Research Reports:

Advance online publication

Impact of F1Fo-ATP-synthase dimer assembly factors on mitochondrial function and organismic aging

Nadia G Rampello1, Maria Stenger2, Benedikt Westermann2, Heinz D Osiewacz1

Download PDF download pdf
Show/hide additional information

    1 Department of Biosciences, Molecular Developmental Biology, Institute of Molecular Biosciences and Cluster of Excellence Frankfurt Macromolecular Complexes, J. W. Goethe University, 60438 Frankfurt, Germany.

    2 Cell Biology and Electron Microscopy, University of Bayreuth, 95440 Bayreuth, Germany.

Keywords: aging, F1Fo-ATP-synthase, membranes, mitochondria, remodeling.


CJ – cristae junction,

IM – inner membrane,

MICOS – mitochondrial contact site and cristae organizing system,

mPTP – mitochondrial permeability transition pore,

mtDNA – mitochondrial DNA,

OM – outer membrane,

OXPHOS – oxidative phosphorylation,

PCD – programmed cell death.
Received originally: 28/11/2017 Received in revised form: 23/01/2018
Accepted: 25/01/2018 Published: 30/01/2018

Heinz D. Osiewacz, Tel: +496979829264;

Conflict of interest statement: The authors declare that they have no conflict of interest.
Please cite this article as: Nadia G Rampello, Maria Stenger, Benedikt Westermann, Heinz D Osiewacz (2018). Impact of F1Fo-ATP-synthase dimer assembly factors on mitochondrial function and organismic aging. Microbial Cell: in press.


In aerobic organisms, mitochondrial F1Fo-ATP-synthase is the major site of ATP production. Beside this fundamental role, the protein complex is involved in shaping and maintenance of cristae. Previous electron microscopic studies identified the dissociation of F1Fo-ATP-synthase dimers and oligomers during organismic aging correlating with a massive remodeling of the mitochondrial inner membrane. Here we report results aimed to experimentally proof this impact and to obtain further insights into the control of these processes. We focused on the role of the two dimer assembly factors PaATPE and PaATPG of the aging model Podospora anserina. Ablation of either protein strongly affects mitochondrial function and leads to an accumulation of senescence markers demonstrating that the inhibition of dimer formation negatively influences vital functions and accelerates organismic aging. Our data validate a model that links mitochondrial membrane remodeling to aging and identify specific molecular components triggering this process.


Mitochondria are eukaryotic organelles involved in a number of essential processes including the synthesis of iron/sulfur clusters, biosynthesis of lipids and amino acids, energy transduction and generation of ATP. In aerobic organisms, most of this universal cellular energy carrier is generated by oxidative phosphorylation (OXPHOS) at the respiratory chain. The protein complexes and supercomplexes of the respiratory chain are located in invaginations of the inner membrane (IM), the so-called cristae, which occur in different shapes (e.g. tubular, lamellar) [1][2][3][4]. At their basis, the cristae junctions (CJ), cristae are connected to the outer membrane (OM), which surrounds the organelle.

F1Fo-ATP-synthase is an IM-bound protein complex that is essential for the electrochemical-driven generation of ATP. The individual proteins of the complex are encoded by the nuclear and by mitochondrial DNA (mtDNA). Mutations in the corresponding genes lead to F1Fo-ATP-synthase deficiency, mitochondrial dysfunction [5] and severe neurodegenerative pathologies like Alzheimer’s and Parkinson’s disease [6][7][8] and have a strong impact on biological aging [9][10][11]. Beside its enzymatic role, the F1Fo-ATP-synthase complex plays a key role in shaping cristae structure [12][13][14]. In particular, rows of F1Fo-ATP-synthase dimers at the tips of the cristae appear to be critical for maintaining their typical convex curvature [15][16]. Recent studies identified the impact of another protein complex, the mitochondrial contact site and cristae organizing system (MICOS) [17], in controlling IM ultrastructure [3][18][19][20]. This complex is localized at the CJ. Despite the distant localization of the two complexes, interactions between them, or at least of components of them, were demonstrated. It was found that Mic10, a core component of MICOS, interacts with the dimeric F1Fo-ATP-synthase and stabilizes the complex [21][22]. The mechanisms regulating these interactions are largely unknown but are of key relevance for the remodeling of mitochondrial ultrastructure that is observed as adaptive response to physiological changes [23][24].

Pronounced changes of the mitochondrial ultrastructure were previously demonstrated to occur during aging of the aging model organism Podospora anserina. Mitochondria from juvenile cultures predominantly contain well-structured lamellar cristae with rows of F1Fo-ATP-synthase dimers at their tips. During aging, the invaginations of the IM recede and the membrane curvature becomes concave forming a system of vesicles in the matrix space. This process of membrane reorganization goes along with a dissociation of F1Fo-ATP-synthase dimers. Occasionally, vesicles in the matrix of old mitochondria are found in close contact with the OM at contact sites. It was suggested that at late age the OM bursts at these sites and releases mitochondrial content to the cytosol inducing programmed cell death (PCD) [25]. The relevance of this series of cellular events observed during P. anserina aging is supported by genetic manipulations of the molecular machinery involved in the control of PCD, the final phase in the life cycle of P. anserina [26][27]. Strikingly, overexpression of a gene coding for the mitochondrial peptidyl prolyl-cis,trans-isomerase, cyclophilin D (CYPD), which is involved in the control of the mitochondrial permeability transition pore (mPTP) opening [28], leads to accelerated aging. In this overexpression strain mitochondria of young chronological age (6-days) display a vesicular ultrastructure that is characteristic for old wild-type mitochondria of 18-days of age [29]. The molecular components involved in this process and its regulation were unknown.

In the yeast Saccharomyces cerevisiae, it was shown that dimer and oligomer formation is mediated by the interaction of two dimer assembly factors, subunit e (Atp21, Su e) and subunit g (Atp20, Su g) of F1Fo-ATP-synthase [30][31]. Deletion of a gene coding for either one of these proteins leads to a loss of dimers and oligomers without influencing the catalytic ATP-synthase activity of the enzyme but inducing a strong alteration of mitochondrial ultrastructure [30][32]. Surprisingly, the downregulation of the gene coding for subunit e or g in HeLa cells affects not only the stability of dimers and oligomers but also the catalytic activity of the enzyme and mitochondrial morphology [33].

Here we report novel data from a study aimed to generate mechanistic insights into the impact of mitochondrial ultrastructure on biological aging. We focused on PaAtpe and PaAtpg encoding the two putative F1Fo-ATP-synthase dimer assembly factors of P. anserina and investigated their age-related expression. Moreover, we analyzed the impact of the ablation of the two dimer assembly factors on biological aging in detail. Our data extend a model describing the age-related mitochondrial membrane remodeling including the role of F1Fo-ATP-synthase dimers and dimer assembly factors PaATPE and PaATPG.


The abundance of F1Fo-ATP-synthase dimers decreases during aging

Previous work revealed an essential role of F1Fo-ATP-synthase dimers in the formation of mitochondrial cristae [12][13][14][16] and a decrease of mitochondria with lamellar cristae accompanied by an increase of those with a vesicular ultrastructure during aging of P. anserina [25][29]. To elucidate the biochemical basis of these microscopic observations, we analyzed mitochondria from batches isolated from 6-days and 16-days old cultures of the P. anserina wild type that previously were used for cryo-electron microscopy [25] and subjected them to BN-PAGE analysis (Fig. 1A). We observed a 20% decrease of F1Fo-ATP-synthase dimers in 16-days old cultures compared to 6-days old cultures. This effect is likely to be underestimated because of the elimination of impaired mitochondria during aging by autophagy, a quality control pathway that increases during aging [34][35]. Apart from a decrease in abundance of F1Fo-ATP-synthase dimers, a marked change of supercomplex amount S1 (I1III2IV1) and S0 (I1III2IV0) is observed during aging (Fig. 1A). In cells of 6-days old cultures S1 predominates while this supercomplex is decreased in 16-days cultures. In contrast, an increase of S0 is observed during aging (Fig. 1A).

FIGURE 1: Age-dependent dimer decrease and analysis of expression of PaAtpe and PaAtpg in P. anserina. (A) Representative BN-PAGE analysis and quantification of mitochondrial protein extracts (V2, F1Fo-ATP-synthase dimers) from three independent 6-days and 16-days old wild-type strains. F1Fo-ATP-synthase dimers were normalized to Coomassie stained gel. Relative dimer content of 6-days old wild-type strains was set to 100%. Mitochondrial protein complexes were stained with Coomassie Blue and complexes and supercomplexes S1, S0, V2, I1, V1, III1 and IV1 are indicated. (B) Transcript analysis of PaAtpe and PaAtpg in three young (4 d) and old (16 d) wild type cultures, respectively. RNA was isolated and gene expression was determined by qRT-PCR analyses. The relative expression was normalized to the expression of PaPorin coding for a mitochondrial outer membrane protein. Error bars represent the standard deviation and the P-values were determined by Student´s t test.

Next, we investigated the age-associated expression of PaAtpe and PaAtpg, coding for two potential factors involved in the control of F1Fo-ATP-synthase dimer formation. A comparative transcript analysis of these genes of young (4-days) and senescent (16-days) P. anserina cultures revealed a reduction of the PaAtpg transcript level but no significant alteration of PaAtpe transcripts (Fig. 1B), suggesting that the age-related regulation or stability of the two putative dimer-specific genes differs. Interestingly, in the young wild type, transcript levels of PaAtpe are considerably lower than those of PaAtpg. These observations let us speculate about different regulatory mechanisms and probably different functions of the two dimer assembly factors. It appears that PaATPE is a limiting but central factor in dimer formation. This idea is supported by different studies with yeast demonstrating that dimer assembly factors bind to the Fo part of ATP-synthase in a sequential manner. First Su e binds to the Fo part followed by the association of Su g [31][36]. It was shown that the presence of Su e is required for stabilization of Su g whereas Su g is not necessary for binding of Su e [37]. Thus, Su e appears to play a key role in ATP-synthase dimer formation while Su g acts as a protein supporting Su e in this function [30][31].

Overall, the observed changes in F1Fo-ATP-synthase dimer quantity and alterations of supercomplexes S1 to S0 indicate mitochondrial membrane reorganization processes during aging of P. anserina. These biochemical data are in concordance with the observations of earlier cryo-electron microscopy studies [25][29].

Ablation of PaATPE and PaATPG affects dimer formation and mitochondrial ultrastructure

Next, we focused on the role of PaATPE and PaATPG in the formation of F1Fo-ATP-synthase dimers. In yeast and HeLa cells the lack of one of the homologues is sufficient to inhibit F1Fo-ATP-synthase dimer formation [30][31][33]. In both model organisms, the deletion of either gene strongly affects mitochondrial ultrastructure. In yeast, onion-like structures of the IM are found [12]. In HeLa cells, the IM forms arch-like or longitudinal cristae [33].

We generated P. anserina strains in which either PaAtpe (P. anserina accession number: Pa_1_3740) or PaAtpg (P. anserina accession number: Pa_1_2480) were replaced by a bifunctional selection marker that mediates phleomycin and blasticidin resistance [38]. Strains were verified by Southern blot analysis using a specific Phleo and PaAtpe or PaAtpg probe (Fig. 2A). Subsequent analysis of mitochondrial extracts from each of the two deletion strains by BN-PAGE revealed the absence of F1Fo-ATP-synthase dimers (Fig. 2B) and demonstrated that the P. anserina proteins encoded by these two genes are indeed involved in the dimerization of F1Fo-ATP-synthase monomers.

Created with GIMP

FIGURE 2: Deletion of PaAtpe or PaAtpg affects F1Fo-ATP-synthase dimer formation and mitochondrial inner membrane ultrastructure. (A) Southern blot analysis of HindIII- and EcoRV-digested genomic DNA (gDNA) of wild-type, ΔPaAtpe and ΔPaAtpg strains. The digested gDNA was hybridized with a specific PaAtpe, PaAtpg and Phleo probe, respectively, and demonstrated a successful deletion of PaAtpe and PaAtpg. (B) Representative BN-PAGE analysis of mitochondrial protein extracts from 6-days old wild-type, ΔPaAtpe and ΔPaAtpg strains. Mitochondrial complexes including S1, V2, I1, V1, III1 and IV1 were visualized by Coomassie staining. (C) EM of isolated mitochondria of wild-type and deletion strains of different age (6 days and 16 days old). The morphology of at least 50 organelles per strain and growth condition was analyzed. Representative images are shown at the same magnification. Scale bar: 0,2 µm.

Subsequently, we analyzed whether the lack of F1Fo-ATP-synthase dimers affects mitochondrial ultrastructure. Electron microscopy of mitochondria isolated from young (6-days) and old (16-days) wild-type strains revealed pronounced remodeling of the IM during aging (Fig. 2C), corresponding to what was described earlier in a cryo-electron microscopy study [29]. While well-separated lamellar cristae with a typical convex curvature at the tips could be readily found in preparations of young wild type mitochondria, mitochondria from old cultures were generally devoid of lamellar cristae and the inner membrane frequently formed septa and vesicular structures (reticulate ultrastructure). Mitochondria isolated from PaAtpe and PaAtpg deletion strains of young chronological age (i.e. 6-days) strikingly resemble old wild type mitochondria (16-days). Importantly, typical lamellar cristae could not be found in mutant or old wild type mitochondria (Fig. 2C). These results clearly demonstrate a direct impact of F1Fo-ATP-synthase dimers on the formation of lamellar cristae and aging-dependent mitochondrial membrane reorganization.

Defects in F1Fo-ATP-synthase dimerization affects mitochondrial function and leads to accelerated aging

In a series of subsequent experiments, we concentrated on the impact of F1Fo-ATP-synthase dimerization on aging of P. anserina. We compared well-known senescent markers in the two deletion strains and the wild type of defined chronological age. Apart from the recently identified ultrastructural reorganization of the IM, changes in mitochondrial morphotype [39], reorganization of the mitochondrial DNA (mtDNA) [40][41][42][43][44], an increase in hydroxide peroxide (H2O2) release from cultures [39][45] and impairments in respiration [46] were analyzed as hallmarks of aging.

Light microscopy analysis identified an accelerated change of mitochondrial morphotypes in the two investigated deletion strains. In contrast to the wild type, in which mitochondria from 3-days old cultures are mainly of a filamentous morphotype, mitochondria of the same chronological age of the two deletion mutants display a punctate morphotype that is characteristic for mitochondria of old (i.e. 16-days old) wild-type strains (Fig. 3A).

FIGURE 3: Impairments of mitochondrial functions affect growth and lifespan in deletion mutants. (A) Comparison of mitochondrial morphology of 3-days and 16-days old wild-type strains with those of ΔPaAtpe and ΔPaAtpg (3 d) by fluorescence microscopy. Mitochondria were stained with MitoTracker® Red and analyzed by confocal fluorescence microscopy. Scale bars: 10 µm. (B) Representative Southern blot analysis of BglII-digested gDNA of wild-type (4-days and 16-days old), ΔPaAtpe and ΔPaAtpg strains (4-days old). The 2500 bp age-specific plDNA (arrow) fragment was detected with a specific plDNA probe. (C) Release of ROS species H2O2 from wild-type (6-days n=3), ΔPaAtpe (6-days n=3) and ΔPaAtpg strains (6-days n = 3) visualized by DAB precipitation. (D) Oxygen consumption (basal respiration) of 6-days old deletion mutant mycelium compared to respiration of 6-days old wild type mycelium (n = 3-4 biological replicates with a total number of 12-16 technical replicates). (E) Relative COX- and AOX-dependent oxygen consumption rate (OCR) of 6-days old wild-type and 6-days old deletion strains mycelium after treatment with KCN (COX-inhibitor) or SHAM (AOX-inhibitor). (F) Relative complex I-dependent OCR of 6-days old wild-type mitochondria compared to mitochondria from 6-days old deletion mutants (n = 4-8 biological replicates with a total number of 15-28 technical replicates). State 4 OCR of mitochondria from wild type was set to 100%. (G) ATP production of 6-days old wild-type and 6-days old deletion mutant mitochondria after removal of samples during state 3 respiration measurements. Samples of three biological replicates and two technical replicates, respectively, were measured three times by a luminescence-based assay. (H) Phenotypic analysis of indicated strains growing on M2 medium for 4 days. (I) Growth rate of wild type (0.58 ± 0.05 cm/d, n = 27), ΔPaAtpe (0.53 ± 0.05 cm/d, n = 25) and ΔPaAtpg (0.53 ± 0.08 cm/d, n =3 3) growing on M2 medium. Growth rate was determined from day 3 to 6 of growth. (J) Lifespan analysis of wild type (mean lifespan = 23.3 d, n = 27), ΔPaATPe (mean lifespan = 15.1 d, n = 25,) and ΔPaATPg (mean lifespan = 13.5 d, n = 33) growing on M2 medium. The error bars represent the standard deviation and the P-values were determined by Student´s t test.

Analysis of mtDNA revealed an accelerated amplification of a mitochondrial plasmid-like DNA (plDNA). In 4-days old PaAtpe and PaAtpg deletion strains this senescent marker is already strongly amplified. In the wild type, plDNA is almost absent from 4-days old cultures and found in strains of much older age (e.g. 16-days) (Fig. 3B).

Next, we analyzed H2O2 release [39]. Incubation of wild-type and deletion strains of the same chronological age (6-days) with a diaminobenzidin (DAB) staining solution revealed an increase of a brown precipitate demonstrating a strong increase in H2O2 release by ΔPaAtpe and ΔPaAtpg cultures (Fig. 3C).

In order to link these different age-dependent changes to mitochondrial functions, we measured respiration of P. anserina deletion strains. Clearly, total oxygen consumption of deletion strains is reduced in comparison to the wild type (Fig. 3D). Furthermore, we determined respiration of wild-type, ΔPaAtpe and ΔPaAtpg strains in the presence and absence of respiration inhibitors potassium cyanide (KCN), inhibiting complex IV (COX), and salicylhydroxamic acid (SHAM), inhibiting the alternative oxidase AOX (Fig. 3E). Notably, in the two deletion strains alternative respiration is slightly increased as compensatory response to OXPHOS impairments and increased mitochondrial stress [46][47][48]. These data are in concordance with studies in yeast in which mutations of several subunits of F1Fo-ATP-synthase like Atp4 [49] or Su e and Su g [50][51] lead to a destabilization of of the complex and a reduced COX activity.

Determination of the relative oxygen consumption rate (OCR) via complex I of isolated mitochondria from wild-type, ΔPaAtpe and ΔPaAtpg strains revealed that state 4 (ADP-independent) as well as state 3 (ADP-dependent) respiration is significantly decreased in deletion mutants. State 3 respiration is most strongly affected (Fig. 3F). An impaired respiration often results in an inefficient ATP production. To test F1Fo-ATP-synthase activity, we removed part of the samples used for state 3 respiration measurements and determined ATP production in this state using a luciferin-luciferase assay. We found that ATP content in deletion strains is significantly reduced compared to the wild type (Fig. 3G) indicating that monomeric F1Fo-ATP-synthase is not as efficient as the dimeric form. Thus, the dimerization of F1Fo-ATP-synthase is not only important for F1Fo-ATP-synthase dimerization and mitochondrial ultrastructure but also for energy transduction. Similar effects were also observed in yeast and HeLa cells. In HeLa cells, downregulation of dimer-specific genes leads to an increase of doubling-times and a reduction of OXPHOS capacity [33]. Yeast cells in which either one of the two dimer assembly factors is ablated display an abnormal mitochondrial morphology, a decreased growth rate on non-fermentable carbon sources and reduced respiration [12][30].

The effect of reduced ATP generation in PaAtpe and PaAtpg deletion strains is not apparent in the first days (e.g. 4 days) of growth. At this time, cultures display the same morphology and radial growth rate as the wild type (Fig. 3H). Later on (days 3 – 6), growth rate of deletion strains becomes slightly, but significantly reduced when compared to the wild type (Fig. 3I). The reduction of the growth rate in the presenescent life phase is another aging marker that together with the described changes in mitochondrial morphology and ultrastructure as well as mitochondria dysfunction, reorganization of mtDNA and the increase in ROS production suggests an acceleration of the aging process in ΔPaAtpe and ΔPaAtpg strains. This conclusion was finally verified by determination of the lifespan of the two deletion strains. In comparison to the wild type, the lifespan of the mutants is strongly reduced by 33% and 42%, respectively (Fig. 3J). Until now, such an effect on biological aging was not reported in any of the different established aging models, including yeast in which F1Fo-ATP-synthase dimerization factors were extensively studied.

Conclusions and perspectives

Here we provide novel data on the identification of individual components involved in the control of mitochondrial inner membrane remodeling and their impact on biological aging. These experimental data extend a model that was proposed from earlier cryo-electron microscopy studies [25] and from data of genetic interventions into the induction of PCD via the overexpression of a gene coding for cyclophilin D, a regulator of the mitochondrial permeability transition (mPT) [29]. In this particular strain, it was demonstrated that autophagy is induced to an extent that leads to autophagic cell death [52]. Significantly, CYPD is known to interact with the lateral stalk of the F1Fo-ATP-synthase decreasing its activity [53]. Moreover, F1Fo-ATP-synthase dimers were demonstrated to be part of the mPTP [54] and that opening of the mPTP correlates with the dissociation of dimers [55]. Overall, these and the data presented in our current study highlight the central role of F1Fo-ATP-synthase in mitochondrial biology. However, the regulatory circuits and the mechanisms involved in the different aspects of F1Fo-ATP-synthase function remain to be unraveled in detail. Concerning the role in mitochondrial ultrastructure remodeling, the identification and the characterization of components involved in this process is crucial. Apart from the role of F1Fo-ATP-synthase dimers at the cristae tips, the MICOS complex has been recently identified [18][19][20]. Interestingly, it was found that both complexes are necessary for cristae formation. Notwithstanding that the core MICOS protein Mic60 and dimer assembly factors Su e and Su g play antagonistic roles [14], the other core MICOS protein, Mic10, was found to interact with Su e of the F1Fo-ATP-synthase [21][22]. Furthermore, the demonstration of a F1Fo-ATP-synthase oligomerization promoting effect of Mic27 [21] also suggests an interplay of the MICOS complex with the F1Fo-ATP-synthase dimer. The elucidation of regulation of these crosstalks will certainly be a key aspect of future investigations.


P. anserina strains and cultivation

In this study wild type ‘s’ [56] and the newly generated deletion strains ΔPaAtpe and ΔPaAtpg were used. Strains were grown on standard cornmeal agar (BMM) at 27°C under constant light [57]. For spore germination, standard cornmeal agar (BMM) supplemented with 60 mM ammonium acetate was used and incubated at 27°C in dark for 2 days. For all experiments strains were cultivated on M2 plates for 2 days at 27°C under constant light and transferred in CM liquid medium for 2 days at 27°C under constant light. Flasks were shaken at 160 rounds per minute (rpm). All strains used in this study were derived from monokaryotic ascospores [57].

Cloning procedures and generation of P. anserina mutants

Deletion of PaAtpe and PaAtpg was performed with the method described by Hamann et al., 2005 [38]. Briefly, a small 5’-flank of genes PaAtpe and PaAtpg, respectively, was amplified with oligonucleotides ATPe_KO1 (5’-GTGGTACCCGCTGTGAGAGCTTCTTC-3’), ATPe_KO2 (5’-GCAAGCTTTTTGAGGAATCTGGGGGC-3’), ATPg_KO1 (5’-CGGGTACCGTGAAGAGCGTATGTTGG-3’) and ATPg_KO2 (5’-GCAAGCTTTTCGAACTTCGGGCACTG-3’). A small 3’-flank of the same genes was amplified with oligonucleotides ATPe_KO3 (5’- GCACTAGTACTGTCCGTCGACGAACT-3’), ATPe_KO4 (5’- AAAGCGGCCGCTCAACGATGTGACATTG-3’), ATPg_KO3 (5’- CTACTAGTTCTTAGCGCAGGGAGGTG-3’) and ATPg_KO4 (5’- CAGCGGCCGCAGGTTGCAACAGTAGTAG-3’). Recognition sites of restriction endonucleases are underlined. The 5’ fragments were digested with KpnI and HindIII and the 3’ fragments with BcuI and NotI and ligated into previously digested plasmid pKO4. The resulting plasmids were termed pAtpeKO1 and pAtpgKO1 and contain a resistance cassette with phleomycin and blasticidin marker genes for fungal and bacterial selection, respectively. The flanked resistance cassettes were digested with NotI and KpnI and used for transformation of Escherichia coli strain KS272 bearing the plasmid pKOBEG [58] and the cosmid 15C5 containing the PaAtpe locus or cosmid 13B10 containing the PaAtpg locus, respectively. Homologous recombination between the flanks of the resistance cassette and cosmid 15C5 and 13B10 leads to generation of ∆Atpe15C5 and ∆Atpg13B10, which contain the two resistance markers surrounded by large flanks. The cosmid was isolated and used for transformation of wild type P. anserina. Selection of positive PaAtpe and PaAtpg deletion strains was performed by growth on medium containing phleomycin. The deletion of PaAtpe and PaAtpg was verified by Southern blot analysis as described below.

Southern blot analysis

Total DNA was isolated according to Lecellier and Silar, 1994 [59]. DNA restriction, gel electrophoresis and Southern blotting were performed according to standard protocols. For Southern blot hybridization and detection, digoxigenin-labeled hybridization probes (‘DIG DNA Labeling and Detection Kit’) were used according to the manufacturer’s instructions. The PaAtpe-specific hybridization probe was amplified by PCR using the oligonucleotides Pa_1_3740-1 (5’-AATGGCCTCTTCCGGAGTC-3’) and Pa_1_3740-2 (5’-CTCGAGGTCGAAGCTTGAG-3’) corresponding to 511 nucleotides of the gene PaAtpe. The PaAtpg-specific hybridization probe was amplified by PCR using the oligonucleotides Pa_1_2480-3 (5’- TCTTTCGCCCTCCTCTCAC-3’) and Pa_1_2480-4 (5’- AGACGATCTTGGCCACCTC-3’) corresponding to 418 nucleotides of the gene PaAtpg. As a hybridization probe specific for the phleomycin resistance gene (Ble), the 1293 bp BamHI-fragment of the plasmid pKO4 [60] was used. As a hybridization probe specific for the plDNA the 2500 bp BamHI-fragment of the plasmid pSP17 [61] was used.

Growth rate and lifespan determination

To determine lifespan and growth rate of P. anserina strains used in this study, monokaryotic ascospores were isolated from crosses of respective strains and germinated for 2 days at 27°C in the dark on BMM supplemented with 60 mM ammonium acetate. After germination mycelia were placed on M2 medium [57] and incubated at 27°C under constant light. The lifespan is defined as the period of linear growth in days (d). The growth rate was measured as growth in centimeters per day (cm/d).

Transcript analysis

Plates containing M2 medium covered with cellophane were inoculated with small pieces of mycelium and incubated for 2 days at 27°C under constant light. Total RNA was isolated from scraped fungal mycelium using the Nucleo Spin® RNA Plant-Kit (Macherey-Nagel). Reverse transcription of 1 mg total RNA was performed with the RevertAid™ M-MuLV reverse transcriptase (ThermoScientific) according to the manufacturer’s instruction. Real-time PCR was realized using iQ SYBR Green Supermix (BioRad) followed by the manufacturer’s protocol. For each gene, the efficiency (E) of the primer pairs was calculated based on a real-time PCR with a dilution series of cDNA according to E = 10[-1 ⁄ Slope] [62]. The relative expression level (normalized to the level of the porin transcript) was calculated according to the following formula: Relative expression= (E(porin)^CP(porin))/(E(target gene)^CP(target gene)) with: E = PCR efficiency of the respective primer pair and CP = crossing point for each transcript.

Mitochondria isolation

Mitochondria of P. anserina cultures were isolated by differential centrifugation for measurement of mitochondrial oxygen consumption and BN-PAGE analysis [57].

Blue-native polyacrylamide gels (BN-PAGE)

BN-PAGE was performed as previously described [63]. For each sample 75-100 µg of mitochondrial protein extracts were solubilized using a digitonin/protein ratio of 3:1 (w/w). Linear gradient gels (4-13%) overlaid with 3.5% stacking gels were used for separation of solubilized mitochondria. Respiratory chain components were subsequently visualized by Coomassie blue staining and assigned as described [64].

Mitochondrial oxygen consumption

Measurement of mitochondrial oxygen consumption was performed at 27°C using two different high-resolution respirometers (Oxygraph-2k series C and G, Oroboros Instruments, Innsbruck, Austria). 200 μg freshly prepared mitochondria were injected into 2 ml air saturated oxygen buffer (0.3 M sucrose, 10 mM KH2PO4, 5 mM MgCl2, 1 mM EDTA, 10 mM KCl, 0.1% BSA; pH = 7.2). To determine the complex I-dependent state 4 respiration (state 4) 20 mM pyruvate and 5 mM malate were added. Thereafter, 1.5 mM ADP was added to determine complex I-dependent state 3 respiration (state 3).

Determination of complex IV- and AOX-dependent oxygen consumption was performed using strains cultivated on M2 medium for 2 days and in CM liquid medium for 2 days as described above. Small pieces of mycelium were subsequently transferred into the respirometer and oxygen consumption was measured in liquid CM medium according to the manufacturer’s instructions. 1 mM KCN was added to inhibit respiration via complex IV. 4 mM salicylhydroxamic acid (SHAM) was added to inhibit respiration via AOX.

Data were analyzed using the manufacturer´s software DatLab 6.

ATP measurement

For determination of ATP production samples were removed after measurement of state 3 respiration. Thereafter samples were boiled in a water bath for 15 minutes. After boiling they were centrifuged for 10 min and 14,000 rpm and transferred into new reaction tubes. The supernatant was diluted (1:30) and ATP amount was measured by using the ATP Bioluminescence Assay Kit (CLS II, Roche) adapted for use in a microtiter plate format. The assay was performed according to the manufacturer’s instructions.

Fluorescence microscopy

P. anserina mycelia were grown on microscope slides with a central depression that is filled with M2 agar medium and incubated for 1-2 days at 27°C and constant light. Hyphae were stained with 1 µM of the mitochondrial specific dye Mito Tracker CMX ROS (Invitrogen) and visualized using a confocal laser scanning microscope (CLSM TCS SP5, Leica).

Electron microscopy

Electron microscopy of chemically fixed isolated mitochondria was performed as described [65].

Hydrogen peroxide release assay

To determine the H2O2 release mycelia were cultivated on M2 medium at 27°C in the dark for 4 days. The plates were flooded with a solution containing 100 mM Tris/HCl pH 6.9 and 2.5 mM diaminobenzidine (DAB) and incubated for 30 min in the dark and 27°C. Subsequently, the solution was poured off and the plates were incubated again for 3 h at 27°C in the dark.

Statistical analysis

All statistical significances were calculated using the Student t-test. P-values <0.05 were considered statistically significant. P ≤ 0.05: *, P ≤ 0.01: **, P ≤ 0.001: ***.


  1. M. Zick, R. Rabl, and A.S. Reichert, "Cristae formation—linking ultrastructure and function of mitochondria", Biochimica et Biophysica Acta (BBA) - Molecular Cell Research, vol. 1793, pp. 5-19, 2009.
  2. S. Cogliati, J.A. Enriquez, and L. Scorrano, "Mitochondrial Cristae: Where Beauty Meets Functionality", Trends in Biochemical Sciences, vol. 41, pp. 261-273, 2016.
  3. M.E. Harner, A. Unger, W.J. Geerts, M. Mari, T. Izawa, M. Stenger, S. Geimer, F. Reggiori, B. Westermann, and W. Neupert, "An evidence based hypothesis on the existence of two pathways of mitochondrial crista formation", eLife, vol. 5, 2016.
  4. H. Rampelt, R.M. Zerbes, M. van der Laan, and N. Pfanner, "Role of the mitochondrial contact site and cristae organizing system in membrane architecture and dynamics", Biochimica et Biophysica Acta (BBA) - Molecular Cell Research, vol. 1864, pp. 737-746, 2017.
  5. A.I. Jonckheere, J.A.M. Smeitink, and R.J.T. Rodenburg, "Mitochondrial ATP synthase: architecture, function and pathology", Journal of Inherited Metabolic Disease, vol. 35, pp. 211-225, 2011.
  6. T. Tatsuta, and T. Langer, "Quality control of mitochondria: protection against neurodegeneration and ageing", The EMBO Journal, vol. 27, pp. 306-314, 2008.
  7. P. Coskun, J. Wyrembak, S.E. Schriner, H. Chen, C. Marciniack, F. LaFerla, and D.C. Wallace, "A mitochondrial etiology of Alzheimer and Parkinson disease", Biochimica et Biophysica Acta (BBA) - General Subjects, vol. 1820, pp. 553-564, 2012.
  8. K. Itoh, K. Nakamura, M. Iijima, and H. Sesaki, "Mitochondrial dynamics in neurodegeneration", Trends in Cell Biology, vol. 23, pp. 64-71, 2013.
  9. M.T. Lin, and M.F. Beal, "Mitochondrial dysfunction and oxidative stress in neurodegenerative diseases", Nature, vol. 443, pp. 787-795, 2006.
  10. B.M. Baker, and C.M. Haynes, "Mitochondrial protein quality control during biogenesis and aging", Trends in Biochemical Sciences, vol. 36, pp. 254-261, 2011.
  11. H.D. Osiewacz, and D. Bernhardt, "Mitochondrial Quality Control: Impact on Aging and Life Span - A Mini-Review", Gerontology, vol. 59, pp. 413-420, 2013.
  12. C. Bornhövd, F. Vogel, W. Neupert, and A.S. Reichert, "Mitochondrial Membrane Potential Is Dependent on the Oligomeric State of F1F0-ATP Synthase Supracomplexes", Journal of Biological Chemistry, vol. 281, pp. 13990-13998, 2006.
  13. M. Strauss, G. Hofhaus, R.R. Schröder, and W. Kühlbrandt, "Dimer ribbons of ATP synthase shape the inner mitochondrial membrane", The EMBO Journal, vol. 27, pp. 1154-1160, 2008.
  14. R. Rabl, V. Soubannier, R. Scholz, F. Vogel, N. Mendl, A. Vasiljev-Neumeyer, C. Körner, R. Jagasia, T. Keil, W. Baumeister, M. Cyrklaff, W. Neupert, and A.S. Reichert, "Formation of cristae and crista junctions in mitochondria depends on antagonism between Fcj1 and Sue/g", The Journal of Cell Biology, vol. 185, pp. 1047-1063, 2009.
  15. K.M. Davies, M. Strauss, B. Daum, J.H. Kief, H.D. Osiewacz, A. Rycovska, V. Zickermann, and W. Kuhlbrandt, "Macromolecular organization of ATP synthase and complex I in whole mitochondria", Proceedings of the National Academy of Sciences, vol. 108, pp. 14121-14126, 2011.
  16. K.M. Davies, C. Anselmi, I. Wittig, J.D. Faraldo-Gomez, and W. Kuhlbrandt, "Structure of the yeast F1Fo-ATP synthase dimer and its role in shaping the mitochondrial cristae", Proceedings of the National Academy of Sciences, vol. 109, pp. 13602-13607, 2012.
  17. N. Pfanner, M. van der Laan, P. Amati, R.A. Capaldi, A.A. Caudy, A. Chacinska, M. Darshi, M. Deckers, S. Hoppins, T. Icho, S. Jakobs, J. Ji, V. Kozjak-Pavlovic, C. Meisinger, P.R. Odgren, S.K. Park, P. Rehling, A.S. Reichert, M.S. Sheikh, S.S. Taylor, N. Tsuchida, A.M. van der Bliek, I.J. van der Klei, J.S. Weissman, B. Westermann, J. Zha, W. Neupert, and J. Nunnari, "Uniform nomenclature for the mitochondrial contact site and cristae organizing system", The Journal of Cell Biology, vol. 204, pp. 1083-1086, 2014.
  18. M. Harner, C. Körner, D. Walther, D. Mokranjac, J. Kaesmacher, U. Welsch, J. Griffith, M. Mann, F. Reggiori, and W. Neupert, "The mitochondrial contact site complex, a determinant of mitochondrial architecture", The EMBO Journal, vol. 30, pp. 4356-4370, 2011.
  19. S. Hoppins, S.R. Collins, A. Cassidy-Stone, E. Hummel, R.M. DeVay, L.L. Lackner, B. Westermann, M. Schuldiner, J.S. Weissman, and J. Nunnari, "A mitochondrial-focused genetic interaction map reveals a scaffold-like complex required for inner membrane organization in mitochondria", The Journal of Cell Biology, vol. 195, pp. 323-340, 2011.
  20. K. von der Malsburg, J. Müller, M. Bohnert, S. Oeljeklaus, P. Kwiatkowska, T. Becker, A. Loniewska-Lwowska, S. Wiese, S. Rao, D. Milenkovic, D. Hutu, R. Zerbes, A. Schulze-Specking, H. Meyer, J. Martinou, S. Rospert, P. Rehling, C. Meisinger, M. Veenhuis, B. Warscheid, I. van der Klei, N. Pfanner, A. Chacinska, and M. van der Laan, "Dual Role of Mitofilin in Mitochondrial Membrane Organization and Protein Biogenesis", Developmental Cell, vol. 21, pp. 694-707, 2011.
  21. K. Eydt, K.M. Davis, C. Behrendt, I.. Wittig, and A.S. Reichert, "Cristae architecture is determined by an interplay of the MICOS complex and the F1Fo ATP synthase via Mic27 and Mic10", Microbial Cell, vol. 4, pp. 259-272, 2017.
  22. H. Rampelt, M. Bohnert, R.M. Zerbes, S.E. Horvath, B. Warscheid, N. Pfanner, and M. van der Laan, "Mic10, a Core Subunit of the Mitochondrial Contact Site and Cristae Organizing System, Interacts with the Dimeric F 1 F o -ATP Synthase", Journal of Molecular Biology, vol. 429, pp. 1162-1170, 2017.
  23. C.A. Mannella, "Structure and dynamics of the mitochondrial inner membrane cristae", Biochimica et Biophysica Acta (BBA) - Molecular Cell Research, vol. 1763, pp. 542-548, 2006.
  24. T. Wai, and T. Langer, "Mitochondrial Dynamics and Metabolic Regulation", Trends in Endocrinology & Metabolism, vol. 27, pp. 105-117, 2016.
  25. B. Daum, A. Walter, A. Horst, H.D. Osiewacz, and W. Kuhlbrandt, "Age-dependent dissociation of ATP synthase dimers and loss of inner-membrane cristae in mitochondria", Proceedings of the National Academy of Sciences, vol. 110, pp. 15301-15306, 2013.
  26. A. Hamann, D. Brust, and H.D. Osiewacz, "Deletion of putative apoptosis factors leads to lifespan extension in the fungal ageing model Podospora anserina", Molecular Microbiology, vol. 65, pp. 948-958, 2007.
  27. A. Hamann, D. Brust, and H.D. Osiewacz, "Apoptosis pathways in fungal growth, development and ageing", Trends in Microbiology, vol. 16, pp. 276-283, 2008.
  28. C.P. Baines, "The molecular composition of the mitochondrial permeability transition pore", Journal of Molecular and Cellular Cardiology, vol. 46, pp. 850-857, 2009.
  29. D. Brust, B. Daum, C. Breunig, A. Hamann, W. Kühlbrandt, and H.D. Osiewacz, "Cyclophilin D links programmed cell death and organismal aging in Podospora anserina", Aging Cell, vol. 9, pp. 761-775, 2010.
  30. I. Arnold, "Yeast mitochondrial F1F0-ATP synthase exists as a dimer: identification of three dimer-specific subunits", The EMBO Journal, vol. 17, pp. 7170-7178, 1998.
  31. K. Wagner, P. Rehling, L.K. Sanjuán Szklarz, R.D. Taylor, N. Pfanner, and M. van der Laan, "Mitochondrial F1Fo-ATP Synthase: The Small Subunits e and g Associate with Monomeric Complexes to Trigger Dimerization", Journal of Molecular Biology, vol. 392, pp. 855-861, 2009.
  32. P. Paumard, J. Vaillier, B. Coulary, J. Schaeffer, V. Soubannier, D.M. Mueller, D. Brèthes, J. di Rago, and J. Velours, "The ATP synthase is involved in generating mitochondrial cristae morphology", The EMBO Journal, vol. 21, pp. 221-230, 2002.
  33. J. Habersetzer, I. Larrieu, M. Priault, B. Salin, R. Rossignol, D. Brèthes, and P. Paumard, "Human F1F0 ATP Synthase, Mitochondrial Ultrastructure and OXPHOS Impairment: A (Super-)Complex Matter?", PLoS ONE, vol. 8, pp. e75429, 2013.
  34. O. Philipp, A. Hamann, J. Servos, A. Werner, I. Koch, and H.D. Osiewacz, "A Genome-Wide Longitudinal Transcriptome Analysis of the Aging Model Podospora anserine", PLoS ONE, vol. 8, pp. e83109, 2013.
  35. L. Knuppertz, A. Hamann, F. Pampaloni, E. Stelzer, and H.D. Osiewacz, "Identification of autophagy as a longevity-assurance mechanism in the aging modelPodospora anserina", Autophagy, vol. 10, pp. 822-834, 2014.
  36. K. Wagner, I. Perschil, C.D. Fichter, and M. van der Laan, "Stepwise Assembly of Dimeric F1Fo-ATP Synthase in Mitochondria Involves the Small Fo-Subunits k and i", Molecular Biology of the Cell, vol. 21, pp. 1494-1504, 2010.
  37. V. Everard-Gigot, C.D. Dunn, B.M. Dolan, S. Brunner, R.E. Jensen, and R.A. Stuart, "Functional Analysis of Subunit e of the F1Fo-ATP Synthase of the Yeast Saccharomyces cerevisiae: Importance of the N-Terminal Membrane Anchor Region", Eukaryotic Cell, vol. 4, pp. 346-355, 2005.
  38. A. Hamann, K. Krause, A. Werner, and H.D. Osiewacz, "A two-step protocol for efficient deletion of genes in the filamentous ascomycete Podospora anserina", Current Genetics, vol. 48, pp. 270-275, 2005.
  39. C. Scheckhuber, N. Erjavec, A. Tinazli, A. Hamann, T. Nyström, and H. Osiewacz, "Reducing mitochondrial fission results in increased life span and fitness of two fungal ageing models", Nature Cell Biology, vol. 9, pp. 99-105, 2006.
  40. U. Stahl, P.A. Lemke, P. Tudzynski, U. Kück, and K. Esser, "Evidence for plasmid like DNA in a filamentous fungus, the ascomycete Podospora anserina.", Molecular & general genetics : MGG, 1978.
  41. D.J. Cummings, L. Belcour, and C. Grandchamp, "Mitochondrial DNA from Podospora anserina. I. Isolation and characterization.", Molecular & general genetics : MGG, 1979.
  42. L. Belcour, O. Begel, M. Moss�, and C. Vierny, "Mitochondrial DNA amplification in senescent cultures of Podospora anserina: Variability between the retained, amplified sequences", Current Genetics, vol. 3, pp. 13-21, 1981.
  43. U. K�ck, U. Stahl, and K. Esser, "Plasmid-like DNA is part of mitochondrial DNA in Podospora anserina", Current Genetics, vol. 3, pp. 151-156, 1981.
  44. H.D. Os�ewacz, and K. Esser, "The mitochondrial plasmid of Podospora anserina: A mobile intron of a mitochondrial gene", Current Genetics, vol. 8, pp. 299-305, 1984.
  45. M. Wiemer, . , H. Osiewacz, . , . , and . , "Effect of paraquat-induced oxidative stress on gene expression and aging of the filamentous ascomycete Podospora anserina", Microbial Cell, vol. 1, pp. 225-240, 2014.
  46. C. Borghouts, A. Werner, T. Elthon, and H.D. Osiewacz, "Copper-Modulated Gene Expression and Senescence in the Filamentous Fungus Podospora anserina", Molecular and Cellular Biology, vol. 21, pp. 390-399, 2001.
  47. S. Lorin, E. Dufour, J. Boulay, O. Begel, S. Marsy, and A. Sainsard-Chanet, "Overexpression of the alternative oxidase restores senescence and fertility in a long-lived respiration-deficient mutant of Podospora anserina", Molecular Microbiology, vol. 42, pp. 1259-1267, 2002.
  48. C.Q. Scheckhuber, K. Houthoofd, A.C. Weil, A. Werner, A. De Vreese, J.R. Vanfleteren, and H.D. Osiewacz, "Alternative Oxidase Dependent Respiration Leads to an Increased Mitochondrial Content in Two Long-Lived Mutants of the Ageing Model Podospora anserina", PLoS ONE, vol. 6, pp. e16620, 2011.
  49. M. PAUL, J. VELOURS, G. ARSELIN de CHATEAUBODEAU, M. AIGLE, and B. GUERIN, "The role of subunit 4, a nuclear-encoded protein of the F0 sector of yeast mitochondrial ATP synthase, in the assembly of the whole complex", European Journal of Biochemistry, vol. 185, pp. 163-171, 1989.
  50. G.M. Boyle, X. Roucou, P. Nagley, R.J. Devenish, and M. Prescott, "Identification of subunit g of yeast mitochondrial F1F0-ATP synthase, a protein required for maximal activity of cytochrome c oxidase", European Journal of Biochemistry, vol. 262, pp. 315-323, 1999.
  51. S. Saddar, M.K. Dienhart, and R.A. Stuart, "The F1F0-ATP Synthase Complex Influences the Assembly State of the Cytochromebc1-Cytochrome Oxidase Supercomplex and Its Association with the TIM23 Machinery", Journal of Biological Chemistry, vol. 283, pp. 6677-6686, 2008.
  52. P. Kramer, A.T. Jung, A. Hamann, and H.D. Osiewacz, "Cyclophilin D Is Involved in the Regulation of Autophagy and Affects the Lifespan of P. anserina in Response to Mitochondrial Oxidative Stress", Frontiers in Genetics, vol. 7, 2016.
  53. V. Giorgio, E. Bisetto, M.E. Soriano, F. Dabbeni-Sala, E. Basso, V. Petronilli, M.A. Forte, P. Bernardi, and G. Lippe, "Cyclophilin D Modulates Mitochondrial F0F1-ATP Synthase by Interacting with the Lateral Stalk of the Complex", Journal of Biological Chemistry, vol. 284, pp. 33982-33988, 2009.
  54. V. Giorgio, S. von Stockum, M. Antoniel, A. Fabbro, F. Fogolari, M. Forte, G.D. Glick, V. Petronilli, M. Zoratti, I. Szabo, G. Lippe, and P. Bernardi, "Dimers of mitochondrial ATP synthase form the permeability transition pore", Proceedings of the National Academy of Sciences, vol. 110, pp. 5887-5892, 2013.
  55. M. Bonora, C. Morganti, G. Morciano, G. Pedriali, M. Lebiedzinska‐Arciszewska, G. Aquila, C. Giorgi, P. Rizzo, G. Campo, R. Ferrari, G. Kroemer, M.R. Wieckowski, L. Galluzzi, and P. Pinton, " Mitochondrial permeability transition involves dissociation of F 1 F O ATP synthase dimers and C‐ring conformation ", EMBO reports, vol. 18, pp. 1077-1089, 2017.
  56. G. RIZET, "[Impossibility of obtaining uninterrupted and unlimited multiplication of the ascomycete Podospora anserina].", Comptes rendus hebdomadaires des seances de l'Academie des sciences, 1953.
  57. H.D. Osiewacz, A. Hamann, and S. Zintel, "Assessing Organismal Aging in the Filamentous Fungus Podospora anserina", Methods in Molecular Biology, pp. 439-462, 2012.
  58. M.K. Chaveroche, J.M. Ghigo, and C. d'Enfert, "A rapid method for efficient gene replacement in the filamentous fungus Aspergillus nidulans.", Nucleic acids research, 2000.
  59. G. Lecellier, and P. Silar, "Rapid methods for nucleic acids extraction from Petri dish-grown mycelia.", Current genetics, 1994.
  60. K. Luce, and H.D. Osiewacz, "Increasing organismal healthspan by enhancing mitochondrial protein quality control", Nature Cell Biology, vol. 11, pp. 852-858, 2009.
  61. C. Borghouts, E. Kimpel, and H.D. Osiewacz, "Mitochondrial DNA rearrangements of Podospora anserina are under the control of the nuclear gene grisea", Proceedings of the National Academy of Sciences, vol. 94, pp. 10768-10773, 1997.
  62. M.W. Pfaffl, "A new mathematical model for relative quantification in real-time RT-PCR.", Nucleic acids research, 2001.
  63. I. Wittig, H. Braun, and H. Schägger, "Blue native PAGE", Nature Protocols, vol. 1, pp. 418-428, 2006.
  64. F. Krause, C.Q. Scheckhuber, A. Werner, S. Rexroth, N.H. Reifschneider, N.A. Dencher, and H.D. Osiewacz, "Supramolecular Organization of CytochromecOxidase- and Alternative Oxidase-dependent Respiratory Chains in the Filamentous FungusPodospora anserina", Journal of Biological Chemistry, vol. 279, pp. 26453-26461, 2004.
  65. A. Unger, S. Geimer, M. Harner, W. Neupert, and B. Westermann, "Analysis of Yeast Mitochondria by Electron Microscopy", Methods in Molecular Biology, pp. 293-314, 2017.


HDO conceived and supervised this study. MS performed electron microscopy and, together with BW, analyzed the data. NGR performed the rest of the experiments and NGR and HDO analyzed data. HDO and NGR wrote the manuscript. BW and MS edited the manuscript. All authors read and approved the final manuscript.


This work was supported by grants of the Deutsche Forschungsgemeinschaft (DFG: Os75/17-1) to HDO and via the Cluster of Excellence ‘Macromolecular Complexes’. We thank Alexandra Werner for preparation of P. anserina mitochondria of defined age.


© 2018

Creative Commons License
Impact of F1Fo-ATP-synthase dimer assembly factors on mitochondrial function and organismic aging by Rampello et al. is licensed under a Creative Commons Attribution 4.0 International License.