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Changes in the Sterol Composition of the Plasma Membrane Affect Membrane Potential, Salt Tolerance and the Activity of Multidrug Resistance Pumps in Saccharomyces cerevisiae

Changes in the Sterol Composition of the Plasma Membrane Affect Membrane Potential, Salt Tolerance and the Activity of Multidrug Resistance Pumps in Saccharomyces cerevisiae

  • Marie Kodedová, 
  • Hana Sychrová
PLOS
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Abstract

We investigated the impact of the deletions of genes from the final steps in the biosynthesis of ergosterol (ERG6, ERG2, ERG3, ERG5, ERG4) on the physiological function of the Saccharomyces cerevisiae plasma membrane by a combination of biological tests and the diS-C3(3) fluorescence assay. Most of the erg mutants were more sensitive than the wild type to salt stress or cationic drugs, their susceptibilities were proportional to the hyperpolarization of their plasma membranes. The different sterol composition of the plasma membrane played an important role in the short-term and long-term processes that accompanied the exposure of erg strains to a hyperosmotic stress (effect on cell size, pH homeostasis and survival of yeasts), as well as in the resistance of cells to antifungal drugs. The pleiotropic drug-sensitive phenotypes of erg strains were, to a large extent, a result of the reduced efficiency of the Pdr5 efflux pump, which was shown to be more sensitive to the sterol content of the plasma membrane than Snq2p. In summary, the erg4Δ and erg6Δ mutants exhibited the most compromised phenotypes. As Erg6p is not involved in the cholesterol biosynthetic pathway, it may become a target for a new generation of antifungal drugs.

Introduction

The plasma membrane, together with the cell wall, protects the yeast cell from environmental changes. A proper plasma-membrane composition is essential and has to be carefully controlled by the cell. The regulation of membrane composition has an important modulatory role and serves as an adaptive response to variations in temperature, pH, hydration etc. [12]. The regular plasma-membrane barrier function is dependent on its permeability and fluidity, which are determined by various aspects, such as the length and saturation of lipid acyl chains and the amount and type of sterols and sphingolipids in the membrane [34]. In yeast cells, sterols not only contribute to the fluidity of lipid membranes, but also ensure many other vital processes including vesicle formation and protein sorting, cytoskeleton organization, endocytosis and mating [2,58].

Yeast cells synthesize their major sterol, ergosterol, in the membrane of the endoplasmic reticulum via a cascade of coupled enzymatic reactions. Ergosterol is then transported from the site of its synthesis to the plasma membrane. However, Saccharomyces cerevisiae is also a facultative anaerobic organism, which becomes a sterol auxotroph in the absence of oxygen. Under these conditions, cells take up sterols from the environment, incorporate them into the plasma membrane and transport them back into the membrane of the endoplasmic reticulum, where the free sterols become esterified and the resulting steryl esters are stored in lipid droplets [7,9]. Surprisingly, the synthesis of ergosterol in lower eukaryotes requires more energy than the synthesis of mammalian cholesterol [10]. Only some less evolutionary advanced species of fungi, which live in an aquatic medium where the hydration is stable, synthesize cholesterol instead of ergosterol [11]. Under special conditions, mammalian cholesterol can substitute for the crucial role of ergosterol, e.g. some pathogenic fungi, such as Candida glabrata and Aspergillus fumigatus, import exogenous cholesterol from the host serum in the presence of oxygen to counteract the toxicity of antifungal agents that target ergosterol and its synthetic pathway [1214]. Both cholesterol and ergosterol increase the mechanical resistance of the plasma membrane to osmotic treatments, but ergosterol and its precursors provide lipids with a better protection against peroxidation than cholesterol [15]. Therefore, the ergosterol biosynthetic pathway might have accompanied the evolution of the fungi kingdom and the properties of sterols were gradually optimized for their function in the biosynthetic pathway [1].

The synthesis of ergosterol in yeast cells is a complex process. Altogether the ergosterol biosynthetic pathway involves over 20 distinct reactions [16]. The early pathway starts with acetyl-CoA and ends with the formation of farnesyl pyrophosphate, an important intermediate which is the starting point for several essential pathways. Therefore mutations in this part of the pathway are lethal, because a number of essential metabolic products cannot be synthesized [16]. The next three steps catalyzed by the enzymes encoded by ERG9 (squalene synthase), ERG1 (squalene epoxidase) and ERG7 (lanosterol synthase) are also essential, and they lead to the synthesis of the first sterol molecule, lanosterol [9,17]. Strains with deletions of genes encoding enzymes for the late steps of ergosterol biosynthesis are viable and accumulate sterols that differ from ergosterol in the number and position of double bonds in the B-ring and the side chain of the sterol molecule [17] as shown in Fig 1.

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Fig 1. Final steps of ergosterol biosynthesis in S. cerevisiae with highlighted targets of studied Erg proteins.

Violet arrows indicate parts of sterol molecules that were changed by the corresponding enzymes.

https://doi.org/10.1371/journal.pone.0139306.g001

Ergosterol plays a crucial role in the architecture of the yeast plasma membrane. The plasma membrane of Saccharomyces cerevisiae is composed of structurally distinct lateral microdomains which are formed through the association of sterols and sphingolipids with proteins. Many membrane proteins are distributed non-homogenously in patterns ranging from discrete ergosterol-enriched MCC patches (membrane compartment of arginine permease Can1p) to nearly continuous MCP networks (membrane compartment of Pma1p) [18]. In addition, dynamic patch-like domains, called MCT (membrane compartment of TORC2), were described for Tor Complex 2 [19]. The domain structure of the plasma membrane has been not only identified in S. cerevisiae but also in Schizosaccharomyces pombe or pathogenic Candida albicans and Cryptococcus neoformans [20]. In yeast cells, these microdomains house a number of biologically important proteins involved in Na+, K+ and pH homeostases, nutrient transport, mating, drug efflux and stress response [20]. Integral plasma membrane proteins with similar functions are often localized to numerous coexisting subdomains that overlap only partially, e.g. Pdr5, Pdr12 and Yor1 proteins (MDR pumps) involved in multidrug resistance as efficient drug exporters [21].

As mentioned above, ergosterol is necessary for the regulation of membrane permeability and fluidity, and for regulating the activity of membrane transporters [16]. Thus, due to its indispensable role in yeast physiology, ergosterol and its biosynthesis became major targets in the development of antifungal drugs over the last sixty-five years [2224]. Some of the drugs used for the treatment of both systemic and superficial fungal infections specifically block ergosterol synthesis and simultaneously have only a small effect on the host cholesterol synthesis. Allylamines inhibit squalene epoxidase (encoded by ERG1), whereas morpholines block two separate steps, C-14 sterol reduction (by the product of ERG24) and C-8 isomerization (by the enzyme encoded by ERG2). Erg11p, catalyzing the demethylation of lanosterol, is a target of azoles, the most widely used and most numerous group of antifungal drugs [2324]. Polyenes (nystatin, amphotericin B) selectively interact with the final product of the pathway, ergosterol, and form membrane pores resulting in cell death [22].

The aim of this work was to estimate how changes in sterol composition influence various physiological parameters, growth capacities and tolerance to various stresses in S. cerevisiae cells, as well as identify a promising candidate among the enzymes involved in ergosterol biosynthesis for the development of new antifungal drugs.

Materials and Methods

Yeast strains

The S. cerevisiae strains used in this study are listed in Table 1. For intracellular pH measurement, we transformed BY4741 and erg mutants with the pHl-U plasmid [25], which enables the expression of pHluorin (a modified version of green fluorescent protein sensitive to pH) [26]. We prepared several independent erg6Δ strains by deletion of the ERG6 gene in BY4741 with the loxP-KanMX-loxP cassette [27], using the primers ScERG6-KanMX-F and ScERG6-KanMX-R. Successful integration of the cassette and deletion of ERG6 was verified by diagnostic PCR. All primers used for deletion and verification are listed in S1 Table. Three independent transformants with the correctly integrated cassette were obtained and verified to exhibit the same phenotypes. One representative of these strains was used in subsequent experiments.

Multicopy plasmids, YEpPDR5 and pGRUPDR5, were constructed for the production of Pdr5p or Pdr5p fused with green fluorescent protein (GFP) at the C-terminus under the control of a constitutive NHA1 promoter. The plasmids YEpPDR5 and pGRUPDR5 are derivatives of YEp352 [28] and pGRU1 [29], respectively. The fragments containing PDR5 were amplified from the genomic DNA of S. cerevisiae BY4741 by PCR with the primers listed in S1 Table. The PCR products were inserted into pNHA1-985 [30] (for YEpPDR5) and pNHA1-985GFP [30] (for pGRUPDR5) using homologous recombination, correct integration of PDR5 was verified by diagnostic PCR.

Media and growth assays

Cells were regularly grown at 30°C on YPD (1% yeast extract, 2% peptone, 2% glucose, 2% agar for solid media) or YNB (0.67% yeast nitrogen base without amino acids, 2% glucose, 2% agar for solid media) media supplemented with Brent Supplement Mix (BSM) after autoclaving. For measurements of intracellular pH, in order to diminish the background fluorescence, cells were cultivated in YNB-pH medium (0.17% yeast nitrogen base without riboflavin and folic acid (MP Biomedicals), 0.4% ammonium sulphate, 2% glucose) supplemented with BSM without uracil. For the selection of S. cerevisiae erg6Δ::loxP-kanMX-loxP transformants, G418 was added to YPD medium at a final concentration of 900 μg/mL.

Growth phenotypes of the strains in the presence of salts and drugs were tested both on solid and in liquid media. For testing lithium tolerance, cells growing overnight in liquid media were diluted to OD600 = 0.2 in YPD with 100 mM LiCl or without LiCl and cultivated at 30°C. The OD600 was measured at 1 h intervals. The plotted values of relative growth after 22 h cultivation are the means ± SD of three independent experiments. To compare the resistance of strains to antifungal drugs, the growth in liquid media was monitored in a 96-well plate reader Elx808 (BioTek) for 24 h at 30°C. 100 μL of YPD media in a well was inoculated with 2 μL of cell suspension OD600 = 1. The OD595 was measured at 1 h intervals. Growth curves were obtained in duplicates in a broad range of drug concentrations and repeated twice, representative results are shown. The plotted values of relative growth after 16 h cultivation are the means ± SD.

Drop tests were performed with fresh cells of each tested strain resuspended in sterile distilled water and adjusted to the same initial OD600 = 0.6. Tenfold serial dilutions were prepared, and 3 μL aliquots of each dilution were spotted on appropriate YPD or YNB agar plates supplemented as indicated in the text. Plates were incubated at 30°C for several days and photographed daily. Each drop test was performed in two parallels and repeated at least three times, representative results are shown.

Disc diffusion tests were performed as previously described [31] for estimating 1) the toxicity of antifungal drugs and 2) the activity of MDR pumps in erg mutants. Yeast cells grown to the exponential phase in liquid YPD medium were washed twice with distilled water and resuspended in 10 mM citrate-phosphate buffer (pH 6.0). They were then diluted into top agar (1% yeast extract, 2% peptone, 2% glucose, 1% agar) to OD600 = 0.2 and poured onto YPG plates (1% yeast extract, 2% peptone, 2% glycerol, 2% agar). Drug solutions (2 μL) at the concentrations indicated in the text were spotted onto paper discs laid on top of the agar. The plates were photographed after 2 days at 30°C and the diameters of the growth inhibition zones were measured. To determine the activity of the Pdr5 and Snq2 MDR pumps in erg strains, fluconazole was added to the discs together with the specific substrates of the pumps (FK506 for Pdr5p, NQO (4-nitroquinoline N-oxide) for Snq2p). Representative results of three independent experiments are shown.

Measurement of relative membrane potential (diS-C3(3) assay)

The relative membrane potential of yeast cells was estimated by a fluorescence assay based on the potential-dependent redistribution of the fluorescence probe diS-C3(3) (3,3’-dipropylthiacarbocyanine iodide) [3233], as described in [31]. Cells from the early exponential growth phase were harvested, washed twice with distilled water and resuspended in an assay buffer to OD600 = 0.2 and the probe was added to a final concentration of 2 × 10−8 M. Fluorescence emission spectra (λex = 531 nm, λem = 560–590 nm) of the cell suspensions were measured in an ISS PC1 spectrofluorimeter equipped with a xenon lamp. The staining curves recorded the dependence of the fluorescence emission maximum wavelength λmax at the time of staining. Representative results of three independent experiments are shown.

Cell size measurements

Cell diameter was estimated for cells growing in YPD to the early exponential growth phase. The cell size was measured before and 20 s after the addition of NaCl (final concentration 1 M) to the sample. A cell counter (CASY model TT; Roche Innovatis AG) with a 60 μm capillary was used. The experiment was repeated four times, each time 3–5 × 104 cells were analyzed for each strain and each set of conditions. Intervals containing the most typical 60% of the cell population were visualized using a box plot diagram with the mean diameter from the observed interval (2.5–9 μm) inside the box. Average results are shown ± SD.

Measurement of intracellular pH

Intracellular pH (pHin) was estimated using the pH-sensitive green fluorescent protein ratiometric pHluorin as described previously [2526,34]. Briefly, cultures expressing cytosolic pHluorin were excited with 400/30 or 485/20 nm light, and the emission was registered at 516/20 nm in a Synergy HT reader (BioTek). In all experiments, the background fluorescence of a wild-type culture not expressing pHluorin was subtracted from both signals independently, before the ratio of the two signals was determined. The pHin was measured 20 min after the addition of NaCl (1 M final concentration) or a corresponding volume of water (as a control) to cell suspensions. The pHin signal was calibrated using washed cells permeabilized with digitonin (300 μg/mL) in phosphate-buffered saline (PBS) for 10 min. Cells were collected by centrifugation, washed with PBS and resuspended to an OD600 of 0.5 in citrate-phosphate buffers with pH values ranging from 5.6 to 7.6 in 96-well microtitre plates. The emission ratios at 516 nm upon excitation at 400 and 485 nm were determined after 30 min of incubation of permeabilized cells in calibration buffers and plotted against the corresponding buffer pH. All pHin measurements were repeated three times (7–16 replicates in each experiment), pHin values are represented as means ± SD.

Fluorescence microscopy

Yeast strains with pGRUPDR5 plasmid were grown to the exponential growth phase in YNB medium supplemented with BSM without uracil and observed with a fluorescence microscope (Olympus AX70).

Statistical analysis

The statistical analyses were performed with SigmaPlot 13. Differences caused by salt stress or antifungal drugs were statistically described using a paired t-test, i.e. a comparison of the values before and after the addition of salt to each strain, or by ANOVA and subsequent post hoc test for finding significant differences among yeast strains.

Results and Discussion

Changes in the sterol composition of the plasma membrane affect growth phenotypes and membrane potential

We studied the impact of deletions of genes from the final steps in the biosynthesis of ergosterol (ERG6, ERG2, ERG3, ERG5, ERG4) on the physiological function of the Saccharomyces cerevisiae plasma membrane. For our study, we used EUROSCARF strains from the KanMX deletion library constructed in the BY4741 background and prepared the erg6Δ mutant. Three independent erg6Δ candidates were verified to have the same growth phenotypes. Further, one representative of these mutants was used. This erg6Δ strain exhibited the slowest growth compared to the other tested erg strains (S1 Fig), and indicated that the product of ERG6 represents a weak spot in ergosterol biosynthesis.

One of the first indicators of plasma membrane damage, due to changes in the properties or lipid and protein content of the plasma membrane, is the inability to maintain plasma-membrane potential. To elucidate whether the accumulation of sterols differing from ergosterol in the plasma membrane of erg mutants affects the level of membrane potential, we used a diS-C3(3) assay [33]. This assay is based on a cationic potentiometric probe, which is able to sensitively reflect very fine changes in the plasma-membrane potential, such as those caused by membrane lateral microdomain structures [35] or by the altered transport activity of mutated versions of the Trk1 potassium uptake system [36]. According to the diS-C3(3) staining of cells, the erg mutants divided into three groups (Fig 2A). While the erg5Δ strain exhibited almost wild-type level of relative membrane potential (only with a very slight hyperpolarization compared to the parental strain); deletion of the other four genes, and mainly ERG6 or ERG4, had a crucial effect on plasma membrane integrity which resulted in a very rapid probe uptake. They were strongly hyperpolarized, the staining curves had steep inclinations and the equilibrium intracellular concentrations of diS-C3(3) were achieved within 10 minutes of staining (Fig 2A). The erg3Δ and erg2Δ mutants exhibited a less dramatic impairment of membrane function accompanied by a lower hyperpolarization, the influx of the probe into these strains was slower, and the final λmax equilibrium was lower than in erg4Δ and erg6Δ cells.

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Fig 2. Strains with hyperpolarized membranes are less tolerant to LiCl and cationic drugs.

(A) Relative membrane potential of BY4741 (black circles), erg2Δ (red squares), erg3Δ (green triangles), erg4Δ (yellow triangles), erg5Δ (blue diamonds) and erg6Δ (cyan hexagons) cells estimated with diS-C3(3) fluorescence probe. (B) Relative growth in liquid YPD medium supplemented with 100 mM LiCl (growth in YPD medium without LiCl = 100%). The P values (*P < 0.05, **P < 0.001) denote statistically significant differences from the wild-type strain. (C) Growth on solid YPD media supplemented with LiCl, hygromycin B and tetramethylammonium (TMA) after 1 day of incubation.

https://doi.org/10.1371/journal.pone.0139306.g002

It is important to note that the fluorescence response of diS-C3(3) to membrane potential is influenced by the activity of the Pdr5 and Snq2 MDR pumps, which actively expel the probe from the cells [37]. It is well known that changes in the composition of the plasma membrane negatively affect the function of many transporters [16,18,38], and thus the observed differences in staining curves (Fig 2A) might be partly due to the different activity of MDR pumps. To verify whether the observed differences in staining reflect purely the hyperpolarization of the membrane, or a decreased activity of MDR pumps, or a combination of both, we performed a series of experiments. First, we complemented the fluorescence measurements of membrane potential with growth assays with lithium chloride in liquid and solid media (Fig 2B and 2C). Toxic lithium cations enter into the cells non-specifically according to the plasma-membrane potential and are actively eliminated from the cytosol by two types of plasma-membrane exporters, Ena1-5 ATPases and the Nha1 cation/H+ antiporter, or by the intracellular Nhx1 cation/H+ antiporter which sequestrates them into the vacuoles [39]. Differences in the relative growth of wild type and erg mutant strains in liquid YPD medium supplemented with 100 mM LiCl (Fig 2B) were in good agreement with the results obtained by diS-C3(3) assay, and confirmed the hyperpolarization of the erg2Δ, erg3Δ, erg4Δ and erg6Δ plasma membranes. The strain lacking ERG6 exhibited the poorest growth in the presence of lithium of all the erg mutants. This hypersensitivity to Li+ has been observed previously [40]. The lithium hypersensitivity of erg6Δ mutants was attributed to increased rates of cation influx and not decreased rates of efflux [40], which also corresponds to the hyperpolarization of the cell plasma membrane. Our results, indicating hyperpolarization of the membranes of at least four erg mutants, were further verified on solid media with LiCl and two cationic drugs, hygromycin B and tetramethylammonium (TMA). It is presumed that an abnormal sensitivity to these toxic cations does not reflect the activity of MDR pumps, but only a change in the plasma-membrane potential of cells [41]. We observed a similar-looking pattern of yeast sensitivity to the presence of lithium and cationic drugs in the growth media (Fig 2C). The wild-type and erg5Δ strains were the most resistant strains, due to their normal or only slightly increased membrane potential, whereas the erg6Δ, erg4Δ, erg2Δ and erg3Δ strains were sensitive to all three tested compounds in proportion to the level of hyperpolarization of their membranes.

Erg mutants differ in their tolerance to hyperosmotic stress caused by NaCl and in their intracellular pH

To further characterize the effects of erg mutations, we estimated two other physiological parameters which might be affected by altered plasma-membrane composition, intracellular pH and cell tolerance to hyperosmotic stress. As shown in Fig 3A, wild-type BY4741 strain, together with the erg5Δ, tolerated a high external concentration of NaCl much better than the other erg mutants. The exposure of yeast cells to saline stress implied exposure to both specific cation toxicity and osmotic stress. Sodium, similarly to lithium, enters cells in a non-specific manner and is actively exported via Ena ATPases and the Nha1 cation/H+ antiporter [39]. The intracellular accumulation of sodium in high concentrations is lethal because of its ability to replace necessary potassium cations and to inhibit specific metabolic pathways [39,42]. Lower resistance of the erg2Δ, erg3Δ, erg4Δ and erg6Δ strains to hyperosmotic stress is independently demonstrated by their inability to grow in the presence of high concentrations of glucose and sorbitol (Fig 3A). High extracellular osmotic pressure is accompanied by a transient loss of intracellular water visible as cell shrinkage. Fig 3B and 3C show that the addition of 1 M NaCl to cell suspensions diminished the cell size of all strains. The shrinkage of mutants from the earlier steps of ergosterol biosynthesis was greater than the shrinkage of erg4Δ and wild-type strains; Fig 3C), which suggested that the native elasticity/rigidity of the membranes of these mutants was severely disturbed. Almost the same level of shrinkage of BY4741 and erg4Δ cells (Fig 3C) was surprising, due to the great difference in their tolerance to NaCl in drop tests (Fig 3A). The sensitivity of erg4Δ cells to sodium cations is markedly connected to their higher (inside negative) relative membrane potential (Fig 2A) which represents a driving force for sodium influx. On the other hand, the ergosterol precursor accumulated in the membranes of erg4Δ cells probably conferred them with a similar elasticity/rigidity to that provided by ergosterol in the wild-type cells (Fig 3C). This result is in agreement with the hypothesis that, during their evolution, the structure of sterol molecules was progressively improved in order to increase their resistance to environmental pressures [1]. It also is worth noting that only the deletion of ERG4 resulted in a significant increase (P < 0.05) in cell size under non-stressed conditions (Fig 3B, empty boxes). YPD-grown cells of all the other mutants had a size similar to those of BY4741. This result is probably related to the earlier observation that ERG4 is required for proper cell morphology, especially shape remodelling and cell fusion during yeast mating [5,8]. Taken together, the results obtained with high concentrations of NaCl, glucose and sorbitol showed, that it is not only the tolerance to toxic sodium cations that differs among the erg mutants, but also their responses to increased osmotic pressure vary according to the sterols present in their membranes.

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Fig 3. Effect of osmotic stress.

(A) Growth on solid YPD medium supplemented with NaCl (recorded after 2 days), with glucose and sorbitol (recorded after 6 days), or adjusted to low pH with tartaric acid (recorded after 1 day). (B) Cell size before (empty boxes) and 20 s after the addition of 1 M NaCl (hatched boxes). The P values (*P < 0.01, **P < 0.001, ***P < 0.0001 based on paired t-test) reflect a statistically significant change in cell size after osmotic shock. (C) The shrinkage of cells after osmotic shock caused by NaCl in % (initial size of cells before exposure to 1 M NaCl = 100%). (D) Intracellular pH of cells expressing pHluorin 20 min after the addition of 33 μL of H2O (control, empty bars) or 33 μL of 4 M NaCl (final concentration 1 M, hatched bars). The P values (*P < 0.05 based on paired t-test) reflect a statistically significant drop in pH after the addition of NaCl.

https://doi.org/10.1371/journal.pone.0139306.g003

As we assumed that changes in the membrane’s physical properties (mainly fluidity and potential) affect the activity of plasma-membrane transporters, and as a result the uptake of nutrients and thus the overall cell metabolism, we measured the intracellular pH with the use of pHluorin expression. We observed a significantly lower (P < 0.05) intracellular pH in all erg mutants exponentially growing in YNB-pH (Fig 3D, empty bars). Further, we tested whether the observed levels of salt tolerance in the mutants and the wild type correlated with the ability to maintain intracellular pH. Indeed, erg mutants had problems maintaining pHin homeostasis upon NaCl stress, they exhibited a considerable drop in pHin, bigger than in the wild-type strain after 20 min treatment with 1 M NaCl (Fig 3D, compare empty and hatched bars). The highest acidification of the cytosol occurred in the strains with the most hyperpolarized plasma membranes, erg6Δ (ΔpHin = 0.24 ± 0.01) and erg4Δ (ΔpHin = 0.23 ± 0.05). Hyperpolarization was the reason for the higher sensitivity of the erg4Δ and erg6Δ cells to toxic cations (Figs 2 and 3A), and it also resulted in a deeper drop in pHin upon NaCl stress. The observed acidification of the cytosol upon salt stress is most probably connected to plasma-membrane proteome changes. Upon the addition of 1 M NaCl, a significant decrease in the abundance of 24 proteins in the S. cerevisiae plasma membrane was observed, and the Pma1 H+-ATPase, which is the main system pumping protons out of cells, was among them [42]. Decreased levels of Pma1p activity in the plasma membrane after salt stress, documented by the acidification of the cytosol (Fig 3D), could be favourable for wild-type cells exposed to toxic sodium ions. A decrease in the activity [31] or amount [42] of Pma1p results in a reduction in the membrane potential (relative depolarization) and a concomitant decrease in the potential-driven influx of toxic sodium cations. On the other hand, the results obtained with erg mutants suggest that the above decrease in Pma1p activity at the plasma membrane is not enough to counteract the hyperpolarization brought about by the changes in sterol composition and hence membrane properties. Moreover, erg mutants differ not only in their ability to maintain pHin homeostasis upon NaCl stress, but also in the sensitivity to low extracellular pH (Fig 3A). The most sensitive to acidic stress were the erg2Δ, erg3Δ and erg6Δ mutants, whereas the erg5Δ strain grew similarly as the wild type.

Erg mutants differ in their susceptibility to antifungal agents

In comparison to the parental BY4741 strain, most of the erg mutants were more sensitive to salt stress or cationic drugs and the level of their sensitivity was connected to the relative hyperpolarization of their plasma membrane (Fig 2 and Fig 3A). We also tested the susceptibility of erg mutants to six antifungal drugs with different structures and mechanisms of action (Fig 4 and S2 Fig). Cycloheximide inhibits protein synthesis due to its binding to eukaryotic ribosomes [43], nystatin binds to ergosterol within the cell membrane to generate pores, causing cell membrane leakage and loss of cytoplasmic content [22,44], and imidazoles (clotrimazole, ketoconazole) and triazoles (fluconazole, itraconazole) act as inhibitors of ergosterol synthesis [24]. Disc diffusion tests showed that the erg6Δ, erg4Δ and erg3Δ strains were more sensitive to cycloheximide than the wild type (Fig 4). The mutant lacking ERG4 was also slightly more sensitive to nystatin than the parental strain, but the deletion of ERG2, ERG6 and to a lesser extent ERG3 conferred a resistance to this polyene, probably due to a lower affinity of this drug for fecosterol, zymosterol and episterol, respectively, which are accumulated in these mutants. The most susceptible strains to azoles were erg6Δ, erg4Δ and erg2Δ (Fig 4). The heterogeneous sensitivity of the tested erg mutants was probably not only influenced by the higher permeability of their membranes for these drugs, but it also suggested a distinct functioning of their MDR pumps.

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Fig 4. Growth inhibition zones of cells exposed to antifungal drugs.

Red frames indicate strains less tolerant to drugs than the wild type, green frames indicate more tolerant strains than the wild type. Diameter of paper discs was 6 mm. The P values (*P < 0.05, **P < 0.01, ***P < 0.001) denote statistically significant differences from the wild-type strain.

https://doi.org/10.1371/journal.pone.0139306.g004

Changes in the sterol composition of the plasma membrane affect the activity of Pdr5p

To investigate how changes in sterol content influenced the ability of Pdr5p and also Snq2p to export drugs from cells, we performed a series of experiments. As mentioned above, the diS-C3(3) fluorescence probe is a substrate of both these pumps, as is CCCP (carbonyl cyanide 3-chlorophenylhydrazone) [31]. Thus in the presence of CCCP, the efflux of the probe via the Pdr5 and Snq2 pumps is inhibited (competitive inhibition between the two substrates) and the cell staining increases. In our experiments, CCCP was only able to effectively block the export of the probe from wild-type, erg5Δ, pdr5Δ and snq2Δ cells (Fig 5A), which suggested that at least one of the two MDR pumps was fully functional in these cells. We did not observe any similar increase in λmax after the addition of 10 μM CCCP to erg4Δ, erg6Δ, erg2Δ and erg3Δ cells (Fig 5B) which indicated a broken activity of the MDR pumps in these strains. As the deletion of the ERG4, ERG6, ERG2 and ERG3 genes significantly altered the cell’s ability to export the fluorescence probe, which is a substrate of at least these two MDR pumps, we used several known substrates of these two pumps to determine whether Pdr5p and Snq2p were influenced by changes in the membrane composition in the same way. Whereas CCCP, fluconazole and the diS-C3(3) probe are substrates of both the Snq2 and Pdr5 pumps [31,37,45], the immunosuppressant FK506 is a specific substrate of Pdr5p [46] and the mutagen 4-nitroquinoline N-oxide (NQO) is a specific substrate of Snq2p [47].

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Fig 5. Activity of Pdr5 and Snq2 pumps.

Changes in diS-C3(3) staining of (A) wild-type BY4741 (black circles), erg5Δ (blue diamonds), pdr5Δ (pink squares), snq2Δ (violet hexagons) and (B) erg2Δ (red squares), erg3Δ (green triangles), erg4Δ (yellow triangles) and erg6Δ (cyan hexagons) cells after addition of 10 μM CCCP (full symbols); control (empty symbols). (C) Changes in diS-C3(3) staining of wild-type cells (grey and black symbols) after addition of CCCP or FK506: 5 μM CCCP (diamonds), 10 μM CCCP (squares), 20 μM CCCP (inverted triangles), 10 μM FK506 (hexagons), 100 μM FK506 (triangles), control (circles) in comparison with staining of pdr5Δ (pink symbols) and snq2Δ cells (violet symbols): 10 μM CCCP (squares), 10 μM FK506 (hexagons), control (circles). (D) Changes in diS-C3(3) staining of wild-type (black circles), erg2Δ (red squares), erg3Δ (green triangles), erg4Δ (yellow triangles), erg5Δ (blue diamonds), erg6Δ (cyan hexagons), pdr5Δ (pink squares) and snq2Δ (violet hexagons) cells after addition of 100 μM FK506 (full symbols); control (empty symbols). Arrows with dotted lines indicate addition of compounds. (E) Growth inhibition zones of cells exposed to 30 mM FK506, 6.5 mM fluconazole, 5 mM NQO and their combinations.

https://doi.org/10.1371/journal.pone.0139306.g005

First we compared the inhibition of the probe efflux by the addition of CCCP or FK506 in the wild-type cells and in the pdr5Δ and snq2Δ mutants. While 10 μM CCCP was sufficient for the inhibition of the probe export, as is evident from a concentration-dependent increase in λmax after the exposure of cells to CCCP, even a tenfold higher concentration of FK506 was not able to cause a similar effect (Fig 5C). This result confirmed that CCCP effectively inhibited the probe export via both MDR pumps, as is also visible from the staining curves of pdr5Δ and snq2Δ cells exposed to CCCP. On the other hand, FK506 only affected Pdr5p (see Fig 5C; a small increase of diS-C3(3) staining of snq2Δ cells after addition of 10 μM FK506). The activity of Snq2 pump was unchanged by this drug (documented in Fig 5C by no change in staining after FK506 addition to pdr5Δ cells), and it was fully able to compensate the FK506-blocked probe export via Pdr5p in the wild-type cells. A similar result, i.e. no effect of FK506 addition was also observed in all erg mutants (Fig 5D). This result indirectly suggested that Snq2p was fully functional, in contrast to Pdr5p. Although some studies minimized the importance of the sterol composition of plasma membrane for the proper functioning of MDR pumps [48], it is generally assumed that the members of this protein family require close contact with neighbour components of the membrane to engage in their regular transport activity, as was demonstrated for Pdr5p [49] or Pdr12p [3]. This close interaction between MDR transporters and the surrounding sterols is limited in erg mutants, which mainly accumulate bended sterols instead of flat ergosterol in their membranes. In other words, the presence of double bonds in the aliphatic tail determines the planarity of the sterol molecules might affect, together with sphingolipids [3], the efflux capabilities of MDR pumps (Fig 1).

To confirm the results obtained in fluorescence measurements, we performed disc diffusion tests (Fig 5E and S3 Fig) and assessments of relative growth in liquid media (S4 Fig) with fluconazole as a substrate of both Pdr5p and Snq2p, FK506 as a specific substrate of Pdr5p, and NQO as a specific substrate of Snq2p. Pdr5p did not exhibit the same activity in all strains, because an increase in the size or clarity of the growth inhibition zones was visible in the presence of FK506, fluconazole and their combination in the erg2Δ, erg3Δ, erg4Δ and erg6Δ mutants (indicated by black frames in Fig 5E and red frames in Fig 4; the statistical analysis of the diameters of growth inhibition zones is shown in S3 Fig) compared to the growth inhibition zones of the parental strain BY4741, erg5Δ and snq2Δ mutants. In contrast to Pdr5p, Snq2p seemed to be fully functional in all strains, because the same size of zones was observed in the presence of NQO and its combination with fluconazole in all erg mutants and the wild type (white ellipses in Fig 5E). The results obtained by disc diffusion tests were confirmed by measurement of relative growth in liquid media. Obtained data are summarized in S4 Fig. Both approaches highlighted the significantly reduced activity of Pdr5p in erg6Δ and erg4Δ mutants. Since it is thought that Pdr5p is localized to ergosterol-rich domains of the plasma membrane [21], changes in the ergosterol content of the plasma membrane as a consequence of the deletion of genes involved in ergosterol biosynthesis have a significant influence on its function, whereas Snq2p seems to be less sensitive to changes in its microenvironment (Fig 5). Similarly, MDR transporters exhibit different lipid affinities in the pathogenic yeast C. albicans, where the inability to synthesize ergosterol leads to a mislocalization of Cdr1p and affects its functionality, whereas another MDR transporter, Mdr1p, remains functional and properly localized within the plasma membrane [50].

We were interested whether the lower activity of Pdr5p observed in several erg mutants resulted from a mislocalization and lower content of this transporter in their plasma membranes. To elucidate this possibility we constructed plasmids enabling overproduction and visualization (GFP-tagging) of Pdr5p. Then, the production and subcellular localization of Pdr5p were observed by monitoring the fluorescence emitted by the fused GFP in the wild type and erg mutants (Fig 6A). Green ring-shaped fluorescence at the cell surface was detected in all strains containing the pGRUPDR5 plasmid. The results indicated successful overproduction and correct localization of Pdr5p. Though deletion of ERG genes did not affect the localization of Pdr5p, the PDR5 overexpression did not improve significantly the cell capacity to export the fluorescence probe in all strains (an example is shown in Fig 6B). Only in the case of the erg2Δ and erg3Δ strains, Pdr5p overproduction improved slightly the capacity to export the probe (diminished level of diS-C3(3) staining of erg2Δ and erg3Δ cells overexpressing Pdr5p, Fig 6B and 6C). Both Erg2p and Erg3p change the B-ring of sterol molecule whereas other enzymes (Erg6, Erg5 and Erg4) modify the side chain of the sterol molecule as shown in Fig 1. This experiment showed that in spite of the correct localization of Pdr5p in erg mutants, its activity is lower than in the wild type, and the Pdr5p overexpression can improve the capacity to export the fluorescence probe only in erg2Δ and erg3Δ cells.

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Fig 6. Overexpression of PDR5.

(A) Deletion of ERG genes does not affect localization of Pdr5p fused with GFP (expressed from pGRUPDR5). The scale bar is 5 μm. (B) diS-C3(3) staining of wild-type BY4741 (black circles), erg2Δ (red squares), erg3Δ (green triangles) and erg4Δ (yellow triangles) cells transformed either with YEpPDR5 (overexpression of Pdr5p; full symbols) or YEp352 (empty plasmid; empty symbols). (C) Difference of Δλmax between staining curves of cells transformed with YEp352 (empty plasmid) and YEpPDR5 illustrates an increase in the probe export caused by the Pdr5 overexpression. Values were calculated from panel B after 30 min of staining.

https://doi.org/10.1371/journal.pone.0139306.g006

In summary, it is evident that the much higher diS-C3(3) staining of erg2Δ, erg3Δ, erg4Δ and erg6Δ mutants observed in the initial experiments (Fig 2A), was due to a combination of two effects–a hyperpolarization of the plasma membrane, and a lower activity of Pdr5p.

We found that the mutants, lacking genes encoding the final steps of ergosterol biosynthesis, differ in a number of parameters. Besides hyperpolarization of their membranes and a connected higher sensitivity to toxic alkali-metal cations and cationic drugs, we also observed differences in their response to high osmotic pressure and the ability to maintain a favourable intracellular pH upon osmotic-stress conditions. Moreover, we obtained a strong indication that the activity of one of the main MDR pumps in S. cerevisiae, Pdr5p, is strongly affected by the changed sterol composition of the plasma membrane.

In almost all the performed experiments, the phenotypes of the erg4Δ and erg6Δ mutants were the most different from the parental-strain phenotypes, suggesting that the accumulation of ergosterol precursors ergosta-5,7,22,24(28)-tetraenol and zymosterol, respectively, changes the properties of S. cerevisiae plasma membrane more significantly than the accumulation of other precursors. Thus ERG6 and ERG4 genes and their protein products may become useful antifungal targets for a new generation of inhibitors of ergosterol biosynthesis. ERG6 is especially interesting, because it encodes sterol C-24 methyltransferase, which is not involved in cholesterol biosynthesis in mammalian cells. The deletion of the ERG6 gene is neither lethal in S. cerevisiae nor in C. albicans [51], nevertheless it results in a series of serious effects. Besides those shown in our study, they include e.g. the inability to import tryptophan and utilize respiratory energy sources, and a hypersensitivity to a number of metabolic inhibitors [16,5152]. The administration of inhibitors of Erg6p would make the pathogenic yeast hypersensitive to currently known and established antifungal agents as well as to new compounds. Because of the increased drug access produced by inhibitors of the sterol C-24 methyltransferase, other antifungal drugs will become more effective and can be clinically applied at reduced dosages, limiting their possible negative side effects. Though some promising compounds with in vitro activities against Erg6p have already been synthesised (e.g. [5354]), much more work is still needed to develop new and efficient antifungal drugs targeting ergosterol biosynthesis, mainly due to a rapidly increasing number of clinical isolates resistant to classical ergosterol-pathway-targeted antifungal drugs [5556].

Supporting Information

S1 Fig. Growth of Saccharomyces cerevisiae wild-type BY4741 and isogenic erg mutant strains on solid media.

Tenfold serial dilutions of saturated cultures were prepared and 3-μL aliquots spotted onto YPD or YNB plates and incubated at 30°C. The erg6Δ strain is a new construct, see Table 1 and Materials and methods.

https://doi.org/10.1371/journal.pone.0139306.s001

(TIF)

S2 Fig. Relative growth in liquid YPD medium supplemented with antifungal drugs.

Cells were cultivated in the presence of (A) 2 nM cycloheximide, (B) 1 μM nystatin, (C) 0.1 μM clotrimazole, (D) 1 μM ketoconazole, (E) 5 μM fluconazole and (F) 0.2 μM itraconazole. Growth without drugs = 100%. The P values (*P < 0.05, **P < 0.01, ***P < 0.001) denote statistically significant differences from the wild-type strain.

https://doi.org/10.1371/journal.pone.0139306.s002

(TIF)

S3 Fig. Diameters of the growth inhibition zones.

The cells were exposed to (A) 30 mM FK506, (B) 6.5 mM fluconazole, (C) 5 mM NQO and their combinations (D) 6.5 mM fluconazole plus 30 mM FK506, (E) 6.5 mM fluconazole plus 5 mM NQO. Diameter of paper discs was 6 mm. The P values (*P < 0.05, **P < 0.01, ***P < 0.001) denote statistically significant differences from the wild-type strain.

https://doi.org/10.1371/journal.pone.0139306.s003

(TIF)

S4 Fig. Relative growth in liquid YPD medium supplemented with antifungal drugs.

Cells were cultivated in the presence of (A) 10 μM fluconazole, (B) 20 μM FK506, (C) 0.1 μM NQO and their combinations (D) 10 μM fluconazole plus 20 μM FK506 and (E) 10 μM fluconazole plus 0.1 μM NQO. Growth without drugs = 100%. The P values (*P < 0.05, **P < 0.01, ***P < 0.001) denote statistically significant differences from the wild-type strain.

https://doi.org/10.1371/journal.pone.0139306.s004

(TIF)

S1 Table. Oligonucleotides used in this study.

https://doi.org/10.1371/journal.pone.0139306.s005

(DOC)

Acknowledgments

We would like to thank Lydie Marešová for sharing the unpublished data with us.

Author Contributions

Conceived and designed the experiments: MK HS. Performed the experiments: MK. Analyzed the data: MK. Wrote the paper: MK HS.

References

  1. 1. Dupont S, Lemetais G, Ferreira T, Cayot P, Gervais P, Beney L. Ergosterol biosynthesis: a fungal pathway for life on land? Evolution. 2012;66: 2961–2968.
  2. 2. Caspeta L, Chen Y, Ghiaci P, Feizi A, Buskov S, Hallström BM, et al. Altered sterol composition renders yeast thermotolerant. Science. 2014;346: 75–78.
  3. 3. Guan XL, Souza CM, Pichler H, Dewhurst G, Schaad O, Kajiwara K, et al. Functional interactions between sphingolipids and sterols in biological membranes regulating cell physiology. Mol Biol Cell. 2009;20: 2083–2095.
  4. 4. Spanova M, Zweytick D, Lohner K, Klug L, Leitner E, Hermetter A. Influence of squalene on lipid particle/droplet and membrane organization in the yeast Saccharomyces cerevisiae. Biochim Biophys Acta. 2012;1821: 647–653.
  5. 5. Aguilar PS, Heiman MG, Walther TC, Engel A, Schwudke D, Gushwa N, et al. Structure of sterol aliphatic chains affects yeast cell shape and cell fusion during mating. PNAS. 2010;107: 4170–4175.
  6. 6. Heese-Peck A, Pichler H, Zanolari B, Watanabe R, Daum G, Riezman H. Multiple functions of sterols in yeast endocytosis. Mol Biol Cell. 2002;13: 2664–2680.
  7. 7. Jacquier N, Schneiter R. Mechanisms of sterol uptake and transport in yeast. J Steroid Biochem Mol Biol. 2012;129: 70–78.
  8. 8. Tiedje C, Holland DG, Just U, Höfken T. Proteins involved in sterol synthesis interact with Ste20 and regulate cell polarity. J Cell Sci. 2007;120: 3613–3624.
  9. 9. Klug L, Daum G. Yeast lipid metabolism at a glance. FEMS Yeast Res. 2014;14: 369–388.
  10. 10. Parks LW, Casey WM. Physiological implications of sterol biosynthesis in yeast. Annu Rev Microbiol. 1995;49: 95–116.
  11. 11. Weete JD, Abril M, Blackwell M. Phylogenetic distribution of fungal sterols. PLoS ONE. 2010;5: e10899.
  12. 12. Bard M, Sturm AM, Pierson CA, Brown S, Rogers KM, Nabinger S, et al. Sterol uptake in Candida glabrata: Rescue of sterol auxotrophic strains. Diagn Microbiol Infect Dis. 2005;52: 285–293.
  13. 13. Hazen KC, Stei J, Darracott C, Breathnach A, May J, Howell SA. Isolation of cholesterol-dependent Candida glabrata from clinical specimens. Diagn Microbiol Infect Dis. 2005;52: 35–37.
  14. 14. Xiong Q, Hassan SA, Wilson WK, Han XY, May GS, Tarrand JJ, et al. Cholesterol import by Aspergillus fumigatus and its influence on antifungal potency of sterol biosynthesis inhibitors. Antimicrob Agents Chemother. 2005;49: 518–524.
  15. 15. Wiseman H. Vitamin D is a membrane antioxidant. Ability to inhibit iron-dependent lipid peroxidation in liposomes compared to cholesterol, ergosterol and tamoxifen and relevance to anticancer action. FEBS Lett 1993;326:285–8.
  16. 16. Daum G, Lees ND, Bard M, Dickson R. Biochemistry, cell biology and molecular biology of lipids of Saccharomyces cerevisiae. Yeast. 1998;14: 1471–1510.
  17. 17. Lees ND, Skaggs B, Kirsch DR, Bard M. Cloning of the late genes in the ergosterol biosynthetic pathway of Saccharomyces cerevisiae–A review. Lipids. 1995;30: 221–226.
  18. 18. Malínský J, Opekarová M, Tanner W. The lateral compartmentation of the yeast plasma membrane. Yeast. 2010;27: 473–478.
  19. 19. Merzendorfer H, Heinisch JJ. Microcompartments within the yeast plasma membrane. Biol Chem. 2013;394: 189–202.
  20. 20. Mollinedo F. Lipid raft involvement in yeast cell growth and death. Front Oncol. 2012;2: 140.
  21. 21. Spira F, Mueller NS, Beck G, von Olshausen P, Beig J, Wedlich-Söldner R. Patchwork organization of the yeast plasma membrane into numerous coexisting domains. Nat Cell Biol. 2012;14: 640–648.
  22. 22. Marty A, Finkelstein A. Pores formed in lipid bilayer membranes by nystatin. J Gen Physiol. 1975;65: 515–526.
  23. 23. Fromtling RA. Overview of medically important antifungal azole derivatives. Clin Microbiol Rev. 1988;1: 187–217.
  24. 24. Shalini K, Kumar N, Drabu S, Sharma PK. Advances in synthetic approach to and antifungal activity of triazoles. Beilstein J Org Chem. 2011;7: 668–677.
  25. 25. Marešová L, Hošková B, Urbánková E, Chaloupka R, Sychrová H. New applications of pHluorin-measuring intracellular pH of prototrophic yeasts and determining changes in the buffering capacity of strains with affected potassium homeostasis. Yeast. 2010;27: 317–325.
  26. 26. Miesenböck G, De Angelis DA, Rothman JE. Visualizing secretion and synaptic transmission with pH-sensitive green fluorescent proteins. Nature. 1998;394: 192–195.
  27. 27. Güldener U, Heck S, Fielder T, Beinhauer J, Hegemann JH. A new efficient gene disruption cassette for repeated use in budding yeast. Nucleic Acids Res. 1996;24: 2519–2524.
  28. 28. Hill JE, Myers AM, Koerner TJ, Tzagoloff A. Yeast/E. coli shuttle vectors with multiple unique restriction sites. Yeast. 1986;2: 163–167.
  29. 29. Myers AM, Tzagoloff A, Kinney DM, Lusty CJ. Yeast shuttle and integrative vectors with multiple cloning sites suitable for construction of lacZ fusions. Gene. 1986;45: 299–310.
  30. 30. Kinclová O, Ramos J, Potier S, Sychrová H. Functional study of the Saccharomyces cerevisiae Nha1p C-terminus. Mol Microbiol. 2001;40: 656–668.
  31. 31. Hendrych T, Kodedová M, Sigler K, Gášková D. Characterization of the kinetics and mechanisms of inhibition of drugs interacting with the S. cerevisiae multidrug resistance pumps Pdr5p and Snq2p. Biochim Biophys Acta. 2009;1788: 717–723.
  32. 32. Denksteinová B, Gášková D, Heřman P, Večeř J, Malínský J, Plášek J, et al. Monitoring of membrane potential changes in S. cerevisiae by diS-C3(3) fluorescence. Folia Microbiol. 1997;42: 221–224.
  33. 33. Gášková D, Brodská B, Heřman P, Večeř J, Malínský J, Sigler K, et al. Fluorescent probing of membrane potential in walled cells: diS-C3(3) assay in Saccharomyces cerevisiae. Yeast. 1998;14: 1189–1197.
  34. 34. Orij R, Postmus J, Ter Beek A, Brul S, Smits GJ. In vivo measurement of cytosolic and mitochondrial pH using a pH-sensitive GFP derivative in Saccharomyces cerevisiae reveals a relation between intracellular pH and growth. Microbiology. 2009;155: 268–278.
  35. 35. Heřman P, Večeř J, Opekarová M, Veselá P, Jančíková I, Zahumenský J, et al. Depolarization affects the lateral microdomain structure of yeast plasma membrane. FEBS Journal. 2015;282: 419–434.
  36. 36. Herrera R, Álvarez MC, Gelis S, Kodedová M, Sychrová H, Kschischo M, et al. Role of Saccharomyces cerevisiae Trk1 in stabilization of intracellular potassium content upon changes in external potassium levels. Biochim Biophys Acta. 2014;1838: 127–133.
  37. 37. Čadek R, Chládková K, Sigler K, Gášková D. Impact of the growth phase on the activity of multidrug resistance pumps and membrane potential of S. cerevisiae: effect of pump overproduction and carbon source. Biochim Biophys Acta. 2004;1665: 111–117.
  38. 38. Ren B, Dai HQ, Pei G, Tong YJ, Zhuo Y, Yang N, et al. ABC transporters coupled with the elevated ergosterol contents contribute to the azole resistance and amphotericin B susceptibility. Appl Microbiol Biotechnol. 2014;98: 2609–2616.
  39. 39. Ariño J, Ramos J, Sychrová H. Alkali metal cation transport and homeostasis in yeasts. Microbiol Mol Biol Rev. 2010;74: 95–120.
  40. 40. Welihinda AA, Beavis AD, Trumbly RJ. Mutations in LIS1 (ERG6) gene confer increased sodium and lithium uptake in Saccharomyces cerevisiae. Biochim Biophys Acta. 1994;1193: 107–117.
  41. 41. Barreto L, Canadell D, Petrezsélyová S, Navarrete C, Marešová L, Peréz-Valle J, et al. A genomewide screen for tolerance to cationic drugs reveals genes important for potassium homeostasis in Saccharomyces cerevisiae. Eukaryot Cell. 2011;10: 1241–1250.
  42. 42. Szopinska A, Degand H, Hochstenbach J-F, Nader J, Morsomme P. Rapid response of the yeast plasma membrane proteome to salt stress. Mol Cell Proteomics. 2011;10: M111.009589.
  43. 43. Käufer NF, Fried HM, Schwindinger WF, Jasin M, Warner JR. Cycloheximide resistance in yeast: the gene and its protein. Nucleic Acids Res. 1983;11: 3123–3135.
  44. 44. Kodedová M, Sigler K, Lemire BD, Gášková D. Fluorescence method for determining the mechanism and speed of action of surface-active drugs on yeast cells. BioTechniques. 2011;50: 58–63.
  45. 45. Anderson JB, Sirjusingh C, Parsons AB, Boone C, Wickens C, Cowen LE, et al. Mode of selection and experimental evolution of antifungal drug resistance in Saccharomyces cerevisiae. Genetics. 2003;163: 1287–1298.
  46. 46. Kralli A, Yamamoto KR. An FK506-sensitive transporter selectively decreases intracellular levels and potency of steroid hormones. J Biol Chem. 1996;271: 17152–17156.
  47. 47. Decottignies A, Lambert L, Catty P, Degand H, Epping EA, Moye-Rowley WS, et al. Identification and characterization of SNQ2, a new multidrug ATP binding cassette transporter of the yeast plasma membrane. J Biol Chem. 1995;270: 18150–18157.
  48. 48. Emter R, Heese-Peck A, Kralli A. ERG6 and PDR5 regulate small lipophilic drug accumulation in yeast cells via distinct mechanisms. FEBS Letters. 2002;521: 57–61.
  49. 49. Kaur R, Bachhawat AK. The yeast multidrug resistance pump, Pdr5p, confers reduced drug resistance in erg mutants of Saccharomyces cerevisiae. Microbiology. 1999;145: 809–818.
  50. 50. Prasad R, Singh A. Lipids of Candida albicans and their role in multidrug resistance. Curr Genet. 2013;59: 243–250.
  51. 51. Jensen-Pergakes KL, Kennedy MA, Lees ND, Barbuch R, Koegel C, Bard M. Sequencing, disruption, and characterization of the Candida albicans sterol methyltransferase (ERG6) gene: drug susceptibility studies in erg6 mutants. Antimicrob Agents Chemother. 1998;42: 1160–1167.
  52. 52. Parks LW, Smith SJ, Crowley JH. Biochemical and physiological effects of sterol alterations in yeast–A review. Lipids. 1995;30: 227–230.
  53. 53. Chung S-K, Lee K-W, Kang HI, Yamashita C, Kudo M, Yoshida Y. Design and synthesis of potential inhibitors of the ergosterol biosynthesis as antifungal agents. Bioorg Med Chem. 2000;8: 2475–2486.
  54. 54. Kristan K, Lanišnik Rižner T. Steroid-transforming enzymes in fungi. J Steroid Biochem Mol Biol. 2012;129: 79–91.
  55. 55. Diekema D, Arbefeville S, Boyken L, Kroeger J, Pfaller M. The changing epidemiology of healthcare-associated candidemia over three decades. Diagn Microbiol Infect Dis. 2012;73: 45–48.
  56. 56. Pfaller MA, Diekema DJ. Epidemiology of invasive candidiasis: a persistent public health problem. Clin Microbiol Rev. 2007;20: 133–163.