Mitochondrial dysfunction and alterations in energy metabolism have been implicated in a variety of human diseases. Mitochondrial fusion is essential for maintenance of mitochondrial function and requires the prohibitin ring complex subunit prohibitin‐2 (PHB2) at the mitochondrial inner membrane. Here, we provide a link between PHB2 deficiency and hyperactive insulin/IGF‐1 signaling. Deletion of PHB2 in podocytes of mice, terminally differentiated cells at the kidney filtration barrier, caused progressive proteinuria, kidney failure, and death of the animals and resulted in hyperphosphorylation of S6 ribosomal protein (S6RP), a known mediator of the mTOR signaling pathway. Inhibition of the insulin/IGF‐1 signaling system through genetic deletion of the insulin receptor alone or in combination with the IGF‐1 receptor or treatment with rapamycin prevented hyperphosphorylation of S6RP without affecting the mitochondrial structural defect, alleviated renal disease, and delayed the onset of kidney failure in PHB2‐deficient animals. Evidently, perturbation of insulin/IGF‐1 receptor signaling contributes to tissue damage in mitochondrial disease, which may allow therapeutic intervention against a wide spectrum of diseases.
Podocyte‐specific PHB2 loss results in severe kidney disease that is alleviated by insulin and IGF‐1 receptors deletion or rapamycin treatment, demonstrating not only a causal link between mitochondrial dysfunction and kidney disease but also putative therapeutic avenues.
Deletion of the mitochondrial protein PHB2 in glomerular podocytes caused progressive proteinuria and death of the animals due to end‐stage kidney failure.
Contrary to generally held beliefs loss of PHB2 did not cause overt defects in mitochondrial respiratory activity or increased production of ROS but was accompanied by hyperactive insulin/IGF‐1 receptor signaling.
Inhibition of the insulin/IGF‐1 signaling system through genetic deletion of insulin receptor alone or in combination with the IGF‐1 receptor or treatment with mTOR inhibitor rapamycin, alleviated renal disease and delayed the onset of kidney failure in PHB2‐deficient animals.
The mitochondrial prohibitin (PHB) protein complex comprises two subunits, PHB1 and PHB2, that assemble into a high molecular weight ring complex in the mitochondrial inner membrane (Back et al, 2002; Tatsuta et al, 2005; Merkwirth & Langer, 2009). PHB proteins have multiple functions, they modulate mitochondrial m‐AAA protease activity (Steglich et al, 1999) and control lipid distribution in the mitochondrial inner membrane (Osman et al, 2009b), and they serve as membrane‐bound chaperones for the assembly of mitochondrial‐encoded proteins (Nijtmans et al, 2000) and recruit membrane proteins to a specific lipid environment (Osman et al, 2009a). Acting as a membrane scaffold, the PHB complex is involved in maintaining mitochondrial integrity, indispensable for cristae morphogenesis, and fusion of the organelles (Kasashima et al, 2008; Merkwirth et al, 2008). Cellular depletion of PHB2 in mouse embryonic fibroblasts (MEFs) led to disorganized and swollen mitochondrial cristae structures (Merkwirth et al, 2008). The conventional knockout of Phb2 in a mouse model resulted in embryonic lethality (Park et al, 2005; Merkwirth et al, 2008) while a conditional, neuron‐specific PHB2 deficiency led to neurodegeneration associated with loss of the mitochondrial genome and severe mitochondrial dysfunction (Merkwirth et al, 2012).
Deregulation of mitochondrial function, impaired energy homeostasis, and the production of reactive oxygen species have been implicated in aging‐associated phenotypes (Nunnari & Suomalainen, 2012; Bratic & Larsson, 2013) and a large variety of human disorders including kidney disease (Imasawa & Rossignol, 2013). The majority of kidney diseases affect the renal filtration unit, the glomerulus, as a consequence of a very limited capacity for regeneration and self‐renewal of terminally differentiated glomerular podocytes (Brinkkoetter et al, 2013). Podocytes are epithelial cells that have interdigitating foot processes to cover the outer surface of glomerular capillaries at the kidney filtration barrier and form the filtration slits. Podocytes are essential components of the kidney filtration unit and responsible for ultrafiltration of protein‐free urine from plasma.
To understand the contribution of mitochondrial dysfunction to kidney disease, we generated podocyte‐specific Phb2 knockout mice. Loss of PHB2 in podocytes inevitably led to progressive proteinuria, glomerulosclerosis, end‐stage renal failure, and death of the animals within 4–5 weeks. Surprisingly, either additional knockout of the insulin and IGF‐1 receptor or treatment with the mTORC1 inhibitor rapamycin partially rescued the phenotype of Phb2 knockout mice and prolonged survival.
Podocyte‐specific Phb2 knockout mice develop albuminuria and die prematurely
To understand the contribution of mitochondrial dysfunction to kidney disease, we deleted the Phb2 gene specifically in podocytes (Phb2pko) by mating a conditional Phb2fl/fl mouse line (Merkwirth et al, 2008) to podocyte‐specific Cre mice (NPHS2.cre) (Moeller et al, 2003). Mice of all genotypes were born following Mendelian rules (Supplementary Fig S1A). At birth, Phb2pko mutants appeared as healthy as wild‐type or heterozygous controls and did not show signs of glomerular dysfunction. The absence of PHB2 resulted in progressive and marked proteinuria reaching an albumin‐to‐creatinine ratio of 470 mg/mg at day 28 (Fig 1A), growth retardation, and massive loss of body weight in comparison with their wild‐type (Phb2fl/fl) and heterozygous littermates (Phb2het) (Fig 1B and C). Phb2pko mutant animals developed renal failure as indicated by a rise in serum creatinine and urea (Fig 1D and E). All animals died prematurely within 31–37 days postpartum (Fig 1F).
Phb2pko mice develop glomerulosclerosis
Histological analyses confirmed a normal renal histology at 14 days after birth but revealed progressive glomerulosclerosis at later stages, a phenotype closely resembling human glomerular disease (Fig 2A). At 28 days, Phb2pko mice presented with marked deposition of protein casts in the tubular system, collapsing glomerular capillaries and global glomerulosclerosis.
It is well established that in podocyte disease, the elaborate cytoarchitecture of podocyte foot processes is altered, leading to loss of the typical slit diaphragm structure. Slit diaphragms form a membrane‐like cell‐to‐cell contact that contains a protein complex of podocin and associated proteins (Brinkkoetter et al, 2013). Consistent with glomerulosclerosis being the result of podocyte disease, immunohistochemistry stainings for podocin showed alterations at 21 days and a dispersed and reduced staining at 28 days (Fig 2B). At 21 days, we observed podocyte effacement, that is, severe changes in foot process organization in all analyzed glomeruli of Phb2pko mice (Fig 2C). Podocyte effacement results in proteinuria, progressive renal damage with glomerular scarring, and eventual loss of renal function, necessitating renal replacement therapy in humans. At 28 days, the podocyte foot process structure was completely lost. As PHB2 is required for maintaining the structure of mitochondrial cristae, we assessed mitochondrial architecture (Fig 2D and E). At 14 days, both mitochondrial cristae structures and overall morphology were unaffected. However, 1 week later, lamellar cristae structures were disorganized or completely lost in mitochondria of Phb2pko podocytes, which is in line with previous reports of mitochondrial changes after deletion of Phb2 in neurons (Merkwirth et al, 2012). At 28 days, we were unable to analyze mitochondrial appearance due to progressive sclerosis and the overall loss of glomerular architecture.
As loss of PHB2 might render podocytes susceptible to apoptosis (Merkwirth et al, 2008, 2012; Baris et al, 2011; Wu & Wu, 2012), we studied whether the development of albuminuria was due to increased levels of apoptotic cell death resulting in reduced podocyte cell number. At 21 days, staining for cleaved caspase‐3 was completely negative (Supplementary Fig S2A). In addition, we quantified podocyte cell number by immunohistochemistry staining for WT‐1 in a blinded manner. Again, there were no differences in the overall podocyte cell number between Phb2fl/fl control and Phb2pko animals (Supplementary Fig S2B and C). In summary, Phb2pko mice did not show signs of increased apoptosis or cell loss at this early time point.
The phenotype of Phb2pko mice is not developmental
Although all relevant phenotypic changes were observed after day 14, at a time glomerulogenesis is completed, a developmental phenotype resulting from PHB2 loss could still not be excluded. We therefore tested whether the induction of PHB2 loss in adulthood might cause a similar phenotype. Phb2fl/fl mice were mated to podocin‐iCreER(T2) mice that allow expression of Cre recombinase activity upon tamoxifen induction (Wang et al, 2010). The resulting podocin‐iCreER(T2) Phb2pko animals (tPod–Phb2pko) received a tamoxifen‐enriched diet and developed progressive glomerulosclerosis (Fig 3A and B) and massive albuminuria (Fig 3C) as observed in non‐inducible Phb2pko mice. Thus, the phenotype of Phb2pko mice does not appear to be the result of altered developmental programs.
Podocyte‐specific knockout of the insulin receptor and IGF‐1 receptor prolongs survival of Phb2pko mice
Studies in yeast and the nematode Caenorhabditis elegans provided an intriguing link of mitochondrial PHB deficiency and altered insulin signaling (Artal‐Sanz & Tavernarakis, 2009; Schleit et al, 2013). In worms, loss of PHB2 decreased survival but prolonged lifespan of long‐lived daf‐2 mutants (Artal‐Sanz & Tavernarakis, 2009). In yeast, Phb2 deficiency activated the mitochondrial unfolded protein response (mtUPR), which was associated with reduced lifespan. This effect could be inhibited by dietary restriction reducing the mtUPR (Schleit et al, 2013). Given the complex, yet ill‐defined interactions of Phb2 deficiency and insulin signaling in model organisms, we tested whether inhibition of insulin and/or IGF‐1 receptor signaling specifically in podocytes modulated latency or severity of the disease phenotype of Phb2pko animals. Surprisingly, genetic deletion of the insulin receptor (Insr) in podocytes but not of the IGF‐1 receptor (Igf1r) attenuated renal disease of Phb2pko mice (Fig 4A and B). Phb2pko mice lacking a functional insulin receptor in podocytes (Insrpko) showed a highly significant survival advantage (Fig 4C). Generation of triple‐knockout animals with a genetic deletion of both insulin receptor and IGF‐1 receptor in addition to PHB2 (Phb2pko/Insrpko/Igf1rpko) significantly alleviated renal disease, enhanced survival (Fig 4D and E), improved kidney function, and delayed the onset of kidney failure (Fig 5A).
To exclude the possibility that the Cre recombinase insufficiently recombines three genes and thereby alleviates the Phb2‐related phenotype in the triple‐knockout animals, we isolated genomic DNA from glomeruli of Phb2pko and Phb2pko/Insrpko/Igf1rpko mice and performed quantitative PCR experiments specific for the deleted Phb2 gene. These studies did not detect any differences in Phb2 gene deletion efficiency between the single‐ and the triple‐knockout mice clearly excluding the possibility of altered recombination efficiency as a basis for the survival advantage (Fig 5B). In line with this, Phb2pko/Insrpko/Igf1rpko mice showed the same mitochondrial structural changes as seen in Phb2pko mice (Fig 5C). Moreover, double‐knockout as well as triple‐knockout mice developed massive albuminuria (Supplementary Fig S3A and B).
Insrpko/Igf1rpko showed normal survival for the time analyzed (until 8 weeks after birth) and did not develop proteinuria or renal disease (Supplementary Fig S4A and B) in contrast to previous observations demonstrating renal disease at later time points in life (Welsh et al, 2010).
Loss of PHB2 leads to changes of mitochondrial morphology
To better understand the beneficial effect of podocyte‐specific insulin signaling deficiency for renal disease and the role of PHB2 on metabolic signaling in podocytes, we next generated a Phb2 knockdown podocyte cell culture model. As Phb2 deficiency leads to a reduced cellular proliferation rate impeding the generation of conventional stable cell lines (Merkwirth et al, 2008), we utilized a doxycycline‐inducible promoter to express short hairpin RNAs directed against Phb2 mRNA in mouse podocytes (Shankland et al, 2007). After doxycycline treatment, decreased mRNA expression of Phb2 but not Phb1 was detected (Supplementary Fig S5A). Western blot analysis revealed an interdependence of protein stability of PHB1 and PHB2 and showed reduced protein levels for both PHB1 and PHB2 in Phb2 knockdown podocytes consistent with previous findings (Artal‐Sanz et al, 2003; Merkwirth et al, 2008) (Supplementary Fig S5B). Knockdown of Phb2 in podocytes resulted in a disrupted reticular mitochondrial network and the accumulation of fragmented mitochondria (Fig 6A and B). The mitochondrial morphology was further analyzed by using morphometric image analysis of the ratio of discrete mitochondrial number to total mitochondrial area as a quantitative measure of mitochondrial length/interconnectivity (Losón et al, 2013). These data showed a significant difference between control and Phb2 knockdown podocytes (Fig 6C). Moreover, we detected less branches and smaller mitochondrial sizes after loss of PHB2 (Fig 6D and E). However, these structural abnormalities were not accompanied by an impaired oxidative phosphorylation (OXPHOS) system. We did not detect any differences in oxygen consumption rates between Phb2‐deficient and control podocytes using complex II substrates (succinate and glycerol‐3‐phosphate) (Fig 6F). Similar results were obtained when complex I substrates (pyruvate, glutamate, and malate) were used (unpublished data). Furthermore, there was no evidence for a compensatory upregulation of mitochondrial number as we did not detect differences in total mitochondrial mass by using both, quantification of mtDNA by qPCR (Fig 6G) and FACS analysis of podocytes stained with the mitochondrial marker MitoTracker (Fig 6H and I). Additionally, we did not detect any change in reactive oxygen species (ROS) in Phb2‐deficient podocytes (Fig 6H and I). These findings are in accordance with previous publications showing an unaltered mitochondrial respiratory function after loss of PHB2 in MEFs (Merkwirth et al, 2008). These results indicated that rather a cellular signaling program than a mitochondrial respiratory function defect may account for the severe podocyte dysfunction and cell loss.
Inhibition of mTOR signaling increases survival of Phb2pko mice
Hyperactive mTOR in podocytes contributes to kidney disease, and genetic reduction of podocyte‐specific mTOR complex 1 (mTORC1) in diabetic animals suppresses the development of diabetic nephropathy (Gödel et al, 2011; Inoki et al, 2011). Therefore, we next investigated the activity of mTOR signaling in the podocyte cell culture model. Western blot analysis of Phb2‐deficient podocytes revealed hyperphosphorylation of S6 ribosomal protein (S6RP), a component of the 40S ribosomal subunit, indicative of a hyperactive mTOR signaling pathway (Fig 7A) (Magnuson et al, 2012). Hyperphosphorylation of S6RP was also observed in Phb2‐deficient glomeruli in vivo (Fig 7B). These data indicated that hyperactivity of mTOR signaling may contribute to the detrimental effects of loss of PHB2 in podocytes. And in fact, hyperphosphorylation was partially reversed in the protected Phb2pko/Insrpko/Igf1rpko triple knockouts, where phosphorylated S6 ribosomal protein was mainly found in non‐podocyte cells (Supplementary Fig S6A) and treatment with a dual insulin receptor/IGF‐1 receptor inhibitor (BMS 536924, Tocris) decreased phosphorylation of S6RP in Phb2‐deficient podocytes in vitro to the level of control podocytes (Supplementary Fig S6B). These data raise the possibility that mitochondrial dysfunction resulting from Phb2 deficiency causes hyperactive insulin/mTOR signaling in podocytes. This hypothesis was further supported by experiments in C. elegans. Heat‐shock treatment of worms results in the nuclear translocation of DAF‐16 independent of insulin signaling (Supplementary Fig S7A). Cytoplasmic redistribution, a process known to be controlled by insulin receptor (DAF‐2) signaling, was used as an indicator of insulin receptor (DAF‐2) signaling in phb‐2‐proficient and phb‐2‐deficient worms (Supplementary Fig S7B–D). Consistent with hyperactive insulin signaling in phb‐2‐deficient animals, loss of PHB‐2 accelerated recovery of the DAF‐2‐dependent cytoplasmic localization of DAF‐16 after heat shock (Supplementary Fig S7A–D), further supporting a role for insulin receptor‐mediated mTOR hyperactivity resulting from the mitochondrial defects.
Taken together, these data suggested the intriguing possibility that the severe kidney disorder in Phb2pko mice may be amenable to a therapeutic intervention with mTOR inhibitors. Treatment with the mTOR inhibitor rapamycin abrogated phosphorylation of S6RP in the cell culture model (Fig 7A). Daily treatment with rapamycin (3 mg/kg) by intraperitoneal injection beginning at week 2 alleviated the kidney disease and significantly enhanced survival of Phb2pko animals (Fig 7C and D) and reversed the hyperphosphorylation of S6RP (Supplementary Fig S8A), suggesting that at least some of the beneficial effects of insulin and IGF‐1 receptor deficiency of podocytes are mediated through preventing mTOR hyperactivity. Interestingly, we did not observe major changes in proteinuria levels which may indicate additional mTOR‐independent effects accounting for the proteinuric phenotype (Supplementary Fig S8B).
Since active mTOR inhibits autophagy in podocytes (Inoki & Huber, 2012), we also quantified accumulation of the autophagosome marker LC3 in podocytes in vitro. Although a trend to less autophagy was seen in Phb2‐deficient podocytes compared to control podocytes (Supplementary Fig S9A), this effect was not statistically significant. Even inhibition of autophagosomal degradation by adding chloroquine to the cells did not result in any significant differences in the accumulation of autophagosomes (Supplementary Fig S9A). This is in accordance with our electron microscopy studies where we did not observe a reduced amount of autophagosomes in Phb2pko mice, suggesting that the mTOR effect may be independent of influencing the level of autophagy.
More than 5% of all human beings worldwide suffer from chronic kidney diseases (CKD) with great impact on quality of life and rising socioeconomic burdens on our societies. Glomerular disorders, with diabetic nephropathy being the leading cause, account for the majority of cases of CKD. In the past several years, accumulating evidence suggested that glomerular podocytes are crucial for the function of the kidney filter and critically involved in the development of glomerulosclerosis and proteinuria (Elger & Kriz, 1998; Brinkkoetter et al, 2013). Work within the last decade suggests that both mitochondrial dysfunction and dysregulated insulin signaling contribute to podocyte injury (Coward et al, 2005; Welsh et al, 2010; Su et al, 2013; Zhou et al, 2013). Our data indicate that cell intrinsic inhibition of the insulin/IGF‐1 signaling system may protect from mitochondria‐mediated disease. The link of PHB2 deficiency and altered metabolism and/or insulin signaling had been suggested in yeast and C. elegans (Artal‐Sanz & Tavernarakis, 2009; Schleit et al, 2013). Here, we used a clinically relevant condition, podocyte‐driven kidney disease, as a model to show that inhibition of insulin signaling, achieved through cell type specific genetic deletion of insulin receptor alone or in combination with the IGF‐1 receptor in podocytes, protects from renal disease, prevents kidney failure, and enhances survival of animals with induced dysfunction of mitochondria. Taken more broadly, these findings provide the intriguing possibility that mitochondrial dysfunction may result in pathological upregulation of insulin/IGF‐1 signaling in non‐classic insulin‐responsive target cells. Whether this is a specific phenomenon for podocytes warrants further investigation.
Staining for the mTORC1 downstream target phosphorylated S6 ribosomal protein revealed enhanced phosphorylation of S6 ribosomal protein in Phb2pko mice, which was reversed after loss of the insulin and IGF‐1 receptor. This raised the intriguing hypothesis that the beneficial effect of the loss of insulin signaling in Phb2pko mice depends on less active mTORC1. In line with this, we also observed that inhibition of mTOR kinase activity with rapamycin protects from disease and robustly increases survival. Our data perfectly complement with recent data provided by Kaeberlein and colleagues who demonstrated a convincing beneficial effect of mTOR inhibition in a rare mitochondrial disease with mainly neurological symptoms (Johnson et al, 2013). Moreover, a recent study in zebrafish linked mutations in electron transfer proteins, which are associated with severe inherited mitochondrial disorders due to defects in β‐oxidation, to increased signaling via mTOR (Kim et al, 2013), further emphasizing the connection between mitochondria and metabolic signaling. Here, we show that defects in the mitochondrial fusion machinery, which become evident after loss of PHB2, lead to hyperactivation of the insulin/IGF‐1 signaling pathway and subsequently mTOR. There is an increasing body of literature that supports the hypothesis that malfunctioning mitochondria may cause diseases by sending pathogenic signals and altering the cellular metabolism rather than by inhibiting respiratory chain activity and lowering energy levels (reviewed in (Raimundo, 2014)).
Our findings may have important implications as mitochondrial dysfunction, impaired metabolism, and alterations in the production of reactive oxygen species have been implicated in renal aging and a large variety of kidney disease, most of them without any available treatment.
Materials and Methods
The antibodies used in this study are listed in Table 1.
Mice in which exons 3 and 4 of the Phb2 gene are flanked by two loxP sequences (Phb2 flox/flox mice; Merkwirth et al, 2008) were mated to either NPHS2.Cre mice (Moeller et al, 2003) or tamoxifen‐inducible podocin‐iCreER(T2) (Wang et al, 2010) to generate podocyte‐specific Phb2 knockout mice Phb2fl/fl;NPHS2.Cre (Phb2pko) or tamoxifen‐inducible podocyte‐specific Phb2 knockout mice Phb2fl/fl; podocin‐iCreER(T2) [podocin‐iCreER(T2) Phb2pko]. We included mice from both genders carrying the conventional NPHS2.cre transgene while only 8‐week‐old male animals were exposed to a tamoxifen‐enriched diet (400 mg/kg; TD.55125; Harlan Laboratories, Indianapolis, IN, USA) ad libitum for 6 weeks to exclude any potential side effects in female animals. Based on a daily intake of 5 g of food per mouse, this corresponded to an oral dose of 2 mg/day tamoxifen per mouse.
To generate double‐ and triple‐knockout mice, first, Phb2 flox/flox mice were mated to Igf1r flox/flox and/or Insr flox/flox mice. Second, these mice were mated to podocyte‐specific Cre mice (NPHS2.cre mice) (Moeller et al, 2003) to obtain mice with a podocyte‐specific deficiency of either Phb2 and Igf1r (Phb2pko/Igf1rpko mice) or Phb2 and Insr (Phb2pko/Insrpko mice) or Phb2 and Insr and Igf1r (Phb2pko/Insrpko/Igf1rpko mice).
All animals were backcrossed onto the C57BL/6 background for at least 10 generations. Mice were housed according to the standardized specific pathogen‐free conditions in the University of Cologne animal facility. The Animal Care Committee of the University of Cologne reviewed and approved the experimental protocol. The mice were sacrificed once they lost 15–20% of their maximal body weight following federal animal care regulations. Urine was analyzed with Coomassie gel stains, ELISA (mouse albumin ELISA kit; Bethyl Labs, Montgomery, TX, USA), and urine creatinine assay (Cayman Chemical, Ann Arbor, MI, USA). Blood samples were collected in the fifth week of life for quantification of serum urea and creatinine by the Institute for Clinical Chemistry of the University Hospital of Cologne, Germany. Renal tissue was embedded in OCT compound (Sakura, Torrance, CA, USA) and frozen at −70°C or fixed in 4% neutral buffered formalin for immunostaining.
For rapamycin injections, the protocol published by Zeng et al (2008) was used with some modifications. Animals received daily i.p. injections of either rapamycin solution (LC Laboratories, Woburn, MA, USA) or vehicle solution [5% (v/v) ethanol, 5% (v/v) Tween® 80, 5% (v/v) PEG400] starting 2 weeks after birth until they were sacrificed because of weight loss or sickness. Phb2pko and control mice were injected with either 3 μg rapamycin solution per g body weight or the same volume of vehicle solution (DMSO). Rapamycin solution was always freshly prepared prior to injection. Animals were randomly assigned to different treatment groups independently of genotyping results.
The sample size for the animal studies was based on ANOVA calculations according to the variable‐criteria sequential stopping rule (SSR). All analyses and quantifications were performed in a blinded fashion, and no animals were excluded from the evaluation or the statistics.
Indirect immunoperoxidase staining was performed on formalin‐fixed tissue. Briefly, 4‐μm‐thin tissue sections were deparaffinized in Xylene (VWR, Darmstadt, Germany) and rehydrated in graded ethanol. Endogenous peroxidase activity was blocked with 3% hydrogen peroxidase (Fischar, Saarbruecken, Germany). Sections were incubated overnight at 4°C with primary antibodies diluted in 1% BSA/TBS. The sections were washed repeatedly in TBS before incubation with biotinylated mouse anti‐rabbit secondary antibody (Jackson Immunoresearch, West Grove, PA, USA) diluted in 1% BSA/TBS for 1 h at room temperature. The ABC kit (Vector, Burlingame, CA, USA) was used for signal amplification, and 3,3′‐diaminobenzamidine (Sigma‐Aldrich, St Louis, MO, USA) was used as a chromogen. Slides were counterstained with hematoxylin (Sigma‐Aldrich), dehydrated, and covered with Histomount (National Diagnostics, Atlanta, GA, USA). Periodic acid Schiff (PAS) staining was performed for the assessment of glomerulosclerosis. Images were acquired with an Axiovert 200 M microscope/EC Plan‐Neofluar ×40/1.3 oil immersion or C‐Apo ×63/1.20 water immersion objective equipped with a charge‐coupled‐device camera (all from Carl Zeiss MicroImaging GmbH, Jena, Germany). Images were further processed using ImageJ/Fiji software version 1.46 (NIH, Bethesda, MD, USA).
Fresh cut frozen sections were fixed with 4% PFA before overnight incubation at 4°C with anti‐phospho‐S6 ribosomal protein (Ser235/236) from Cell Signaling, Danvers, MA, diluted in 5% NDS/PBS+Triton X‐100. The sections were washed repeatedly with PBS before incubation with fluorescently labeled anti‐rabbit secondary antibody (Jackson Immunoresearch) diluted in PBS for 1 h at room temperature. Anti‐Podocin from Sigma‐Aldrich was directly labeled with a fluorescent dye according to the manufacturer's instructions (Zenon® Rabbit IgG Labeling Kit; Life Technologies, Carlsbad, CA, USA). Sections were mounted with ProLong® Gold antifade reagent (Life Technologies).
Cells were fixed with 4% PFA before overnight incubation at 4°C with the primary antibody diluted in 5% NDS/PBS+Triton X‐100. The sections were washed repeatedly with PBS before incubation with the fluorescently labeled secondary antibody (Jackson Immunoresearch) diluted in PBS for 1 h at room temperature. Mounting was done with ProLong® Gold antifade reagent (Life Technologies). Images were acquired with an Axiovert 200 M microscope/EC Plan‐Neofluar ×40/1.3 oil immersion or C‐Apo ×63/1.20 water immersion objective equipped with a charge‐coupled‐device camera (all from Carl Zeiss MicroImaging GmbH) or an LSM 710/Axiobserver Z1 confocal microscope ×63/1.4 oil immersion objective operated by ZEN 2009 software. Images were further processed and analyzed using ImageJ/Fiji software version 1.46 (NIH; Schindelin et al, 2012). For morphometric analysis, images were processed using median and Mexican hat filtering (http://rsb.info.nih.gov/ij/plugins/mexican-hat/index.html). Mitochondria were then thresholded and binarized for subsequent analysis. Branching on skeletonized binary images was measured using the Analyse Skeleton plugin (Arganda‐Carreras et al, 2010).
Mice were perfused with electron microscopy fixation buffer (4% paraformaldehyde and 2% glutaraldehyde in 0.1 M sodium cacodylate, pH 7.4) and the kidneys post‐fixed in the same buffer for two weeks at 4°C. Samples were osmicated with 1% OsO4 in 0.1 M cacodylate and dehydrated in a graduated ethanol series. Infiltration with Epon and flat embedding was performed according to standard procedures. Thin (30 nm) cross sections were taken on an Ultracut UCT ultramicrotome (Reichert, Heidelberg, Germany). The sections were stained with 1% aqueous uranylic acetate and lead citrate and examined with a Zeiss EM 902 electron microscope (LEO, Oberkochen, Germany). Images were further processed with Adobe Photoshop CS4 version 220.127.116.11. (Adobe Systems, San Jose, CA, USA).
Conditionally immortalized podocytes were generated as previously described (Shankland et al, 2007) and cultured in RPMI media supplemented with 10% FBS and IFNγ. Mycoplasm contamination was excluded by PCR testing. Short hairpin RNAs (shRNAs) against PHB2 were designed based on the prediction of a publicly available prediction program (RNAi Designer; Invitrogen, Carlsbad, CA, USA). shRNAs were selected for efficient knockdown by using a Dual‐luciferase® reporter assay (Promega, Madison, WI, USA). Podocytes containing either a doxycycline‐inducible scrambled shRNA (5′‐TGCTGAAATGTACTGCGCGTGGAGACGTTTTGGCCACTGACTGACGTCTCCACGCAGTACATTT‐3′) or two Phb2 shRNAs (5′‐TGCTGAGCTAAGTCCTTCAAGTTCTGGTTTTGGCCACTGACTGACCAGAACTTAGGACTTAGCT‐3′ and 5′‐TGCTGTAACAATGGACGGCAGCACTCGTTTTGGCCACTGACTGACGAGTGCTGGTCCATTGTTA‐3′) were generated by means of the T‐Rex™ System by Invitrogen (Invitrogen). If not indicated otherwise, differentiation of podocytes was induced by culturing the cells at 37°C on Primaria plastic plates (BD Biosciences, San Jose, CA, USA) in the absence of IFNγ. After 10 days of differentiation, 2 μg/ml doxycycline was added to the medium and exchanged every 24 h. Experiments were performed after 96 h of doxycycline treatment. In our inhibition experiments, cells were treated either for 2 h with 10 ng/ml rapamycin (LC Laboratories) or for 24 h with 10 μM BMS 53692 (Tocris).
Autophagy experiments were carried out with undifferentiated podocytes at 33°C after treatment with 2 μg/ml for 96 h. Undifferentiated podocytes were used for this experiment because LC3 levels were below the detection limit in cultured differentiated podocytes. In this experiment, cells were treated with 10 ng/ml rapamycin for 24 h and 25 μM chloroquine for 2 h.
All results are expressed as means ± SEM. Statistical significance was evaluated using GraphPad Prism version 4.00c for Macintosh and OASIS (Online Application for the Survival Analysis of Lifespan Assays) (Yang et al, 2011). Unpaired Student's t‐test was applied in most experiments. A Log rank test (Bewick et al, 2004) was performed for survival curves, and a chi‐square test was applied for the subcellular localization of DAF‐16::GFP. A P‐value < 0.05 was considered significant.
For more detailed Materials and Methods, see Supplementary Information.
The paper explained
Diseases of the kidney glomerular filter are a major cause of end‐stage renal disease in humans. Mitochondrial dysfunction and alterations in energy metabolism as well as dysregulated insulin signaling have been implicated in many of these diseases.
In the present study, we used four different mouse models to investigate the role of the mitochondrial protein prohibitin‐2 (PHB2) and insulin signaling in glomerular podocytes. Loss of PHB2 caused progressive proteinuria and premature death of the animals due to end‐stage kidney failure and was associated with hyperactive insulin/IGF‐1 receptor and subsequently mTOR signaling. We did not observe overt defects in mitochondrial respiratory activity or increased production of reactive oxygen species. Inhibition of the insulin/IGF‐1 signaling system through genetic deletion of insulin receptor alone or in combination with the IGF‐1 alleviated renal disease and delayed the onset of kidney failure in PHB2‐deficient animals. Similar effects were achieved by treatment with mTOR inhibitor rapamycin.
Here, we used a clinically relevant condition, podocyte‐driven kidney disease, as a model to show that inhibition of insulin signaling protects from renal disease, prevents kidney failure and enhances survival of animals with induced dysfunction of mitochondria. These findings provide the intriguing possibility that mitochondrial dysfunction may result in pathological upregulation of insulin/IGF‐1 signaling in non‐classic insulin‐responsive target cells and may allow therapeutic intervention against a wide spectrum of glomerular diseases.
CI, TB, and PTB conceived the study; CI, SK, SB, HH, MK, BS, CD, ORB, FF, AL, and WB carried out the experiments; CI, CM, MH, WB, BS, ORB, RJW, JCB, CEK, R‐UM, TL, TB, and PTB designed experiments and analyzed the data; CI, TB, and PTB wrote the manuscript with input from all other authors. All authors approved the manuscript.
Conflict of interest
The authors declare that they have no conflict of interest.
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We thank N. Urban, S. Kunath, K. Heckmann, B. Maar, C. Hoffmann, J. Hausmann, B. Martiny, G. Rappl, M. Brütting, R. Herzog, A. Köser, and P. Kirschner for excellent technical support, Arnaud Mourier for helping with the oxygen consumption measurements, and the nephrology research laboratory Cologne for discussions. We thank F. Danesh (Baylor College of Medicine, Houston, TX) for providing us with the podocin‐iCreER(T2) mice and S. Shankland (University of Washington, Seattle, WA) for an immortalized mouse podocyte cell line. We are grateful to A. Trifunovic (University of Cologne, Cologne, Germany) for discussions, technical support, and reading the manuscript. Thanks to the Caenorhabditis Genetics Center for providing the reporter strain. C. Ising was supported by a fellowship from the International Graduate School in Development Health and Disease at the University of Cologne, Germany. B. Schermer obtained funding from the Deutsche Forschungsgemeinschaft (SCHE1562/2 and SFB832). T. Benzing received funding from the Deutsche Forschungsgemeinschaft (SFB635 and SFB829). P. T. Brinkkoetter received funding from the Deutsche Forschungsgemeinschaft (BR2955/4‐1) and Köln Fortune Program of the University of Cologne, Germany.
FundingInternational Graduate School in Development Health and Disease at the University of Cologne, Germany
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- © 2015 The Authors. Published under the terms of the CC BY 4.0 license