Genome-wide analysis of intracellular pH reveals quantitative control of cell division rate by pHc in Saccharomyces cerevisiae
© Orij et al.; licensee BioMed Central Ltd. 2012
Received: 30 March 2012
Accepted: 26 September 2012
Published: 26 September 2012
Because protonation affects the properties of almost all molecules in cells, cytosolic pH (pHc) is usually assumed to be constant. In the model organism yeast, however, pHc changes in response to the presence of nutrients and varies during growth. Since small changes in pHc can lead to major changes in metabolism, signal transduction, and phenotype, we decided to analyze pHc control.
Introducing a pH-sensitive reporter protein into the yeast deletion collection allowed quantitative genome-wide analysis of pHc in live, growing yeast cultures. pHc is robust towards gene deletion; no single gene mutation led to a pHc of more than 0.3 units lower than that of wild type. Correct pHc control required not only vacuolar proton pumps, but also strongly relied on mitochondrial function. Additionally, we identified a striking relationship between pHc and growth rate. Careful dissection of cause and consequence revealed that pHc quantitatively controls growth rate. Detailed analysis of the genetic basis of this control revealed that the adequate signaling of pHc depended on inositol polyphosphates, a set of relatively unknown signaling molecules with exquisitely pH sensitive properties.
While pHc is a very dynamic parameter in the normal life of yeast, genetically it is a tightly controlled cellular parameter. The coupling of pHc to growth rate is even more robust to genetic alteration. Changes in pHc control cell division rate in yeast, possibly as a signal. Such a signaling role of pHc is probable, and may be central in development and tumorigenesis.
Cytosolic pH (pHc) determines the relative protonation state of all weak acid compounds of the cytosol and affects many, if not all, processes in the cell. It is known to affect redox equilibria , metabolic rates and energy storing or generating gradients [2, 3], protein interactions [4–7], as well as signal transduction [8–10], and it is an important thermodynamic constraint on metabolic reactions . Furthermore, pHc homeostasis is intricately connected with that of other cations, with membrane potentials, and therefore with cellular energy homeostasis [12, 13].
Only relatively recently, with the development of green fluorescent protein (GFP)-based pH sensors, has it become possible to study pH in live, unperturbed cells, in an organelle specific fashion [14–18]. The use of this technology is generating increased insight into intracellular pH (pHi) control, such as the interaction between plasma membrane and vacuolar proton transport [16, 19], and nutrient signaling and pHi control . That pHc itself directly controls signal transduction and cellular transcriptional responses to environmental conditions was shown recently. A decrease of pHc from 7 to 6.8, induced by carbon source depletion, abolishes the interaction of the transcription factor Opi1p with phosphatidic acid through direct protonation of the phosphate headgroup of this membrane phospholipid . Considering the known and emerging importance of this parameter, it is remarkable how little is understood of the genetic basis of its control. We decided to carefully study pHc in growing cultures of the yeast deletion collection , to determine the genes that are involved in pHc control during normal, fermentative growth on glucose. This revealed that pHc is controlled by the interplay of cation pumps and the mitochondria, even in fermenting cultures. Additionally, we determined that pHc quantitatively controls yeast cell division rate. Remarkably, deletion of 19 genes could abolish this control, suggesting that pHc functions as a true signal, transmitting information about external conditions to control cellular decisions.
pHc is dynamic during growth
Cytosolic pH of yeast cultures is not a static but a highly dynamic parameter. Re-addition of glucose to starved cells leads to a rapid acidification of the cytosol in approximately 30 seconds followed by an alkalinization to neutral pH before growth recommences [18, 21, 22]. This rapid acidification, which is believed to be the cause of initiation of glycolysis [10, 23], is followed by an alkalinization as a result of the activation of the plasma membrane H+-ATPase Pma1p [24, 25].
Identification of pHc mutants
We failed to identify several mutants that we expected to have an altered pHc. We separately tested several of these, among which were trk1, trk2, nha1, nhx1. In our analysis, cells growing on defined media with glucose available, these mutants did not have a significantly deviating pHc. We have shown before  that, in such conditions, a PMA1 hypomorph ygl007c and a trk1 deletion strain do not have a pHc phenotype, and that such a phenotype only becomes apparent when the cells are challenged with low external pH. At an external pH (pHex) of 3.0, trk1, trk2, nha1 and nhx1 had pHc values of 6.93 ± 0.02, 7.02 ± 0.06, 6.99 ± 0.01 and 7.08 ± 0.10, respectively (with average Z-values of -2.77, -0.99, -1.32 and 0.02), which indicates a significant pHc deviation for trk1 only. This suggests that, although the gene products have well defined functions in cation homeostasis, deletion of these genes when sufficient cellular energy can be generated does not cause a pHc decrease.
Profiling of mutants with aberrant pHc under additional stress conditions reveals involvement of vacuole and mitochondria in pHc control
Mitochondrial proton pumping functions, as well as functions related to mitochondrial biogenesis and inheritance, were strongly enriched, despite the fact that respiration is not required for energy generation during fermentative growth on glucose. To see if this mitochondrial role in pHc homeostasis is related to the role of the mitochondria in energy generation, we assessed the pHc of all pHc mutants during respiratory growth in glycerol- and ethanol-containing medium (Figure 3b). The average parent pHc on respiratory medium was reduced by 0.27 pH units, and similarly almost all mutants tested had a lower pHc on respiratory medium. However, only 13 of the 73 strains with a significantly low pHc on glucose were also significantly low during respiratory growth, when compared to wild type. Eleven of these (msf1Δ, aep3Δ, pet100Δ, atp7Δ, mss116Δ, mtg2Δ, mnn9Δ, plc1Δ, dep1Δ, rpl21aΔ, and snf2Δ) had extremely low growth rates on glycerol/ethanol medium, and were indeed previously shown to have severely reduced growth on respiratory media or to be respiratory growth deficient [28–30]. Only vps66Δ and kre28Δ had low pHc on respiratory and fermentative carbon sources but were able to grow relatively normally on respiratory media compared to fermentative conditions. The other 60 strains with low pHc during fermentative growth had normal or even high pHc during respiratory growth. This apparent rescue of most low pHc phenotypes shows that pHc regulation in fermenting cells is very different from that in respiring cells, as suggested before . Together, our data establish the major importance of the vacuole and mitochondria in pH control, and reveal these organelles as central controllers of cytosolic ion concentrations [16, 19, 31, 32].
pHc controls growth rate
To positively demonstrate that pHc dictates growth rate, we postulated that it should then be possible to titrate pHc, which should allow us to set the growth rate to the values predicted by the quantitative relationship previously determined (Figure 4a). In wild-type strains, the plasma membrane ATPase ensures pHc control in different pHex conditions [18, 33], and titration of pHex leads to only minute changes in pHc (Figure S1 in Additional file 3). However, in a mutant with a hypomorphic allele of PMA1 (pma1-007), with approximately 50% reduced plasma membrane ATPase levels and activity [7, 34], acidification of the culture medium with HCl from pH 5.0 to pH 2.0 resulted in a pHc decrease from 7.0 to 6.2 (Figure 4b), while nutrient abundance is not affected. Cultivation in these conditions revealed that growth was also progressively decreased (Figure 4c). Direct comparison of growth rate and pHc revealed that the growth rate was decreased exactly to the extent expected from the lowering of pHc (Figure 4d), thus showing that pHc determines the growth rate.
pHc appears to have a signaling role
Mutations that reduce growth control by pHc
Inositol phosphate biosynthetic process
Inositol phosphate biosynthetic process
Rho protein signal transduction
Lipid biosynthetic process
Fatty acid metabolic process
Retrograde transport, endosome to Golgi
Isoleucine biosynthetic process
Biological process unknown
Complex control of a simple parameter
It is becoming apparent that pHc is controlled not just by simply pumping protons out of the cytosol into the vacuole or across the plasma membrane. The pH of the various compartments is heavily influenced by that of others . Vacuolar ATPases are not only important for maintenance of the low pH in the secretory pathway, but also for control of cytosolic pH. This could be a buffering activity, a transient and rapid mode of removing protons from the cytosol, to be made permanent by true proton efflux. It should be noted, however, that a transient storage of protons in the secretory pathway or the vacuole conserves the energy in the cell as a membrane potential. Most of the components of the vacuolar ATPases have been identified based on the vma phenotype, which comprises the inability to grow at high extracellular pH and at high Ca2+ concentrations [40, 41]. It is remarkable, therefore, that not all vma mutants have a pHc phenotype at a pHex of 5.0, and of the ones that do, not all have a pHc phenotype at a pHex of 7.5 (2 out of 7). Similarly, we found very little correlation between our screen for pHc and a recent screen for mutations leading to deviating vacuolar pH, although conditions were different . This suggests that even if the mechanisms for pHc control share components with those for vacuolar pH control, the organelles control their pH independently.
While the role of vacuolar proton pumping in pHc homeostasis has been relatively well studied, the important role of the mitochondria is novel. In an analysis of mutations affecting the 'ionome' of yeast, a similar enrichment of both vacuolar and mitochondrial genes was observed , suggesting that the homeostasis of cations in general requires the proper function of both organelles. However, this analysis does not distinguish the organelle-specific ion concentrations. A role for mitochondria in pHc homeostasis is less surprising if one considers the fact that proton translocation over the mitochondrial inner membrane is the driving force for energy generation in mitochondria. However, in the glucose-rich conditions of our screen the mitochondrial respiratory chain is not required for energy generation in yeast. Still, we identified a large number of mutants in mitochondrial genes in which pHc was affected. The genes were classified as part of the proton translocating machinery and the mitochondrial respiratory chain, but also as involved in mitochondrial translation and biogenesis. The same mutations did not necessarily affect pHc in respiratory conditions, which suggests that the role of these genes in pHc homeostasis is indeed not linked to energy generation.
Clearly, the control of pHc in yeast, and in other eukaryotes [32, 43] is distributed over various organelles, as is control of organellar pH. Also, the same functions are not responsible for pHc control in different conditions. This shows that pHc is a seemingly simple outcome of diverse and intricate regulation. This renders pHc an excellent signal of cellular status.
pHc as a signal integrating multiple environmental cues to control growth
In yeast it has long been known that pHc transiently responds to the addition of nutrients [18, 23]. The transient pHc reduction upon glucose addition plays a role in the activation of the nutrient signaling, growth-promoting activation of protein kinase A . How exactly pHc functions in the activation of protein kinase A is not yet fully understood, but it is clear that a lowered pHc promotes the activity of the adenylate cyclase Cyr1p through the activity of Ira2p and Ras2p , and possibly also the increase in the affinity of Cyr1p for ATP upon a decrease in pHc . Additionally, the gradual decrease of pHc upon glucose depletion was shown to lead to inactivation of protein kinase A, through the disassembly of the vacuolar proton ATPases [10, 19]. Decrease of pHc upon glucose depletion also affects other signal transduction pathways. The activation of inositol biosynthetic gene transcription upon inositol depletion is inhibited in the absence of a proper energy source, through direct control of the activity of the transcriptional inhibitor Opi1p. This inhibitor is recruited to phosphatidic acid in membranes upon inositol depletion, directly binding to the negatively charged phospholipid. Upon pHc decrease the phosphate headgroup of the phospholipid is protonated, and Opi1p is released [7, 47]. Therefore, as phosphates can be protonated at physiological pHc values, and this can affect interactions with proteins, it is very likely that other phosphate groups, such as those on proteins or those on small metabolites, may be protonated and this protonation could then affect recognition by enzymes or effector proteins.
There is some evidence that pHc varies during the cell cycle [48, 49], but others have not been able to confirm this . We show that pHc quantitatively controls cell division rate. This may or may not be through cell cycle phase-dependent fluctuations. However, the fact that the changes in pHc that we observed are in the range at which phosphate groups can be protonated, and the observation that such protonation can interfere with protein interactions , would allow many opportunities for pHc interference with cell cycle signaling.
Previously, is has been shown that the Vip1p pyrophosphorylation of InsP6 is important for phosphate regulation of growth [51, 52]. Interestingly, they reveal an inhibitory interaction of inositol pyrophosphate with the alternative CDK Pho85p, suggesting that such interactions could control kinase function [39, 52]. We now show that Kcs1p-mediated pyrophosphorylation of InsP6 is important for pHc signaling to set growth rate. It is tempting to speculate that these inositol pyrophosphate species appear to integrate signals from two major regulatory metabolites to determine growth rate. Indeed, a recent publication shows that inositol pyrophosphates contribute to cellular energy control , which is completely in line with the potential role of pHc in nutrient status sensing. The authors find that inositol pyrophosphates affect mitochondrial function and fermentation rates to control cellular ATP content. This suggests that pHc, inositol pyrophosphates and mitochondria function in an interdependent network to control cell division, resource distribution, and therefore potentially the balance between growth and cellular robustness [53–57].
The implications of pHc as a signal for growth and more
In humans, pHc changes have been implicated in tumorigenic transformation and tumor growth and metastasis [58–60]. The reduction of oxygen availability in solid tumors causes a fermentative metabolism, described already in 1927 by Otto Warburg. This change leads to the production of lactate, which causes the acidification of the tumor exterior space and the surrounding tissue. Tumor cells themselves almost invariably overexpress pH homeostatic pumps [61, 62], leading to a selective advantage of transformed over non-transformed cells. Interestingly, our data suggest that the acidification of the non-transformed cells might result in a growth suppression, but also that the slightly alkaline tumor cell cytosol might have growth promoting activity. Indeed, it has been suggested that tumor alkalinization might already be a very early event in tumorigenic transformation , and an even slightly increased replication rate of the alkalinized cells could benefit the accumulation of mutations promoting the transformation to malignancy.
Intracellular pH is a determinant of the properties of the molecules that make up living cells, and changes in pHc rapidly and reversibly alter these properties. In yeast, pHc is highly dynamic. Although intracellular pH is hardly affected by changes in extracellular pH, it is affected by the changes occurring during normal growth on glucose (Figure 1), and decreases as a consequence of CO2 produced by cellular metabolism. In respiratory conditions, either after glucose depletion or during growth on glycerol- and ethanol-containing media, pH is much lower than during fermentation.
To understand the genetic basis of pHc control during growth on glucose, we expressed the pH-sensitive GFP pHluorin in all strains of the yeast haploid deletion collection. We analyzed pHc in liquid cultures of these strains during the exponential growth phase, and identified 177 mutants in which pHc deviated significantly from wild type. The genes affecting pHc control were strongly enriched for functions in the vacuole, including vacuolar proton pumping, but also for many mitochondrial functions, both in proton pumping and energy generation as well as in mitochondrial translation, biogenesis and inheritance. The fact that the same mutations did not lead to pHc alterations in respiratory conditions indicates that pHc control is condition dependent.
The most striking functional enrichment of the mutants was in very general growth-related functions. This could imply that pHc is reduced as a consequence of reduction in growth rate or as a consequence of the metabolic conditions that lead to a reduced growth rate, but it also opens up the possibility that growth rate is reduced as a consequence of the reduction in pHc. We note that while conditions that decrease growth rate also generally reduce pHc, mutations that reduce growth rate do not necessarily reduce pHc. Also, pHc responds much more rapidly to external conditions than growth rate does. This suggests that either environmental conditions affect pHc and metabolism that sets growth rate in parallel, or that pHc in fact controls growth rate. To distinguish between these two options, we titrated pHex with strong acid in cultures of the plasma membrane ATPase hypomorph pma1-007 that were otherwise unaffected in nutrient availability, and thereby reduced pHc. This indeed led to a reduction of growth rate, quantitatively matching the relationship between pHc and growth rate observed in wild type. This proves that pHc directly controls growth rate. A further analysis of the genetic basis of this control shows that it was relaxed in only 19 out of 177 mutants. The fact that pHc control can be relaxed demonstrates that pHc must function as a signal, whereas the fact that this signal is not properly sensed in only 19 mutants suggests that it has evolved to be robust to mutation, and therefore that it is central and important.
Indeed, there is evidence that similar control takes place in mammalian cells. Although a link between pH control and tumorigenesis has been established, most research in this field focuses on the acidified cell exterior, which appears to affect metastatic propensity . Very little is known about the role of the alkalinization of the cell interior. However, recent literature also suggests that, in mammalian cells too, pHc affects signal transduction [8, 9] and cell division rate [63–65]. The fact that we now show that cytosolic pH controls growth rate, and functions as a signal to do so, suggests that the relevance of pHc for growth control is conserved. How exactly this quantitative signal is controlled, and how it is transmitted to control the cell cycle, remains to be elucidated, but the involvement of the inositol pyrophosphate kinase Kcs1p, and of Plc1p gives promising targets for investigation.
Materials and methods
In all experiments strains were pre-cultured by transfer from solid medium to liquid and incubated overnight (o/n) in round-bottom 96-well microplates (Greiner Bio-One, Kremsmünster, Austria)) stacked in microplate holders (New Brunswick, Enfield, CT, USA) under constant shaking at 30°C in 200 μl low fluorescence synthetic defined monosodium glutamate medium buffered at pH 5.0 with 25 mM sodium citrate. This medium contained 1.7 g yeast nitrogen base without (w/o) ammonium sulfate, w/o folic acid, w/o riboflavin (MP Biochemicals, Santa Ana, CA, USA), 1 g L-glutamic acid sodium salt hydrate (Sigma-Aldrich, St. Louis, MO, USA), 2 g drop-out amino acids supplement powder mixture without uracil (Sigma-Aldrich; Acros Organics, Geel, Belgium; Thermo Fisher Scientific, Waltham, MA, USA), 20 g glucose (Thermo Fisher Scientific) and 7.35 g sodium citrate (Sigma-Aldrich) per liter. For pH titration experiments, strains were cultivated in 500 ml batch fermenters with a steady airflow (500 ml minute-1) and stirring rate (600 r.p.m.). The pH of batch fermenter cultures was controlled by titration with 0.2 M KOH using an Applikon ADI 1030 controller (Applikon Biotechnology, Foster City, CA, USA).
The plasmid pYES-PACT1-pHluorin  was introduced into the MAT α query strain Y7092 and crossed with the MAT a DMA using SGA technology , yielding a complete set of mutants expressing pHluorin in the cytosol. Mutants that displayed a slow growing phenotype were set up in a separate array, allowing for longer incubation times on the different SGA media.
Ethanol, acetate, succinate and pyruvate concentrations in the medium were determined by high pressure liquid chromatography. To this extent, 1.0 ml of sample was quenched with 100 μl of 35% perchloric acid followed by a neutralization with 55 μl of 7 M KOH. Samples were analyzed on a Phenomenex Rezex ROA-Organic Acid H+ column (Phenomenex, Utrecht, The Netherlands) using 7.2 mM H2SO4 as mobile phase.
Screening for mutants with deviating pHc
Unless stated otherwise, strains were pre-cultured o/n in microplates, diluted 10-fold into fresh medium in CELLSTAR black polystyrene clear-bottom 96-well microplates (Greiner Bio-One) and grown for 4 hours to ensure exponential growth. Plates were transferred to the Automated Cell, Compound and Environment Screening System (ACCESS)  and incubated at 30°C under constant shaking until automatically transferred to a Safire2 microplate reader (Tecan, Männedorf, Switzerland). Optical density at 600 nm (OD600) was measured followed by two fluorescence measurements at 390 nm and 470 nm excitation, both with 512 nm emission. After background subtraction the ratio of the two fluorescence measurements was compared to a calibration curve to determine pHc as described in . The array was screened twice and the 2,136 wild-type measurements were used to determine an average wild-type pHc with according standard deviation. For every mutant in the array the average pH was converted to a Z-value defined as the number of standard deviations their measured pH was removed from the average wild-type pHc in that replicate. Mutants with a Z-value at least higher than 2 or lower than -2 once and higher than 1 or lower than -1 in the other screening were selected as 'candidate hits' and combined with the slow grower array for additional confirmatory screening. Candidate hits and slow grower arrays were precultured as described and subjected to six rescreening runs where OD600 was measured with a SpectraMax Plus384 microplate spectrophotometer (Molecular Devices, Sunnyvale, CA, USA) followed by pHluorin fluorescence measurements using a SpectraMax Gemini XS microtitre plate spectrofluorometer (Molecular Devices). In each of these replicates, mutant pHc values were converted to Z-values with respect to average and standard deviation of the wild-type population in that replicate. Significant scores were determined based on a two-tailed t-test of these rescreening Z-values compared to the wild-type data (P < 0.01). For the analysis of the candidate hits based on the initial two genome-wide screens, for rigidity we did not include the pHc values used for identification in the determination of significance. Doing so would have improved P-values for all pHc mutants identified. For the slow growing mutants, to avoid bias originating from outliers, we performed a second analysis discarding the lowest and highest replicate value for each mutant (Jackknife), and retesting significance. Mutants with P-values > 0.1 in this analysis were discarded as significant. Both average Z-values and average pHc values are presented. All mutants identified as significant were subjected to microscopical analysis: strains were grown in microplates for at least 2 hours as described above. After washing with phosphate-buffered saline, cells were transferred to agarose-coated glass slides. Images were obtained using a Canon A620 camera (Canon, Tokyo, Japan) on an Axiovert 40 CFL microscope with a Plan Neofluar 100 X/NA 1.3 oil objective (Carl Zeiss, Oberkochen, Germany), using Endow GFP narrow-band excitation filter sets (Chroma Technology, Bellows Falls, VT, USA) for fluorescent images.
Profiling of mutants with aberrant pHc under additional stress conditions
After o/n inoculation in described conditions, cells were transferred to fresh medium buffered at pH 3.0 with 25 mM potassium citrate (Sigma-Aldrich), pH 7.5 with 25 mM MOPS (Sigma-Aldrich) or 2% ethanol and 2% glycerol as the carbon source. These experiments were conducted at least three times. Deviation was determined using t-tests comparing to the parent strain.
Hypergeometric distribution analysis
Enrichment of data sets for gene ontology terms was performed using the Yeast GO-term finder .
Growth curve analysis
After o/n inoculation hits identified in the initial screen were re-inoculated and subsequently monitored for 16 hours by OD600 and pHc measurements every 10 minutes in a FLUOstar OPTIMA microplate reader (BMG labtech, Ortenberg, Germany). Growth data were corrected for the non-linearity of optical recording at higher cell densities similar to the method in , correcting OD600 values recorded in the microplate reader (ODobs) to reflect linear OD600 determinations of the same cultures in a Novaspec II spectrophotometer (Pharmacia LKB Biochrom, Cambridge, UK) (always diluting the cultures to yield measured values between 0.05 and 0.3 OD units) using the formula ODcor = 1.1252(ODobs)2 + 0.6808(ODobs) - 0.0002. Growth rates of cultures in time were determined by calculating the slope of six consecutive data points (1 hour) of the entire ln(ODcor) curve.
where a was determined be to -7.24 ± 0.06, and b to 0.73 ± 0.08. We used this fit to predict the growth rate at each time point based on the pHc measured at that time, for all wild-type and mutant strain time courses. We next determined the biological variance at each time point of the measured μ values around the predicted μ values of the 190 individual wild-type replicates, resulting in a mean and standard deviation of the wild-type divergence from the prediction at each time point. Using this mean and standard deviation, we transformed individual wild-type and mutant curves to Z-values at all time points. t-Test analyses of the average mutant Z-values compared to all wild-type replicates for all time points between t = 4 h to t = 9 h was multiplied by a correction factor to eliminate false positives based on P-values of wild-type time courses in a same t-test. Z-values of mutant and wild-type μ/pHc curves, from t = 4 h to t = 9 h, were hierarchically clustered using Euclidean distances with full linkage.
deletion mutant array
green fluorescent protein
open reading frame
synthetic genetic array.
We thank Azmat Ullah, Wing Kit Man, Nydia van Dyk and Lawrence Heisler for assistance with experiments. This work was partially funded by Unilever (RO and GJS). Work in CN and GG's laboratory is supported by the NHGRI and CIHR (MOP-81340 and MOP-84305) and the Canadian Cancer Society (020380); work in CB and FV's laboratory was supported by the CIHR (MOP-97939)
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