Oxidative Medicine and Cellular Longevity

Volume 2013 (2013), Article ID 139491, 6 pages

http://dx.doi.org/10.1155/2013/139491

Review Article

Roles of Mitochondrial Dynamics under Stressful and Normal Conditions in Yeast Cells

Dmitry A. Knorre,1,2 Konstantin Y. Popadin,³ Svyatoslav S. Sokolov,1,2 and Fedor F. Severin1,2

¹Belozersky Institute of Physico-Chemical Biology, Moscow State University, Vorobyevy Gory 1, Moscow 119992, Russia

²Institute of Mitoengineering, Moscow State University, Vorobyevy Gory 1, Moscow 119992, Russia

³Department of Genetic Medicine and Development, University of Geneva Medical School, 1 rue Michel-Servet, 1211 Geneva, Switzerland

Received 7 May 2013; Accepted 25 June 2013

Academic Editor: Cristina Mazzoni

Copyright © 2013 Dmitry A. Knorre et al. 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.

Abstract.

Eukaryotic cells contain dynamic mitochondrial filaments: they fuse and divide. Here we summarize data on the protein machinery driving mitochondrial dynamics in yeast and also discuss the factors that affect the fusion-fission balance. Fission is a general stress response of cells, and in the case of yeast this response appears to be prosurvival. At the same time, even under normal conditions yeast mitochondria undergo continuous cycles of fusion and fission. This seems to be a futile cycle and also expensive from the energy point of view. Why does it exist? Benefits might be the same as in the case of sexual reproduction. Indeed, mixing and separating of mitochondrial content allows mitochondrial DNA to segregate and recombine randomly, leading to high variation in the numbers of mutations per individual mitochondrion. This opens a possibility for effective purifying selection-elimination of mitochondria highly contaminated by deleterious mutations. The beneficial action presumes a mechanism for removal of defective mitochondria. We argue that selective mitochondrial autophagy or asymmetrical distribution of mitochondria during cell division could be at the core of such mechanism.

1. Introduction

Almost all eukaryotic cells harbor mitochondria—the distant descendants of endosymbiotic alphaproteobacteria (see [1] for review). In most types of eukaryotic cells, mitochondria are organized in complex reticular structures with dynamically changing topology. Changes of the structures are usually referred to as mitochondrial dynamics. These changes include events of mitochondria fission and fusion, as well as active transport of individual filaments. Importantly, defects of mitochondrial dynamics are associated with defects in mechanisms of mitochondrial DNA (mtDNA) maintenance [2]. This makes the baker’s yeast Saccharomyces cerevisiae a useful tool for studies of mitochondrial dynamics mechanisms. Importantly, in contrast to most of animal cells, yeasts are able to proliferate without a functional respiratory chain and ATP-synthase. Such cells still have basal mitochondrial morphology, membrane potential, and metabolic activities. Moreover, yeast cells lacking mitochondrial DNA can be easily cultivated in medium containing a fermentable carbon source (e.g., glucose). This allowed performing several large-scale screenings aimed at identification of genes involved in mitochondrial dynamics and maintenance of reticular mitochondrial morphology [2, 3]. It was found that proteins involved in the molecular mechanisms of mitochondrial fusion and fission in yeast have many similarities to such mechanisms in animals (see [4] for review). The molecular mechanisms of mitochondrial fusion, fission, and movement were reviewed in detail recently [4–8].

In this review we briefly discuss these mechanisms focusing on the role of mitochondrial dynamics in cell physiology under stressful and normal conditions using an example of Saccharomyces cerevisiae yeast cells.

2. Mitochondrial Dynamics: Mechanisms and Stress Response

Mitochondrial fission is an active process organized by several proteins (see [9] for review). The key role is played by GTPase Dnm1p, which is capable of oligomerization on the lipid surface: it was shown that Dnm1p forms ~80 nm spirals on liposomes [10, 11]. A subsequent GTP hydrolysis results in a conformational change of Dnm1p, constriction of the spirals, and fission of the lipid vesicles [11]. Fis1p is localized at the outer membrane of mitochondria and recruits Dnm1p on the mitochondrial surface by means of adaptor proteins: Caf4p and its paralog Mdv1p [12]. It was shown that during membrane scission Dnm1p-dependent constriction is accompanied by longitudinal tension of lipid vesicles [13]. This implies that mitochondrial movement along the cytoskeleton could be an important factor for mitochondrial fission. Interestingly, for some stressful conditions fission of mitochondrial reticulum was observed even in the absence of the DNM1 gene. Kitagaki and colleagues [14] have shown that high (15%) concentration of ethanol facilitates fission of yeast mitochondria even on Δdnm1 background. Possibly, severe changes in ion composition of cytoplasm and mitochondrial matrix or significant change in mitochondrial lipid composition leads to mechanical division of mitochondria into small compartments. Indeed, most of the protocols of mitochondria isolation do not allow preserving native structure of mitochondrial reticulum.

Mitochondrial fusion in yeast is orchestrated by another set of proteins including Fzo1p, Mdm30, Ugo1p, and Mgm1p. Studies on isolated mitochondria show that the process of fusion occurs in several stages [15, 16]: docking of mitochondria and fusion of the outer membranes followed by fusion of the inner membranes (Figure 1). Docking of mitochondria in yeast is controlled by outer membrane protein Fzo1p. Fzo1p is a GTPase [17] that forms trans-dimers allowing anchoring of separate mitochondrial vesicles. According to the model of Anton and colleagues [16], this process requires GTP binding, whereas hydrolysis of GTP allows moving to the next stage—fusion of the outer membranes. While mitochondrial fusion requires GTP, Meeusen and McCaffery [15] have shown that the rate of mitochondrial fusions could be as high as 50% of the maximum level with energy regeneration system in the absence of exogenous GTP. This indicates that low concentration of endogenous GTP is sufficient to maintain physiological rates of mitochondrial fusion. At the same time, the uncoupler FCCP (Carbonyl cyanide-4-(trifluoromethoxy)phenylhydrazone) and the ionophore valinomycin were found to be effective inhibitors of fusion of isolated yeast [15] and human [18] mitochondria. Accordingly, FCCP [19] and also other uncouplers and inhibitors of respiratory chain were found to induce mitochondrial reticulum fission in various human cell lines (see [20] for review). Another important factor regulating mitochondrial fusion is cellular redox state. Very recently, it was shown that docking of mitochondria is regulated by the ratio of reduced/oxidized glutathione: GSSG induces the generation of disulphide-mediated mitofusin oligomers and in this way promotes fusion [21]. It was found that C684A mutation of cysteine in Mfn2 inhibits mitochondrial fusion, pointing to a role of this residue in oligomerization of mitofusin and docking of mitochondria [22]. As S. cerevisiae genome contains a homolog of Mfn2, FZO1, the redox-dependent mechanism of regulation is likely to be conserved also in yeast. At the same time, treatment of human cells with hydrogen peroxide [22] or treatment of yeast cells with the drug amiodarone that induces endogenous formation of reactive oxygen species [23] causes mitochondrial fission. This apparent contradiction could be explained by the fact that high concentration of hydrogen peroxide inhibits the respiratory chain, thus counteracting the stimulating effect on mitochondria fusion [24]. Another explanation is based on the importance of the lipid composition for mitochondrial fusion; the inactivation of genes encoding enzymes of mitochondrial biosynthesis of lipids, phosphatidylethanolamine and cardiolipin (PSD1 and CRD1, correspondingly), inhibits mitochondrial fusion [25, 26]. Therefore, peroxidation of cardiolipin induced by hydrogen peroxide could also retard mitochondrial fusion.

Figure 1: Proteins driving the cycle of mitochondrial fusion and fission. Mitochondrial fusion starts with the docking mediated by Fzo1 and Ugo1. Docking is followed by the outer membrane fusion mediated by Mdm30 and Ugo1. The inner membrane fusion is likely to be dependent on Mgm1 and Ysp2. Caf4, Mdv1 and Fis1 make a platform for fission which is being executed by Dnm1 oligomers.

To conclude this part, it should be noted that stresses generally tip the mitochondrial dynamics towards fission. This is not surprising; local damage to fused mitochondria might depolarize the whole cellular mitochondrial content [27]. In other words, cells with fissed mitochondria seem to be more resistant to stresses; at least a minor fraction of the mitochondrial vesicles might be lucky to escape the damage. In theory, a cell with fragmented mitochondria is as resistant as the one with separated mitoplasts surrounded by an intact outer membrane. We have recently shown that such morphology can be observed in Δysp2 cells in stationary phase [28]. The YSP2 gene was previously discovered as a genetic factor that decreases resistance to amiodarone and acetic acid [29]. This is consistent with a possible role of Ysp2p in mitochondrial inner membrane fusion (Figure 1).

3. Role of Mitochondrial Dynamics under Normal Conditions

It must be noted that mitochondrial fusion and fission not only happen under stress, but also constantly occur under normal conditions. This is true not only for yeast cells, but also for cells of higher organisms. Both processes consume energy. Thus the question arises about the biological role of these processes under stress-free conditions.

It has been suggested that fusion-fission cycle can maintain high quality of mitochondrial protein components, keeping mitochondrial vesicles with low membrane potential out of the process of fusion into the mitochondrial reticulum and their consequent elimination by mitophagy (mitochondria-specific autophagy; see [30] for review). This filtering will keep the average quality of the mitochondrial respiratory chain on a constant level and work against ROS-induced protein damage but will not affect mtDNA quality if segregation of proteins and mtDNA is independent during fusion-fission process. However, since mtDNA is a subject to high mutation rate [31], the effective purifying selection which eliminates de novo deleterious mutations is required to maintain the quality of mtDNA. Thus, it has been proposed that the fusion-fission process can not only select mitochondria on the level of phenotypes (proteins), but also contribute to preferential elimination of mtDNA with deleterious mutations [32]. However, the functional link between mitochondrial phenotypes (protein components) and genotypes (mtDNA) is necessary for establishment of this kind of selection on a genetic level. For example, low mitochondrial membrane potential needs to be determined by deleterious mutations in mtDNA. There are two not mutually exclusive ways to develop such phenotype-genotype linkage. The first is purely mechanistic and based on passive membrane colocalization of mtDNA and proteins encoded by the mtDNA. Indeed, the inner membrane proteins were shown to have significantly lower mobility than proteins localized in the outer membrane [33]. Thus the local quality of the mitochondrial membrane is expected to be linked to the quality of the neighboring mtDNA attached to the membrane. This membrane linkage will lead to the formation of fissed mitochondria with correlated quality of phenotypes and genotypes, making a “fusion quality filter” effective in elimination of mtDNA with deleterious mutations (see [34] for review).

The second mechanism is based on active expression of mtDNA in fissed mitochondria and subsequent incorporation of newly synthesized proteins into mitochondrial membrane, so that genotype fitness influences phenotype fitness. This scenario does not depend on passive inheritance of mtDNA in complex with their protein products but requires long periods of existence of fissed mitochondria sufficient for incorporation of newly synthesized proteins into the mitochondrial membrane. The mechanism of purification of mitochondria from mutant copies of DNA during the fusion-fission process resembles the mechanism proposed to explain the existence of sexual reproduction (mutational deterministic hypothesis; [35, 36]). The fusion-fission process (as well as genetic recombination) restores high variability in the numbers of mutant mtDNAs per mitochondrial vesicle (number of deleterious mutations per offspring), making selection more effective (Figure 2). Indeed, elimination of the minimal numbers of mitochondrial vesicles maximally contaminated by mutant mtDNA will keep the heteroplasmy level low and will be energetically less expensive than elimination of large numbers of moderately contaminated mitochondria. The mutational deterministic hypothesis depends on high mutation rate and a negative epistasis between deleterious mutations [35–37]. Since both parameters are poorly known for the mitochondrial genome, future experimental studies are required to test the importance of the mechanism.

Figure 2: Hypothetical scheme illustrating how the mitochondrial fusion-fission cycle helps to maintain mitochondrial DNA. Rearrangements of the DNA induced by mitochondrial fission-fusion and recombination result in appearance of mutation-free mitochondrial genomes. Removal of genomes with high levels of deleterious mutations inhibits the high rate of mtDNA damage (see text for details).

The relative influence of the first (passive) and the second (active) mechanisms on the maintenance of the mtDNA quality during the fusion-fission process depends on the frequency of fusion-fission events and the rate of mtDNA transcription and translation, and thus they can be different in various cells.

Is there any experimental evidence that mitochondrial dynamics counterbalance the high rate of deleterious mutation accumulation in yeast? It was recently shown that the FIS1 and MDV1 genes appear to be involved in maintenance of heteroplasmy in diploid yeast cells acquired after mating of haploids cells with different mitochondrial markers [38]. Although the authors did not observe this effect in Δdnm1/Δdnm1 diploid, the results indicated that mitochondrial dynamics affect redistribution of different variants of the mitochondrial genome. The knockouts of genes involved in mitochondrial dynamics increase the chance of petite mutation in yeast. Petite mutation refers to inability of growth on medium with a nonfermentable carbon source (ethanol, glycerol, etc.), and it is usually associated with deletions or complete loss of mtDNA (see [39] for review). The inactivation of a fusion protein-encoding gene (FZO1) results in quick degradation of the mitochondrial genome [40], whereas the deletions of fission genes DNM1 or FIS1, while increasing rate of petite mutation, still allow maintenance of the functional copies of mtDNA in the cells.

To draw parallels between sexual reproduction and fusion-fission dependent recombination of mtDNAs one should consider the ways of elimination of nonfunctional mitochondria. Apparently, the functional mtDNA could outcompete the damaged one by advantages in replication. Although the opposite situation is described in the literature as suppressive petite mutation [41], the latter is not a common case. An alternative explanation comes from experiments with human cell lines. In 2008, Twig and colleagues [42] showed that after fission mitochondria can depolarize and get targeted to an autophagosome. The process of selective elimination of mitochondria unable to maintain their own transmembrane potential was called mitophagy. Mitophagy attracted a lot of attention because the mutations in PINK1 and Parkin (involved in marking the malfunctioning mitochondria for mitophagy) were found to be linked to Parkinson disease (see [43, 44] for review). It was suggested that mitophagy is necessary for quality control of mitochondria, to remove damaged protein complexes [8] or damaged mtDNA [32]. There are no homologs of PINK1 or Parkin in Saccharomyces cerevisiae. However, certain conditions, including nitrogen starvation or rapamycin treatment, induce selective mitochondrial autophagy in Atg32-dependent manner. Atg32 is located on the outer mitochondrial membrane and initiates the assembly of the autophagic complex which includes several ubiquitin ligases and adaptor proteins [45, 46]. Moreover, treatment of cells with mitochondrial respiratory chain inhibitors Antimycin A or KCN triggers a general increase of autophagy [47]. Intriguingly, this increase was shown to be Atg32 dependent [47]. Recently, it was shown that mitophagy indeed plays a role in maintaining mitochondrial quality in yeast [48].

Interestingly, it was shown that mitochondrial fission is not a necessary prerequisite for mitophagy in yeast [49]. This underscores the importance the “futile” fission-fusion cycle; the mitophagy of fully fused mitochondria can be lethal for the cells (yeast cannot live without mitochondria).

Another possible way to remove mtDNA with deleterious mutations relies on asymmetrical division of yeast cells (see [50] for review). It was shown that a complex molecular mechanism (based on the polarisome) fulfills bud-to-mother transport of damaged macromolecules in yeast cells [51]. Moreover, it was recently reported that mitochondria with higher rate of superoxide production are retained in the mother cells [52]. Such selective retention is not surprising because actin cables anchor mitochondria via Mmm1p and Mdm10p [53], which in turn form a protein complex spanning both mitochondrial membranes and being capable of binding mtDNA (see [54] for review). The machinery responsible for mother-bud distribution of mitochondria also includes mitochondrial anchor in the mother cell (cortical protein Num1 [55] and myosin-related motor which moves mitochondria towards the bud (Myo2, [56]). Possibly, multiple rounds of asymmetrical distribution of malfunctioning mitochondria lead to a decrease of mtDNA stability in replicatively old cells. In accordance with this hypothesis, it was shown that the chances of petite mutation significantly increased with replicative age [57].

Replicatively old yeast cells demonstrate slower growth and increased chance of viability loss [58]. Some authors argue that the death of a replicatively old mother cell could be an active process similar to apoptosis of mammalian cells [59]. Therefore, if asymmetrical redistribution of mitochondria indeed exists, damaged mtDNA is constantly eliminated by replicative aging.

Is there any evidence linking yeast replicative aging and mitochondrial dynamics? Recently it was found that replicatively old yeast cells harbor fissed mitochondria with decreased transmembrane potential [60]. Earlier Scheckhuber and colleagues [61] showed that replicatively aged yeast cells have fissed mitochondria and that the deletions of either DNM1 or FIS1 genes provide a certain increase in S. cerevisiae lifespan. Indeed, mitochondrial dynamics appear to be necessary for asymmetrical redistribution of mitochondria. Theoretically, if the dynamics are lost due to mutations, then the old mother cells of the mutants gain some advantage over the wild type ones carrying accumulating copies of damaged mtDNA. However, this benefit is obviously canceled by a moderate decrease in competitive fitness of the mutant cells; high-throughput screening [62] has shown a decrease in competitive fitness of strains lacking FIS1, CAF4, DNM1, or FZO1 compared to the wild type strain.

4. Conclusions

To conclude, it appears that mitochondrial dynamics in yeast play different roles under stress and under normal conditions and normal aging. A single onset of fission followed by recovery of the reticulum seems to be required for the stress-resistances. Alternatively, multiple “futile cycles” of fusion and fission contribute to maintenance of mitochondrial genomes in the long term under stress-free conditions.

Acknowledgment

This work was supported by the Russian Foundation for Basic Research Grant 12-04-01412.

References

M. W. Gray, G. Burger, and B. Franz Lang, “The origin and early evolution of mitochondria,” Genome Biology, vol. 2, no. 6, pp. 1018.1–1018.5, 2001.

T. Hanekamp, M. K. Thorsness, I. Rebbapragada et al., “Maintenance of mitochondrial morphology is linked to maintenance of the mitochondrial genome in Saccharomyces cerevisiae,” Genetics, vol. 162, no. 3, pp. 1147–1156, 2002.

K. S. Dimmer, S. Fritz, F. Fuchs et al., “Genetic basis of mitochondrial function and morphology in Saccharomyces cerevisiae,” Molecular Biology of the Cell, vol. 13, no. 3, pp. 847–853, 2002.

J. Zhao, U. Lendahl, and M. Nistér, “Regulation of mitochondrial dynamics: convergences and divergences between yeast and vertebrates,” Cellular and Molecular Life Sciences, vol. 70, no. 6, pp. 951–976, 2013.

H. Otera and K. Mihara, “Molecular mechanisms and physiologic functions of mitochondrial dynamics,” Journal of Biochemistry, vol. 149, no. 3, pp. 241–251, 2011.

R. J. Braun and B. Westermann, “Mitochondrial dynamics in yeast cell death and aging,” Biochemical Society Transactions, vol. 39, no. 5, pp. 1520–1526, 2011.

J. R. Lovas and X. Wang, “The meaning of mitochondrial movement to a neuron’s life,” Biochimica et Biophysica Acta, vol. 1833, no. 1, pp. 184–194, 2013.

B. Westermann, “Mitochondrial fusion and fission in cell life and death,” Nature Reviews Molecular Cell Biology, vol. 11, no. 12, pp. 872–884, 2010.

L. L. Lackner and J. M. Nunnari, “The molecular mechanism and cellular functions of mitochondrial division,” Biochimica et Biophysica Acta, vol. 1792, no. 12, pp. 1138–1144, 2009.

E. Ingerman, E. M. Perkins, M. Marino et al., “Dnm1 forms spirals that are structurally tailored to fit mitochondria,” Journal of Cell Biology, vol. 170, no. 7, pp. 1021–1027, 2005.

J. A. Mears, L. L. Lackner, S. Fang, E. Ingerman, J. Nunnari, and J. E. Hinshaw, “Conformational changes in Dnm1 support a contractile mechanism for mitochondrial fission,” Nature Structural & Molecular Biology, vol. 18, no. 1, pp. 20–26, 2011.

Q. Guo, S. Koirala, E. M. Perkins, J. M. McCaffery, and J. M. Shaw, “The mitochondrial fission adaptors Caf4 and Mdv1 are not functionally equivalent,” PloS One, vol. 7, no. 12, Article ID e53523, 2012.

A. Roux, K. Uyhazi, A. Frost, and P. De Camilli, “GTP-dependent twisting of dynamin implicates constriction and tension in membrane fission,” Nature, vol. 441, no. 7092, pp. 528–531, 2006.

H. Kitagaki, Y. Araki, K. Funato, and H. Shimoi, “Ethanol-induced death in yeast exhibits features of apoptosis mediated by mitochondrial fission pathway,” FEBS Letters, vol. 581, no. 16, pp. 2935–2942, 2007.

S. Meeusen, J. M. McCaffery, and J. Nunnari, “Mitochondrial fusion intermediates revealed in vitro,” Science, vol. 305, no. 5691, pp. 1747–1752, 2004.

F. Anton, J. M. Fres, A. Schauss et al., “Ugo1 and Mdm30 act sequentially during Fzo1-mediated mitochondrial outer membrane fusion,” Journal of Cell Science, vol. 124, no. 7, pp. 1126–1135, 2011.

G. J. Hermann, J. W. Thatcher, J. P. Mills et al., “Mitochondrial fusion in yeast requires the transmembrane GTPase Fzo1p,” Journal of Cell Biology, vol. 143, no. 2, pp. 359–373, 1998.

A. C. Schauss, H. Huang, S.-Y. Choi et al., “A novel cell-free mitochondrial fusion assay amenable for high-throughput screenings of fusion modulators,” BMC Biology, vol. 8, article 100, 2010.

F. Legros, F. Malka, P. Frachon, A. Lombès, and M. Rojo, “Organization and dynamics of human mitochondrial DNA,” Journal of Cell Science, vol. 117, no. 13, pp. 2653–2662, 2004.

C. Sauvanet, S. Duvezin-Caubet, J.-P. di Rago, and M. Rojo, “Energetic requirements and bioenergetic modulation of mitochondrial morphology and dynamics,” Seminars in Cell and Developmental Biology, vol. 21, no. 6, pp. 558–565, 2010.

T. Shutt, M. Geoffrion, R. Milne, and H. M. McBride, “The intracellular redox state is a core determinant of mitochondrial fusion,” EMBO Reports, vol. 13, no. 10, pp. 909–915, 2012.

V. P. Skulachev, L. E. Bakeeva, B. V. Chernyak et al., “Thread-grain transition of mitochondrial reticulum as a step of mitoptosis and apoptosis,” Molecular and Cellular Biochemistry, vol. 256-257, no. 1-2, pp. 341–358, 2004.

A. I. Pozniakovsky, D. A. Knorre, O. V. Markova, A. A. Hyman, V. P. Skulachev, and F. F. Severin, “Role of mitochondria in the pheromone- and amiodarone-induced programmed death of yeast,” Journal of Cell Biology, vol. 168, no. 2, pp. 257–269, 2005.

A. C. Nulton-Persson and L. I. Szweda, “Modulation of mitochondrial function by hydrogen peroxide,” The Journal of Biological Chemistry, vol. 276, no. 26, pp. 23357–23361, 2001.

A. Joshi, M. Thompson, N. Fei, M. Huttemann, and M. L. Greenberg, “Cardiolipin and mitochondrial phosphatidylethanolamine have overlapping functions in mitochondrial fusion in Saccharomyces cerevisiae,” The Journal of Biological Chemistry, vol. 287, no. 21, pp. 1–20, 2012.

E. Y. L. Chan and G. A. McQuibban, “Phosphatidylserine decarboxylase 1 (Psd1) promotes mitochondrial fusion by regulating the biophysical properties of the mitochondrial membrane and alternative topogenesis of mitochondrial genome maintenance protein 1 (Mgm1),” The Journal of Biological Chemistry, vol. 287, no. 48, pp. 40131–40139, 2012.

A. A. Amchenkova, L. E. Bakeeva, Y. S. Chentsov, V. P. Skulachev, and D. B. Zorov, “Coupling membranes as energy-transmitting cables. I. Filamentous mitochrondia in fibroblasts and mitochondrial clusters in cardiomyocytes,” Journal of Cell Biology, vol. 107, no. 2, pp. 481–495, 1988.

D. A. Knorre, S. M. Ojovan, V. B. Saprunova, S. S. Sokolov, L. E. Bakeeva, and F. F. Severin, “Mitochondrial matrix fragmentation as a protection mechanism of yeast Saccharomyces cerevisiae,” Biochemistry, vol. 73, no. 11, pp. 1254–1259, 2008.

S. Sokolov, D. Knorre, E. Smirnova et al., “Ysp2 mediates death of yeast induced by amiodarone or intracellular acidification,” Biochimica et Biophysica Acta, vol. 1757, no. 9-10, pp. 1366–1370, 2006.

R. Youle and A. van der Bliek, “Mitochondrial fission, fusion, and stress,” Science, vol. 337, no. 6098, pp. 1062–1065, 2012.

C. Richter, J.-W. Park, and B. N. Ames, “Normal oxidative damage to mitochondrial and nuclear DNA is extensive,” Proceedings of the National Academy of Sciences of the United States of America, vol. 85, no. 17, pp. 6465–6467, 1988.

S. Vidoni, C. Zanna, M. Rugolo, E. Sarzi, and G. Lenaers, “Why mitochondria must fuse to maintain their genome integrity,” Antioxidants & Redox Signaling, vol. 19, no. 4, 2013.

V. M. Sukhorukov, D. Dikov, K. Busch, V. Strecker, I. Wittig, and J. Bereiter-Hahn, “Determination of protein mobility in mitochondrial membranes of living cells,” Biochimica et Biophysica Acta, vol. 1798, no. 11, pp. 2022–2032, 2010.

A. Kowald and T. B. L. Kirkwood, “Evolution of the mitochondrial fusion—fission cycle and its role in aging,” Proceedings of the National Academy of Sciences of the United States of America, vol. 108, no. 25, pp. 10237–10242, 2011.

A. S. Kondrashov, “Selection against harmful mutations in large sexual and asexual populations,” Genetical Research, vol. 40, no. 3, pp. 325–332, 1982.

A. S. Kondrashov, “Deleterious mutations and the evolution of sexual reproduction,” Nature, vol. 336, no. 6198, pp. 435–440, 1988.

A. S. Kondrashov, “Classification of hypotheses on the advantage of amphimixis,” Journal of Heredity, vol. 84, no. 5, pp. 372–387, 1993.

E. Bradshaw, M. Yoshida, and F. Ling, “Mitochondrial fission proteins Fis1 and Mdv1, but not Dnm1, play a role in maintenance of heteroplasmy in budding yeast,” FEBS Letters, vol. 586, no. 8, pp. 1245–1251, 2012.

V. Contamine and M. Picard, “Maintenance and integrity of the mitochondrial genome: a plethora of nuclear genes in the budding yeast,” Microbiology and Molecular Biology Reviews, vol. 64, no. 2, pp. 281–315, 2000.

D. Rapaport, M. Brunner, W. Neupert, and B. Westermann, “Fzo1p is a mitochondrial outer membrane protein essential for the biogenesis of functional mitochondria in Saccharomyces cerevisiae,” The Journal of Biological Chemistry, vol. 273, no. 32, pp. 20150–20155, 1998.

B. Ephrussi, H. de Margerie-Hottinguer, and H. Roman, “Suppressiveness: a new factor in the genetic determinism of the synthesis of respiratory enzymes in yeast,” Proceedings of the National Academy of Sciences of the United States of America, vol. 41, no. 12, pp. 1065–1071, 1955.

G. Twig, A. Elorza, A. J. A. Molina et al., “Fission and selective fusion govern mitochondrial segregation and elimination by autophagy,” EMBO Journal, vol. 27, no. 2, pp. 433–446, 2008.

M. Müller and A. S. Reichert, “Mitophagy, mitochondrial dynamics and the general stress response in yeast,” Biochemical Society Transactions, vol. 39, no. 5, pp. 1514–1519, 2011.

G. Twig and O. S. Shirihai, “The interplay between mitochondrial dynamics and mitophagy,” Antioxidants & Redox Signaling, vol. 14, no. 10, pp. 1939–1951, 2011.

I. Bhatia-Kiššová and N. Camougrand, “Mitophagy in yeast: actors and physiological roles,” FEMS Yeast Research, vol. 10, no. 8, pp. 1023–1034, 2010.

K. Suzuki, “Selective autophagy in budding yeast,” Cell Death and Differentiation, vol. 20, no. 1, pp. 43–48, 2013.

M. Deffieu, I. Bhatia-Kissová, B. Salin et al., “Increased levels of reduced cytochrome b and mitophagy components are required to trigger nonspecific autophagy following induced mitochondrial dysfunction,” Journal of Cell Science, vol. 126, part 2, pp. 415–426, 2013.

Y. Kurihara, T. Kanki, Y. Aoki et al., “Mitophagy plays an essential role in reducing mitochondrial production of reactive oxygen species and mutation of mitochondrial DNA by maintaining mitochondrial quantity and quality in yeast,” The Journal of Biological Chemistry, vol. 287, no. 5, pp. 3265–3272, 2012.

N. Mendl, A. Occhipinti, M. Müller, P. Wild, I. Dikic, and A. S. Reichert, “Mitophagy in yeast is independent of mitochondrial fission and requires the stress response gene WHI2,” Journal of Cell Science, vol. 124, no. 8, pp. 1339–1350, 2011.

K. A. Henderson and D. E. Gottschling, “A mother's sacrifice: what is she keeping for herself?” Current Opinion in Cell Biology, vol. 20, no. 6, pp. 723–728, 2008.

B. Liu, L. Larsson, A. Caballero et al., “The polarisome is required for segregation and retrograde transport of protein aggregates,” Cell, vol. 140, no. 2, pp. 257–267, 2010.

J. R. McFaline-Figueroa, J. Vevea, T. C. Swayne et al., “Mitochondrial quality control during inheritance is associated with lifespan and mother-daughter age asymmetry in budding yeast,” Aging Cell, vol. 10, no. 5, pp. 885–895, 2011.

I. Boldogh, N. Vojtov, S. Karmon, and L. A. Pon, “Interaction between mitochondria and the actin cytoskeleton in budding yeast requires two integral mitochondrial outer membrane proteins, Mmm1p and Mdm10p,” Journal of Cell Biology, vol. 141, no. 6, pp. 1371–1381, 1998.

J. C. Xin and R. A. Butow, “The organization and inheritance of the mitochondrial genome,” Nature Reviews Genetics, vol. 6, no. 11, pp. 815–825, 2005.

T. Klecker, D. Scholz, J. Förtsch, and B. Westermann, “The yeast cell cortical protein Num1 integrates mitochondrial dynamics into cellular architecture,” Journal of Cell Science, vol. 126, no. 13, pp. 2924–2930, 2013.

J. Förtsch, E. Hummel, M. Krist, and B. Westermann, “The myosin-related motor protein Myo2 is an essential mediator of bud-directed mitochondrial movement in yeast,” Journal of Cell Biology, vol. 194, no. 3, pp. 473–488, 2011.

J. R. Veatch, M. A. McMurray, Z. W. Nelson, and D. E. Gottschling, “Mitochondrial dysfunction leads to nuclear genome instability via an iron-sulfur cluster defect,” Cell, vol. 137, no. 7, pp. 1247–1258, 2009.

D. Sinclair, K. Mills, and L. Guarente, “Aging in Saccharomyces cerevisiae,” Annual Review of Microbiology, vol. 52, pp. 533–560, 1998.

P. Laun, A. Pichova, F. Madeo et al., “Aged mother cells of Saccharomyces cerevisiae show markers of oxidative stress and apoptosis,” Molecular Microbiology, vol. 39, no. 5, pp. 1166–1173, 2001.

A. L. Hughes and D. E. Gottschling, “An early age increase in vacuolar pH limits mitochondrial function and lifespan in yeast,” Nature, vol. 492, no. 7428, pp. 261–265, 2012.

C. Q. Scheckhuber, N. Erjavec, A. Tinazli, A. Hamann, T. Nyström, and H. D. Osiewacz, “Reducing mitochondrial fission results in increased life span and fitness of two fungal ageing models,” Nature Cell Biology, vol. 9, no. 1, pp. 99–105, 2007.

A. Baryshnikova, M. Costanzo, Y. Kim et al., “Quantitative analysis of fitness and genetic interactions in yeast on a genome scale,” Nature Methods, vol. 7, no. 12, pp. 1017–1024, 2010.