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Journal of Amino Acids
Volume 2013 (2013), Article ID 461901, 7 pages
Metabolic Fate of the Increased Yeast Amino Acid Uptake Subsequent to Catabolite Derepression
The Institute of Urology and Nephrology, University College London, Charles Bell House, 67 Riding House Street, London W1W 7EY, UK
Received 14 November 2012; Revised 31 December 2012; Accepted 31 December 2012
Academic Editor: Hieronim Jakubowski
Copyright © 2013 John S. Hothersall and Aamir Ahmed. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Catabolite repression (CCR) regulates amino acid permeases in Saccharomyces cerevisiae via a TOR-kinase mediated mechanism. When glucose, the preferred fuel in S. cerevisiae, is substituted by galactose, amino acid uptake is increased. Here we have assessed the contribution and metabolic significance of this surfeit of amino acid in yeast undergoing catabolite derepression (CDR). L-[U-14C]leucine oxidation was increased 15 ± 1 fold in wild type (WT) strain grown in galactose compared to glucose. Under CDR, leucine oxidation was (i) proportional to uptake, as demonstrated by decreased uptake and oxidation of leucine in strains deleted of major leucine permeases and (ii) entirely dependent upon the TCA cycle, as cytochrome c1 (Cyt1) deleted strains could not grow in galactose. A regulator of amino acid carbon entry into the TCA cycle, branched chain ketoacid dehydrogenase, was also increased 29 ± 3 fold under CCR in WT strain. Protein expression of key TCA cycle enzymes, citrate synthase (Cs), and Cyt1 was increased during CDR. In summary, CDR upregulation of amino acid uptake is accompanied by increased utilization of amino acids for yeast growth. The mechanism for this is likely to be an increase in protein expression of key regulators of the TCA cycle.
In S. cerevisiae and other yeast, growth in glucose as the carbon source represses transcription of numerous genes (termed glucose repression or carbon catabolite repression, CCR) [1, 2]. Yeast grown with alternate carbon source (e.g., galactose or glycerol) undergoes catabolite derepression. During catabolite derepression (a condition akin to metabolic stress) yeast metabolism shifts from fermentative to respiratory and carbon is shunted to the mitochondrial TCA cycle thus increasing electron transport and respiration [3, 4].
We recently reported that during catabolite derepression (with galactose or glycerol as carbon source), there is an increase in yeast amino acid permease gene and protein expression, amino acid uptake, and oxygen consumption . We further demonstrated that the signalling involved in the coordination of this process, via TOR1 , a phenomenon that is distinct from that involved in diauxic shift, the recurring life cycle in the natural history of yeast . It has also been known for some time that synthesis of respiratory enzymes is increased in the presence of galactose compared to glucose . Based upon these observations we put forward a prima facie model  suggesting that the surfeit of amino acids during catabolite derepression in yeast may serve as reductive substrates for the TCA cycle providing an electron source for mitochondrial energy transduction. Little information exists on the utilization of the increased amino acids under conditions of stress such as catabolite derepression in yeast.
In this paper we have tested our proposed model  by addressing the following question regarding the metabolic fate of increased uptake of amino acids under catabolite derepression: are the accumulated amino acids surplus to the altered metabolic requirement during catabolite derepression or do they serve as a fuel in biochemical pathways related to the observed increase in oxygen consumption? We used the WT yeast and strains with genetic alterations grown under CCR and catabolite derepressed conditions to investigate whether the increase in amino acid uptake during catabolite derepression is accompanied by (i) increase in the oxidation of amino acids and (ii) increase in the activity and expression of TCA cycle enzymes. Our results show a direct corelation between the increase in amino acid uptake and an increase in the trans- and deamination of amino acids during catabolite derepression accompanied by oxidative cell metabolism and increase in the TCA cycle turn-over during catabolite derepression. Furthermore, this increase in the TCA cycle turn-over is accompanied by an increase in the activity and protein expression of key TCA cycle and amino acid metabolizing enzymes. We demonstrate that the TOR mediated increase in amino acid uptake serves as a fuel for energy provision, thus providing a mechanism of yeast metabolic adaptation during conditions of stress.
2. Materials and Methods
L-[U-14C]leucine (10.9 GBq/mmol) was purchased from Amersham Pharmacia Biotech, UK. Nitrocelluose filters (0.45 μm pore size) were purchased from Whatman, UK, or Millipore, UK. Chemicals were obtained from Merck, UK, unless otherwise stated.
2.2. Yeast Strains and Growth Conditions
Wild type S. cerevisiae strains S288C variant M3750 (MATaura3; ), BY4741 (MATahisΔ31 leu2Δ0 met15Δ0 ura3Δ0; purchased from the Yeast Knockout Collection (YKO)  through Open Biosystems, USA), and EY0986 (MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0  purchased from the Yeast-GFP clone collection, Invitrogen, UK) were used in this study. Amino acid permease deleted yeast has been described earlier  and details of the genotype of the amino acid permease deleted strains used in this study are given in Supplementary Table 1 (see Supplementary Material available online at http://dx.doi.org/10.1155/2013/461901). Growth conditions are detailed elsewhere . Oxygen consumption and L-[U-14C]leucine uptake were measured as described previously . Glucose concentration in the culture supernatant of O/N yeast cultures was measured using a chemiluminescence assay  and was found to be mM (). For some experiments, yeast was grown on solid medium by adding 2% select agar (Invitrogen) to the YNB medium plus the carbohydrate source described above.
2.3. Leucine Oxidation
Leucine is a common substrate for all the neutral amino acid permeases upregulated during catabolite derepression under the control of TOR . We therefore used L-[U-14C]leucine as a paradigm substrate for amino acid oxidation. L-[U-14C]leucine oxidation assay is similar to that described previously [13, 14]. Briefly, O/N cultures were harvested by centrifugation at 1000 ×g for 10 min at room temperature and washed with YNB medium without carbohydrates. Care was taken to remove all the media and the cell pellet was washed and resuspended in fresh YNB-CSM (without L-leucine) medium containing either glucose or galactose. In some instances carbohydrate substrate was omitted and in others the nonmetabolizable analogue of glucose, namely, 2-deoxyglucose (DOG), was used. Each corresponding suspension (5 mL) was added to L-[U-14C]leucine (750 μM, 94 μmoles/μCi) in a 50 mL Erlenmeyer flask fitted with a 2 mL centre well, sealed with silicone rubber Suba seals, and placed in an orbital shaking incubator at 30°C (120 rpm). After 1 h the reaction was stopped by injecting through the Suba seal 200 μL 5 N HCl into the flask and into the centre well 500 μL of hyamine hydroxide (1.0 M in methanol, Packard (Caversham, Berks, UK). The flasks were returned to the incubator for a further 1 h to equilibrate 14CO2 absorption into the hyamine. The contents of the centre well were transferred to a scintillation vial together with the results of a 1 mL wash with methanol. Corresponding blanks without yeast were used to measure L-[U-14C]leucine background release of 14CO2 and a sample from the flask was taken for specific activity calculation. Samples were counted in a Beckman LS6000 liquid scintillation counter (Beckman-Coulter, UK).
2.4. Amino Acid Transport Assay
Yeast cells were recovered by centrifugation, washed in 0.6 mL of a HEPES based transport buffer , and finally resuspended to OD600 = 0.7 − 0.8. Radio-labelled amino acid uptake was measured using techniques described previously [5, 15].
2.5. Enzyme Assay
The basal activity of branched-chain α-keto acid dehydrogenase (BckDH, E.C.18.104.22.168) was measured in cell homogenates from yeast. The assay medium (pH 7.4) contained 30 mM potassium phosphate, 2 mM DTT, 5 mM MgCl2, 3 mM NAD+, 0.4 mM reduced CoA, thiamine pyrophosphate, and 0.05% (v/v) Triton X-100. Nonspecific reductive activity was assessed at 340 nm in a Beckman DU650 spectrophotometer (Beckman-Coulter, UK). Specific BCKD activity was measured upon addition of 0.5 mM α-ketoisovalerate. Activity was calculated from NADH formed using an extinction coefficient (Σ340) of 6220 M−1 cm−1. Intracellular glutamate was measured using a NADH/glutamate dehydrogenase linked assay in hydralazine buffer pH 9.0 according to the method of Bergmeyer .
2.6. Direct Fluorescence Microscopy of Green Fluorescent Protein (GFP) Tagged Yeast Strains
Yeast with GFP-tagged cytochrome c1 (Cyt1, YOR065W), citrate synthase (Cs, YNR001C), and dihydrolipoamide dehydrogenase (Lpd1, YFL018C) were grown either in glucose or galactose containing media. Fluorescence for Cyt1-GFP and Cs-GFP was performed using a Zeiss LSM510 confocal system (Zeiss, Germany) with an argon laser line (488 nm) and a transmitted light detector for bright-field images or a Bio-Rad Radiance 2100 confocal system (Bio-Rad) coupled to a Nikon TE300 inverted microscope equipped with a Nikon 60x oil-immersion lens (numerical aperture = 1.4) with an argon laser line (488 nm) and a transmitted light detector for bright-field images and analysed using ImageJ software (http://rsb.info.nih.gov/ij/). Experiments were performed in at least 3 different preparations with triplicate or quadruplicate measurements. Results are expressed as means ± SEM. Statistical analysis, where applicable, was performed using a Student’s -test.
There was a large increase in the L-leucine uptake and also in the oxygen consumption in yeast grown under catabolite derepression, as reported previously . There was a -fold increase in L-[U-14C]leucine oxidation in yeast undergoing catabolite derepression than those grown in glucose under CCR (Figure 1(a)). The accompanying 15-fold increase in the oxygen consumption in the WT yeast grown in galactose compared to glucose medium, we have reported previously , was also observed for other WT strains used in this study (data not shown).
Is the pool of oxidized leucine derived largely from the increased L-leucine uptake during catabolite derepression? If the source of oxidized leucine was largely derived from the increased uptake, there should be a decrease in the leucine oxidation in yeast from which major amino acid permeases were deleted. The rate of leucine oxidation was proportionally decreased in strains from which the major TOR regulated amino acid permeases BAP1, TAT1, and GNP1 were deleted (Figure 1(a)). There was a good corelation between the decrease in leucine oxidation and the decrease in uptake (Figure 1(b)) when normalized to L-[U-14C]leucine oxidation and uptake, respectively, in the appropriate strain. These results indicate that the rate of leucine oxidation is correlated to the uptake during catabolite derepression.
The α-ketoglutarate/glutamate oxido-reductive deamination reaction catalysed by glutamate dehydrogenase plays a key role in nitrogen flow and hence amino acid carbon entry into oxidative metabolism. Concomitant with the increase in leucine oxidation we also observed a significant increase in intracellular glutamate concentration in galactose grown yeast (glucose and galactose , , ).
An interesting corollary is that in WT yeast 14CO2 production from L-[U-14C]leucine is dependent upon the presence of glucose or galactose (Figure 2). Yeast incubated with L-[U-14C]leucine but without a carbohydrate source (–CHO) released only nominal amounts of 14CO2. Addition of glucose or galactose to yeast from either ± CCR cultures (+CHO) resulted in measurable leucine oxidation (Figure 2). Deoxyglucose (+DOG) did not mimic this response indicating the requirement for a metabolizable carbohydrate source to achieve measurable leucine oxidation.
Transamination of leucine results in the formation of the branched chain keto acid, α-ketoisocaproate (α-KIC). The key regulatory enzyme controlling entry of keto acids into oxidative metabolism is BckDH. The basal activity of BckDH was measured in whole cell extracts (after 0.05% treatment with Triton X-100 to release the enzyme from mitochondria) of WT yeast grown in 2% glucose or galactose medium; the BckDH activity determined was basal rather than total (dephosphorylated). The activity of BckDH was linear for at least 6 min (Figure 3). There was approximately a 30-fold increase in the basal BckDH activity in yeast grown in 2% galactose compared to those grown in glucose.
BckDH is a member of the 2-oxo acid dehydrogenase multienzyme complexes that contains dihydrolipoamide dehydrogenase (Lpd1). An increase in protein expression, measured by fluorescence microscopy, for Lpd1 was also observed. Analysis of images (not shown) from Lpd1-GFP strains indicates a -fold increase Lpd1 expression in yeast grown in galactose compared to those grown in glucose. These results indicate that leucine catabolic pathways are upregulated during catabolite derepression.
The yeast grown with galactose as sole carbon source is in an oxidative state of metabolism with increased oxygen consumption . To confirm if the yeast relied upon the activity of TCA cycle during catabolite derepression for growth and that any residual fermentative component of metabolism did not account for growth we used a strain with the cytochrome c1 gene deletion. Cyt1 is a subunit of complex III in the mitochondrial electron transport chain. There was no regression in growth of Δcyt1 strain compared to WT when grown in medium with 2% glucose (Figure 4). However, there was no growth visible for the Δcyt1 yeast when grown in galactose medium (Figure 4), even after 72 hours of incubation. Similar results were observed for growth in liquid medium (data not shown). These results indicate that reductive substrate-electron transfer is critical for growth with galactose as the sole carbon source. We further investigated the role of the TCA cycle and electron transport by examining the expression of citrate synthase and Cyt1 from the Yeast-GFP clone collection  in yeast grown in 2% glucose or galactose medium. The Yeast-GFP clone collection is designed to express full-length proteins, tagged at the carboxy-terminal end with GFP, from their endogenous promoters. A very faint GFP signal was observed for Cyt1 protein in yeast grown in 2% glucose (Figure 5(a)). This expression was increased by -fold when WT yeast was grown in 2% galactose YNB (Figure 5(c)). Cs1 expression was visible in WT yeast grown in 2% glucose medium (Figure 5(e)); however this was significantly (, ) increased by % in yeast grown in galactose medium (Figure 5(g)).
4.1. Coordination of Nitrogen and Carbon Metabolism
Catabolite derepression, from a genetic point of view, results in transcription of numerous genes, by upstream activation sites (UAS) such as CCAAT box, R box, or CSRE element which are known to be involved in oxidative metabolic pathways  or PKA pathway [18, 19], and from a metabolic and functional point of view results in enhanced uptake of amino acids via TOR signal transduction . Our results indicate a level of coordination between the genes activated during catabolite derepression via the UAS and via signal transduction through TOR, although the precise nature of this coordination remains an outstanding question.
In this paper we have investigated the molecular mechanisms underlying the integration of nitrogen and carbon metabolism in S. cerevisiae during conditions of stress. We have demonstrated that amino acid transport and oxidation, via the TCA cycle, play a vital role in yeast survival and growth during catabolite derepression. With regards to amino acid metabolism, we propose that during catabolite derepression, the following three major steps involving genetic and metabolic reprogramming occur: (1) TOR mediated upregulation of amino acid permeases, (2) increase in the uptake of amino acids, and (3) increase in the capacity of the oxidative metabolic machinery. This model suggests that catabolite derepression is modulated via the TOR signalling pathway, which in turn increases the transcription of specific permease genes to induce permease protein expression. This allows the cell to utilise the extracellular amino acids which are fed into an already activated TCA cycle via key enzymes such as 2-oxo acid dehydrogenase multienzyme complexes and consumed for energy production.
4.2. Metabolic Fate of Increased Amino Acid Intake during Catabolite Derepression
Amino acids commonly provide a carbon source for entry into the TCA cycle beyond the point of 2-carbon incorporation at the citrate synthase step. Some of the amino acids whose uptake is increased during catabolite derepression by TOR mediated signalling, such as leucine, are common intermediates of major catabolic pathways such as acetyl CoA, pyruvate, or 2-oxoglutarate. Subsequent entry into intermediary metabolism, with concurrent mitochondrial electron transfer is the main route by which cellular energy is utilized from amino acids. This is achieved either by being an anaplerotic source in a complete TCA cycle, or as a direct bioenergetic substrate in a truncated cycle . As a result, to achieve complete oxidation (CO2 release from all carbons) a source of acetyl CoA is required. In this respect, the only known pathway for the terminal oxidation of leucine is through acetoacetate to acetyl-CoA and hence subsequent oxidation in the TCA cycle.
We have also observed, for the first time, an absolute requirement of a carbon source (e.g., glucose or galactose), in situ, for the increased oxidative metabolism of leucine to take place. It is particularly intriguing as the presence of carbohydrate is not necessary for the increase in L-[U-14C]leucine uptake observed during catabolite derepression (Figure 1). It is also not essential at the first irreversible (and rate limiting) step in leucine oxidation, that is, the activity of BckDH multienzyme complex (Figure 5), in cell extracts. BckDH oxidatively decarboxylates α-KIC to form isovaleryl-CoA and allows entry of the carbon skeleton of the increased cellular leucine into the TCA cycle. It is therefore likely that during catabolite derepression, an alternative nonamino acid carbon source is required for the entry of leucine into the TCA cycle downstream of BckDH. Alternatively it may be a strict requirement in situ; a possibility that remains to be investigated. It must be noted that under the O/N culture conditions generally employed for yeast growth in the laboratory and those used in our study, there is a significant amount of carbohydrate present in the growth medium.
We believe the integration of amino acid transport with oxidative metabolism, demonstrated here at the molecular level, is an important advance in our understanding of intermediary metabolism, particularly the role amino acids may play in contributing to the overall balance of carbon provision for cell maintenance, growth, and proliferation during conditions of stress. Our demonstration that amino acid transport and subsequent catabolism contribute to oxidative energy supply during catabolite derepression also highlights the importance of mitochondrial redox in this control. The resultant changes to mitochondrial redox (NAD(P)+/NAD(P)H), evoked by both catabolism and oxidative deamination of ketoacid derived amino acid, has clear implications in other cellular processes such as modulation of histone deacetylase  and life span in S. cerevisiae.
This work was supported by the Wellcome Trust (award to A. Ahmed), UK, and St Peter’s Trust for Kidney, Bladder & Prostate Research. The authors would like to thank J. Hansen and M. Kielland-Brandt for some of the yeast strains used in this study. The authors are also grateful to Peter Munro and Richard Wu for help with confocal microscopy and George Peter for useful discussions. The authors also thank Sophie Ridge-Ahmed for help in preparing the figures.
- M. Carlson, “Glucose repression in yeast,” Current Opinion in Microbiology, vol. 2, no. 2, pp. 202–207, 1999.
- J. M. Gancedo, “The early steps of glucose signalling in yeast,” FEMS Microbiology Reviews, vol. 32, no. 4, pp. 673–704, 2008.
- P. W. Coschigano and B. Magasanik, “The URE2 gene product of Saccharomyces cerevisiae plays an important role in the cellular response to the nitrogen source and has homology to glutathione S-transferases,” Molecular and Cellular Biology, vol. 11, no. 2, pp. 822–832, 1991.
- S. J. Lin, M. Kaeberlein, A. A. Andalis et al., “Calorie restriction extends Saccharomyces cerevisiae lifespan by increasing respiration,” Nature, vol. 418, no. 6895, pp. 344–348, 2002.
- G. J. Peter, L. Düring, and A. Ahmed, “Carbon catabolite repression regulates amino acid permeases in Saccharomyces cerevisiae via the TOR signaling pathway,” The Journal of Biological Chemistry, vol. 281, no. 9, pp. 5546–5552, 2006.
- J. L. DeRisi, V. R. Iyer, and P. O. Brown, “Exploring the metabolic and genetic control of gene expression on a genomic scale,” Science, vol. 278, no. 5338, pp. 680–686, 1997.
- E. S. Polakis, W. Bartley, and G. A. Meek, “Changes in the activities of respiratory enzymes during the aerobic growth of yeast on different carbon sources,” Biochemical Journal, vol. 97, no. 1, pp. 298–302, 1965.
- L. Düring-Olsen, B. Regenberg, C. Gjermansen, M. C. Kielland-Brandt, and J. Hansen, “Cysteine uptake by Saccharomyces cerevisiae is accomplished by multiple permeases,” Current Genetics, vol. 35, no. 6, pp. 609–617, 1999.
- E. A. Winzeler, D. D. Shoemaker, A. Astromoff et al., “Functional characterization of the S. cerevisiae genome by gene deletion and parallel analysis,” Science, vol. 285, no. 5429, pp. 901–906, 1999.
- W. K. Huh, J. V. Falvo, L. C. Gerke et al., “Global analysis of protein localization in budding yeast,” Nature, vol. 425, no. 6959, pp. 686–691, 2003.
- B. Regenberg, L. Düring-Olsen, M. C. Kielland-Brandt, and S. Holmberg, “Substrate specificity and gene expression of the amino acid permeases in Saccharomyces cerevisiae,” Current Genetics, vol. 36, no. 6, pp. 317–328, 1999.
- S. Igarashi and W. L. Hinze, “Luminol chemiluminescent determination of glucose or glucose oxidase activity using an inverted micellar system,” Analytical Chemistry, vol. 60, no. 5, pp. 446–450, 1988.
- K. Tanaka, R. Mandell, and V. E. Shih, “Metabolsim of [1-(14)C] and [2-(14)C] leucine in cultured skin fibroblasts from patients with isovaleric acidemia. Characterization of metabolic defects,” The Journal of Clinical Investigation, vol. 58, no. 1, pp. 164–172, 1976.
- J. S. Hothersall, A. L. Greenbaum, and P. McLean, “The functional significance of the pentose phosphate pathway in synaptosomes: protection against peroxidative damage by catecholamines and oxidants,” Journal of Neurochemistry, vol. 39, no. 5, pp. 1325–1332, 1982.
- A. Ahmed, F. Sesti, N. Ilan, T. M. Shih, S. L. Sturley, and S. A. N. Goldstein, “A molecular target for viral killer toxin: TOK1 potassium channels,” Cell, vol. 99, no. 3, pp. 283–291, 1999.
- H. U. Bergmeyer, Methods of Enzymatic Analysis, Chemie Gmbh, Academic Press, New York, NY, USA, 1963.
- H. J. Schüller, “Transcriptional control of nonfermentative metabolism in the yeast Saccharomyces cerevisiae,” Current Genetics, vol. 43, no. 3, pp. 139–160, 2003.
- D. Livas, M. J. H. Almering, J. M. Daran, J. T. Pronk, and J. M. Gancedo, “Transcriptional responses to glucose in Saccharomyces cerevisiae strains lacking a functional protein kinase A,” BMC Genomics, vol. 12, article 405, 2011.
- M. G. Slattery, D. Liko, and W. Heideman, “Protein kinase A, TOR, and glucose transport control the response to nutrient repletion in Saccharomyces cerevisiae,” Eukaryotic Cell, vol. 7, no. 2, pp. 358–367, 2008.
- J. K. Kelleher, B. M. Bryan 3rd. B.M., R. T. Mallet, A. L. Holleran, A. N. Murphy, and G. Fiskum, “Analysis of tricarboxylic acid-cycle metabolism of hepatoma cells by comparison of 14CO2 ratios,” Biochemical Journal, vol. 246, no. 3, pp. 633–639, 1987.