Inhibition of growth of Zymomonas mobilis by model compounds found in lignocellulosic hydrolysates
© Franden et al.; licensee BioMed Central Ltd. 2013
Received: 15 March 2013
Accepted: 24 June 2013
Published: 9 July 2013
During the pretreatment of biomass feedstocks and subsequent conditioning prior to saccharification, many toxic compounds are produced or introduced which inhibit microbial growth and in many cases, production of ethanol. An understanding of the toxic effects of compounds found in hydrolysate is critical to improving sugar utilization and ethanol yields in the fermentation process. In this study, we established a useful tool for surveying hydrolysate toxicity by measuring growth rates in the presence of toxic compounds, and examined the effects of selected model inhibitors of aldehydes, organic and inorganic acids (along with various cations), and alcohols on growth of Zymomonas mobilis 8b (a ZM4 derivative) using glucose or xylose as the carbon source.
Toxicity strongly correlated to hydrophobicity in Z. mobilis, which has been observed in Escherichia coli and Saccharomyces cerevisiae for aldehydes and with some exceptions, organic acids. We observed Z. mobilis 8b to be more tolerant to organic acids than previously reported, although the carbon source and growth conditions play a role in tolerance. Growth in xylose was profoundly inhibited by monocarboxylic organic acids compared to growth in glucose, whereas dicarboxylic acids demonstrated little or no effects on growth rate in either substrate. Furthermore, cations can be ranked in order of their toxicity, Ca++ > > Na+ > NH4+ > K+. HMF (5-hydroxymethylfurfural), furfural and acetate, which were observed to contribute to inhibition of Z. mobilis growth in dilute acid pretreated corn stover hydrolysate, do not interact in a synergistic manner in combination. We provide further evidence that Z. mobilis 8b is capable of converting the aldehydes furfural, vanillin, 4-hydroxybenzaldehyde and to some extent syringaldehyde to their alcohol forms (furfuryl, vanillyl, 4-hydroxybenzyl and syringyl alcohol) during fermentation.
Several key findings in this report provide a mechanism for predicting toxic contributions of inhibitory components of hydrolysate and provide guidance for potential process development, along with potential future strain improvement and tolerance strategies.
KeywordsZymomonas mobilis High-throughput screening Cell growth assay Bioscreen C Inhibitor Hydrolysate Lignocellulosic biomass Ethanol
From a process economic consideration, two of the biggest challenges for a cost competitive cellulosic ethanol operation involve achieving high sugar yields from the hydrolysis of cellulose and hemicellulose in the pretreatment and enzymatic saccharification steps and subsequent fermentation of those sugars to ethanol at high yields. Pretreatment processes are designed to break down the cellulose, hemicellulose and lignin matrix, releasing monosaccharides and providing access of polysaccharides for enzymatic conversion and they often result in the introduction of toxic compounds which are also inhibitory to microbial fermentations [1–6], and so the two challenges have appeared to be mutually exclusive.
Inhibitors fall into several categories: furans, phenols, carboxylic and inorganic acids, aldehydes and alcohols [6–8]. Organic acids (primarily acetic acid) are released from the deacetylation of xylan and lignin breakdown during pretreatment [1, 9]. The furans, HMF and furfural, result from the degradation of hexose and pentoses, respectively. Other degradation products include formic, 2-furoic, and levulinic acids. Phenols identified in lignocellulosics include acids, alcohols, aldehydes and ketones . The extent of inhibitor formation is often a function of pretreatment severity, a combined factor that includes reaction time, temperature, and catalyst concentration. More severe pretreatment conditions generally produce pretreated solids that are easily saccharified by enzymes, but such conditions often cause greater sugar degradation losses and require costly detoxification steps, often referred to as conditioning.
Most of the published work focusing on mitigating the negative influence of inhibitors in hydrolysates has relied on chemical, physical or biological methods for their removal or abatement. These methods include overliming, ion-exchange chromatography, the use of polymeric sorbents, or treatments with enzymes or microorganisms . A more systematic approach to this problem would involve the identification and potency of inhibitors, understanding the basis of their formation, and identifying alternative pretreatment conditions and/or techniques to prevent their production. The efficacy of conditioning treatments can be determined by benchmarking the fermentation of the conditioned hydrolysate to a control, consisting of a reference medium supplemented with pure sugars. While these assessments provide guidance, they provide little information about the type and quantity of the inhibitors removed and the potential synergistic effects between various inhibitory components that may be present.
Because of the many variables reported for hydrolysate toxicity measurements, such as fermentation organisms, inoculum levels, fermentation conditions, biomass feedstocks, and pretreatment conditions [11–14], it is difficult to interpret published data and properly evaluate the toxic nature of hydrolysates. The contribution of individual compounds to the overall toxic level and the underlying toxicity mechanisms are not well understood at the level required for optimization of the pretreatment conditions or effectively engineering tolerant strains. Some work has been conducted analyzing the inhibitory effects of model compounds in Z. mobilis, E. coli, S. cerevisiae, etc. [4, 5, 13, 15–18]. For example, the recombinant strain E. coli LY01 was tested for growth and ethanol production inhibitions by a wide range of aldehydes, acids, and alcohols [16–18]. In these works, inhibitory activity was closely related to hydrophobicity. Aldehydes tended to be more toxic than acids, which were more toxic than alcohols.
Little is known of the toxic effects of inhibitory compounds on Z. mobilis growth and fermentation, although some preliminary studies have evaluated the effects of furans, aldehydes in glucose with a wild-type Z. mobilis ATCC 10988 and with a recombinant plasmid-bearing strain Z. mobilis CP4/pZB5 . Z. mobilis ZM4 has been shown to be more robust in its enhanced sugar utilization rates and tolerance to ethanol [14, 19]. Z. mobilis 8b, a recombinant xylose utilizing strain derived from ZM4 , was shown to have improved tolerance to acetic acid . Nevertheless, the toxic effects on Z. mobilis cell growth by hydrolysates or inhibitors have not been investigated systematically. To this end, we developed a quantitative, high-throughput biological growth assay using an automated turbidometer to obtain detailed inhibitory kinetic data for individual compounds . Growth is widely used to evaluate the toxicity of various inhibitor compounds on microbial fermentation and is associated with ethanol production by recombinant S. cerevisiae, E. coli and Z. mobilis. Inhibition of cell growth has been shown to be strongly correlated with inhibition of ethanol production for many inhibitory compounds [4, 5, 16, 17, 23, 24].
In this study, we examined model inhibitor compounds that include five aldehydes, fourteen organic acids and two alcohols, for their effect on growth rates as well as final cell mass using either glucose or xylose as the substrate. Since, inorganic salts can also be introduced during the acid or alkali pretreatment processes and subsequent neutralization or conditioning steps preceding saccharification, we also compared four cations and four inorganic anions for their inhibitory potential as well. We further investigated synergistic potentials of HMF, furfural, acetate and formate. Furfural was found to inhibit growth and fermentation synergistically with phenols in E. coli[16–18] and with acetic acid in S. cerevisiae.
Results and discussion
We previously reported a method for examining growth inhibition with individual compounds as well as hydrolysate using a high throughput assay and described the inhibition on growth and final cell densities of Z. mobilis by four compounds: acetate, ethanol, HMF and furfural . We continued to use this method for a more detailed analysis of the effect of compounds that are either produced or introduced as a result of the pretreatment and conditioning steps. This was done in order to determine the relative toxicity among the inhibitors and provide guidance for improvements in both biomass processing steps or in the robustness of the ethanologen.
Effect of inhibitors on growth of Z. mobilis in glucose
Hydrophobicity values (logP octanol/water coefficients), millimolar inhibitory concentrations (IC 25 , IC 50 , IC 75 and IC 100 ) for growth rate inhibitions by 25%, 50%, 75% and 100%, respectively in glucose and xylose
Organic acids 9
Vanillic acid 10
4-Hydroxybenzoic acid 10
4-Hydroxycinnamic acid 11 (ρ-Coumaric acid)
Caproic (Hexanoic) acid
Inorganic acids 9
Each compound elicited a distinct growth rate inhibition profile which is either sigmoidal or hyperbolic in shape. Lactic acid, which is sometimes introduced by contamination of lactic acid bacteria in biomass fermentations, is tolerated by Z. mobilis up to 500-600 mM (Figure 1A). Levulinic, succinic, acetic, itaconic and 2-furoic share similar minimum inhibitory concentrations (MIC) of 300-475 mM (Figure 1A and B). MIC is defined as the lowest concentration of inhibitor that completely inhibits growth within a 24 hour period. However, at concentrations below 100 mM, succinic and itaconic were less inhibitory than acetic, levulinic and 2-furoic acids. Due to low solubilities of vanillic, 4-hydroxybenzoic, and 4-hydroxycinnamic (ρ-coumaric) acids, concentrations causing more than 50% inhibition were not tested; therefore MICs were extrapolated from the inhibition curves (Figure 1C and D). Caproic (hexanoic) acid was most inhibitory at concentrations as low as 34 mM, followed by 4-hydroxycinnamic, oxalic, 4-hydroxybenzoic, vanilic, ferulic, formic, 2-furoic, itaconic, succinic, acetic, levulinic and lactic acid. Oxalic acid is not recognized as a component of lignocellulosic hydrolysate but was included in this study because it has been used or considered for some pretreatment processes .
Of the inorganic salts studied, ammonium chloride is the least toxic and ammonium nitrate is the most toxic. Ammonium phosphate is slightly less toxic than ammonium sulfate (Figure 1E). Sulfuric and phosphoric acid are divalent and trivalent, respectively, and would contain additional ammonium ions increasing its ionic strength as well as the osmolarity of the medium. Sulfuric acid is often used in dilute acid pretreatment processes and ammonium sulfate at concentrations above 300 mM (~40 g/L) completely inhibits Z. mobilis growth.
The aldehydes were far more toxic than the organic acids used in this study with the exception of caproic acid. The most toxic aldehyde was vanillin, followed by 4-hydroxybenzaldehyde, syringaldehyde, furfural and HMF (Figure 1F). Furfuryl alcohol was examined in this study as it has been shown to be a product of furfural conversion in Z. mobilis (Additional file 1: Figure S1A and Additional file 2: Figure S2C) and is approximately one fourth as inhibitory as furfural (Figure 1C).
Relationship of compound hydrophobicity to growth of Z. mobilis
Hydrophilic organic acids tended to be less inhibitory than the hydrophobic ones, though some compounds with negative logP values did not follow this trend. Although oxalic acid, a dicarboxylic acid with pKa values of 1.3 and 4.3) is very hydrophilic, it was extremely toxic to Z. mobilis. Oxalic acid has been used as a catalyst for pretreatment of biomass . It is a very strong acid and forms insoluble precipitates with many metal ions, including magnesium, which is essential for many important enzymes (pyrophosphatase, pyruvate kinase, enolase, membrane ATPase, and others) [27–30]. Lactic, levulinic, acetic, succinic and formic acids have similar partition coefficients yet vary significantly in their inhibitory level. Formic acid, a degradation product of HMF and furfural, is also very toxic to Z. mobilis and has also been observed to be toxic to E. coli. . It has been proposed that its higher toxicity may be a result of its high permeability through the cell membrane [31, 32]. Compounds with lower hydrophobicity (i.e. when logP(octanol/water) < 1) generally had lower toxicity. Other less inhibitory organic acids included lactic acid, followed by levulinic and acetic acid.
Relationship of growth rates to final cell densities
Growth rates for selected compounds at varied concentrations are plotted with the relative growth yield taken after 24 hours (Additional file 3: Figure S3). The relative growth yield is the ratio of the maximum cell density +/- inhibitor, correcting values for non-linear response . Results for growth rates and final cell densities for acetate, HMF, furfural and ethanol were reported previously . All of the compounds tested caused a decrease in final cell densities, but displayed different inhibitory profiles. Only representative compounds are shown (Additional file 3: Figure S3). Formic (Additional file 3: Figure S3A), caproic, and benzoic acid as well as syringaldehyde caused significant reductions in final cell mass relative to the reduction in growth rates. This is similar to the pattern observed with acetic acid . For most of the other acids and alcohols as well as 4-hydroxybenzaldehyde and vanillin, final cell density was reduced to a level consistent with the decrease in growth rates for increasing concentrations of inhibitor as shown for itaconic acid in Additional file 3: Figure S3B. On the other hand, whereas growth rates in HMF were reduced, cell mass at the end of fermentation (24 hours) was not affected until concentrations exceeded 12 mM (1.5 g/L)  and then the reduction in growth rates for increasing inhibitor concentrations exceeded the reduction in cell density. This signified that the compounds did not affect the stoichiometry of the conversion of substrates into cellular material, only the conversion rate. Similarly, growth rates in furfural were more affected than final cell density . Other compounds showing a similar pattern include: 4-hydroxycinnamic acid, 4-hydroxybenzoic acid (Additional file 3: Figure S3C), and vanillic acid and possibly ferulic acid.
For the inorganic acids, relative final cell densities were proportional to growth rates, with the possible exception of sulfate, which did not reduce final cell mass even when growth rates were reduced (Additional file 3: Figure S3D).
Growth inhibition and carbon source
pK a values of compounds and relative toxicities for glucose and xylose were calculated by dividing the mean of inhibitor concentrations at IC 25 , IC 50 , IC 75 and IC 100 when grown in glucose divided by the mean inhibitor concentration at respective IC when grown in xylose
Average ratio of IC in RMG/IC in RMX
4.5 +/- 0.5
4.1 +/- 1.3
3.7 +/- 0.4
3.2 +/- 0.8
Caproic (Hexanoic) acid
2.2 +/- 0.4
1.9 +/- 0.4
1.9 +/- 0.4
1.4 +/- 0.1
1.4 +/- 0.1
1.3 +/- 0.2
1.1 +/- 0.06
0.9 +/- 0.1
1.0 +/- 0.2
0.9 +/- 0.04
0.8 +/- 0.2
0.7 +/- 0.1
0.6 +/- 0.1
1.1 +/- 0.1
1.0 +/- 0.1
0.8 +/- 0.1
0.9 +/- 0.1
1.5 +/- 0.4
1.6 +/- 0.1
1.0 +/- 0.1
1.0 +/- 0.1
The mechanism of toxicity for weak acids for bacteria and yeast is shown to be due to the passage of the protonated form of the acid, which is highly permeable, through the cell membrane [33–35]. Cells lose energy if the acid is deprotonated in the higher pH of the cytoplasm (loss of protonmotive force) or if the acid is actively pumped out of the cell. The intracellular pH for Z. mobilis has been reported to be between 5.4- 5.6 in pH 5 medium in Z. mobilis 113  and 6.2-5.3 for Z. mobilis CP4 during batch fermentation . This is above the pKa for the weak monocarboxylic acids evaluated in this study thus allowing for the disassociation of acid within the cell, resulted in a subsequent drop in internal pH and disruption of the transmembrane potential. Dicarboxylic acids with pKa values above and below physiological pH are expected to be partially protonated and therefore less toxic due to lower permeability through the cell membrane. The observation that monocarboxylic acids were more inhibitory in xylose-grown cells than in glucose-grown cells was unexpected. The increased inhibitory action of monocarboxylic acids on xylose growth may possibly be the result of an already reduced energy state from inefficient xylose metabolism compounded by further disruption of the transmembrane potential, although further investigation is needed to support this hypothesis.
Cation effect on inhibitor toxicity
We also examined the inhibitory profiles for four inorganic acids and two organic acids (sulfate, chloride, phosphate, nitrate, acetate and formate) using different cations, in order to determine what contribution cations have in hydrolysate toxicity. Both ammonia and calcium have been used in neutralization and conditioning steps following pretreatment and prior to saccharification and were examined along with potassium and sodium. Calcium sulfate and phosphate were not tested due to their low solubilities.
The examination of inorganic acids arose from the need to understand the contribution of salts towards hydrolysate toxicity that are introduced during pretreatment and subsequent neutralization/conditioning steps. Approximately, 250 to 400 mM of the anions (chloride, sulfate, nitrate and phosphate) caused complete inhibition of growth. An analysis of some dilute acid corn stover pretreated material conditioned with ammonium hydroxide used in a previous report  revealed concentrations of sulfate up to 200 mM would cause approximately 75% growth inhibition by itself without additional inhibitors. Lower acid pretreatment conditions reduce the introduction of inorganic salts and can benefit ethanologen growth and fermentation (unpublished results) though the lower severity pretreatment can have a negative impact on cellulose and hemicellulose hydrolysis.
In our analysis of cations, we discovered calcium to be the most toxic, followed by sodium, ammonium and potassium. Calcium overliming has been shown to provide advantages at least in part through the reduction in the levels of sulfate, HMF and furfural as well as other phenolics, but at the same time introduces new inhibitors, especially calcium ions that are particularly inhibitory in Z. mobilis, when paired with acetate or formate. Calcium’s role in toxicity may arise from its ability to form a wide variety of complexes in biological systems and compete directly with magnesium for many important enzymes [27–30]. Calcium toxicity may explain why Z. mobilis performs better in ammonium conditioned hydrolysates rather than in calcium overlimed hydrolysates .
Effect of combined acetate, formate, HMF and furfural on Z. mobilis growth in glucose and xylose
We investigated inhibitory synergism among four compounds (HMF, furfural, acetate and formate), chosen because of their inhibitory potential and concentration in acid pretreated corn stover hydrolysate. We performed a two-level, four-factor factorial design using growth rate as the response factor and used concentrations of inhibitors which would cause 20% inhibition for each based on glucose substrate (10 mM HMF, 5 mM furfural, 125 mM acetate and 50 mM formate). Two center points were included containing half the concentrations above combining all the inhibitors.
Combinations of HMF, furfural and acetate resulted in additive rather than synergistic inhibition. These results differ from published results using E. coli in which furfural and HMF were shown to act synergistically with a number of compounds [4, 17]. In S. cerevisiae strain 259ST, however, furfural, ethanol and acetate combinations were found to have additive inhibition to growth but synergistic inhibition for ethanol production . Further investigation is needed to determine whether ethanol production is synergistically inhibited in Z. mobilis by these compounds and whether some of the other compounds act synergistically to inhibit growth and/or ethanol production.
Aldehyde conversion by Z. mobilis
Fermentation performance by Z. mobilis 8b in glucose and xylose in the presence of inhibitors at 1X MIC
Complete inhibition of growth does not necessarily reflect cell death nor inhibition of fermentation, particularly with more concentrated inocula. To investigate whether ethanol could still be produced at inhibitor concentrations that prevent growth, we conducted small scale fermentation experiments (4 mL) in the presence of either 5% glucose or 5% xylose over a 24 or 48 hour period for glucose and xylose, respectively.
When xylose is used in place of glucose as the substrate, growth rates and final cell mass are significantly reduced [21, 22, 39]. Even with no inhibitors present, Z. mobilis 8b was only able to reach a final cell density of ~ 2.7, less than one half of the cell density achieved from glucose cultures. Approximately 97% of the available xylose was consumed and produced 83% of theoretical ethanol yields. Ethanol yields were lower than typically observed in pH controlled fermentations which could be attributed to the lack of pH control. Although some inhibitors caused uncoupled ethanol production from growth in glucose, all compounds that completely inhibited growth in xylose also inhibited ethanol production. Some growth was evident in the presence of 4-hydroxybenzoic and 4-hydroxycinnamic acid from 48 to 72 hours following an initial lag with concomitant ethanol production. None of the other cultures exhibited a similar lag of growth or fermentation.
In mini-fermentations, Z. mobilis 8b was able to grow and produce ethanol at 1X MIC in the remaining compounds (ferulic, furoic, vanillic, 4-hydroxybenzoic, 4- hydroxycinnamic, and sulfuric acids in addition to syringaldehyde, vanillin, HMF and furfural), although final cell densities were lower than observed with the control. One possible explanation might be that the presence of high cell concentration might enhance the capacity to bind extracellular inhibitors, thus reducing the bioavailability. It is also possible that the intracellular concentration of these inhibitors is lower when they are distributed among a larger number of cells. It is also conceivable that growth conditions are different enough in ini-fermentations compared to Bioscreen C growth assays to account for differences. As described earlier, Z. mobilis is capable of converting some inhibitors to a less toxic product. This appears to be the case with the apparent reduction of key aldehydes to the corresponding alcohol. This phenomenon was also observed in fermentation experiments conducted in the presence of aldehydes added at the IC50 concentration. Z. mobilis was capable of reducing toxic amounts furfural, vanillin, 4-hydroxybenzaldehyde and some syringaldehyde to the apparent alcohol product. Although Z. mobilis 8b was able to convert 4-hydroxybenzaldehyde, it was not able to overcome growth and fermentation inhibition at 1X MIC. Further investigation will be needed to determine whether Z. mobilis is capable of converting the other phenolics studied in this report. Previous reports have observed the reduction of HMF and furfural concentrations during fermentation in shake flask studies with Z. mobilis ATCC 10988 . We will be conducting additional studies to determine the gene(s) responsible for conversion of these aldehydes. Enhanced conversion of toxic aldehydes with engineered strains could reduce process costs by improving ethanol yields or by reducing fermentation time.
Comparison of Zymomonas to other ethanologens
Although some preliminary studies have evaluated the effects of model compounds present in hydrolysates on Z. mobilis, the strains, media and methods used to assess toxicity varied significantly [11–14]. The data are compiled and presented in Additional file 5: Table S1 for comparison purposes. Since the ranges of concentrations were limited in previous publications, information on MIC has not been reported. From our examination, Z. mobilis 8b performed better in acids and aldehydes using growth as the criteria than when compared with E. coli, Thermoanerobacter mathranii, Candida shehateae, and Pichia stipitis[7, 16, 17].
Z. mobilis 8b, derived from Z. mobilis ZM4, performed much better than Z. mobilis CP4/pZB5 [11–14] and ZM4 (ATCC31821) has been shown to perform much better in ethanol fermentations than CP4 [40, 41]. Thus it is not surprising that 8b outperformed better in HMF, furfural, vanillin, syringaldehyde and acetic acid. Similar tolerance levels to HMF, furfural, vanillin and acetate were observed for Z. mobilis 10988, ZM4 and 8b [11, 13, 14, 21, 42].
What was a surprising observation in this study and has not been previously demonstrated, was that sensitivities to monovalent acids, was particularly strong when xylose was used as the sole substrate. Thus, the challenges of engineering a strain for efficient utilization of pentose sugars are compounded by the additional burden of increased toxicity by these common inhibitors. Clearly, future genetic engineering efforts of Z. mobilis should be directed towards improving growth and thus fermentation performance in organic acid (particularly acetate) through an understanding of the mechanism of organic acid toxicity in both glucose and xylose.
This is the first comprehensive report on the inhibitory effects of model compounds on Z. mobilis using a systematic approach based on inhibitory growth profiles. Using data obtained in this report, we have established a toxicity database for various compounds. Combined with analysis of hydrolysate composition, we are able to make predictions on the contribution of each compound towards toxicity and can begin to prioritize inhibitors based on their relative importance to overall toxicity in hydrolysates for microorganisms. Guidance can then be provided, accordingly, for potential process development, along with potential future strain improvement and tolerance strategies.
Reagents and strains
The Z. mobilis strain used in this study was the recombinant strain 8b engineered for xylose utilization . The following chemicals were obtained from Sigma-Aldrich (St. Louis, MO): calcium acetate, calcium nitrate, succinic acid, sodium sulfate, sodium chloride, ammonium chloride, potassium chloride, calcium chloride, 2-furoic acid, ferulic acid, formic acid, L (+) lactic acid, potassium nitrate, ammonium nitrate, monobasic ammonium phosphate, dibasic potassium phosphate, furfural, syringaldehyde, MES (4-morpholineethanesulfonic acid) and methyl sulfoxide (DMSO), levulinic acid, benzoic acid, potassium sulfate, hexanoic (caproic) acid, 4-hydroxycinnamic (ρ-coumaric) acid, 4-hydroxybenzoic acid, vanillic acid, oxalic acid, furfuryl alcohol, HMF (5-hydroxymethylfufural), vanillin and 4-hydroxybenzaldehyde. The following chemicals were obtained from JT Baker: acetic acid, ammonium sulfate, dibasic ammonium phosphate, and monobasic potassium phosphate.
Culture conditions and growth rate studies
Cultures were grown in RM medium (10 g/L yeast extract, 2 g/L KH2PO4) supplemented with either 2% (w/v) glucose (RMG) or 2% (w/v) xylose (RMX) for inhibitor studies. The pH of all media was adjusted to pH5.8 and was filter sterilized. Media were prepared from stock solutions of yeast extract and monobasic potassium phosphate, and when possible, inhibitor stock solutions were prepared and titrated to pH 5.8. Two compounds (4-hydroxycinnamic acid and syringaldehyde) were prepared from stock solutions in 100% DMSO due to their low solubility in water. The total amount of DMSO in the final medium ranged from 0.1-5.0% (v/v) for 4-hydroxycinnamic acid and 0.1%-3% (v/v) in syringaldehyde. Inhibitor studies with DMSO alone did not detect notable inhibitions on growth or final cell mass (data not shown).
Ammonium salts were prepared by titrating the acids with concentrated ammonium hydroxide, except for the anions: sulfate, chloride, nitrate, acetate, phosphate. Calcium formate was prepared by titrating formic acid with lime. Phosphate stocks were made by preparing 1 M stock solutions of monobasic phosphate and titrating the medium to pH of 5.8 with 1 M dibasic solution.
As a consequence of precipitation of monobasic potassium phosphate with calcium, it was not included in medium containing calcium. In this case, 50 mM MES, pH 5.8, was provided to supply some buffering capacity. Growth rates in RMG or RMX with 50 mM MES, pH 5.8, and no potassium phosphate were similar to those obtained in media with potassium phosphate which indicated that yeast extract in rich media could supply sufficient phosphorous for growth at the 2% sugar level (data not shown).
Overnight cultures in RMG medium were either started from single colonies or from glycerol stocks. Optical densities were measured using a Beckman DU-640 spectrophotometer (Beckman Coulter, Inc., Brea, CA) for inoculation. Growth rates were obtained from the Bioscreen C analyzer purchased from Growth Curves USA (Piscataway, NJ). Procedures for inoculation, growth conditions, measurement, recording of final cell densities and calculations used to correct for non-linear response at high cell densities were previously reported . In brief, log phase cultures of Z. mobilis 8b (a recombinant xylose-utilizing strain of ZM4) were obtained by inoculating overnight cultures in RMG at 30°C and allowing the cells to grow to an OD600 ~ 1.0. Cells were then spun down at 3840 × g, for 10 min at RT and resuspended in RMG or RMX with inhibitor at the desired concentration such that the starting cell density distributed to Bioscreen C microplates after appropriate dilutions with inhibitors was OD600 = 0.05 (~5 × 106 cells/mL=) in a total volume of 300 μL. Incubations were performed at 30°C and absorbance readings were taken every 10 min. Operation of the Bioscreen C and collection of turbidity measurements (OD420–580) were computer automated with EZ Experiment. Data were collected and exported to Microsoft Excel spreadsheets.
Cultures for mini-fermentation studies at 1X MIC were inoculated with Z. mobilis 8b from seed cultures at an OD600 of 1.0 described above, in 4.5 mL of RM medium containing 5% glucose or 5% xylose and inhibitor compounds at a concentration which would cause 100% inhibition of growth rates (1X MIC) in 6 mL HPLC vials at 30°C, 150 rpm, and were vented with an 18 gauge needle and 0.2 micron syringe filter. Samples (0.5 mL) were removed at 0, 24 and 48 hours post inoculation for OD600 and HPLC analysis.
Cultures for aldehyde conversion studies were inoculated with Z. mobilis 8b at an OD600 of 1.0 in 100 mL of RMG containing 5% glucose in 125 mL unbaffled shake flasks containing aldehyde inhibitors at a concentration that would cause 50% inhibition of growth rates at 30°C, 125 rpm. Samples were removed at 0, 24 and 48 hours for HPLC and growth analysis. Flasks containing inhibitor medium without cells were included to assess abiotic loss due to instability or volatility.
High performance liquid chromatography (HPLC) analysis of aldehydes and aldehyde conversion products
Aldehydes and their conversion products were analyzed by reverse-phase HPLC with photodiode array detection (Agilent 1100, Agilent Technologies, Santa Clara, CA) on a C-18 column (Phenomenex, Luna, 150 × 4.6 mm; Torrance, CA) using a linear gradient of acetonitrile-water over 35 min at a flow rate of 0.5 mL/min.
Gas chromatography-mass spectroscopy (GC/MS) analysis of aldehydes and aldehyde conversion products
Aldehydes and their conversion products from same samples analyzed above were also analyzed by GC/MS on an Agilent 6890 GC equipped with a 5973 MS (Agilent Technologies, Palo Alto, CA). Sample compounds were separated using a HP-5MS column (Agilent 122-5532, 30 m × .25 mm × .25 μm HP-5MS column). HP MSD Chemstation software (Agilent) equipped with NIST database Rev. D.03.00 was used to determine the identity of the unknown compounds found within the samples. Each sample was placed on an auto-sampler (Agilent) and injected at a volume of 1 uL. The GC/MS method consisted of a front inlet temperature of 285°C, MS transfer line temperature of 280°C, and a scan range from 35 m/z to 450 m/z. A constant flow of 1 ml/min was held throughout the run. A starting temperature of 35°C was held for 3 minutes and then ramped at 15°C/min to a temperature of 225°C and held for 1 minute, then continued at a ramped rate of 15°C/min to 300°C and held for 5 minutes. The method resulted in a run time of 26.67 minutes for each sample.
Minimum inhibitor concentration
Gram per liter
Inhibitor concentration causing x% growth inhibition
High performance liquid chromatography
Optical density at 600 nanometers.
We would like to acknowledge the funding support from the BioEnergy Technologies Office (BETO), a program in DOE EERE. We also would like to thank Bill Michener from the National Bioenergy Center at the National Renewable Energy Laboratory for GC-MS analysis of aldehydes and their conversion products.
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