol Bioeng 1999, 66: 35-41.View ArticleGoogle Scholar
- Väljamäe P, Kipper K, Pettersson G, Johansson G: Synergistic cellulose hydrolysis can be described in terms of fractal-like kinetics. Biotechnol Bioeng 2003, 84: 254-257. 10.1002/bit.10775View ArticleGoogle Scholar
- Zaccai G: The effect of water on protein dynamics. Philos Trans R Soc Lond B Biol Sci 2004, 359: 1269-1275. 10.1098/rstb.2004.1503View ArticleGoogle Scholar
- Bruce LJ, Daugulis AJ: Solvent selection-strategies for extractive biocatalysis. Biotechnol Prog 1991, 7: 116-124. 10.1021/bp00008a006View ArticleGoogle Scholar
- Moritz JW, Duff SJB: Simultaneous saccharification and extractive fermentation of cellulosic substrates. Biotechnol Bioeng 1996, 49: 504-511.View ArticleGoogle Scholar
- Jeoh T, Ishizawa CI, Davis MF, Himmel ME, Adney WS, Johnson DK: Cellulase digestibility of pretreated biomass is limited by cellulose accessibility. Biotechnol Bioeng 2007, 98: 112-122. 10.1002/bit.21408View ArticleGoogle Scholar
- Tanaka M, Nakamura H, Taniguchi M, Morita T, Matsuno R, Kamikubo T: Elucidation of Adsorption Processes of Cellulases During Hydrolysis of Crystalline Cellulose. Appl Microbiol Biotechnol 1986, 23: 263-268. 10.1007/BF00261926Google Scholar
- Stutzenberger F, Lintz G: Hydrolysis Products Inhibit Adsorption of Trichoderma-Reesei C30 Cellulases to Protein-Extracted Lucerne Fibers. Enzyme Microb Technol 1986, 8: 341-344. 10.1016/0141-0229(86)90132-8View ArticleGoogle Scholar
- Kumar R, Wyman CE: An improved method to directly estimate cellulase adsorption on biomass solids. Enzyme Microb Technol 2008, 42: 426-433. 10.1016/j.enzmictec.2007.12.005View ArticleGoogle Scholar
- Kristensen JB, Felby C, Jørgensen H: Determining yields in high solids enzymatic hydrolysis of biomass. Appl Biochem Biotechnol 2009, 156: 127-32. 10.1007/s12010-008-8375-0View ArticleGoogle Scholar
- Ooshima H, Ishitani Y, Harano Y: Simultaneous saccharification and fermentation of cellulose: Effect of ethanol on enzymatic saccharification of cellulose. Biotechnol Bioeng 1985, 27: 389-397. 10.1002/bit.260270402View ArticleGoogle Scholar
- Väljamäe P, Pettersson G, Johansson G: Mechanism of substrate inhibition in cellulose synergistic degradation. Eur J Biochem 2001, 268: 4520-4526. 10.1046/j.1432-1327.2001.02377.xView ArticleGoogle Scholar
- Fenske JJ, Penner MH, Bolte JP: A simple individual-based model of insoluble polysaccharide hydrolysis: the potential for autosynergism with dual-activity glycosidases. J Theor Biol 1999, 199: 113-118. 10.1006/jtbi.1999.0938View ArticleGoogle Scholar
- Huang XL, Penner MH: Apparent substrate inhibition of the Trichoderma reesei cellulase system. J Agric Food Chem 1991, 39: 2096-2100. 10.1021/jf00011a042View ArticleGoogle Scholar
- Oh KK, Kim SW, Jeong YS, Hong SI: Bioconversion of cellulose into ethanol by nonisothermal simultaneous saccharification and fermentation. Appl Biochem Biotechnol 2000, 89: 15-30. 10.1385/ABAB:89:1:15View ArticleGoogle Scholar
- Sluiter A: Determination of structural carbohydrates and lignin in biomass. NREL Laboratory Analytical Procedures. National Renewable Energy Laboratory, Golden, CO, USA; 2004.Google Scholar
- Wood T, Bhat KM: Methods for measuring cellulase activities. In Biomass – Part A: Cellulose and hemicellulose. San Diego: Academic Press; 1988:87-112.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an open access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.