Rapid total volatile organic carbon quantification from microbial fermentation using a platinum catalyst and proton transfer reaction-mass spectrometry
© The Author(s) 2016
Received: 25 September 2016
Accepted: 28 September 2016
Published: 5 October 2016
A novel analytical system was developed to rapidly and accurately quantify total volatile organic compound (VOC) production from microbial reactor systems using a platinum catalyst and a sensitive CO2 detector. This system allows nearly instantaneous determination of total VOC production by utilizing a platinum catalyst to completely and quantitatively oxidize headspace VOCs to CO2 in coordination with a CO2 detector. Measurement of respiratory CO2 by bypassing the catalyst allowed the total VOC content to be determined from the difference in the two signals. To the best of our knowledge, this is the first instance of a platinum catalyst and CO2 detector being used to quantify the total VOCs produced by a complex bioreactor system. Continuous recording of these CO2 data provided a record of respiration and total VOC production throughout the experiments. Proton transfer reaction-mass spectrometry (PTR-MS) was used to identify and quantify major VOCs. The sum of the individual compounds measured by PTR-MS can be compared to the total VOCs quantified by the platinum catalyst to identify potential differences in detection, identification and calibration. PTR-MS measurements accounted on average for 94 % of the total VOC carbon detected by the platinum catalyst and CO2 detector. In a model system, a VOC producing endophytic fungus Nodulisporium isolate TI-13 was grown in a solid state reactor utilizing the agricultural byproduct beet pulp as a substrate. Temporal changes in production of major volatile compounds (ethanol, methanol, acetaldehyde, terpenes, and terpenoids) were quantified by PTR-MS and compared to the total VOC measurements taken with the platinum catalyst and CO2 detector. This analytical system provided fast, consistent data for evaluating VOC production in the nonhomogeneous solid state reactor system.
KeywordsFungal endophyte Proton transfer reaction-mass spectrometry Solid state fermentation Total volatile organic carbon
Fungi and bacteria produce hundreds of volatile organic compounds (VOCs) with industrial applications including biofuels, insecticides, quorum sensing and biocontrol, flavor and aroma compounds, antibacterials and antifungals (Hung et al. 2015; Kai et al. 2009; Morath et al. 2012; Strobel 2014). Bioprospecting has identified many new microorganisms that produce valuable VOCs, and the types and amounts of these compounds often change with substrate, culturing conditions and growth phase (Bunge et al. 2008; Kai et al. 2009; Morath et al. 2012; Strobel 2014). Higher yields of most microbial VOCs must be achieved to make these bioprocesses industrially viable, but fast and accurate analytical methods to determine the type and amount of VOCs produced are lacking (Morath et al. 2012). Efficient ways to screen new and genetically modified strains, and changes in culture conditions, are required to rapidly identify improvement to VOC yields (Morath et al. 2012).
Solid phase microextraction (SPME) coupled with gas chromatography–mass spectrometry (GC–MS) has been used to identify compounds produced by microbial fermentation (Mallette et al. 2012; Morath et al. 2012). With little sample preparation, SPME GC–MS readily identifies VOCs using compound libraries, but does a poor job of quantifying the amounts of compounds produced (Luchner et al. 2012; Mallette et al. 2012; Morath et al. 2012) and is not well suited to screen for increased yields of VOCs. Traditional extraction techniques to concentrate VOCs can be time intensive, and large organic solvent volumes may lead to poor resolution of volatile compounds (Kai et al. 2009; Morath et al. 2012). Further, extraction techniques may identify fewer VOCs than SPME GC–MS (Kai et al. 2009; Morath et al. 2012). Another analytical method, proton nuclear magnetic resonance can quantify VOCs quickly, but has poor sensitivity, cannot determine carbon length and some oxygenated VOCs cannot be measured because signals are confounded with sugar peaks (Mallette et al. 2014).
Proton transfer reaction-mass spectrometry (PTR-MS) is an effective analytical technique for measuring VOCs in the headspace of both liquid and nonhomogeneous solid state microbial reactor systems (Bunge et al. 2008; Ezra et al. 2004b; Luchner et al. 2012; Mallette et al. 2012). With PTR-MS, many VOCs can be quantified down to the 10–100 parts per trillion range with reliable results (Biasioli et al. 2011; de Gouw et al. 2003; Lindinger et al. 1998). PTR-MS provides data quickly including a likely compound identification, without the extensive preparatory laboratory work required for extractions (Ammann et al. 2004; Luchner et al. 2012). With real-time gas phase measurement capability, the PTR-MS readily ties VOC data to experimental conditions and temporal changes, and can non-invasively utilize reactor off-gas for measurements (Luchner et al. 2012; Romano et al. 2015).
Previously, PTR-MS has been used to explore microbial systems, but estimates of error in VOC quantification can be between 15 and 40 % depending on system conditions (Bunge et al. 2008; Ezra et al. 2004b; Luchner et al. 2012; Mallette et al. 2012; Romano et al. 2015; Schmidberger et al. 2014; Singer et al. 2009). Quantification of total VOC production with PTR-MS can be improved with calibration, but significant uncertainties may remain due to compounds that are not readily detected by PTR-MS (e.g. alkanes) and complex mixtures where multiple compounds with different sensitivity (calibration) factors contribute to the same mass to charge ratio.
Alternatively, the platinum catalyst and sensitive CO2 detector provide a robust VOC quantification system (Baasandorj et al. 2015; Veres et al. 2010) that confidently provides the total amount of gas phase organic carbon in complex mixtures of VOCs produced by microbial systems. The platinum catalyst oxidizes VOCs completely to CO2, which allows a sensitive CO2 detector to accurately quantify the total VOC production in real-time, as well as record respiratory CO2. This accurate VOC total can be used to quantify headspace carbon for carbon balances and as a real-time process monitoring tool. Additionally, the total VOC measurements can be compared to less certain total quantifications performed with other instruments, such as PTR-MS, to identify discrepancies in the system. To the best of our knowledge, this is the first time the combination of a platinum catalyst and CO2 detector has been used to quantify total headspace VOC production from a complex bioreactor system.
This paper demonstrates total VOC quantification in a non-homogenous solid state reactor system, where both growth phase and VOC data can be cumbersome to collect (Desgranges et al. 1991; Krishna 2005). The system described here provides a virtually instantaneous method for quantifying total VOC production.
Materials and methods
Solid state fungal reactor system
Solid state reactors constructed from a 2-L, air tight, borosilicate glass container with three stainless steel mesh shelves were inoculated with 250 mg of biomass as determined by a correlation with protein concentration using a modified Bradford method (Bradford 1976). As a substrate, 50 g of beet pulp were autoclaved for 20 min with 250 mL of water and allowed to cool. The reactor, hydration flask and all tubing were autoclaved at 121 °C for 20 min before use. Fungal biomass was added to the beet pulp, mixed by inversion and evenly distributed to the three shelves of the reactor. Biological triplicate experiments were run for approximately 5 days each until total VOC production approached zero.
The solid state reactor (see Fig. 1) was continuously sparged with 100 mL/min of hydrated medical grade compressed air. The air was delivered via a stainless steel tube (0.5 cm I.D.) running to the bottom center of the reactor. Inlet air pressure forced reactor gas out of the top of the reactor. Reactor off-gas was then diluted with 900 mL/min of dry medical grade air to keep water from condensing in the system and to keep concentrations within the linear range of the CO2 detector and PTR-MS. A portion of the diluted flow stream, ~200 mL/min, was then pulled through the CO2 detector and PTR-MS with the PTR-MS diaphragm pump.
Nodulisporium isolate TI-13 was discovered as an endophyte of Cassia fistula in the highlands of Thailand using established collection and isolation methods as described previously (Ezra et al. 2004a). The TI-13 ITS1-5.8 S-ITS2 ribosomal gene sequence is available in GenBank as KJ558391, and the filamentous fungus is stored as sample NRRL 50502 in the Agriculture Research Service Culture Collection at the US Department of Agriculture (Nigg et al. 2014). The fungus was characterized as having the perfect stage of Hypoxylon sp. and as Nodulisporium sp. based on ITS1-5.8 S-ITS2 ribosomal gene sequence information (Nigg et al. 2014).
Inoculum cultures were generated by growing the fungus on potato dextrose agar until hyphae covered ≥60 % of the plate surface. A 20 % glycerol solution (10 mL) was added to each plate, scraped with a sterile glass rod and the suspended fungal biomass solution was collected. The solution was mixed thoroughly, added to Microbank microbead vials, and stored at −80 °C until use.
The composition of the inoculum medium was 60 g/L glucose and 0.5 g/L yeast extract. Two hundred and fifty millilitre of sterile filtered (0.22 µm) medium was added to 500 mL sterile baffled flasks. Three microbeads were added to each inoculum culture and grown for 9 days at 160 rpm and 30 °C. All inoculum flasks were covered with sterile Kimguard (Kimberly-Clark; Roswell, GA, USA) to allow gas exchange, but prevent microbial contamination.
CO2 detector calibration and verification
An LI-840 CO2/H2O non-dispersive infrared gas analyzer (Li-cor Biosciences; Lincoln, NE, USA), quantified CO2 in the reactor off-gas continuously without impacting it. This optical technique is non-destructive and allowed the PTR-MS to be placed in series after the CO2 detector. The CO2 detector was calibrated using a certified CO2 free gas standard to set the zero point (1 % methane, balance nitrogen Scotty Analyzed Gases, Plumsteadville, PA, USA) and another gas standard for the span (a gas standard of 1010 ppm CO2, balance nitrogen, Scotty Analyzed Gases, Plumsteadville, PA, USA). Linearity of the CO2 detector was assessed by diluting the gas standard (1010 ppm CO2, balance nitrogen) with medical grade compressed air using mass flow controllers to produce final CO2 concentrations of 50.5, 101, 505 and 1010 ppm. The CO2 detector response agreed with the prepared gas standard to within 3.3 % for the four values measured, with values creating a line with a slope of 1.0006 and an R2 value of 0.9998 when plotting measured concentration versus expected concentration (data not shown).
Platinum catalyst VOC conversion verification
Complete oxidation of VOCs to CO2 by a heated platinum catalyst (Shimadzu, Kyoto, Japan, High Sensitivity Catalyst 630-00996 maintained at 400 °C) was confirmed by diluting a gas standard (0.1 % propane, balance air, Cal Gas Direct, Huntington Beach, CA, USA) and medical grade compressed air with mass flow controllers to produce final propane concentrations in the range of 10–100 ppm, which spanned the total VOC concentration presented to the catalyst in the diluted sample flow. Based on the tenfold dilution of the bioreactor effluent and accounting for the three carbons in propane, this experiment produced a test matrix that was equivalent to total bioreactor VOC concentration of 300–3000 ppm C. Overall, the platinum catalyst and CO2 detector measurement agreed with the gas standard for conversion of propane to CO2 by the platinum catalyst to within 5 % for the four measured values, and created a line with a slope of 0.95 and an R2 value of 0.9991 when measured concentration was plotted against expected concentration. The catalyst exhibited near complete conversion efficiency for propane concentrations up to 50 ppm of propane, which decreased to 95 % at the highest, 100 ppm test point. This experiment established the effective maximum working concentration of the employed catalyst system at 1500 ppm C after adjusting for dilution. Catalyst systems employing higher temperatures and greater amounts of catalyst could be used to achieve higher maximum working concentrations. Similar catalyst systems have been used previously to confirm concentrations of calibration gases with high accuracy (Baasandorj et al. 2015; Veres et al. 2010).
The reactor off-gas flow path was alternated with a valve on a 3 h timer to run either directly to the CO2 detector or through the platinum catalyst to oxidize VOCs to CO2 before the CO2 detector. By alternating the air stream either around or through the platinum catalyst every 3 h, a near-continuous record of respiratory CO2 and total gas phase carbon (CO2 and VOC) production was created for each experiment. The CO2 detector measurement was recorded once per second during the experiments. Background CO2 and VOCs measurements for each tank of medical grade compressed air were subtracted from these values.
Proton transfer reaction-mass spectrometry (PTR-MS)
PTR-MS was used to provide compositional information about the VOCs in the reactor off-gas. PTR-MS uses H3O+ ions to protonate molecules (e.g. VOCs) with proton affinities greater than water (Lindinger et al. 1998). The singly charged ions are then typically detected as protonated molecules (ions with a mass-to-charge ratio, m/z, equal to the molecular weight plus 1 for the proton) by a quadrupole mass spectrometer (Lindinger et al. 1998). Identity is assigned based on the mass of the ion and prior knowledge of the likely products of a specific reactor system (Luchner et al. 2012). Constituents of air like O2, N2 and CO2 have proton affinities lower than water so are not protonated and do not interfere with measurements. Alkanes also have proton affinities lower than water, so PTR-MS does not efficiently detect alkanes (Lindinger et al. 1998).
Initial experiments with this solid state system showed the major VOC products were ethanol, methanol, acetaldehyde and monoterpenes, so care was taken to calibrate the PTR-MS for these compounds. Quantification was performed using sensitivity factors derived from calibration experiments by dynamically diluting a multicomponent standard containing methanol, acetaldehyde and terpenes (Apel-Riemer Environmental Inc., Broomfield, CO, USA). Ethanol calibration was performed separately using a permeation tube at a variety of humidities as described below. Sensitivity factors of 4.1, 17.4, 18.2 and 2.2 ncps (normalized counts per second)/ppbv for ethanol (m47, m65, m93), methanol (m33, m51), acetaldehyde (m45) and terpenes and terpenoids (m137) were used, respectively. The off-gas of the abiotic control and fungal cultures were both analyzed by the PTR-MS. The total VOCs measured in the abiotic control were subtracted from the fungal VOC production measurements.
Ethanol PTR-MS calibration
Ethanol calibrations were performed using a calibrated permeation tube (KIN-TEK; La Marque, TX, USA) at a variety of humidity values approaching dry air as the experiments were performed with 90 % dry air. Compressed air (19.5 mL/min) was sparged through a temperature-controlled oven (50 °C) holding a calibrated ethanol permeation tube (emission rate 209 ng/min at 50 °C). Mass flow controllers were used to control medical grade compressed air flowing through the permeation tube and a second dilution stream, introduced after the permeation tube, to produce concentrations of 101, 199, 484 and 924 ppb of ethanol based on the calibrated permeation tube emission rate. The concentration of ethanol produced with the permeation tube was checked using the platinum catalyst system as described previously (Baasandorj et al. 2015) resulting in a line with a slope of 1.1 and an R2 value of 0.997 (data not shown). The temperature of the permeation tube was then increased to 80 °C to produce ethanol concentrations comparable to those observed in the fungal experiment (1.2–6.2 ppm). The humidity of the air was varied by utilizing a hydration flask before the dilution. Humidity was monitored via the ratio of the H3O+(H2O) to H3O+ ion intensities with calibration experiments performed under conditions that closely matched the humidity in the fungal experiments. At low humidity, the sensitivity factor had a relatively constant value of approximately 4.0. Calibrations were repeated after the experiments and yielded a sensitivity factor of approximately 3.9.
Additionally for these data, we can examine the VOC content quantified with PTR-MS for comparison to the total VOC production measured by the platinum catalyst and CO2 detector. Figure 4 shows a difference PTR-MS spectrum, where a background spectrum (obtained by measuring reactor off-gas passed through the catalyst) was subtracted from the off-gas measurements, from late stationary phase (119 h into experiment 3). Additional reactor off-gas VOC ions are present in the spectra, but they represented less than three percent of the ion intensity before death phase and were not quantified. Results show counts for ethanol (m/z 47, 65, 93) were highest for most spectra. Large amounts of methanol (m/z 33, 51) and acetaldehyde (m/z 45) ions are present in this spectrum. The terpene and terpenoid (m/z 81, 137) peaks and concentrations are smaller, despite accounting for more carbon per mole since they have ten carbons per molecule, compared to one or two carbon compounds like methanol and ethanol. Higher counts of two ions (m/z 57, 71), each of up to three percent of total ion intensity, and small but increased amounts of several other ions (less than one percent of total ion intensity each) were detected in death phase spectra (data not shown).
The compounds quantified by the PTR-MS (acetaldehyde, ethanol, methanol and terpenes) were multiplied by their carbon number and summed to determine the total concentration of VOCs in ppm C. This concentration was then divided by the total VOC production in ppm C determined by the platinum catalyst and CO2 detector to calculate recovery as shown by the height of the bars compared to one on the right axis in Fig. 3. Ideally, recovery ratios would be 1.0 if the PTR-MS detected all carbon containing compounds in the headspace. The average recovery ratio observed here was 0.945 ± 0.047 (average and standard error; see Additional file 1: Table S1) indicating that any unidentified VOC products constitute only a small fraction of the total VOC production. Recovery ratios were furthest from 1.0 at lag and death phases. Total VOC production was also lowest during lag and death phases, so small inaccuracies in CO2 concentration differences between bypass and catalyst measurements likely contributed to the recovery ratio error. Additionally, multiple small intensity ion signals that were not quantified appeared in death phase, which is expected due to cellular degradation and changing metabolism (Hazelwood et al. 2008). Fungal production of small concentrations of alkanes, which are undetectable by the PTR-MS, and small errors in calibration of the CO2 detector and PTR-MS may also contribute to errors in total quantification.
Two types of deviations from the anticipated response appeared in the CO2 detector signals later in the experiments. “Rolling” deviations in the CO2 signal were observed when switching between modes in which the signal exhibited some hysteresis and was slow to achieve a steady measurement immediately following the change in flow paths. This is most readily apparent starting in late-exponential phase (about 60 h) as observed in Fig. 2. The rolling characteristic was observed only in this experimental set and is likely due to pressure variations that occurred when switching between lines. Yegneswaran et al. (1990) observed similar patterns of CO2 concentrations and determined they were caused by small pressure changes in the bioreactor, but quickly returned to steady state. This type of deviation could be avoided by using two CO2 detectors. Additionally, some noise was observed in the infrared based CO2 measurements starting in late stationary phase and increased until the end of the experiments, but no cause was determined for this deviation. While this deviation persisted in later experiments, a definitive cause has not been determined. The combined momentary inaccuracies are estimated at less than 5 % of the signal, and do not significantly influence total VOC calculations for the majority of each experiment. During death phase, these perturbations were larger compared to the total signal and may contribute to less accurate death phase VOC recovery results.
Respiratory CO2, VOC production and reproducibility
Three biological replicate experiments were performed to assess the reproducibility of the system. Total respiratory CO2, total organic carbon in the headspace (from VOCs) and substrate percentage of carbon converted to VOCs and CO2 were very reproducible for the three experiments. The total amount of respiratory CO2 produced was 0.73 ± 0.040 carbon g with three biological replicates (average and standard error) calculated by integrating the lower respiratory CO2 line in Fig. 2 as described above. Total VOC production was calculated in an analogous fashion by integrating data such as that shown in Fig. 3. Overall, 0.087 ± 0.0055 carbon g of total VOC were produced in each experiment. The average amount of beet pulp carbon (43 % carbon) (Stoppok and Buchholz 1985) converted to respiratory CO2 and VOCs was 3.8 ± 0.19 %. A biomass measurement assay was not utilized in these experiments. Whole experiment headspace selectivity was calculated as 0.12 ± 0.0080 by dividing the VOCs by the respiratory CO2 as measured by the CO2 detector throughout the experiment as described above.
The combination of PTR-MS, platinum catalyst and sensitive CO2 detector allowed for real-time VOC sampling with a quantitative determination of the compounds produced. The system described provides a robust measurement of the total VOC production as well as composition of major species produced by the non-homogenous solid state reactor system. To the best of our knowledge, this is the first time the total gas phase VOC content of a solid state reactor has been reported.
The platinum catalyst provides an accurate measurement of total headspace VOC production in complex microbial systems. Catalyst systems are effective at oxidizing nearly all the VOCs present in a sample, and are routinely used to purify air of VOCs for background measurements in PTR-MS (de Gouw and Warneke 2007) and to measure total organic carbon (Sugimura and Suzuki 1988). The platinum catalyst and CO2 detector agreed with the propane gas standard to within 5 % in our verification, and similar systems used to verify gas calibration standards agree to within 4–5 % of standards (Baasandorj et al. 2015; Veres et al. 2010). Catalyst systems are more accurate at measuring VOCs under many conditions than other detection systems currently available, such as PTR-MS and GC–MS (Ammann et al. 2004; Baasandorj et al. 2015; de Gouw et al. 2003; Kajos et al. 2015; Veres et al. 2010). An accurate total VOC measurement allows confident determination of the fraction one compound represents in a VOC mixture. Also, the platinum catalyst and CO2 detector are an affordable system to accurately quantify total headspace VOC carbon and respiratory CO2 for carbon balances. However, the platinum catalyst and CO2 detector do not provide any information on the identity of the VOCs present in a sample.
The platinum catalyst can also be used as an assessment tool to determine if the majority of VOCs produced are being detected, accurately identified and accurately quantified by the PTR-MS. A difference in the total VOC content determined by the platinum catalyst and CO2 detector from that provided by the PTR-MS can alert the user to check for issues such as the following: additional ions with significant carbon content may need to be quantified in the PTR-MS spectrum, some compounds (e.g. alkanes) are not being detected, sensitivity factors may be inaccurate, or identification of the VOC precursor responsible for part or all of an ion’s intensity may be incorrect. Ideally, all but one of these issues would be ruled out using prior system knowledge before using this assessment tool to identify discrepancies in PTR-MS VOC quantification. In this system, the PTR-MS total VOC content agreed on average to within 5.5 ± 4.7 % of that determined with the platinum catalyst and CO2 detector, which is considered to be excellent agreement. This level of agreement suggests that the PTR-MS quantification is providing an accurate measurement of VOC composition and that there are no significant errors in the calibration of the four major products, especially the detailed calibration of the major product, ethanol. The system described here is rapid and efficient at measuring the composition of VOCs with high confidence compared to other available measurement methods.
Identifying and quantifying headspace metabolites with PTR-MS throughout growth phases may aid in understanding metabolic processes (Bunge et al. 2008; Crespo et al. 2011; Luchner et al. 2012) and improve monitoring in production systems (Schmidberger et al. 2014). For example, acetaldehyde production appears to be an early marker of impending robust growth in some bacterial and fungal species and can be detected before increases in cell dry weight (Bunge et al. 2008) or respiratory CO2. Similarly, total VOC measurements can help verify robust growth, product formation and aid in understanding novel processes. This system can also determine headspace selectivity and productivity for total VOC production or individual compounds. For facilities without a PTR-MS, utilizing a platinum catalyst and CO2 detector in conjunction with SPME GC–MS could be employed. This would provide real-time respiratory CO2 and total VOC production rates, with SPME GC–MS used to identify specific compounds in complex VOC mixtures. While SPME GC–MS does not provide reliable quantification, it can be used in coordination with other assays to measure products (Mallette et al. 2012).
This total VOC quantification system can be applied in many different types of bioreactors. Bioremediation projects could utilize the detection system to quantify VOC removal in soil, water, or air samples. This system has applications in screening VOC producing organisms, VOC yield changes from varying process conditions, identifying appropriate target genes for genetic engineering and verifying increased VOC production in genetically engineered strains. The VOC measurement system could also be used for online process monitoring of bioreactors (Schmidberger et al. 2014), especially in solid state reactor systems where accurate and immediate online measurements are extremely difficult (Lui 2013). Similarly, many novel biological systems under study present challenges to traditional rapid monitoring methods, where complications with standard methods arise from a number of conditions such as complex carbon sources, fungi growing with pellet morphology and biofilms. These systems can benefit from utilizing the method described here to provide additional metabolic data in real-time.
WBK designed the experiments. HRS performed experiments and drafted the manuscript. All three authors interpreted data and edited the manuscript. All authors read and approved the final manuscript.
This research was supported in part by the National Science Foundation (NSF) EFRI Program under Grant No. 0937613. Any opinion, findings and conclusions or recommendations expressed in this material are those of the authors and do not necessarily reflect the views of the NSF. Thank you to the Montana State University Center for Biofilm Engineering, the Chemistry and Biochemistry Department and the Chemical and Biological Engineering Department for support. The authors would also like to thank Drs. Gary Strobel and Natasha Mallette for sound technical advice.
The authors declare that they have no competing interests.
This research was supported in part by the National Science Foundation (NSF) EFRI Program under Grant No. 0937613, as well as the Montana State University Chemistry and Biochemistry Department, Chemical and Biological Engineering Department, and Center for Biofilm Engineering.
This article does not contain any studies with human participants or animals performed by any of the authors.
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- Ammann C, Spirig C, Neftel A, Steinbacher M, Komenda M, Schaub A (2004) Application of PTR-MS for measurements of biogenic VOC in a deciduous forest. Int J Mass Spectrom 2–3:87–101. doi:10.1016/j.ijms.2004.08.012 View ArticleGoogle Scholar
- Baasandorj M, Millet DB, Hu L, Mitroo D, Williams BJ (2015) Measuring acetic and formic acid by proton-transfer-reaction mass spectrometry: sensitivity, humidity dependence, and quantifying interferences. Atmos Meas Tech 3:1303–1321. doi:10.5194/amt-8-1303-2015 View ArticleGoogle Scholar
- Biasioli F, Gasperi F, Yeretzian C, Märk TD (2011) PTR-MS monitoring of VOCs and BVOCs in food science and technology. TrAC Trends Anal Chem 7:968–977. doi:10.1016/j.trac.2011.03.009 View ArticleGoogle Scholar
- Bradford MM (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem 1–2:248–254. doi:10.1016/0003-2697(76)90527-3 View ArticleGoogle Scholar
- Bunge M, Araghipour N, Mikoviny T, Dunkl J, Schnitzhofer R, Hansel A, Schinner F, Wisthaler A, Margesin R, Märk TD (2008) On-line monitoring of microbial volatile metabolites by proton transfer reaction-mass spectrometry. Appl Environ Microbiol 7:2179–2186. doi:10.1128/AEM.02069-07 View ArticleGoogle Scholar
- Crespo E, Cristescu SM, de Ronde H, Kuijper S, Kolk AHJ, Anthony RM, Harren FJM (2011) Proton transfer reaction mass spectrometry detects rapid changes in volatile metabolite emission by Mycobacterium smegmatis after the addition of specific antimicrobial agents. J Microbiol Methods 1:8–15. doi:10.1016/j.mimet.2011.01.025 View ArticleGoogle Scholar
- de Gouw J, Warneke C (2007) Measurements of volatile organic compounds in the earth’s atmosphere using proton-transfer-reaction mass spectrometry. Mass Spectrom Rev 26:223–257. doi:10.1002/mas.20119 View ArticlePubMedGoogle Scholar
- de Gouw J, Warneke C, Karl T, Eerdekens G, van der Veen C, Fall R (2003) Sensitivity and specificity of atmospheric trace gas detection by proton-transfer-reaction mass spectrometry. Int J Mass Spectrom. doi:10.1016/S1387-3806(02)00926-0 Google Scholar
- Desgranges C, Vergoignan C, Georges M, Durand A (1991) Biomass estimation in solid state fermentation I. Manual biochemical methods. Appl Microbiol Biotechnol 2:200–205. doi:10.1007/BF00184686 Google Scholar
- Ezra D, Hess WM, Strobel GA (2004a) New endophytic isolates of Muscodor albus, a volatile-antibiotic-producing fungus. Microbiology 12:4023–4031. doi:10.1099/mic.0.27334-0 View ArticleGoogle Scholar
- Ezra D, Jasper J, Rogers T, Knighton B, Grimsrud E, Strobel G (2004b) Proton transfer reaction-mass spectrometry as a technique to measure volatile emissions of Muscodor albus. Plant Sci 6:1471–1477. doi:10.1016/j.plantsci.2004.01.022 View ArticleGoogle Scholar
- Hazelwood LA, Daran J-M, van Maris AJ, Pronk JT, Dickinson JR (2008) The Ehrlich pathway for fusel alcohol production: a century of research on Saccharomyces cerevisiae metabolism. Appl Environ Microbiol 8:2259–2266. doi:10.1128/AEM.02625-07 View ArticleGoogle Scholar
- Hung R, Lee S, Bennett JW (2015) Fungal volatile organic compounds and their role in ecosystems. Appl Microbiol Biotechnol 8:3395–3405. doi:10.1007/s00253-015-6494-4 View ArticleGoogle Scholar
- Kai M, Haustein M, Molina F, Petri A, Scholz B, Piechulla B (2009) Bacterial volatiles and their action potential. Appl Microbiol Biotechnol 6:1001–1012. doi:10.1007/s00253-008-1760-3 View ArticleGoogle Scholar
- Kajos MK, Rantala P, Hill M, Hellén H, Aalto J, Patokoski J, Taipale R, Hoerger CC, Reimann S, Ruuskanen TM, Rinne J, Petäjä T (2015) Ambient measurements of aromatic and oxidized VOCs by PTR-MS and GC-MS: intercomparison between four instruments in a boreal forest in Finland. Atmos Meas Tech 10:4453–4473. doi:10.5194/amt-8-4453-2015 View ArticleGoogle Scholar
- Krishna C (2005) Solid-state fermentation systems—an overview. Crit Rev Biotechnol 1–2:1–30. doi:10.1080/07388550590925383 View ArticleGoogle Scholar
- Lindinger W, Hansel A, Jordan A (1998) On-line monitoring of volatile organic compounds at pptv levels by means of proton-transfer-reaction mass spectrometry (PTR-MS) medical applications, food control and environmental research. Int J Mass Spectrom Ion Process 3:191–241. doi:10.1016/s0168-1176(97)00281-4 View ArticleGoogle Scholar
- Luchner M, Gutmann R, Bayer K, Dunkl J, Hansel A, Herbig J, Singer W, Strobl F, Winkler K, Striedner G (2012) Implementation of proton transfer reaction-mass spectrometry (PTR-MS) for advanced bioprocess monitoring. Biotechnol Bioeng 12:3059–3069. doi:10.1002/bit.24579 View ArticleGoogle Scholar
- Lui L (2013) Process engineering of solid-state fermentation. CRC Press, Boca RatonGoogle Scholar
- Mallette N, Pankratz EM, Parker AE, Strobel GA, Busse SC, Carlson RP, Peyton BM (2014) Evaluation of cellulose as a substrate for hydrocarbon fuel production by Ascocoryne sarcoides (NRRL 50072). J Sustain Bioenergy Syst 01:33–49. doi:10.4236/jsbs.2014.41004 View ArticleGoogle Scholar
- Mallette ND, Knighton WB, Strobel GA, Carlson RP, Peyton BM (2012) Resolution of volatile fuel compound profiles from Ascocoryne sarcoides: a comparison by proton transfer reaction-mass spectrometry and solid phase microextraction gas chromatography–mass spectrometry. AMB Express 1:23. doi:10.1186/2191-0855-2-23 View ArticleGoogle Scholar
- Morath SU, Hung R, Bennett JW (2012) Fungal volatile organic compounds: a review with emphasis on their biotechnological potential. Fungal Biol Rev 2–3:73–83. doi:10.1016/j.fbr.2012.07.001 View ArticleGoogle Scholar
- Nigg J, Strobel G, Knighton WB, Hilmer J, Geary B, Riyaz-Ul-Hassan S, Harper JK, Valenti D, Wang Y (2014) Functionalized para-substituted benzenes as 1,8-cineole production modulators in an endophytic Nodulisporium species. Microbiology 8:1772–1782. doi:10.1099/mic.0.079756-0 View ArticleGoogle Scholar
- Romano A, Capozzi V, Spano G, Biasioli F (2015) Proton transfer reaction-mass spectrometry: online and rapid determination of volatile organic compounds of microbial origin. Appl Microbiol Biotechnol 9:3787–3795. doi:10.1007/s00253-015-6528-y View ArticleGoogle Scholar
- Schmidberger T, Gutmann R, Bayer K, Kronthaler J, Huber R (2014) Advanced online monitoring of cell culture off-gas using proton transfer reaction mass spectrometry. Biotechnol Prog 2:496–504. doi:10.1002/btpr.1853 View ArticleGoogle Scholar
- Singer W, Gutmann R, Dunkl J, Hansel A (2009) PTR-MS technology for process monitoring and control in biotechnology. J Process Anal Chem 1:1–4Google Scholar
- Stoppok E, Buchholz K (1985) Continuous anaerobic conversion of sugar beet pulp to biogas. Biotechnol Lett 2:119–124. doi:10.1007/BF01026682 View ArticleGoogle Scholar
- Strobel GA (2014) Methods of discovery and techniques to study endophytic fungi producing fuel-related hydrocarbons. Nat Prod Rep 2:259–272. doi:10.1039/C3NP70129H View ArticleGoogle Scholar
- Sugimura Y, Suzuki Y (1988) A high-temperature catalytic oxidation method for the determination of non-volatile dissolved organic carbon in seawater by direct injection of a liquid sample. Mar Chem 24:105–131. doi:10.1016/0304-4203(88)90043-6 View ArticleGoogle Scholar
- Veres P, Gilman J, Roberts J, Kuster W, Warneke C, Burling I, Gouw Jd (2010) Development and validation of a portable gas phase standard generation and calibration system for volatile organic compounds. Atmos Meas Tech 3:683–691. doi:10.5194/amt-3-683-2010 View ArticleGoogle Scholar
- Yegneswaran PK, Gray MR, Thompson BG (1990) Kinetics of CO2 hydration in fermentors: pH and pressure effects. Biotechnol Bioeng 36:92–96. doi:10.1002/bit.260360112 View ArticlePubMedGoogle Scholar