Dap1p, a Heme-Binding Protein That Regulates the Cytochrome P450 Protein Erg11p/Cyp51p in Saccharomyces cerevisiae

Yeast strains and growth conditions.All strains were isogenic with W303 (leu2-3,112 his3-11,15 ura3-1 ade2-1 trp1-1 can1-100 rad5-535) (32). For the strains used in this study, the rad5-535 allele was replaced with the wild-type RAD5 gene by crossing and was tested by PCR as described elsewhere (6). All genetic manipulations and transformations with plasmid DNA were performed as previously described (13). The yeast strains RCY407-12d and RCY409-2a (both wild type) and RCY407-1d and RCY409-4b (both dap1Δ::LEU2) have been described previously (14). The erg2Δ strain JRY7187 was a gift from Jasper Rine's laboratory.

Plasmids.The plasmids used in this study are summarized in Table 1. The ERG11 gene was amplified using the primers ERG11-300F-Hind and ERG11+1650R-Bam. The sequences of all primers used in this study are available at the website www2.mc.uky.edu/Pharmacology/rjc_research.asp . The PCR product was digested with HindIII and BamHI and ligated to the plasmid YEplac195 (12), which was digested with the same enzymes. The resulting plasmid (called pRH4) contained the entire ERG11 open reading frame, along with 300 bp of its upstream sequence. The ERG1 gene was amplified by PCR using the primers ERG1-290F-Bam and ERG1+1524R-Hind, and the resulting PCR product was subcloned into the plasmid YEplac195, forming the plasmid pJM60.

For epitope tagging the ERG11 open reading frame, the entire ERG11 gene was amplified using W303a genomic DNA as a template with the primers ERG11-300F-Hind and ERG11+1650-MYCR-Bam. The PCR product was digested with BamHI and HindIII and cloned into the corresponding sites of the single-copy plasmid pRS316. The resulting plasmid was called pRH7.

For DAP1 mutagenesis, DAP1 was amplified by PCR using the primers DAP-200F and DAP+470R and subcloned into the plasmid pCR3.1 (Invitrogen), forming the plasmid pRC31. The Dap1p-D91G mutation was created with the ExCite mutagenesis kit (Stratagene) using the manufacturer's instructions and the primers DAP1-D91G-F and DAP1+265R with pRC31 as a template, forming the plasmid pRC34. After confirming the integrity of the D91G mutation, the DAP1-D91G mutant was subcloned into the XhoI and EcoRI sites of the plasmid pRS313, forming the plasmid pRC39. The wild-type gene was similarly cloned into pRS313, forming the plasmid pRC41.

For production of a Dap1p fusion protein with glutathione S-transferase, the DAP1 open reading frame from bp 4 to 459 was amplified by PCR using the primers DAP1+4F-Bgl and DAP1+457R-Xho, with W303a genomic DNA as a template. The PCR product was then subcloned into the BamHI and XhoI sites of the plasmid pGEX-4T-1 (Amersham), forming the plasmid pGC5. The DAP1-D91G mutant was subcloned similarly. To construct the plasmid encoding the Dap1p protein containing the D91G mutation, the mutated DAP1 open reading frame was amplified using the same primers with pRC34 as a template and subcloned into the same sites of pGEX-4T-1. The resulting plasmid was called pGC4. The sequences of all cloned genes were confirmed by automated sequencing using core facilities at the University of North Carolina at Chapel Hill and the University of Cincinnati.

Fusion protein purification and measurement of heme binding.Bacteria harboring the pGC4 and pGC5 plasmids were grown to an A ₆₀₀ of 0.3, treated with isopropyl-β-d-thiogalactopyranoside for 4 h, and collected by centrifugation. Bacteria were lysed by incubation in the B-PER reagent (Pierce) and bound to glutathione-agarose columns for 2 to 20 h at 4°C. The columns were then washed three times with phosphate-buffered saline. A 100-μg aliquot of fusion protein was liberated with 1 U of thrombin (Fisher) by incubation at 37°C for 2 h with agitation. The glutathione-agarose column was then removed by centrifugation, and the A ₄₀₀ of the supernatant was measured in a microtiter plate reader. Measurements were performed in triplicate using three separate aliquots of fusion protein. At the onset of the experiment, the absorption spectrum from 300 to 700 nm for Dap1p was determined using a Spectronics Genesys 5 spectrophotometer (Spectronics Instruments), before and after the addition of 0.5 mg of sodium dithionate (a kind gift of Todd Porter, originally from Sigma).

Growth assays.The ability of various strains to grow on itraconazole and MMS was determined using a spotting assay as previously described (14). Briefly, overnight cultures were serially diluted 1:10 and spotted on plates lacking histidine or uracil, as indicated in the figure legends. Where indicated, plates also contained 0.01 to 0.015% MMS (Sigma) or were overlaid with 0.2 mg of itraconazole (Ortho Biotech)/ml. For some experiments, 13 μg of hemin (Sigma; diluted from a 1.3-mg/ml stock in 50% ethanol and 0.1 N NaOH in water)/ml was added to the plates prior to testing viability. Before performing the spotting assay, yeast strains were maintained for 3 to 5 days on yeast extract-peptone-dextrose (YPD) plates containing 13 μg of hemin/ml to ensure uptake of heme.

To calculate 50% lethal dose (LD₅₀) values, liquid yeast cultures were grown overnight and then diluted to an A ₆₀₀ of 0.1, and 50 μl of diluted culture was added to a 96-well culture dish. An additional 50 μl of medium containing 0 to 0.016% MMS was then added to each well, and the cells were grown at 30°C with shaking until the A ₆₀₀ of cells that were not treated with MMS reached 0.5. The A ₆₀₀ of all of the wells was then measured using a Thermo Lab System Multi-Scan MCC/340 microtiter plate reader. The effect of each dose of MMS on each strain was measured in triplicate, and the LD₅₀ was calculated using Microsoft Excel. The standard deviation of three independent measurements was compared for the separate strains. To validate the assay, we calculated the LD₅₀ values for wild-type (RCY409-2a), dap1Δ (RCY409-4b), and dun1Δ (RCY144-1a) strains. The LD₅₀ for the wild-type strain was 0.013% MMS, while the LD₅₀ for dap1Δ was 0.005% and for dun1Δ it was 0.003%. The difference between wild-type and dap1Δ strains was highly significant (P = 0.0004; t test).

Sterol analysis.Sterol profiles were analyzed using the KOH-n-heptane extraction procedure of Molzahn and Woods (25) as previously described (14). Cells were grown in liquid medium and harvested for sterol analysis at an A ₆₀₀ of 0.8. Cells were pelleted, washed once with distilled water (dH₂O), and resuspended in 4.5 M KOH-60% ethanol. Cells were then refluxed in a round-bottom flask at 88 to 90°C for 1 h. A 95% ethanol solution was then added, and the cells were refluxed for an additional hour and then cooled to room temperature. The mixture was then extracted with n-heptane and dH₂O, and the n-heptane layer was analyzed by gas chromatography. Each sample was injected twice, and a representative profile is shown. Sterols were analyzed by gas chromatography with a Hewlett-Packard HP5890 series II chromatograph as described elsewhere (14). In some cases, cells were pregrown for 50 generations on YPD plates containing 13 μg of hemin/ml and then grown in liquid YPD containing hemin for sterol analysis.

Protein analysis.Yeast cells were diluted and grown to early log phase, then centrifuged, washed once with water, and lysed by incubation in the Y-PER reagent (Pierce) containing 1 mM phenylmethylsulfonyl fluoride and 10 μg of the protease inhibitors aprotinin and leupeptin (Fisher)/ml. Cells were incubated for 5 min at room temperature and then clarified by centrifugation at 14,000 × g for 10 min at 4°C. For each sample, 25 μg was separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis in a 4 to 20% acrylamide gradient gel, transferred to Immobilon P (Millipore), probed with an appropriate antibody, and detected by chemiluminescence using the West Pico substrate (Pierce). The antibody to the Myc epitope tag sequence was 9B11 from Cell Signaling. The antibody to α-tubulin was developed by J. Frankel and was obtained from the Developmental Studies Bank at the University of Iowa under the auspices of the National Institute of Child Health and Human Development. The polyclonal antibody to Erg11p was raised to the 15 amino-terminal amino acids of Erg11p and was used at a dilution of 1:1,000.

Reverse transcriptase PCR (RT-PCR).RNA was isolated from log-phase yeast cells by phenol-chloroform extraction as described elsewhere (www.microarrays.org ). Following extraction and analysis by agarose gel, 6 μg of RNA was converted to cDNA by using SuperScript II reverse transcriptase (Invitrogen), according to the manufacturer's instructions. Following cDNA synthesis, the ERG11 transcript was amplified using the primers ERG11+350F and ERG11+642R. The SCS2 and TUB1 transcripts were not altered by sterol pools and were used as controls for RNA loading. SCS2 expression was analyzed using the primers SCS2+300F and SCS2+480R, and TUB1 was analyzed using the primers TUB1+1F and TUB1+220R. The PCRs were prepared as a common pool and then divided into equal thirds in separate tubes. During the PCR, the tubes were removed at three different cycle numbers to ensure that the transcript was being monitored during the linear phase of the PCR. PCRs were separated on a 1.5% agarose 1000 gel (Invitrogen) and photographed.

Dap1p is a heme-1 domain protein that binds to heme.Dap1p is part of a widely conserved group of proteins that share sequence similarity with cytochrome b ₅ (23), a heme-binding protein that activates multiple cytochrome P450 proteins (30). Because of the similarity between Dap1p and cytochrome b ₅, we analyzed heme binding by Dap1p purified in Escherichia coli. When glutathione S-transferase fusion proteins with Dap1p were bound to glutathione-agarose columns, they had a brown appearance (data not shown), a characteristic of heme-binding proteins. Purified Dap1p was liberated from the column (Fig. 2A) and exhibited strong absorbance at 400 nm, indicating heme binding. Furthermore, when the reducing agent dithionate was added to Dap1p, the absorbance peak shifted to 420 nm (data not shown). We conclude that Dap1p binds to heme, like the related protein cytochrome b ₅ and the Dap1p homologue IZAg (24).

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FIG. 2.

Dap1p is a heme-binding protein, and heme binding is required for Dap1p-mediated damage resistance. (A) The highly conserved Asp91 residue of Dap1p was mutated to Gly, and wild-type Dap1p and Dap1p^D91G proteins were purified as fusion proteins with glutathione S-transferase. (B) Dap1p bound to heme (left bar), while the Dap1p^D91G lost heme-binding activity (right bar). (C) DAP1 complements the dap1Δ phenotype, while DAP1 ^D91G does not. The entire DAP1 open reading frame, along with 300 bp of promoter sequence, was subcloned in the single-copy plasmid pRS313, as was the DAP1 ^D91G mutant. Wild-type cells (rows 1 to 3 and 7 to 9) and dap1Δ strains (rows 4 to 6 and 10 to 12) were transformed with either a control plasmid (VEC., rows 1, 4, 7, and 10), a DAP1-containing plasmid (rows 2, 5, 8, and 11), or the DAP1 ^D91G-containing plasmid (rows 3, 6, 9, and 12). Cells were grown on medium lacking histidine to force retention of the plasmids. Growth was analyzed by spotting 10-fold dilutions on plates lacking histidine (top panel) or on the same plates containing 0.01% MMS (bottom panel).

Cytochrome b ₅ binds to heme through a binding pocket composed of four α-helices (30). The sequences bridging these helices are highly conserved between cytochrome b ₅ and the Dap1p-related proteins. We mutated the conserved residue of Dap1p, Asp91, to glycine and purified the Dap1p^D91G fusion protein. Like the wild-type protein, Dap1p^D91G was readily purified (Fig. 2A, lane 2), but Dap1p^D91G-containing agarose columns were not brown in color, and Dap1p^D91G exhibited no absorbance at 400 nm. Figure 2B shows the relative absorbances of Dap1p and Dap1p^D91G. Heme-binding measurements were performed in triplicate, and the difference in heme binding between Dap1p and Dap1p^D91G has been confirmed in multiple protein preparations. We conclude that the D91 residue is required for heme binding by Dap1p.

The D91G mutation within the Dap1p heme-1 domain inactivates Dap1p.To assess the biological importance of heme binding for Dap1p, we subcloned the wild-type DAP1 and mutant DAP1 ^D91G genes into single-copy CEN plasmids for expression in yeast. The resulting plasmids were called DAP1-CEN and DAP1 ^D91G-CEN. Both plasmids were introduced into wild-type and dap1Δ yeast strains and tested for damage resistance. MMS had little effect on wild-type strains containing a control plasmid, DAP1-CEN, or DAP1 ^D91G (Fig. 2C, rows 7 to 9). In dap1Δ strains, cells containing the control plasmid were sensitive to MMS (Fig. 2C, row 10), while DAP1-CEN complemented the dap1Δ phenotype (Fig. 2C, row 11). In contrast, the DAP1 ^D91G-CEN plasmid was unable to complement the dap1Δ phenotype (Fig. 2C, row 12). We conclude that sequences within Dap1p that are required for heme binding are critical for Dap1p function in damage resistance.

MMS sensitivity in dap1Δ strains is suppressed by exogenous hemin.Next, we examined whether heme is the primary target for Dap1p or whether the heme-1 motif is a structural domain utilized by ligands other than heme, as suggested previously (23). We tested the model that heme binding is the target of Dap1p by adding exogenous hemin to wild-type and dap1Δ cells and then measuring MMS sensitivity.

To ensure uptake of hemin, wild-type and dap1Δ cells were maintained for approximately 50 generations on solid YPD medium, with or without hemin. Cells were then diluted and tested for growth on YPD, YPD containing hemin, YPD plus MMS, and YPD containing hemin plus MMS (Fig. 3). Pregrowth on solid YPD medium containing hemin suppressed MMS sensitivity in dap1Δ strains (Fig. 3C and D, bottom rows), while the growth of these strains was unaffected by hemin under normal conditions (Fig. 3B). As a control, we maintained a dun1Δ strain on similar plates containing hemin and measured MMS resistance. DUN1 (damage uninducible) encodes a protein kinase that is required for signaling following DNA damage, and dun1Δ strains are damage sensitive (38). Growth on hemin had no effect on MMS resistance in the dun1Δ strain (data not shown), indicating that suppression of MMS sensitivity by heme is not a general property of damage resistance genes.

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FIG. 3.

MMS sensitivity in dap1Δ cells is suppressed by the addition of exogenous heme. Wild-type (RCY409-2a) and dap1Δ (RCY409-4b) cells were pregrown on YPD plates or YPD plates containing 13 μg of hemin/ml and then spotted on YPD plates (A), YPD plates containing 13 μg of hemin/ml (B), YPD plates containing 0.015% MMS (C), or YPD plates containing 13 μg of hemin/ml and 0.015% MMS (D). Pregrowth on hemin had no detectable effect on the growth of dap1Δ cells but suppressed MMS sensitivity in dap1Δ cells.

To quantitate the ability of hemin to suppress MMS sensitivity in dap1Δ strains, we measured the LD₅₀ in dap1Δ strains before and after hemin addition. The LD₅₀ is the dose of MMS at which 50% of the culture survives. As expected, dap1Δ cells had a lower LD₅₀ value than wild-type cells (0.005% MMS versus 0.013%) (see Materials and Methods), and hemin suppressed MMS sensitivity in dap1Δ cells (0.005 versus 0.013%; P = 0.00002). We conclude that dap1Δ strains are deficient in MMS resistance because of defects in the targeting of heme to specific reactions or pathways.

Next, we examined sterol intermediates by gas chromatography in wild-type and dap1Δ cells in the absence and presence of hemin. Pregrowth in hemin had little effect on the accumulation of sterol intermediates in wild-type cells, except for a minor decrease in squalene concentrations (Fig. 4A and B). In dap1Δ cells grown on YPD, we detected elevated lanosterol, ergosta-5,7-dienol, episterol, and squalene levels (compare Figs. 4A and C), as observed in previous studies (14). While most of the sterol intermediates were detected as single peaks, ergosta-5,7-dienol coeluted closely with episterol and appeared as a shoulder on the episterol peak. Because of this overlapping elution profile, we have designated the episterol and ergosta-5,7-dienol peaks as a single peak. When dap1Δ cells were maintained on heme-containing plates, we detected decreased levels of lanosterol and squalene (compare Fig. 4C and D). We also detected elevated levels of zymosterol (Fig. 4C and D) and modest increases in ergosta-5,7-dienol and episterol (Fig. 4C and D), sterol intermediates that are downstream of lanosterol (Fig. 1). These findings indicate that Erg11p/Cyp51p/lanosterol demethylase function is attenuated in dap1Δ mutants and is partially restored by the addition of heme.

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FIG. 4.

Heme suppresses sterol synthetic defects in dap1Δ mutant strains. Wild-type (A and B) and dap1Δ (C and D) cells were maintained in YPD medium or in YPD supplemented with 39 μg of hemin/ml, and sterol intermediates were analyzed by gas chromatography. As previously noted, dap1Δ cells contain increased levels of lanosterol (la) and squalene (sq) relative to wild-type cells and decreased levels of zymosterol (zy) (compare panels A and C) (see also reference 14). The dap1Δ mutants also had increased levels of episterol and ergosta-5,7-dienol (di+ep). Growth in heme-containing medium caused a decrease in squalene and lanosterol in dap1Δ cells (D) and an increase in zymosterol. Similar changes were observed in cells maintained in 13 μg of hemin/ml.

ERG11 is a multicopy suppressor of sterol biosynthesis and damage sensitivity in dap1Δ mutants.In some cases, overexpression of a downstream component of a genetic pathway is capable of suppressing a mutation in an upstream gene (13). For that reason, we tested the hypothesis that multiple copies of ERG11 would suppress dap1Δ phenotypes. The entire ERG11 open reading frame, along with 300 bp of upstream promoter sequence, was cloned into the multiple-copy plasmid YEplac195, resulting in the plasmid YEp-ERG11. Wild-type or dap1Δ mutants expressing the ERG11 plasmid did not have altered growth under normal conditions (Fig. 5A, upper panel, rows 2 and 4). In contrast, YEp-ERG11 completely suppressed the sensitivity of dap1Δ mutants to the antifungal agent itraconazole, a clinical Erg11p inhibitor (Fig. 5A, middle panel, compare rows 3 and 4). YEp-ERG11 also increased itraconazole resistance in wild-type cells (Fig. 5A, middle panel, rows 1 and 2). The result is consistent with Erg11p acting downstream of Dap1p in conferring itraconazole resistance.

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FIG. 5.

Multiple copies of ERG11/lanosterol demethylase, but not ERG1/squalene epoxidase, suppress sensitivity of dap1Δ mutants to azole inhibitors and MMS-induced damage. (A) Log-phase cells were serially diluted 1:10 and spotted onto plates containing synthetic medium lacking uracil (upper panel), the same medium overlaid with 0.2 mg of itraconazole/ml (middle panel), or the same medium containing 0.015% MMS (lower panel). The strains tested were RCY432 (the wild-type strain RCY409-2a harboring the plasmid YEplac195 [wild-type + YEp]), RCY433 (RCY409-2a harboring the ERG11 multiple copy plasmid pRH4 [wild-type + YEp-ERG11]), RCY434 (the dap1Δ strain RCY409-4b harboring the plasmid YEplac195 [dap1Δ + YEp]), and RCY435 (RCY409-4b harboring pRH4 [dap1Δ + YEp-ERG11]). Multiple copies of ERG11 had little effect on normal growth of wild-type or dap1Δ strains on SD-ura (upper panel). As expected, dap1Δ strains harboring YEplac195 were sensitive to itraconazole and MMS (middle and lower panels, third rows). Multiple copies of ERG11 suppressed the sensitivity of dap1Δ strains to itraconazole and MMS (middle and lower panels, fourth rows). (B) Cells were grown, spotted, and diluted similarly to those shown in panel A. The strains tested were RCY409-2a/wild-type cells harboring the control plasmid YEplac195 (rows 1, wild-type + VEC.), the ERG1 multicopy plasmid pJM60 (rows 2, wild-type + YEp-ERG1), and the ERG11 multicopy plasmid pRH4(rows 3, wild-type + ERG11), and the RCY409-4b/dap1Δ strain harboring the control plasmid YEplac195 (rows 4, dap1 + VEC.), the ERG1 multicopy plasmid pJM60 (rows 5, dap1 + Yep-ERG1), and the ERG11 multicopy plasmid pRH4 (rows 6, dap1 + ERG11). While multiple copies of ERG11 suppressed MMS sensitivity in dap1Δ cells, multiple copies of ERG1 did not.

In addition to suppressing itraconazole sensitivity, YEp-ERG11 suppressed the partial ergosterol synthetic defect in dap1Δ cells. Gas chromatographic analysis of wild-type and dap1Δ strains harboring YEplac195 demonstrated elevated levels of squalene and lanosterol and decreased levels of zymosterol in dap1Δ cells (Fig. 6, compare panels A and C), as expected from previous experiments (14). As noted for Fig. 4, we detected elevated levels of episterol and ergosta-5,7-dienol in dap1Δ mutants, suggesting a defect in the reaction catalyzed by Erg5p. The YEp-ERG11 plasmid did not have a marked effect on sterol synthesis in wild-type cells, although there was a detectable increase in squalene (Fig. 6, compare panels A and B). In contrast, YEp-ERG11 led to profound changes in sterol levels in dap1Δ cells, with levels of zymosterol and lanosterol resembling those in wild-type cells (Fig. 6D). YEp-ERG11 also led to an elevated accumulation of episterol and ergosta-5,7-dienol, further suggesting defective Erg3p and Erg5p function in dap1Δ cells.

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FIG. 6.

Multiple copies of ERG11 suppress sterol synthetic defects in dap1Δ mutant cells. The levels of sterol synthetic intermediates in four yeast strains were measured by gas chromatography. (A and B) Wild-type cells harboring either a control plasmid (A) or the multicopy ERG11 plasmid YEp-ERG11 (B) contained normal levels of sterol synthetic intermediates. However, we note that ERG11 overexpression caused a marked accumulation of squalene (B). (C) Cells lacking Dap1p contained elevated levels of lanosterol, ergosta-5,7-dienol, episterol, and squalene. (D) Overexpression of ERG11 decreased the levels of lanosterol in dap1Δ cells but caused an increase in the lanosterol metabolites ergosta-5,7-dienol, episterol, and zymosterol. The elevated levels of squalene observed in dap1Δ cells (C) (14) were unaffected by ERG11 overexpression (D).

Because YEp-ERG11 restored sterol biosynthesis in dap1Δ cells, we examined the effect of YEp-ERG11 on damage resistance. We compared growth of dap1Δ mutants harboring YEplac195 and YEp-ERG11 on plates containing 0.015% MMS. YEp-ERG11 completely suppressed MMS resistance in dap1Δ mutants, while the same strain harboring YEplac195 (Fig. 5, VEC) was sensitive to the drug (Fig. 5A, lower panel, compare rows 3 and 4). Furthermore, the LD₅₀ of MMS was significantly different in dap1Δ cells containing the YEplac195 and YEp-ERG11 plasmids (0.005 versus 0.018% MMS; P = 0.0008). Similar to the itraconazole sensitivity assay, YEp-ERG11 also caused a slight increase in MMS resistance in wild-type cells (Fig. 5A, lower panel, rows 1 and 2). We conclude that ERG11 is an efficient multicopy suppressor of damage sensitivity and sterol synthetic defects in dap1Δ mutants.

ERG1, ERG5, and CYB5 are not multicopy suppressors of dap1Δ damage sensitivity.Sterol synthesis profiles suggested that Erg1p and Erg5p may require Dap1p, because elevated levels of their substrates were detected in dap1Δ mutants (Fig. 4 and 6) (14). We cloned ERG1 and ERG5 into a multicopy plasmid, YEplac195, forming the plasmids YEp-ERG1 and YEp-ERG5, and introduced the plasmids into wild-type and dap1Δ strains. Unlike ERG11, multiple copies of ERG1 and ERG5 did not confer MMS resistance to dap1Δ cells (Fig. 5B, lower panel, fifth row, and data not shown). ERG1 overexpression suppressed the accumulation of squalene in dap1Δ cells (data not shown) but did not affect lanosterol accumulation, as expected from the order of the ergosterol synthetic pathway (Fig. 1). We conclude that Erg1p and Erg5p are not targets for Dap1p in MMS resistance.

Dap1p shares a heme-binding domain with the CYB5/cytochrome b ₅ protein (23). Like Dap1p, Cyb5p regulates resistance to azole antifungal agents (33), possibly because Cyb5p and Cyb5p reductase can substitute for the Erg11p reductase Ncp1p (20). Unlike ERG11, multiple copies of CYB5 did not suppress MMS or azole sensitivity in dap1Δ mutant cells (data not shown). We conclude that Dap1p and Cyb5p do not have redundant functions in MMS resistance.

Multiple copies of ERG11 do not suppress damage sensitivity in checkpoint mutants or sterol biosynthesis mutants downstream of ERG11.We examined the ability of the multicopy YEp-ERG11 plasmid to suppress MMS sensitivity in strains lacking the damage checkpoint proteins MEC1 (1, 36) and DUN1 (38). Strains harboring the mec1-21 and dun1Δ mutations are sensitive to MMS, and MMS sensitivity was not restored by ERG11 overexpression in these strains (data not shown). Thus, ERG11 is not a general suppressor of damage-sensitive mutants. Next, we examined the ability of YEp-ERG11 to suppress additional lesions in the sterol biosynthetic pathway. As expected from the work of other labs, erg2Δ mutants are sensitive to MMS (3), and we found that ERG11 overexpression did not suppress MMS sensitivity in erg2Δ strains (data not shown). Our results suggest that ERG11 suppresses damage sensitivity through the ergosterol synthetic pathway.

Dap1p is required for maintenance of Erg11p levels.The transcription of ERG11 is altered in response to oxygen, glucose, and heme (7). We analyzed the transcription of the ERG11 gene by RT-PCR in wild-type and dap1Δ cells to determine the extent to which Dap1p regulates ERG11 transcription. We used two different genes, SCS2 and TUB1, as controls for loading and analyzed ERG11 expression at multiple PCR cycles (Fig. 7A). The analysis was performed in triplicate. We conclude that DAP1 does not significantly alter ERG11 transcription.

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FIG. 7.

Dap1p is required for expression of the Erg11p protein. (A) Dap1p does not regulate ERG11 transcription. RNA was isolated from the strains RCY409-2a/wild type (lanes 1, 3, 5, 7, and 8) and RCY409-4b/dap1Δ (lanes 2, 4, 6, and 9) and reverse transcribed. ERG11 expression was analyzed by RT-PCR (upper band) with SCS2 gene transcription as a control for loading (lower panel). To ensure that samples were analyzed in the linear phase of the reaction, samples were withdrawn at 22, 25, and 28 cycles of the PCR. To control against PCR products arising from contaminating genomic DNA in the sample, parallel reactions in which RT was omitted from the reaction mixture were analyzed using the same procedure for 28 cycles of PCR. Lane 7 is identical to lane 8, but RT was added. (B) Two pairs of wild-type and dap1Δ strains from different genetic crosses were lysed, and expression of the Erg11p protein was analyzed by Western blotting. The strains RCY409-2a (lane 1), RCY-409-4b (lane 2), RCY407-12d (lane 3), and RCY407-1d (lane 4) were analyzed for Erg11p (upper panel) or tubulin as a loading control (lower panel). The presence of Dap1p in the strains is indicated, and the migration of a molecular mass marker is on the left side of the upper panel. Erg11p was decreased by 5.0- and 3.1-fold in the two dap1Δ strains compared to wild type. (C) The Erg11p open reading frame was cloned in frame with the myc epitope tag sequence on a single-copy plasmid, and wild-type (lanes 1 and 3) and dap1Δ (lanes 2 and 4) strains were transformed with either a control plasmid (lanes 1 and 2) or the Erg11p-myc-containing plasmid (lanes 3 and 4). The strains were lysed and analyzed by Western blotting with antibodies to myc (upper panel) and tubulin (lower panel). (D) Expression levels of Erg11p (top panel) or the loading control tubulin (bottom panel) were analyzed by Western blotting. The wild type (lanes 1 and 3) and dap1Δ strains (lanes 2 and 4) RCY409-2a and RCY409-4b, respectively, were grown in YPD medium (lanes 1 and 2) or YPD medium containing 13 μg of heme/ml for 1 h and then lysed and analyzed. Erg11p expression was decreased approximately fourfold in dap1Δ cells grown in YPD, while addition of heme restored Erg11p expression to wild-type levels (compare lanes 2 and 4).

Next, we analyzed protein samples from wild-type and dap1Δ strains by using an anti-Erg11p antibody. Erg11p levels were decreased approximately fourfold in dap1Δ haploid strains compared to matched wild-type strains from two separate genetic crosses (Fig. 7B, upper panel; lanes 1 and 3 contain proteins from wild-type cells and lanes 2 and 4 contain proteins from dap1Δ cells). In addition, a wild-type diploid strain had markedly higher Erg11p levels than a dap1Δ diploid strain constructed from progeny from the same genetic cross (data not shown).

To ensure that our assignment of the 55-kDa band to Erg11p was correct, we prepared a single-copy (CEN) plasmid containing the ERG11 open reading frame fused to the myc epitope tag and introduced this plasmid into wild-type and dap1Δ strains. As expected, Erg11p-myc migrated as a single 55-kDa band that was detected only in strains harboring the appropriate plasmid (Fig. 7C, upper panel, compare lanes 3 and 4 to control strains in lanes 1 and 2). Wild-type strains expressed Erg11p-myc at approximately fourfold-higher levels than a dap1Δ strain (Fig. 7C, upper panel, lanes 3 and 4), similar to the result shown in Fig. 7B. We conclude that Dap1p is required for wild-type expression levels of Erg11p.

Both addition of heme and ERG11 overexpression suppress MMS sensitivity in dap1Δ cells (Fig. 3 and 5). We examined whether heme addition affected Erg11p stability in dap1Δ cells by Western blotting with the anti-Erg11p antibody. As noted in Fig. 7B, Erg11p was expressed at lower levels in dap1Δ cells than in comparable wild-type cells (Fig. 7D, lanes 1 and 2). By growing the same cells in 13 μg of heme/ml for 1 h, we detected a sharp increase in Erg11p stability in dap1Δ cells (Fig. 7D, compare lanes 2 and 4). Our results are consistent with a model in which heme suppresses MMS sensitivity in dap1Δ cells by stabilizing Erg11p. However, we have not excluded the possibility that heme may alter the stability of proteins other than Erg11p.