Logo of aemPermissionsJournals.ASM.orgJournalAEM ArticleJournal InfoAuthorsReviewers
Appl Environ Microbiol. Jan 2003; 69(1): 113–121.
PMCID: PMC152411

Oxygen Consumption by Anaerobic Saccharomyces cerevisiae under Enological Conditions: Effect on Fermentation Kinetics


The anaerobic growth of the yeast Saccharomyces cerevisiae normally requires the addition of molecular oxygen, which is used to synthesize sterols and unsaturated fatty acids (UFAs). A single oxygen pulse can stimulate enological fermentation, but the biochemical pathways involved in this phenomenon remain to be elucidated. We showed that the addition of oxygen (0.3 to 1.5 mg/g [dry mass] of yeast) to a lipid-depleted medium mainly resulted in the synthesis of the sterols and UFAs required for cell growth. However, the addition of oxygen during the stationary phase in a medium containing excess ergosterol and oleic acid increased the specific fermentation rate, increased cell viability, and shortened the fermentation period. Neither the respiratory chain nor de novo protein synthesis was required for these medium- and long-term effects. As de novo lipid synthesis may be involved in ethanol tolerance, we studied the effect of oxygen addition on sterol and UFA auxotrophs (erg1 and ole1 mutants, respectively). Both mutants exhibited normal anaerobic fermentation kinetics. However, only the ole1 mutant strain responded to the oxygen pulse during the stationary phase, suggesting that de novo sterol synthesis is required for the oxygen-induced increase of the specific fermentation rate. In conclusion, the sterol pathway appears to contribute significantly to the oxygen consumption capacities of cells under anaerobic conditions. Nevertheless, we demonstrated the existence of alternative oxygen consumption pathways that are neither linked to the respiratory chain nor linked to heme, sterol, or UFA synthesis. These pathways dissipate the oxygen added during the stationary phase, without affecting the fermentation kinetics.

The physiological constraints that limit the fermentative activity of the yeast Saccharomyces cerevisiae are not fully understood. Several studies have shown that the lipids or molecular oxygen that are required for lipid biosynthesis are essential for growth (3, 4), plasma membrane integrity (1, 59), and the maintenance of high glycolytic and ethanol production rates (16, 52). In fact, fermentative efficiency and resistance to ethanol are generally linked to: (i) an increase in the ergosterol/phospholipid ratio and (ii) a decrease in the saturation index of the fatty acids in yeast cells (17, 53). Molecular oxygen is required for the conversion of squalene into ergosterol: 1 O2 molecule is required for the conversion of squalene to lanosterol, 9 O2 molecules are required for the conversion of lanosterol to zymosterol, and 2 O2 molecules are required for the conversion of zymosterol to ergosterol (6, 7, 11, 23, 34, 44, 45). However, only one acyl coenzyme A Δ9-desaturase is responsible for the biosynthesis of unsaturated fatty acids (UFAs) (palmitoleate and oleate): 1 O2 molecule is required for the formation of each double bond (47). During enological and brewery fermentations, the addition of air or oxygen is legally permitted as an often common practice. During brewing fermentations, oxygen is generally added during the growth phase to improve biomass synthesis (36). However, under enological conditions, oxygen is used to increase the fermentation rate in the case of sluggish fermentation (52). This is only efficient at the end of the cell growth phase (49, 51). The oxygen requirement is low and has been estimated to be 1.5 to 3.5 mg per g (dry mass) of yeast for enological fermentations (14, 49). Sterol biosynthesis requires 0.1 to 0.3 mg of dissolved oxygen per g (dry mass) of yeast (38), and UFA synthesis requires about 0.35 mg of oxygen per g (dry mass) of yeast (37) during high-gravity brewing fermentations. In contrast, during enological fermentations, the oxygen consumption linked to the sterol biosynthesis pathway can reach 0.5 mg of oxygen per g (dry mass) of yeast, whereas a negligible amount of oxygen is required for UFA synthesis (54).

However, even if ergosterol and UFAs are added to the medium, yeast cells can consume much more oxygen during alcoholic fermentation without affecting the ethanol yield (42, 43, 54). The oxygen consumption capacity of anaerobically grown cells has not been yet characterized under these conditions. Nevertheless, it is partially sensitive to KCN (0.5 to 1 mM) and represents 1 to 5% of the respiratory capacity of fully derepressed aerobically grown cells (28, 48, 54, 62). Some authors believe that the oxygen consumption observed in anaerobically grown repressed cells is mainly due to the classical respiratory chain (25, 43). As the respiratory enzymes, which are subject to glucose catabolite repression, exhibit basal activity (about 1% of the derepressed activity) (25, 30), such ambiguities were reinforced by the fact that some genes (CYC7 and COX5b) encoding respiratory chain components (iso-2 cytochrome c and the cytochrome c oxidase subunit Vb, respectively) are induced under anaerobic conditions. This suggests the existence of an electron flux across cytochrome c oxidase following the addition of oxygen (2, 15, 18). However, recent studies have demonstrated that, despite the fact that they are sensitive to cyanide, promitochondria do not contain any classical respiratory chain activity and do not contribute significantly to the overall oxygen consumption capacities of anaerobic cells (E. Rosenfeld, J. Schaeffer, B. Beauvoit, and J. M. Salmon, submitted for publication). The apparent consumption of excess oxygen by yeast cells is correlated with the hypoxic induction of several genes (HEM13, ERG11, CPR1, and OLE1) (39) and with the cytochrome b5 and P450 contents of microsomal fractions (28, 33, 64). These observations support the partial functioning of heme and microsomal lipid synthesis. Sterol and UFA synthesis may exhibit a temporal priority during the respiratory adaptation to oxygen for mitochondrial membrane biogenesis (19, 28). Nevertheless, the roles of the hypoxic genes that are involved in lipid metabolism remain unknown in the absence of respiratory chain induction (i.e., under hypoxic conditions, following oxygen pulses or following oxygenation of the respiratory-deficient [rho0] mutant strain). This is especially true during the stationary phase (nitrogen starvation) and when the lipid content of the medium is not limiting for growth.

The aim of this work was thus to determine which pathways are the main oxygen-consuming pathways during anaerobic growth during alcoholic fermentation. The fermentation kinetics and the oxygen consumption capacity of the erg1 and ole1 mutant strains were measured to determine how sterol and UFA synthesis may contribute to the response of anaerobic cells to oxygen pulse. Finally, we investigated the potential effect of this oxygen consumption on yeast physiology during anaerobic growth.


Strains, vectors, and culture conditions. (i) Yeast strains.

The S. cerevisiae strain used in this study was V5 (MATa ura3), which was derived from a diploid industrial wine strain. The ura3 genotype was introduced into the V5 strain at the haploid stage. This strain was obtained from the Collection Nationale de Cultures de Microorganismes (Institut Pasteur, Paris, France), reference no. I-1222. The V5-[rho0] respiratory-deficient mutant was obtained by ethidium bromide induction (57). We ensured that strain V5-[rho0] completely lacked mitochondria by checking for a lack of fluorescence inside the cytoplasm after staining with the fluorescent dye DAPI (4′-6′-diamidino-2-phenylindole) (63). Both the V5 and V5-[rho0] strains are ura3 auxotrophs.

(ii) Culture media.

All media were heat sterilized (110°C, 20 min). Unless otherwise specified, yeast strains were grown in the standard nutrient medium (YPD), which contained 1% yeast extract (Difco), 2% Bacto peptone (Difco), and 5% glucose. YNB medium contained 0.17 g of yeast nitrogen base (YNB without amino acids and ammonium sulfate; Difco) liter−1, 5 g of glucose liter−1, 1.15 g of NH4Cl liter−1, and 20 mg of uracil liter−1. A synthetic fermentation medium (Medium Synthetic [MS]) that was strongly buffered to pH 3.3 was used to simulate a standard grape juice (13). This medium contained 200 g of glucose liter−1, 6 g of citric acid liter−1, 6 g of d,l-malic acid liter−1, 20 mg of uracil liter−1, 750 mg of KH2PO4 liter−1, 500 mg of K2SO4 liter−1, 250 mg of MgSO4 · 7H2O liter−1, 155 mg of CaCl2 · 2H2O liter−1, 200 mg of NaCl liter−1, 4 mg of MnSO4 · H2O liter−1, 4 mg of ZnSO4 liter−1, 1 mg of CuSO4 · 5H2O liter−1, 1 mg of KI liter−1, 0.4 mg of CoCl2 · 6H2O liter−1, 1 mg of H3BO3 liter−1, 1 mg of (NH4)6Mo7O24 · 2H2O liter−1, 20 mg of myo-inositol liter−1, 2 mg of nicotinic acid liter−1, 1.5 mg of calcium pantothenate liter−1, 0.25 mg of thiamine-HCl liter−1, 0.25 mg of pyridoxine-HCl liter−1, 0.003 mg of biotin liter−1, and 300 mg of ammoniacal nitrogen (NH4Cl) liter−1. Unless otherwise specified, 15 mg of ergosterol liter−1 dissolved in 1 ml of Tween 80-pure ethanol (50:50, vol/vol) was added to the medium. Approximately 71% of the molar mass of Tween 80 consists of oleic acid (32). When required, Tergitol NP-40 was used to dissolve ergosterol instead of Tween 80 (1 ml of Tergitol NP-40-pure ethanol [50:50, vol/vol]).

(iii) Growth conditions.

In the absence of anaerobic growth factors (i.e., when oxygen was required for growth), yeast cells were precultured at 28°C under hypoxic conditions without agitation. They were grown in small Erlenmeyer flasks with a liquid-to-air ratio of 9/10. In the presence of anaerobic growth factors, yeast cells were precultured in small penicillin flasks (125-ml volume) containing 50 ml of fermentation medium. After inoculation, flasks were tightly closed with a penicillin septum, and pure sterile argon (NP; Air-liquide) (O2 contamination, <2 ppm) was flushed through a needle into the fermentation medium for 5 min. In control experiments (cell-free systems), the decolorization of resazurin (2 mg liter−1) was monitored to ensure that the conditions were indeed anaerobic. Yeast cells were cultured anaerobically in handmade glass fermentors (1.25-liter working volume) fitted with fermentation locks (CO2 bubbling outlets filled with water) (51, 54). The fermentation medium was strongly deoxygenated by bubbling pure sterile argon for 30 min before inoculation. The medium was always inoculated with 106 cells ml−1. After inoculation, the flasks were bubbled with pure sterile argon (NP; Air-liquide) for 40 min to restore anaerobic conditions. In control experiments (cell-free systems), the decolorization of resazurin (2 mg liter−1) was monitored to check anaerobiosis. Fermentations were carried out under isothermal conditions (28°C) with continuous magnetic stirring (500 rpm). A disposable test (Anaerotest; Merck, Darmstadt, Germany) was fitted in the fermentor headspace to ensure that anaerobic conditions were maintained. When required, oxygen was added through a silicone membrane tube as described previously (14). During oxygenation, the culture medium was pumped by way of a peristaltic pump (flow rate, 10 liters h−1) through a silicone tube (length = 2.2 m) set in a jar previously saturated with pure oxygen. The dissolved oxygen transfer rate to the culture medium was 0.8 mg min−1 liter−1 (14). Oxygen additions were repeated several times without significant fouling or changing of silicone membrane properties.

Genetic methods. (i) Disruption of the OLE1 gene.

OLE1 was disrupted by deleting the open reading frame (ORF) as described by Güldener et al. (26). A 1.7-kb fragment containing a dominant resistance module (kanMX) was amplified by PCR with plasmid pUG6-kanMX4 as a template and two oligonucleotides (5′-CTT TAA TGG GCT CCA AGG AAA TGG TTT CCG TGG AAT TCG ACA AGA TTC GTA CGC TGC AGG TCG AC-3′ and 5′-ATC AGC CAA GAC ATT TTG AGC GGC ATT TGA GTG ACG GTA GAC ACC GCA TAG GCC ACT AGT GGA TCT G-3′) that are homologous to the pUG6-kanMX4 multicloning site. These primers also contained 45 nucleotide extensions that were homologous to regions downstream of the start codon (nucleotides 161 to 205) or surrounding the stop codon (nucleotides 1396 to 1440) of the OLE1 ORF (1,533 nucleotides). The PCR product was used to directly transform strain V5 by the lithium acetate method (56). Cells were incubated at 28°C in YPD medium for 14 h and then plated out on YPD medium containing 150 mg of G418 (geneticin) liter−1.

(ii) Disruption of the ERG1 gene.

ERG1 was disrupted by a similar method: the two oligonucleotides 5′-ATG TCT GCT GTT AAC GTT GCA CCT GAA TTG ATT AAT GCC GAC AAC TTC GTA CGC TGC AGG TCG AC-3′ and 5′-TTA ACC AAT CAA CTC ACC AAA CAA AAA TGG GGT GAA TAC TCT AAT GCA TAG GCC ACT AGT GGA TCT G-3′ were homologous to the pUG6-kanMX4 multicloning site. These primers had 45 nucleotide extensions that were homologous to regions downstream of the start codon (nucleotides 1 to 45) or surrounding the stop codon (nucleotides 1447 to 1491) of the ERG1 ORF (YGR175C, 1,491 nucleotides). Due to the aerobic exclusion of sterols (41), the erg1 mutant was unable to grow under aerobic conditions. This phenotype of the erg1 mutant was systematically monitored before use, as mutations in the heme synthesis pathway (spontaneous hem mutants) can suppress this growth phenotype by allowing the efficient uptake of sterols under aerobic conditions (41).

Correct replacement of the OLE1 and ERG1 ORFs by the kanMX4 cassette was checked by PCR on lysed cells (31).

Analytical methods. (i) Number and volume of cells.

Cell numbers and volume were determined by using an electronic particle counter (model ZB2; Beckman-Coulter, Margency, France) fitted with a 100-μm-diameter probe after sonication (30 s, 10 W).

(ii) Cell dry mass.

The cell dry mass was determined by filtering 50 ml of culture medium through membrane filters (pore size, 1.2 μm). Filters were rapidly rinsed three times with 1 ml of distilled water and desiccated at 105°C until reaching a constant weight (24 h).

(iii) Cell viability.

Cell viability was determined by plating out about 250 cells on petri dishes containing YPD agar medium (20 g of agar liter−1, 10 g of yeast extract [Difco] liter−1, 20 g of Bacto peptone [Difco] liter−1, 50 g of glucose liter−1, and anaerobic growth factors). Petri dishes were then incubated at 28°C for 60 h. When necessary, the cells were grown under anaerobic conditions by storing the plates in anaerobic jars fitted with Anaerocult A (Merck). When specified in the text, viability was directly determined on harvested cells by an epifluorescent method with the magnesium salt of 1-anilino-o-naphthalene sulfonic acid (35). For each assay, at least 300 cells were numbered in random microscopic fields.

(iv) Fermentation kinetics.

The amount of CO2 released was determined by automatic measurement of fermentor weight loss every 20 min (50). Loss of ethanol and water due to CO2 stripping represented less than 2% of the total weight loss. The CO2 production rate was calculated by polynomial smoothing of the last ten measurements of fermentor weight loss. The frequent acquisition of CO2 release and the precision of the balance (0.01 g) allowed calculation of the CO2 production rate with good precision and reproducibility [coefficient of variation for d(CO2/dt)max = 0.8%] (13). The fermentation progress (FP) was calculated from the amount of CO2 released from the culture medium according to the following equation: FP = CO2,t/CO2,max, where CO2,t is the cumulative amount of CO2 released at any time t, and CO2,max is the total observed amount of CO2 released at the end of complete fermentation. The use of fermentation progress instead of fermentation time allows a normalization of the fermentation kinetics, which is closely linked to the disappearance of the substrate from the medium. Fermentation was considered to be completed when the medium contained less than 2 g of residual glucose liter−1. In the present study, no fermentation stopped before 99% completion.

(v) Measurement of oxygen consumption.

Oxygen consumptions were measured at 28°C by using a high-resolution oxygraphic system (Oroboros, Innsbruck, Austria). Data were recorded at sampling intervals of 1 s (Datlab Acquisition software; Oroboros, Innsbruck, Austria) (27). After harvesting, cells were quickly washed twice in cold physiological saline (9 g of NaCl liter−1). Oxygen consumption by yeast cells (about 90 × 106 cells ml−1) was then rapidly measured under normoxic conditions (between 3.75 and 7.5 mg of O2 liter−1) in a buffer containing 31 mM citric acid, 45 mM d,l-malic acid, 10 mM KH2PO4 (pH 3.3), and 10% (wt/vol) glucose.


Determination of lipid and oxygen requirements of S. cerevisiae V5 for anaerobic growth.

First, we studied the effect of anaerobic growth factors (ergosterol and Tween 80) on the anaerobic growth of S. cerevisiae V5. As expected, the presence of sterols and fatty acids in the medium resulted in normal fermentation and a final biomass of 170 × 106 cells ml−1 (Fig. (Fig.1).1). In their absence, anaerobic cells only divided 2.8 to 3 times (7 × 106 to 8 × 106 cells ml−1) in 30 h (Fig. (Fig.1A),1A), whereas the yeast population remained viable at this time (92% ± 3%). This residual growth has previously been observed by several other authors (3, 24, 32) and has been attributed to the transfer of sterols and UFAs from the inoculum (24). Under these conditions (45 h of culture, 87% ± 4% cell viability), the addition of 5 mg of oxygen liter−1 restored a normal fermentation (Fig. (Fig.1B)1B) and the cells divided about four more times (final population, 120 × 106 cells ml−1) (Fig. (Fig.1A).1A). At the time of oxygen addition, the oxygen consumption rate (resistant to antimycin A) of the cells was about 2.9 mg of O2 h−1 per 1010 viable cells, which corresponds to 8.4 mg of O2 h−1 g (dry mass) of yeast−1. From the total amount of oxygen added and the cell biomass, we estimated that all of the added oxygen was consumed between 20 min and 5 h before growth resumed. We used this experimental approach (addition of growth factors after 45 h of culture in a synthetic lipid-depleted medium, after cells had entered a true stationary phase) to quantify the oxygen, oleic acid, and ergosterol requirements for strain V5 growth (Fig. (Fig.2).2). About 5 to 7.5 mg of oxygen liter−1 was required for the optimal growth of V5 (Fig. (Fig.2A).2A). These values are compatible with previous data obtained under enological (49) or brewery (21) conditions. Similar values were obtained in the presence of antimycin A, suggesting that the respiratory chain is not induced during oxygen pulses (data not shown). In the presence of excess oleic acid (1 ml of Tween 80-pure ethanol [50:50, vol/vol] liter−1, corresponding to 74 mg of total oleic acid liter−1), maximal growth was achieved with 5 mg of ergosterol liter−1, which is in agreement with previous results (32) (Fig. (Fig.2B).2B). As all the supplied ergosterol is incorporated into yeast cells (22), ergosterol accounted for about 0.18% of the final biomass (148 × 106 cells ml−1, about 2.8 g [dry mass] of yeast liter−1). This is the average ergosterol content found in anaerobically grown glucose-repressed S. cerevisiae cells (8, 9, 20, 46). When the medium contained excess ergosterol, 15 mg of oleic acid liter−1 sustained maximal growth (Fig. (Fig.2C).2C). This value is very similar to that obtained by Barber and Lands (10) but lower than that obtained by Verduyn et al. (61). The oxygen equivalence of ergosterol and oleic acid requirements were calculated and are listed in Table Table1.1. The oxygen required for the growth of V5 exactly matched the cellular requirements for both ergosterol and UFA under anaerobic conditions. Moreover, 75% of the oxygen requirements accounted for sterol synthesis. However, the potential accumulation of sterol intermediates would probably lower the total amount of oxygen required for sterol biosynthesis. This was not considered in our calculations. Nevertheless, these results appear to contradict previous results obtained under brewery conditions, which suggested that only 20 to 30% of the available oxygen was used for the synthesis of lipids (37, 43). As a consequence, we further studied the effect of oxygen addition during alcoholic fermentation in a synthetic medium containing an excess of all of the anaerobic factors essential for the growth of V5 (15 mg of ergosterol liter−1 and 1 ml of Tween 80-pure ethanol [50:50, vol/vol] liter−1).

FIG. 1.
Variations in cell population (A) and CO2 production rate (B) as a function of the lipid composition of MS medium. The V5 strain was anaerobically cultured in the presence ([filled triangle]) or absence (•, [filled square]) of anaerobic growth factors (1 ml ...
FIG. 2.
Effect of adding oxygen (A), ergosterol (B), or oleic acid (C) to wild-type strain V5 grown as described in the legend to Fig. Fig.11 for 50 h under anaerobic conditions in MS synthetic lipid-depleted medium without anaerobic growth factors. The ...
Comparison of the amounts of oxygen, ergosterol, and oleic acid required for the anaerobic growth of S. cerevisiae V5

Effect of oxygen on fermentation of S. cerevisiae V5 in the presence of anaerobic growth factors.

The punctual addition of oxygen (5 mg liter−1) during the growth phase (at 26 or 44 h) led to a low but reproducible increase in both biomass synthesis (Table (Table2)2) and fermentation rates (Fig. (Fig.3).3). Similar results were obtained with oxygen additions in the range 1 to 10 mg liter−1 (data not shown). However, when oxygen was added during the stationary phase (50.5 and 61 h), an increase in the fermentation rate was observed (Fig. (Fig.3),3), but the cell population was not affected (Table (Table2).2). The specific fermentation rate was more increased when oxygen was added during the stationary phase than when it was added during the growth phase (Table (Table2).2). This was accompanied by a long-term increase in cell viability during the stationary phase (Fig. (Fig.4A).4A). This phenomenon has also been observed during industrial fermentations but never explained. This is especially true in the presence of excess ergosterol and oleic acid (49, 51). Identical results were obtained following the addition of antimycin A (5 μM) or when the respiratory-deficient V5-[rho0] mutant was used, indicating that this effect is not due to the function of the classical respiratory chain (data not shown). We also confirmed that the oxygen pulses (1 to 10 mg liter−1) did not induce any respiratory chain activity, as revealed by the full antimycin A resistance of oxygen consumption by [rho+] cells measured under normoxic conditions (data not shown). Moreover, the stimulation of fermentation by oxygen pulse (5 mg liter−1) during the stationary phase was still observed in the presence of cycloheximide (data not shown). This suggests that such stimulation of the fermentation rate by oxygen does not require de novo protein synthesis. As this phenomenon may be of great importance for industrial fermentations with regards to the acquisition of ethanol tolerance mechanisms, we further studied the effect of oxygen during the stationary phase.

FIG. 3.
Changes in the CO2 production rate by V5 cultured anaerobically in MS synthetic medium in the presence of anaerobic growth factors. For the control experiment (•), arrows indicate the addition of dissolved oxygen (5 mg liter−1) at 26 h ...
FIG. 4.
Changes in percent cell viability as a function of fermentation progress. The wild-type V5 (A) and ole1::kan (B) and erg1::kan (C) mutant strains were anaerobically cultured in MS synthetic medium in the presence of anaerobic growth factors. Cell viability ...
Effect of adding oxygen (5 mg liter−1) during anaerobic fermentation of S. cerevisiae V5 in the presence of excess anaerobic growth factorsa

Involvement of de novo lipid synthesis in S. cerevisiae strain V5 during oxygen addition in the presence of anaerobic growth factors.

To determine the importance of sterol and UFA neosynthesis in the observed response to oxygen addition, two mutant strains were derived from the wild-type V5 strain. First, we disrupted ERG1, which encodes squalene epoxidase, the first enzyme involved in the oxygen-dependent parts of the ergosterol biosynthesis pathway (29, 55). Due to the aerobic exclusion of sterols (41), the resulting ERG1 null allele strain (V5 erg1::kan) was unable to grow under aerobic conditions and required the presence of both oleic acid and ergosterol for anaerobic growth (Fig. (Fig.5).5). Second, we disrupted the OLE1 gene, which encodes the microsomal Δ9 fatty acid desaturase (58). The resulting mutant strain (V5 ole1::kan) clearly required oleic acid for growth (Fig. (Fig.5).5). Under anaerobic conditions, both mutant strains reached a similar final cell number (about 160 × 106 cells ml−1) when grown in a complete synthetic medium containing excess oleic acid and ergosterol. The fermentation kinetics of the two mutants were similar to those of the wild-type strain, except that both mutants exhibited an additional 8-h lag phase. The addition of oxygen (5 mg liter−1) during the stationary phase did not have any effect on the fermentation kinetics of the erg1 strain, showing that the ERG1 gene product is essential for the effect of oxygen on fermentation rates (Fig. (Fig.6B).6B). On the contrary, the OLE1 gene product is not involved in this response (Fig. (Fig.6A).6A). Similar results were obtained in terms of cell viability (Fig. (Fig.4).4). Indeed, when oxygen was added during the early stationary phase, a high proportion (about 60%) of wild-type and ole1 mutant cells remained viable at the end of the fermentation period (Fig. 4A and B). Considerably fewer erg1 mutant cells were viable under the same conditions (Fig. (Fig.4C)4C) (36% ± 8%). These data are consistent with the hypothesis that sterols play a specific role in ethanol resistance and in the increase in the specific fermentation rate following the addition of oxygen (17, 22, 60).

FIG. 5.
Comparison of the phenotypes of wild-type V5 (A) and the ole1::kan (B) and erg1::kan (C) mutant strains on different types of solid media. Strains were grown for 96 h at 28°C. When required, 1 ml of Tween 80 liter−1, 15 mg of ergosterol ...
FIG. 6.
Effect of oxygen addition on the fermentation of ole1::kan (A) and erg1::kan (B) mutant strains grown under anaerobic conditions in MS synthetic culture medium in the presence of anaerobic growth factors. Filled circles denote the control experiment. ...

Although erg1 cell viability (estimated by the epifluorescence method) was not affected by a 5-mg liter−1 oxygen addition during the stationary phase (Fig. (Fig.4C),4C), the viability of resting cells was progressively affected in response to exposure to normoxia (data not shown). In fact, the strict anaerobe erg1 strain only seems able to tolerate oxygen when low quantities are added during fermentation.

Contribution of lipid biosynthesis to overall oxygen consumption.

In parallel to the analysis of fermentation kinetics, a high-resolution oxygraph was used to determine the overall oxygen consumption capacities of the wild-type and mutant strains. Oxygen consumption capacities were measured on washed cells in the absence of ergosterol throughout the entire fermentation period (Fig. (Fig.7).7). It is noteworthy that these capacities are not related to the classical respiratory chain functionality, as they were not inhibited by specific inhibitors of the bc1 complex (5 to 50 μM antimycin A or 1 to 4 μM myxothiazol) (data not shown). Moreover, the contribution of heme biosynthesis to oxygen consumption is probably negligible because cells grown on glucose have low heme and porphyrin requirements (about 50 nmol g [dry mass] of yeast−1) (40).

FIG. 7.
Changes in the cell number (filled symbols) and specific oxygen consumption capacities (JO) (open symbols) of V5 (circles), ole1::kan (squares), and erg1::kan (triangles) strains that had been anaerobically cultured in MS synthetic culture medium in the ...

Interestingly, the impairment of sterol synthesis in the erg1 mutant strain resulted in a 40% decrease in oxygen consumption (Fig. (Fig.7).7). On the contrary, the oxygen consumption capacity of the ole1 mutant and of the wild type were similar over the entire fermentation period. This result is consistent with the fermentation kinetics data, which suggest a strong involvement of de novo sterol biosynthesis and the dispensability of the OLE1 gene in the cellular response to moderate oxygen pulses during nitrogen starvation. This last observation was reinforced by the fact that the hypoxic induction of OLE1 does not occur in respiration-deficient strains (as shown by Kwast et al. [39]), whereas the V5-[rho0] strain exhibits an oxygen consumption capacity similar to that of the wild type (about 2 μmol of O2 min−1 g [dry mass] yeast−1 during the early stationary phase).

The contribution made by the sterol pathway in the oxygen consumption capacities of the wild-type and mutant strains was also investigated by measuring the effects of several inhibitors. As expected, this contribution was considerable in the wild type and the ole1 mutant (Table (Table3).3). The oxygen consumption capacity of the erg1 mutant was not inhibited by terbinafine or fenpropimorph, which inhibited several crucial steps of the sterol pathway. This unusual oxygen consumption capacity of the erg1 mutant might be explained by hydroxylation-desaturation reactions (dependent or not on cytochrome P450) from intermediate sterols to ergosterol. However, this is unlikely to occur, as the added ergosterol did not contain significant amounts of other sterols (22) and the oxygen consumption rates of viable erg1 washed cells (suspended in lipid-free media) were almost constant for several hours (data not shown). Therefore, although the erg1 mutant is a strict anaerobe, it is still able to transiently consume oxygen, probably by unknown oxygen consumption pathways. These pathways (which account for a significant amount of the oxygen consumption abilities of the wild-type, [rho0], and ole1 strains) are partially sensitive to cyanide (Table (Table3).3). However, the interpretation of this effect is difficult because cyanide probably has several targets. Finally, we postulate that the uncharacterized oxygen consumption retained by anaerobically grown cells may dissipate the added oxygen (moderate pulse) without having any significant effect on fermentation kinetics (as shown in Fig. Fig.6B6B).

Effect of sterol biosynthesis inhibitors on oxygen consumption of anaerobically grown cellsa


Anaerobic cells retain a capacity to consume oxygen. This capacity may be related to the anaerobic induction of several genes encoding enzymes involved in oxygen utilization (39). However, the relative oxygen fluxes passing through the numerous pathways implicated (e.g., sterol, UFA and heme synthesis, classical or alternative respiratory chain, and soluble oxidases, etc.) have yet to be described. Moreover, whereas the addition of oxygen stimulates enological fermentation (52), the oxygen consumption pathways involved in these phenomena had not been identified.

The first part of the present study looked at the effect of oxygen addition on anaerobic batch fermentation kinetics (enological conditions) as a function of the lipid composition of the medium. We demonstrated that a pulse of dissolved oxygen (1 to 10 mg liter−1) can stimulate alcoholic fermentation, even in the presence of excess ergosterol and oleic acid and without the functioning or induction of the mitochondrial respiratory chain. This phenomenon appeared to contradict outwardly the well-known Pasteur effect (i.e., inhibition of glycolysis by mitochondrial respiration). However, such an oxygen pulse stimulates fermentation only moderately but finally has an influence on long-term fermentative capacities. We showed that de novo sterol synthesis (in the presence of excess ergosterol) is required for the increase of the specific fermentation rate, whereas de novo UFA or protein synthesis is not required. The sterol molecule responsible for this effect has yet to be identified. The use of other erg mutants may lead to the identification of this molecule rather than the use of the anaerobic addition of sterols, which also implies the addition of detergents. The major effect of moderate oxygen additions was on yeast survival (long-term response). Therefore, we hypothesize that a de novo sterol synthesis increased the cellular tolerance to ethanol. However, the short-term response to the oxygen pulse suggests that endogenous sterols have a specific role in the maintenance of the high fermentative capacities of viable cells. Newly synthesized sterols may incorporate plasmalemma microdomains, which may in turn enhance glucose uptake, especially during the stationary phase.

The strong involvement of sterol synthesis during oxygenation of stationary-phase anaerobically grown cells was also quantified in terms of oxygen consumption capacity. By using terbinafine and fenpropimorph, we showed that the sterol pathway accounts for about 30% of the overall oxygen consumption capacity developed in the presence of anaerobic growth factors (but measured in their absence). As anaerobic cells seem to retain a high apparent affinity for oxygen, the sterol pathway may play a crucial role both in hypoxic conditions and during the early stages of normoxic growth. However, it is important to remember that normoxia and the addition of moderate amounts of oxygen exert two distinct and cumulative long-term effects on glucose metabolism, namely the induction of respiratory chain activity despite the strong glucose repression (Rosenfeld et al., submitted) and the stimulation of fermentation rate (this study). These two effects required distinct mechanisms of sterol distribution among cellular membranes. Our study also demonstrated that anaerobically grown cells retain a relatively high oxygen consumption capacity, which seems linked to neither (i) classical respiratory chain activity, (ii) heme biosynthesis, nor (iii) sterol and UFA synthesis. The corresponding alternative cellular pathways also seem to retain high oxygen affinities and likely permit the dissipation of the added oxygen. The subcellular localization, characterization, and analysis of the physiological role of these unusual oxygen consumption pathways are currently under way in our laboratory.


1. Alexandre, H., I. Rousseaux, and C. Charpentier. 1994. Relationship between ethanol tolerance, lipid composition and plasma membrane fluidity in Saccharomyces cerevisiae and Kloeckera apiculata. FEMS Microbiol. Lett. 124:17-22. [PubMed]
2. Allen, L. A., X. J. Zhao, W. Caughey, and R. O. Poyton. 1995. Isoforms of yeast cytochrome c oxidase subunit V affect the binuclear reaction center and alter the kinetics of interaction with the isoforms of yeast cytochrome c. J. Biol. Chem. 270:110-118. [PubMed]
3. Andreasen, A. A., and T. J. B. Stier. 1953. Anaerobic nutrition of Saccharomyces cerevisiae. I. Ergosterol requirement for growth in a defined medium. J. Cell. Comp. Physiol. 41:23-36. [PubMed]
4. Andreasen, A. A., and T. J. B. Stier. 1954. Anaerobic nutrition of Saccharomyces cerevisiae. II. Unsaturated fatty acid requirement for growth in a defined medium. J. Cell. Comp. Physiol. 43:271-281. [PubMed]
5. Aoyama, Y., Y. Yoshida, R. Sato, M. Susani, and H. Ruis. 1981. Involvement of cytochrome b5 and a cyanide-sensitive monooxygenase in the 4-demethylation of 4,4-dimethylzymosterol by yeast microsomes. Biochim. Biophys. Acta 663:194-202. [PubMed]
6. Aoyama, Y., Y. Yoshida, and R. Sato. 1984. Yeast cytochrome P-450 catalyzing lanosterol 14α-demethylation. II. Lanosterol metabolism by purified P-450 14DM and by intact microsomes. J. Biol. Chem. 259:1661-1666. [PubMed]
7. Aoyama, Y., Y. Yoshida, Y. Sonoda, and R. Sato. 1989. Role of the 8-double bond of lanosterol in the enzyme-substrate interaction of cytochrome P-450(14DM) (lanosterol 14 alpha-demethylase). Biochim. Biophys. Acta 1001:196-200. [PubMed]
8. Aries, V., and B. H. Kirsop. 1978. Sterol biosynthesis by strains of Saccharomyces cerevisiae in the presence and absence of dissolved oxygen. J. Inst. Brew. 84:118-121.
9. Arneborg, N., C. E. Hoy, and O. B. Jorgensen. 1995. The effect of ethanol and specific growth rate on the lipid content and composition of Saccharomyces cerevisiae grown anaerobically in a chemostat. Yeast 11:953-959. [PubMed]
10. Barber, E. D., and W. E. M. Lands. 1973. Quantitative measurement of the effectiveness of unsaturated fatty acids required of the growth of Saccharomyces cerevisiae. J. Bacteriol. 115:543-551. [PMC free article] [PubMed]
11. Bard, M., D. A. Bruner, C. A. Pierson, N. D. Lees, B. Biermann, L. Frye, C. Koegel, and R. Barbuch. 1996. Cloning and characterization of ERG25, the Saccharomyces cerevisiae gene encoding C-4 sterol methyl oxidase. Proc. Natl. Acad. Sci. USA 93:186-190. [PMC free article] [PubMed]
12. Barrett-Bee, K., and G. Dixon. 1995. Ergosterol biosynthesis inhibition: a target for antifungal agents. Acta Biochim. Pol. 42:465-479. [PubMed]
13. Bely, M., J. M. Sablayrolles, and P. Barre. 1990. Description of alcoholic fermentation kinetics: its variability and significance. Am. J. Enol. Vitic. 40:319-324.
14. Blateyron, L., E. Aguera, C. Dubois, C. Gerland, and J. M. Sablayrolles. 1998. Control of oxygen additions during alcoholic fermentations. Vitic. Enol. Sci. 53:131-135.
15. Burke, P. V., D. C. Raitt, L. A. Allen, E. A. Kellog, and R. O. Poyton. 1997. Effect of oxygen concentration on the expression of cytochrome c and cytochrome c oxidase genes in yeast. J. Biol. Chem. 272:14705-14712. [PubMed]
16. Casey, G. P., C. A. Magnus, and W. M. Ingledew. 1984. High-gravity brewing: effects of nutrition on yeast composition, fermentative ability and alcohol production. Appl. Environ. Microbiol. 48:639-646. [PMC free article] [PubMed]
17. Chi, Z., and N. J. Arneborg. 1999. Relationship between lipid composition, frequency of ethanol-induced respiratory deficient mutants, and ethanol tolerance in Saccharomyces cerevisiae. Appl. Microbiol. 86:1047-1052. [PubMed]
18. Dagsgaard, C., L. E. Taylor, K. M. O'Brien, and R. O. Poyton. 2001. Effects of anoxia and the mitochondrion on expression of aerobic nuclear COX genes in yeast: evidence for a signalling pathway from the mitochondrial genome to the nucleus. J. Biol. Chem. 276:7593-7601. [PubMed]
19. Damsky, C. H. 1976. Environmentally induced changes in mitochondria and endoplasmic reticulum of Saccharomyces carlsbergensis yeast. J. Cell Biol. 71:123-135. [PMC free article] [PubMed]
20. Daum, G., G. Tuller, T. Nemec, C. Hrastnik, G. Balliano, L. Cattel, P. Milla, F. Rocco, A. Conzelmann, C. Vionnet, D. E. Kelly, S. Kelly, E. Schweizer, H. J. Schuller, U. Hojad, E. Grenier, and K. Finger. 1999. Systematic analysis of yeast strains with possible defect in lipid metabolism. Yeast 15:601-614. [PubMed]
21. David, M. H., and B. H. Kirsop. 1973. A correlation between oxygen requirement and the products of sterol synthesis in strains of Saccharomyces cerevisiae. J. Gen. Microbiol. 77:529-531. [PubMed]
22. Fornairon-Bonnefond, C., V. Demaretz, E. Rosenfeld, and J. M. Salmon. 2002. Oxygen addition and sterol synthesis in Saccharomyces cerevisiae during enological fermentation. J. Biosci. Bioeng. 93:176-182. [PubMed]
23. Gachotte, D., R. Barbuch, J. Gaylor, E. Nickel, and M. Bard. 1998. Characterization of the Saccharomyces cerevisiae ERG26 gene encoding the C-3 sterol dehydrogenase (C-4 decarboxylase) involved in sterol biosynthesis. Proc. Natl. Acad. Sci. USA 95:13794-13799. [PMC free article] [PubMed]
24. Gordon, P. A., and P. R. Stewart. 1972. Effect of lipid status on cytoplasmic and mitochondrial protein synthesis in anaerobic cultures of Saccharomyces cerevisiae. J. Gen. Microbiol. 72:231-242. [PubMed]
25. Groot, G. S. P., L. Kovác, and G. Schatz. 1971. Promitochondria of anaerobically grown yeast. V. Energy transfer in the absence of an electron transfer chain. Proc. Natl. Acad. Sci. USA 68:308-311. [PMC free article] [PubMed]
26. Güldener, U., A. Hech, T. Fiedler, J. Beinhauer, and J. H. Hegemann. 1996. A new efficient gene disruption cassette for repeated use in budding yeast. Nucleic Acids Res. 24:2519-2524. [PMC free article] [PubMed]
27. Haller, T., M. Ortner, and E. Gnaiger. 1994. A respirometer for investigating oxidative cell metabolism: towards optimization of respiratory studies. Anal. Biochem. 218:338-342. [PubMed]
28. Ishidate, K., K. Kawaguchi, K. Tagawa, and B. Hagihara. 1969. Hemoproteins in anaerobically grown yeast cells. J. Biochem. 65:375-383. [PubMed]
29. Jandrositz, A., F. Turnowsky, and G. Hogenauer. 1991. The gene encoding squalene epoxidase from Saccharomyces cerevisiae: cloning and characterization. Gene 107:155-160. [PubMed]
30. Jenkins, R. O., T. G. Cartledge, and D. Lloyd. 1984. Respiratory adaptation of anaerobically grown Saccharomyces uvarum: changes in distribution of enzymes. J. Gen. Microbiol. 130:2809-2816.
31. Jesnowski, R., J. Naehring, and K. Wolf. 1995. A rapid and reliable method for PCR-based amplification of chromosomal and mitochondrial DNA from intact yeast cells. Curr. Genet. 27:318-319. [PubMed]
32. Jollow, D., G. M. Kellerman, and A. W. Linnane. 1968. The biogenesis of mitochondria. III. The lipid composition of aerobically and anaerobically grown Saccharomyces cerevisiae as related to the membrane systems of the cells. J. Cell Biol. 37:221-230. [PMC free article] [PubMed]
33. Kawaguchi, K., K. Ishidate, and K. Tagawa. 1973. Non-mitochondrial electron transfer system in anaerobically grown yeast cells. J. Biochem. (Tokyo) 74:817-826. [PubMed]
34. Kelly, S. L., D. C. Lamb, B. C. Baldwin, A. J. Corran, and E. K. Diane. 1997. Characterization of Saccharomyces cerevisiae CYP61, sterol Δ22-desaturase, and inhibition by azole antifungal agents. J. Biol. Chem. 272:9986-9988. [PubMed]
35. King, L. M., D. O. Schisler, and J. J. Ruocco. 1981. Epifluorescent method for detection of nonviable yeasts. J. Am. Soc. Brew. Chem. 39:52-54.
36. Kirsop, B. H. 1974. Oxygen in brewery fermentation. J. Inst. Brew. 80:252-259.
37. Kirsop, B. H. 1977. Oxygen and sterol synthesis during beer fermentations, p. 41-42. In J. Oksanen and H. Soumalainen (ed.), Proceedings of the EUCHEM Conference on Metabolic Reactions in the Yeast Cell in Anaerobic and Aerobic Conditions, 13 to 16 June 1977, Helsinki, Finland. Alko Offset, Helsinki, Finland.
38. Kirsop, B. H. 1982. Developments in beer fermentation. Top. Enzyme Ferment. Biotechnol. 6:79-131.
39. Kwast, K. E., P. V. Burke, B. T. Staahl, and R. O. Poyton. 1999. Oxygen sensing in yeast: evidence for the involvement of the respiratory chain in regulating the transcription of a subset of hypoxic genes. Proc. Natl. Acad. Sci. USA 96:5446-5451. [PMC free article] [PubMed]
40. Labbe, P. 1971. Synthèse du protohème par la levure Saccharomyces cerevisiae. I. Mise en évidence de différentes étapes de la synthèse du protohème chez la levure cultivée en anaérobiose. Influence des conditions de culture sur cette synthèse. Biochimie 53:1001-1014. [PubMed]
41. Ness, F., T. Achstetter, C. Duport, F. Karst, and R. Spagnoli. 1998. Sterol uptake in Saccharomyces cerevisiae heme auxotrophic mutants is affected by ergosterol and oleate but not by palmitoleate or sterol esterification. J. Bacteriol. 180:1913-1919. [PMC free article] [PubMed]
42. O'Connor-Cox, E. S. C., E. J. Lodolo, and B. C. Axcell. 1993. Role of oxygen in high-gravity fermentations in the absence of unsaturated lipid biosynthesis. J. Am. Soc. Brew. Chem. 51:97-107.
43. O'Connor-Cox, E. S. C., E. J. Lodolo, and B. C. Axcell. 1996. Mitochondrial relevance to yeast fermentative performance: a review. J. Inst. Brew. 102:19-25.
44. Osumi, T., T. Nishino, and H. Katsuki. 1979. Studies on the delta 5-desaturation in ergosterol biosynthesis in yeast. J. Biochem. (Tokyo) 85:819-826. [PubMed]
45. Parks, L. W. 1978. Metabolism of sterols in yeast. Crit. Rev. Microbiol. 6:301-341. [PubMed]
46. Quain, D. E., and R. S. Tubb. 1982. The importance of glycogen in brewing yeast. Tech. Q. Master Brew. Assoc. Am. 19:29-33.
47. Ratledge, C., and C. T. Evans. 1989. Lipids and their metabolism, p. 367-455. In A. H. Rose and J. S. Harrison (ed.), The yeasts: metabolism and physiology of yeasts, 2nd ed. Academic Press, San Diego, Calif.
48. Rogers, P. J., and P. R. Stewart. 1973. Mitochondrial and peroxisomal contributions to the energy metabolism of Saccharomyces cerevisiae in continuous culture. J. Gen. Microbiol. 79:205-217. [PubMed]
49. Sablayrolles, J. M., and P. Barre. 1986. Evaluation des besoins en oxygène de fermentations alcooliques en conditions oenologiques simulées. Sci. Alim. 6:373-383.
50. Sablayrolles, J. M., P. Barre, and P. Grenier. 1987. Design of a laboratory automatic system for studying alcoholic fermentations in anisothermal enological conditions. Biotechnol. Tech. 1:181-184.
51. Sablayrolles, J. M. 1990. Besoins en oxygène lors des fermentations œnologiques. Rev. Fr. Oenol. 124:77-79.
52. Sablayrolles, J. M., C. Dubois, C. Manginot, J. L. Roustan, and P. Barre. 1996. Effectiveness of combined ammoniacal nitrogen and oxygen additions for completion of sluggish and stuck wine fermentations. J. Ferment. Bioeng. 82:377-381.
53. Sajbidor, J., Z. Ciesarova, and D. Smogrovicova. 1995. Influence of ethanol on the lipid content and fatty acid composition of Saccharomyces cerevisiae. Folia Microbiol. (Prague) 40:508-510. [PubMed]
54. Salmon, J. M., C. Fornairon, and P. Barre. 1998. Determination of oxygen utilization pathways in an industrial strain of Saccharomyces cerevisiae during enological fermentation. J. Ferment. Bioeng. 86:154-163.
55. Satoh, T., M. Horie, H. Watanabe, Y. Tsuchiya, and T. Kamei. 1993. Enzymatic properties of squalene epoxidase from Saccharomyces cerevisiae. Biol. Pharm. Bull. 16:349-352. [PubMed]
56. Schiestl, R. H., and R. D. Gietz. 1989. High efficiency transformation of intact cells using single stranded nucleic acid as carrier. Curr. Genet. 16:339-446. [PubMed]
57. Slonimski, P. P., G. Perrodin, and J. H. Croft. 1968. Ethidium bromide-induced mutation of yeast mitochondria: complete transformation of cells into respiratory deficient nonchromosomal “petites.” Biochem. Biophys. Res. Commun. 30:232-239. [PubMed]
58. Stukey, J. E., V. M. McDonough, and C. E. Martin. 1990. The OLE1 gene of Saccharomyces cerevisiae encodes a delta 9 fatty acid desaturase and can be functionally replaced by the rat stearoyl-CoA desaturase gene. J. Biol. Chem. 265:20144-20149. [PubMed]
59. Thomas, D. S., J. A. Hossack, and A. H. Rose. 1978. Plasma-membrane lipid composition and ethanol tolerance in Saccharomyces cerevisiae. Arch. Microbiol. 117:239-245. [PubMed]
60. Valero, E., M. C. Millan, and J. M. Ortega. 2001. Influence of skin maceration and oxygen on anaerobic fermentation of grape musts with high sugar content. Microbios 106:111-127. [PubMed]
61. Verduyn, C., E. Postma, W. A. Scheffers, and J. P. van Dijken. 1990. Physiology of Saccharomyces cerevisiae in anaerobic glucose-limited chemostat cultures. J. Gen. Microbiol. 136:395-403. [PubMed]
62. Visser, W., A. A. van der Baan, W. Batenburg-van der Vegte, W. Scheffers, R. Kramer, and J. P. van Dijken. 1994. Involvement of mitochondria in the assimilatory metabolism of anaerobic Saccharomyces cerevisiae cultures. Microbiology 140:3039-3046. [PubMed]
63. Williamson, D. H., and D. J. Fennell. 1975. The use of fluorescent DNA-binding agent for detecting and separating yeast mitochondrial DNA. Methods Cell. Biol. 12:335-351. [PubMed]
64. Yoshida, Y., H. Kumaoka, and R. Sato. 1974. Studies on the microsomal electron-transport system of anaerobically grown yeast. I. Intracellular localization and characterization. J. Biochem. 75:1201-1210. [PubMed]

Articles from Applied and Environmental Microbiology are provided here courtesy of American Society for Microbiology (ASM)
PubReader format: click here to try


Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


  • Compound
    PubChem Compound links
  • MedGen
    Related information in MedGen
  • PubMed
    PubMed citations for these articles
  • Substance
    PubChem Substance links

Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...