Polycystin 2 is increased in disease to protect against stress-induced cell death

Abstract

Polycystin 2 (PC2 or TRPP1, formerly TRPP2) is a calcium-permeant Transient Receptor Potential (TRP) cation channel expressed primarily on the endoplasmic reticulum (ER) membrane and primary cilia of all cell and tissue types. Despite its ubiquitous expression throughout the body, studies of PC2 have focused primarily on its role in the kidney, as mutations in PC2 lead to the development of autosomal dominant polycystic kidney disease (ADPKD), a debilitating condition for which there is no cure. However, the endogenous role that PC2 plays in the regulation of general cellular homeostasis remains unclear. In this study, we measure how PC2 expression changes in different pathological states, determine that its abundance is increased under conditions of cellular stress in multiple tissues including human disease, and conclude that PC2-deficient cells have increased susceptibility to cell death induced by stress. Our results offer new insight into the normal function of PC2 as a ubiquitous stress-sensitive protein whose expression is up-regulated in response to cell stress to protect against pathological cell death in multiple diseases.

Introduction

Polycystin-2 (PC2 or TRPP1, formerly TRPP2) is a Transient Receptor Potential (TRP) channel most well-known for its associated pathology. When mutated, PC2 causes autosomal dominant polycystic kidney disease (ADPKD), a debilitating condition leading to bilateral renal cyst formation and eventual kidney failure1. Located primarily on the endoplasmic reticulum (ER) and primary cilia of all cell and tissue types2,3,4,5, PC2 is a calcium (Ca2+)-permeant cation channel whose expression level directly affects Ca2+ release from the ER5. As such, PC2 is thought to play a key role in regulating Ca2+-regulated homeostasis and signaling pathways6. This is supported by findings showing that polycystin-deficient cells exhibit dysregulated Ca2+ mobilization and Ca2+-regulated signaling pathways5,7, including pathologically increased cAMP levels8,9 and changes in mitochondrial Ca2+ uptake10,11. The aberrant Ca2+ signaling caused by loss of polycystins is therefore often pointed to as a central cause of enhanced apoptosis12,13, excess fluid secretion14,15, and metabolic abnormalities10,11,16,17,18 seen in cystic kidney cells. Given the importance of PC2 in ADPKD development, most studies of PC2 have focused on its function in the kidney. However, the ubiquitous expression of PC2 in all cell types suggests that it is important in maintaining Ca2+ homeostasis in tissues beyond the kidney.

The tight regulation of intracellular Ca2+ is necessary for many physiological functions, including protecting cells against outside stressors. Oxidative and ER stress responses require Ca2+ influx from both the extracellular environment and intracellular stores as a key initial step for combating cell damage19,20,21,22. This elevated intracellular Ca2+ coordinates many physiological functions, such as changes in Ca2+-dependent gene transcription and activation of pro-survival pathways23. Because altered Ca2+ signaling occurs in cells with differential PC2 expression5, it follows that cells with changed PC2 levels may exhibit altered cellular homeostasis in response to stress. Indeed, beyond ADPKD, the polycystins have been linked to multiple extrarenal pathologies involving dysregulated Ca2+ and stress, including the development of liver24 and pancreatic25 cysts, cerebral aneurysms26,27, cardiac disease28, and cancer29. For instance, increased PC2 levels enhance colorectal cancer aggressiveness via modulation of cancer cell proliferation and migration through aberrant Ca2+-modulated signaling pathways30. Conversely, decreased PC2 corresponds to increased interstitial fibrosis and heightened sensitivity to injury in response to kidney ischemia31. It is established that the gene encoding for PC2, Pkd2, is differentially expressed during animal development to coordinate left-right axis determination in mice32,33 and zebrafish34. However, despite reports of altered PC2 expression in pathological states31,35,36,37, the conditions under which PC2 levels are regulated after development and into adulthood remain incompletely understood. Furthermore, how transcriptionally-regulated changes in PC2 levels influence the cellular response to stress remains unexplored. An understanding of how PC2 levels are regulated in somatic cells will give further insight into its involvement in maintaining normal cellular homeostasis, and may provide potential new targets for the treatment of ADPKD and other diseases affected by polycystin or Ca2+ dysfunction.

Given that increased PC2 levels correlate with enhanced cell viability and proliferation30, and that elevated Ca2+ promotes the activation of pro-survival pathways38, we hypothesized that PC2 expression is enhanced under conditions of stress to help protect against cell death. In this study, we found that levels of PC2 increase in disease states with ER and oxidative stress. PC2 up-regulation occurred under pathological conditions in multiple tissue types, including the kidney, liver, brain, and hearts of both humans and animal models. Finally, PC2 knock-down and knock-out cells showed increased susceptibility to stress-induced cell death. Collectively, our results indicate that PC2 acts in all tissues as a ubiquitous stress response protein whose expression levels correlate with cell survival in response to stress.

Results

PC2 levels are increased in kidneys with acute kidney injury

As one of its main functions, PC2 modulates intracellular Ca2+ signaling. Studies demonstrate that the expression level of PC2 directly impacts the amount of ER Ca2+ released in response to inositol 1,4,5-trisphosphate (InsP3)-dependent stimuli39,40,41. Because kidney tubules afflicted with ischemia-induced acute kidney injury (AKI) exhibit intracellular Ca2+ overload and altered Ca2+ dynamics42, we tested whether the expression level of PC2 was changed in AKI-afflicted kidneys. To model injury, mice were subjected to renal unilateral ischemia/reperfusion (I/R) injury with nephrectomy in which the right renal pedicle was clamped for 27 minutes, reperfused, then sacrificed 72 hours later and the right kidney collected. Left nephrectomized kidney was used as sham control (pre-injury). Increased 4-hydroxynonenal (4-HNE) and nuclear factor kappa-light-chain-enhancer of activated B cells (NFκB), and degradation of inhibitor of kappa (IκBα) confirmed the induction of AKI in I/R kidneys compared to nephrectomy controls (Figs. 1A,B, S1A–C). Strikingly, PC2 abundance was also significantly increased in kidneys with I/R injury (Fig. 1A,C), consistent with work showing increased levels of PC2 in rat kidneys with AKI31,35. We then tested whether this increase was occurring transcriptionally by measuring the mRNA levels of Pkd2 in nephrectomy control and AKI kidneys. We found that the kidneys afflicted with AKI had significantly higher levels of Pkd2 mRNA (Fig. 1D), indicating that both PC2 transcript and protein are increased with stress. To confirm the translational relevance of this response in humans, we performed immunofluorescent staining for PC2, collecting ducts (staining for the lectin Dolichos biflorus agglutinin [DBA]), and mitochondria (staining for the voltage-dependent anion channel [VDAC]) in normal human kidneys (NHK) or kidneys from patients diagnosed with acute tubular injury (AKI; Figs. 1E, S1D; patient information included in Table S1). Quantification of PC2 intensity per cell area revealed that, as in the murine response to AKI, PC2 was significantly increased in human kidney tubules with AKI (Fig. S1E).

Figure 1
figure1

PC2 levels are increased in pathologically stressed kidneys. (A) Normal (Sham) and AKI-afflicted mouse kidneys were immunoblotted for 4-HNE and PC2. Each band represents one biological replicate. Full-length blots shown in Fig. S6. (B,C) Quantification of 4-HNE and PC2 protein abundance in Sham and AKI kidneys, normalized to actin. *p < 0.05 as determined by Mann Whitney U test. Data presented as median with range. Sample size n = 3 biological replicates per group. (D) Normalized mRNA expression of Pkd2 in Sham and AKI-afflicted mouse kidneys. Gapdh used as internal control. Sample size n = 8 biological replicates per group. ***p < 0.001 as determined by Mann Whitney U test. Data presented as median with range. (E) Normal human kidneys (NHK) or kidneys with acute kidney injury (AKI) were stained for PC2 (green), DBA (red), a marker for collecting ducts, and VDAC (blue), an outer mitochondrial membrane protein. Scale bar, 75 μm.

PC2 is increased in livers with non-alcoholic fatty liver disease

Whereas kidney cyst development with ADPKD is well-established, pathologies caused by mutations to PKD2 do not exclusively affect the kidneys. The development of cysts arising from hepatic epithelial cells is a common extrarenal result of ADPKD24. Like cystic kidney cells, PC2-null cystic liver cells exhibit altered intracellular Ca2+ handling and changes in intracellular signaling pathways, indicating the importance of PC2 in tissues outside of the kidney43. To investigate whether PC2 abundance also changes in liver cells with stress, we fed mice a normal diet (ND) as control, or high-fat diet (HFD) to induce insulin resistance and hepatic stress44. After 8 weeks, mice were subjected to glucose tolerance tests, and the HFD-fed mice were found to be glucose intolerant compared to ND-fed mice (Fig. 2A,B). Livers from these mice were collected and showed increased levels of 4-HNE and C/EBP Homologous Protein (CHOP; Figs. 2C, S2A,B), indicating the induction of stress in HFD-fed mice. Immunoblotting for PC2 showed a significant increase in stressed livers from HFD-fed mice (Figs. 2C, S2C). Additionally, qPCR analysis of liver mRNA from mice fed ND or HFD showed a significant increase in Pkd2 mRNA in the HFD-fed mouse livers (Fig. 2D), demonstrating that stress-related Pkd2 up-regulation is not restricted to renal tissue.

Figure 2
figure2

PC2 levels are increased in livers with NAFLD. (A) Plasma blood glucose levels and (B) quantified area under the curve during glucose tolerance tests of mice fed ND or HFD for 8 weeks. Shown are the mean area under the curve ± SD of 5 mice per group. **p < 0.01 as determined by Mann Whitney U test. (C) Mouse livers from ND- or HFD-fed mice were immunoblotted for PC2, 4-HNE, and CHOP. Each lane represents one biological replicate; sample size n = 4 per group. Full-length blots shown in Fig. S7. (D) Normalized mRNA expression of Pkd2 in livers of mice fed ND or HFD for 14 months. Gapdh used as internal control. Sample size n = 3 biological replicates per group. *p < 0.05 as determined by Mann Whitney U test. Data presented as median with range. (E) Normal human livers (NHL) or livers with non-alcoholic steatohepatitis (NASH) were stained for PC2 (green) and VDAC (red). Scale bar, 100 μm. LD = lipid droplet. Asterisks depict lipid accumulation within the liver. (F) PC2 intensity normalized to cell area was quantified in human NHK and NASH livers. ***p < 0.001 as determined Mann Whitney U test. Quantification is of 5 images per sample; sample number NHL n = 6, NASH n = 9.

The translational relevance of these findings was verified by performing immunofluorescent staining of normal human livers (NHL) and livers from patients with diet-induced non-alcoholic steatohepatitis (NASH; Figs. 2E, S2D; patient information included in Table S2). Quantification of PC2 fluorescence per cell area demonstrated that human livers afflicted with non-alcoholic fatty liver disease (NAFLD) likewise have increased abundance of PC2 (Fig. 2F), supporting the hypothesis that PC2 retains critical function in tissues beyond the kidney.

PC2 is up-regulated with stress in cardiac tissue

Although the most striking symptom of ADPKD is the formation of bilateral renal cysts, the most common cause of death in ADPKD patients is a consequence of cardiac abnormalities45,46. Due to the expression of PC2 in cardiac tissue and the apparent importance of the polycystins in heart function, PC2 levels were examined in a murine model of cardiomyopathy and were found to be increased in isoproterenol (ISO)-treated hearts compared to healthy controls36. We observed that cellular stress was induced in the hearts of these ISO-treated mice as indicated by increased 4-HNE levels (Fig. S3A,B), confirming that, as in kidney and liver tissue, increased PC2 was accompanied by cellular stress in the ISO-treated hearts. To test whether PC2 was also transcriptionally up-regulated in the hearts of stressed mice, we compared mRNA levels of Pkd2 in left ventricular (LV) tissue samples from control (sham-operated) and stressed (subjected to transverse aortic constriction [TAC]) mice47. Unlike the ISO-treated mice, TAC mice develop cardiac hypertrophy induced by a physical rather than chemical stressor. Compared to sham-operated mice, LV samples from TAC mice showed an increase in Pkd2 mRNA (Fig. S3C), confirming that PC2 is up-regulated transcriptionally in stressed mouse hearts using multiple methods of stress induction.

To determine whether up-regulation of PC2 with stress is conserved in human disease, we compared levels of PC2 in left ventricular (LV) tissue samples from non-failing (NF) human hearts and LV samples of failing human hearts, obtained from patients with ischemic cardiomyopathy (ICM) or non-ischemic cardiomyopathy (NICM; patient information included in Table S3)48. PC2 was largely increased in the LV samples of ICM and NICM versus NF hearts (Figs. 3A, S3D), and levels of 4-HNE and CHOP were significantly increased in NICM hearts and trending toward increased in ICM samples (Fig. S3E,F). However, because these stress markers were not significantly increased in ICM samples, we questioned whether the up-regulation of PC2 correlated to the degree of stress in these heart samples. We therefore plotted the relative protein levels of PC2 versus CHOP and found a significant correlation between the expression of these proteins (Fig. 3B), demonstrating that although statistical analyses of 4-HNE and CHOP levels do not show a significant increase in ICM samples, the degree of stress in the heart directly correlates with levels of PC2. Plotting relative PC2 versus 4-HNE levels showed a trend toward correlation, but this was not statistically significant due to an outlier in the NICM group (Fig. S3G).

Figure 3
figure3

PC2 expression is up-regulated with stress and correlates with ISR pathway activation. (A) Left ventricular (LV) tissue samples from non-failing (NF) human hearts and from heart failure patients with non-ischemic cardiomyopathy (NICM) or ischemic cardiomyopathy (ICM) were immunoblotted for PC2, 4-HNE, and CHOP. Each lane represents one biological replicate; data shown are representative of n = 8 for each condition. Full-length blots shown in Fig. S8. (B) Normalized protein expression of PC2 was plotted against its corresponding normalized CHOP expression. Linear regression analysis demonstrated that PC2 levels significantly correlated with stress induction as measured by CHOP abundance. (C) RNA-Seq RPKM values from human NF LV samples and in heart failure patients diagnosed with ICM or NICM were log2 transformed and their fold change determined. PKD2 transcripts were increased in the LV of ICM and NICM, compared to NF, hearts. *p < 0.05 and **p < 0.01 as determined by one-way ANOVA. Data presented as mean ± SD. (D) Curated lists of ER- and oxidative-stress associated genes were used to generate a heat map of stress-related gene expression in NF, ICM, and NICM samples. All genes shown exhibited significant differential expression (p < 0.05) amongst groups. A color legend is pictured with a scale from −2 to +2-fold change. (E) Genes that were overlapping between MetaCore and IPA-curated lists were used to generate ‘overlapping’ ER and ‘overlapping’ oxidative stress lists. These lists were cross-referenced, and 6 genes appeared in both lists, which were classified as ISR pathway genes. (F) Linear regression analysis demonstrated that one of the two ISR genes differentially expressed amongst NF, ICM, and NICM samples, NFE2L2, significantly correlated with PKD2 expression. (G) Human iPSC-CMs were treated with increasing concentrations of H2O2 for 2 hours and immunoblotted for 4-HNE and PC2. Each lane represents one independent experiment; sample size n = 3 independent experiments per group. Full-length blots shown in Fig. S9. (H) Quantification of PC2 abundance in untreated (Ctrl) versus H2O2-treated iPSC-CMs. **p < 0.01 as determined by one-way ANOVA. Data presented as mean ± SD.

To test if the increased PC2 seen in NICM and ICM LV tissues was due to differential gene expression, we compared the mRNA levels of PKD2 in these samples versus NF LV samples. Transcript levels of PKD2 were elevated in LV samples from ICM and NICM patients (Fig. 3C), indicating that PC2 increase with stress occurs via transcriptional up-regulation in human hearts. To see if there were differences in cellular stress levels associated with increased PKD2 in the ICM and NICM failing hearts, curated lists of genes associated with cellular responses to ER and oxidative stress were collected from MetaCore (Clarivate Analytics) and Ingenuity Pathway Analysis (Ingenuity Systems, QIAGEN Bioinformatics). Genes from these lists were compiled (Tables S4 and 5, “Compiled”) and used to generate an expression heat map of NF, ICM, and NICM transcripts. All transcripts depicted in the heat map are significantly (p < 0.05) changed among the samples. Transcripts were sorted via hierarchical clustering and demonstrate distinct differential expression patterns in the stress genes of NF compared to ICM and NICM samples (Fig. 3D), demonstrating that up-regulation of PKD2 correlates with altered stress response genes in human hearts.

Because elevated PC2 was associated with increases in canonical markers of both ER (CHOP) and oxidative (4-HNE) stress (Figs. 1A,B, 2C, Fig. S2A,B, Fig. 3A,B, and Fig. S3D–F), we hypothesized that PKD2 expression was changed as part of the integrated stress response (ISR) pathway, an essential adaptive pathway that is activated in response to both ER and oxidative stressors49,50,51,52,53. To explore this idea, we cross-referenced the compiled ER and oxidative stress gene lists to develop a more stringent list of stress-associated genes (Tables S4 and 5, “Overlapping”), and cross-referenced these overlapping lists to identify genes involved in both responses. Between 11 ER stress- and 32 oxidative stress-associated genes, there were 6 genes present in both groups (Fig. 3E), two of which were differentially expressed in the NF versus ICM and NICM heart samples (Fig. S3H,I). We then used correlation analysis with a cutoff of 70% correlation or higher and discovered that one of the ISR genes, NFE2L2, positively correlated with PKD2 expression (Fig. 3F; correlation = 79.2%). NFE2L2, also known as Nrf2, is a transcription factor that binds the antioxidant response element (ARE) and activates the expression of genes involved in the response to cellular insults54,55,56,57. The other ISR gene that was changed in ICM and NICM samples, ATP2A2, did not pass the 70% correlation cutoff (Fig. S3J). We tested whether these correlations were conserved in the LV from stressed mouse hearts and discovered that, like the human hearts, stressed TAC mice had decreased levels of Atp2a2 (Fig. S3K) and a trend toward increased Nfe2l2 (Fig. S3L). These data suggest that, unlike other stress response proteins, PKD2 up-regulation is non-promiscuous and thus is directly associated with specific ISR pathways.

To then investigate whether PC2 expression increases as a direct consequence of cellular stress, we treated human induced pluripotent stem cell-derived cardiomyocytes (iPSC-CMs) with increasing concentrations of hydrogen peroxide (H2O2) to induce cell stress in vitro. H2O2 treatment led to increased levels of oxidative stress in iPSC-CMs as measured by 4-HNE (Figs. 3G, S3M). Immunoblotting for PC2 levels in iPSC-CMs showed two distinct bands, as has been previously observed58. It is thought that the higher band depicts the full-length, N-glycosylated form of PC2, with the lower band depicting a potentially cleaved, inactive form of PC2. Quantification of full-length PC2 levels showed an increase after 2 hours of H2O2 treatment in iPSC-CMs, establishing that increased PC2 occurs as a direct consequence of cellular insult (Fig. 3G,H).

PC2 expression is increased in stressed brains

Having determined that PC2 abundance changes with stress in tissues known to rely on PC2 for proper function, we questioned whether its role as a stress-sensitive protein was conserved in tissues less studied in the context of PC2. Expression of PC2 in the brain led us to test whether its abundance is also altered with stress in the central nervous system. As a model of pathologically altered Ca2+ signaling and cell stress in the brain59,60, we used kainic acid to induce acute seizures in mice61. Systemic injections of kainate cause epileptiform seizures in the hippocampus and induce hippocampus-restricted neuropathology comparable to that seen in patients with temporal lobe epilepsy61. Mice were injected intraperitoneally with saline (Sal) or kainic acid (KA; Fig. S4A), and their seizures scored according to a modified Racine scale every 10 minutes for 120 minutes (Fig. 4A, Table S6). Hippocampal lysates collected from randomly-paired, weight- and age-matched mice were found to have increased expression of PC2 in epileptic compared to saline-treated brains (Fig. 4B). Pkd2 and Nfe2l2 mRNA expression was likewise tested from hippocampi of saline- and KA-treated mice and found to be significantly increased with KA induction of epileptic seizures (Figs. 4C, S4B).

Figure 4
figure4

PC2 is increased in stressed brains. Mice were given injections of saline (Sal) or kainic acid (KA) to induce epileptic seizures and oxidative stress in the brain. (A) Seizure scores following injections were measured according to a modified Racine scale. Data shown are mean ± SD of 6 mice per group. (B) TOP: Hippocampal tissue was collected and immunoblotted for PC2 24 hours following injections. Each lane represents one biological replicate; sample size n = 6 per group. Full-length blots shown in Fig. S11. BOTTOM: Quantification of PC2 protein abundance in Saline and KA-treated hippocampi, normalized to actin. *p < 0.05 as determined by Mann Whitney U test. Data presented as median with range. Sample size n = 6 biological replicates per group. (C) Normalized mRNA expression of Pkd2 in hippocampi from mice injected with saline or KA. Gapdh used as internal control. Sample number Saline n = 6, KA n = 5. **p < 0.01 as determined by Mann Whitney U test. Data presented as median with range. (D) RNA-Seq FPKM values from different structures (LE, leading edge; HBV, hyperplastic blood vessel; MVP, microvascular proliferation) of human glioblastoma samples were log2 transformed and their fold change determined. PKD2 transcripts were increased in HBV and MVP samples compared to LE. ****p < 0.0001 as determined by one-way ANOVA. Data presented as mean ± SD. (E) Linear regression analysis demonstrated that the ISR gene NFE2L2 significantly correlates with PKD2 in human glioblastoma tissues.

We then determined whether this increase was translatable to human disease by investigating if PC2 expression correlates with stress in human brains. Using the RNA-Seq dataset provided by the Allen Institute Ivy Glioblastoma Atlas Project62, we examined PKD2 expression in 3 different glioblastoma structures (hyperplastic blood vessels, microvascular proliferation, and leading edge; patient information included in Table S7). Leading edge (LE) samples showed relatively low amounts of PKD2 expression, whereas hyperplastic blood vessels (HBV) and microvascular proliferation (MVP) samples expressed relatively high amounts of PKD2 (Fig. 4D). These findings correlated with differential expression of the ISR genes NFE2L2 and ATP2A2 in the different glioblastoma structures (Fig. S4C,D), indicating altered ISR levels amongst these structures. We then used correlation analysis (correlation ≥ 70%) and found that, like in human hearts, PKD2 levels positively correlated with NFE2L2 in human brains (Fig. 4E; correlation = 76.8%), but not with ATP2A2 (Fig. S4E).

PC2 up-regulation protects cells against stress-induced cell death

Although we determined that PC2 expression is up-regulated as a consequence of cellular insult in multiple tissue types, whether this increase is detrimental or favorable for the cell remained unclear. To test this, we utilized a kidney epithelial cell line (LLC-PK1) with wild-type levels of PC2 (WT) or PC2 knocked down (PC2 KD; Fig. S5A) to assess PC2’s role in the cellular stress response. Cells were serum-starved (SS) to induce stress (Fig. S5A,B)63,64,65 and, consistent with our findings in animal and human tissues, cells showed increased PC2 mRNA and protein expression following serum starvation (Fig. 5A–C, S5A,C) and treatment with tunicamycin (TM), an inducer of ER stress (Fig. S5D–F). We then measured cell viability of WT and PC2 KD cells under basal and stressed conditions. When stress was induced through serum starvation or with TM treatment, PC2 KD cells showed decreased cell viability compared to WT cells (Figs. 5D, S5G), consistent with previous work showing that loss of PC2 renders kidney cells hyper-sensitive to stress31, and indicating that up-regulation of PC2 occurs as a protective mechanism. To test our hypothesis that PC2 up-regulation protects against cell stress by enhancing intracellular Ca2+ signaling, we measured cell viability in serum-starved cells treated concurrently with the intracellular Ca2+ chelator BAPTA-AM. When Ca2+ signaling was blunted in SS WT cells through BAPTA-AM treatment, cell viability decreased to levels of SS PC2 KD cells (Fig. 5D). However, in SS KD cells treated with BAPTA-AM, there was no further decrease in cell viability (Figs. 5D, S5H), indicating that a PC2-dependent Ca2+ response plays a significant role in the cells’ ability to combat stress. Finally, we measured the degree of stress-induced apoptosis through immunofluorescence and western blot analyses of cleaved caspase-3 activation and found that, compared to WT cells, PC2 KD cells had increased levels of apoptosis when stressed (Figs. 5CE,F, S5A,D,I). The same results were observed when testing another cell line (mIMCD-3) containing normal levels of PC2 (WT) or with PC2 knocked out via CRISPR/Cas9 (PC2 KO; Fig. S5J–L). These data demonstrate that PC2 up-regulation serves to protect cells against stress, and that with inadequate levels of PC2, cells are rendered hyper-susceptible to stress-induced cell death.

Figure 5
figure5

PC2 protects against stress-induced cell death. (A) Kidney epithelial LLC-PK1 cells were grown in normal culture medium (Control) or base medium not supplemented with FBS (Serum Starved, SS) for 24 hours, then stained for DAPI (blue), phalloidin (red), and PC2 (cyan). Scale bar, 25 μm. (B) PC2 intensity normalized to cell area was quantified in control and serum-starved (SS) LLC-PK1 cells. **p < 0.01 as determined by Mann Whitney U test. Quantification is of 5 images per sample; n = 10 samples per group. Data presented as median with range. (C) Fold change mRNA expression of Pkd2 in serum-starved WT, and control and serum-starved PC2 KD cells compared to WT control cells. Actin used as internal control. n = 3 independent experiments per group. ***p < 0.001 as determined by one-way ANOVA. Data presented as mean ± SD. (D) Viability of WT and PC2 KD (KD) cells was tested via CellTiter-Glo assay under normal (Ctrl) and stressed (SS) conditions with or without 24-hour co-treatment of 100 nM BAPTA-AM (BAPTA). *p < 0.05, **p < 0.01, and ****p < 0.0001 as determined by one-way ANOVA. n = 3 independent experiments per group with 10 replicates per experiment. Data presented as mean ± SD. (E) WT and PC2 KD cells were grown in normal culture medium (Ctrl) or serum starved (SS) for 24 hours, then stained for DAPI (blue) and cleaved caspase 3 (green). Images shown are representative of 10 control and 10 serum-starved samples from both WT and PC2 KO cell lines. Scale bar, 25 μm. (F) Cleaved caspase 3 intensity normalized to cell area was quantified. ***p < 0.001 and ****p < 0.0001 as determined by one-way ANOVA. Quantification is of 5 images per sample; n = 10 samples per group. Data presented as mean ± SD.

Discussion

In this study, we establish that PC2 is a stress-responsive protein whose expression is elevated in a variety of cell types under multiple pathological conditions. Its up-regulation is a direct consequence of ER and oxidative stress, and its mRNA expression significantly correlates with Nfe2l2, a transcription factor that is part of the ISR pathway66. Loss of PC2 resulted in a Ca2+-mediated decrease in cell viability in response to stress and increased levels of stress-induced apoptosis. Collectively, these findings demonstrate that PC2 plays an important role in general cell homeostasis in numerous tissue types, and that up-regulation of PC2 helps protect cells against stress-induced cell death under pathological conditions.

The importance of PC2 in the maintenance of cellular homeostasis is well-supported by the pathological dysfunctions that occur in cystic ADPKD cells. Our findings indicate that PC2 is increased transcriptionally with cell stress, and that this occurs in response to specific signaling pathways. The function of PC2 as a modulator of Ca2+ signaling fits well with these findings, as Ca2+ mobilization is a critical step in the cell’s ability to respond to and protect against pathological stressors. As our data indicate, enhanced Ca2+ signaling facilitated by PC2 following cell stress contributes significantly to the cell’s adaptive response, whereas blunted Ca2+ through intracellular chelation or the absence of PC2 causes hypersensitivity of the cells to outside stressors. Though changes in PC2 levels have been noted in different pathological conditions, the causes for its differential expression after development remained incompletely explored. In support of our findings, previous studies have shown that both Pkd2 transcript and protein levels are increased in kidneys following ischemia/reperfusion injury, and that mice with decreased levels of PC2 are more sensitive to injury in both kidney and smooth muscle cells31,67,68,69. The correlation we discovered between PKD2 and NFE2L2 levels suggests that PKD2 may be up-regulated via Nrf2, a transcription factor that is increased following cellular insults including oxidative stress70. Much of what is known regarding the transcriptional regulation of Pkd2 is based upon its cis-acting promoter region, which contains putative binding sites for developmentally-regulated transcription factors such as Sp1, NF-1, and AP-271,72. However, trans-regulatory effects on Pkd2 expression have not been described and may contain additional regulatory elements to alter PC2 levels.

Our results demonstrate that PC2 KD and KO renders cells susceptible to stress-induced death. It therefore logically follows that cystic cells characterized by loss the of PC2 would exhibit decreased cell viability in response to stress. In support of this, a standard phenotype associated with ADPKD is enhanced apoptosis during cyst development69,73,74, where cellular stress levels are high due to many pathological factors, including renal ischemia and altered cell metabolism. In fact, treatment of ADPKD mice with caspase inhibitors (inhibitors of apoptosis) results in decreased cyst volume and cell proliferation74. Additionally, PC2 haploinsufficient (Pkd2+/-) kidney cells that express decreased overall levels of PC2 show hypersensitivity to cell stress. Pkd2+/- mice develop larger, more pronounced kidney cysts when treated with Tumor Necrosis Factor alpha (TNFα, an inflammatory cytokine) to induce stress as compared to wild-type littermates, whereas treatment of Pkd2+/- mice with TNFα inhibitor blocked cyst formation75. Additional studies seeking effective treatment for kidney disease have identified resveratrol, a potent activator of Nrf276, as a potentially compelling therapeutic agent for slowing cyst progression in ADPKD77,78. Whereas these studies have focused on the effects of resveratrol in ameliorating the inflammatory response associated with cyst development, it is possible that resveratrol may act through Nrf2 to help restore normal ISR activity in these cells as well.

Although renal cyst formation and kidney failure are arguably the most well-known symptoms of PC2 dysfunction, multiple extrarenal pathologies are also known to occur in patients with loss-of-function PKD2 mutations. Indeed, ADPKD patients commonly present with numerous manifestations of the disease, including colonic diverticula79,80, hernia81,82, cerebral aneurisms83, and the development of hepatic84, pancreatic25, and seminal vesicle85,86 cysts. Most notably, however, rather than renal failure, the major cause of death in patients with ADPKD is due to cardiac dysfunction83. Studies seeking to elucidate how the loss of PC2 affects the heart have shown that with increased age, decreased PC2 levels result in cardiac dysfunction independent of renal abnormalities87. Additionally, in agreement with our findings, PC2 levels are enhanced in cardiomyocytes with cardiac injury, and Pkd2+/- mice show a diminished capacity to recover from injury following the cessation of stress36. It has been suggested that the extrarenal manifestations seen in ADPKD patients are merely secondary effects caused by the main pathology of renal cysts. However, our findings highlight the importance of PC2 as a ubiquitous protein essential for proper cell function not only in the kidney, but in all tissue types. Based on this, the role of PC2 in numerous Ca2+-associated stress pathologies may prove to be a promising target by which to restore normal Ca2+ and/or ISR homeostasis.

Our in vitro data suggest that PC2 regulation of Ca2+ signaling is required to maintain cell viability in the face of stress. Whereas the function of PC2 as a Ca2+-permeable cation channel is well-established, there currently exists controversy over where PC2 exerts its intrinsic channel function. It is thought that due to the ER retention signal within its C-terminal tail, the majority of PC2 is located on the ER5,88, with the rest being localized to the primary cilia in association with PC189 or TRPV490, where it exerts its anti-cystogenic function91. However, others have suggested that PC2 is also present and functions as a Ca2+ channel on the plasma membrane92,93. In the context of our findings, we believe that PC2 exerts its stress response function from its localization on the ER based upon (1) immunofluorescent imaging demonstrating that PC2 localization remains intracellular, even under stressed conditions (Figs. S1D and S2D) and (2) the up-regulation of PC2 with stress in terminally-differentiated neurons and cardiomyocytes, whose cilia are stumpy, essentially vestigial organelles. Nevertheless, the localization of PC2 does not ultimately influence the findings of this manuscript, as PC2 is believed to facilitate enhanced cytoplasmic Ca2+ signaling whether functioning on the ER, primary cilia, or plasma membrane.

Additionally, though PC2 is itself can form a Ca2+-permeable cation channel, it is known to interact with other cation channels to enhance intracellular Ca2+ signaling (including the inositol 1,4,5-trisphosphate receptor39,40,94, ryanodine receptor95, and other TRP channels90,96). Therefore, whether PC2 is altering intracellular Ca2+ signaling through its intrinsic channel activity or through interactions with other channels remains unclear. Interestingly, PC2 channel activity has been shown to be sensitive to H2O2, whose treatment caused an up-regulation of PC2 in human iPSC-CMs. Because the reported IC50 of this inhibition is ~193 μM97, we do not believe that the H2O2 concentration used in our experiment (up to 200 μM) would be sufficient to completely eliminate a Ca2+ current through PC2. Nonetheless, if it were the case that PC2 is fully inhibited with stress, our data showing that BAPTA-AM treatment (Fig. 5D) in PC2 KD cells has no effect on cell viability compared to WT cells demonstrates the requirement for PC2-mediated Ca2+ signaling in the response to cell stress, whether this is through PC2’s intrinsic channel activity or its interactions with other channels.

Our study is limited by the variability of sample size throughout the different types of tissues and stress. For all conditions, we tested at least n = 3 samples to ensure that proper statistics could be performed during analyses. When possible, we maximized the sample size to increase the power of our study. However, the sample size of human and mouse tissues varied depending upon availability. Variables affecting this included limited access to human pathological samples with specific diagnoses, and the survival of mice undergoing stress procedures. Additionally, though our data point to a potential link between PKD2 and NFE2L2 expression, we do not presume to state that NFE2L2 directly causes PKD2 up-regulation based on our results. Rather, our data show that PKD2 expression correlates with the activation of the ISR pathway due to its role as a stress response protein. The possibility remains that 1) increased Nrf2 may influence PKD2 expression directly, 2) NFE2L2 transcription may be increased due to altered signaling in cells with increased PC2, 3) PKD2 and NFE2L2 are up-regulated under similar stress conditions, but neither one directly affects the expression of the other, or 4) increased PKD2 mRNA is independent of its transcription, but rather is a consequence of post-transcriptional changes such as mRNA stability. Consequently, if and how PC2 and Nrf2 influence one another’s expression, along with the exact mechanism of increased PKD2 transcript will require further in-depth mechanistic studies.

Collectively, we describe a new functional role for PC2 as a stress-sensitive protein that is up-regulated in response to cellular insults in multiple disease states and tissue types. Moreover, loss of PC2 is sufficient to render cells hypersusceptible to stress-induced cell death, implicating altered stress response pathways in the development of polycystin-related pathologies. The ubiquitous expression of PC2 throughout the body raises the possibility that PC2 may contribute to disease states in other tissues where the ISR is induced or disrupted, and may provide a novel target to help ameliorate the progression of these diseases.

Materials and Methods

Reagents and antibodies

Anti-PC2 (sc-47734; for immunoblotting), anti-NFκB (sc-8008), and anti-IκBα (sc-1643) antibodies were purchased from Santa Cruz Biotechnology. Anti-PC2 antibody for immunofluorescent imaging was a kind gift from Dr. Stefan Somlo (Yale). Mouse anti-beta-Actin (#3700), rabbit anti-beta-Actin (#4970), anti-CHOP (#2895), anti-cleaved caspase-3 (#9664), and anti-GAPDH (#2118) antibodies were purchased from Cell Signaling Technology. Anti-4-Hydroxynonenal (ab48506), anti-eIF2α (ab50733), anti-phospho-eIF2α (ab32157) antibodies, and kainic acid (ab120100) were purchased from Abcam. Anti-VDAC (PA1-954A) antibody was purchased from Thermo Fisher Scientific. Hydrogen peroxide (H325-100) and BAPTA-AM (B1205) were purchased from Thermo Fisher Scientific. Tunicamycin (T7765), and Dimethyl sulfoxide (DMSO; W387520) were purchased from Sigma-Aldrich.

Animal studies

The Yale University and University of Illinois at Urbana-Champaign Institutional Animal Care and Use Committees (IACUC) approved the animal housing conditions and the experimental procedures conducted in this study. All experiments were performed in accordance with relevant guidelines and regulations. C57BL/6 mice were kept under standard laboratory conditions with free access to food and water. Control mice were provided 2018S Teklad global rodent diet (Envigo). For diet-induced obesity, mice were fed TD.06414 Teklad diet containing 60% kcal/fat (Envigo) for 8 weeks-14 months, as described in the figure legends, beginning at 10 weeks of age. All animal experiments were performed in a blinded manner.

Renal ischemia/reperfusion mouse model

Male 8- to 10-week-old C57BL/6 mice (National Institutes of Health/National Cancer Institute) were anesthetized with i.p. ketamine (100 mg/kg) and xylazine (10 mg/kg) then subjected to renal ischemia reperfusion (I/R) using a modified approach of that described previously98. Briefly, the right renal pedicle was isolated through a midline abdominal incision and clamped for 27 minutes using a nontraumatic microaneurysm clip (B-2, Fine Science Tools). The left kidney was removed and collected immediately before I/R of the right kidney (Sham, nephrectomized kidney). Mice were kept at 37 °C at all times during the procedure, and reperfusion of kidneys was confirmed after clamp release. Mice were given 1 ml normal saline intraperitoneally to prevent dehydration and were euthanized 72 hours after I/R. Kidney tissue was harvested for immunoblotting as described below.

Glucose tolerance testing

At 18 weeks of age, mice were fasted for 16 hours before glucose tolerance testing. Glucose was administered via i.p. injection (1.5 g/kg body weight). Blood glucose measurements were taken immediately before injection and at 15, 30, 60, and 120 minutes following injection. Blood was collected using a lateral tail nick and glucose levels were measured using blood glucose strips and OneTouch glucometer (LifeScan).

Kainic acid-induced acute seizure mouse model

At 8–10 weeks of age, male C57BL/6 J mice (Jackson Laboratory, Stock Number: 000664) received an i.p. injection of kainic acid (30 mg/kg body weight) or an equal volume of 0.9% saline as described99. Mice were returned to their cages and monitored for behavioral seizures every 10 minutes for 2 hours following injection. Behavioral seizures were scored according to a modified Racine scale as described previously100,101. At 24 hours post injection, mice were euthanized by CO2 inhalation and brains stored at −80 °C until use.

Brain lysate preparation

The dissected brain regions per mouse were homogenized in ice-cold homogenization buffer (Solution A) containing (in mM): 320 sucrose, 1 NaHCO3, 1 MgCl2, 0.5 CaCl2, 0.4 HEPES (pH 7.4) and Halt protease inhibitors (Thermo Fisher Scientific) as previously described99. After centrifuging at 1400 x g for 10 minutes at 4 °C, the homogenate supernatant (S1) was separated from insoluble tissue and nuclear pellet (P1). The S1 fraction was then centrifuged at 13,800 x g for 10 min at 4 °C. The supernatant with cytosolic soluble proteins (S2) was removed, and the remaining pellet with transmembrane proteins and membrane-bound proteins (P2 membrane fraction) was resuspended in ice-cold solution B containing (in mM): 160 sucrose, 6 Tris-HCl, 0.5% Triton-X (pH 8.0) and Halt protease inhibitors. Pierce BCA assay (Thermo Fisher Scientific) was performed to normalize protein concentrations to 1 mg/ml in Solution B (pH 7.4). The S1, S2, and P2 fractions were stored at −80 °C until use.

Western blot

Lysates of mouse kidneys, hearts, livers and human hearts were prepared by homogenization in radioimmunoprecipitation assay (RIPA) buffer containing SDS (Santa Cruz Biotechnology) with Halt protease and phosphatase inhibitor cocktail (Thermo Fisher). Lysates of mouse hippocampi were prepared as described above and the P2 fractions were run for western blotting. Cultured cells were lysed directly in M-PER mammalian protein extraction reagent (Thermo Fisher) supplemented with Halt protease and phosphatase inhibitor cocktail. Equal amounts of protein were loaded, and electrophoresis was performed in NuPAGE 4–12% gradient bis-tris polyacrylamide protein gels (Thermo Fisher). Proteins were transferred to PVDF membrane and blocked with 5% milk in phosphate-buffered saline with Tween-20 for 1 hour. Membranes were then incubated overnight with primary antibody at 4 °C. Blots were washed and incubated with secondary antibody for 1 hour at room temperature. After washing, the secondary antibody was visualized by Pierce ECL chemiluminescence reagents (Thermo Fisher) or using a LI-COR Odyssey imaging system (LI-COR Biosciences).

Human tissue

Human kidney and liver tissues were identified and obtained through the Department of Pathology at the Yale School of Medicine. All experimental protocols and the use of these tissues for research were approved by the Yale Institutional Review Board. All methods were carried out in accordance with relevant guidelines and regulations. Informed consent was obtained from all subjects donating samples. Tissues were fixed with 4% paraformaldehyde at 4 °C overnight, embedded in paraffin, and 5 μm sections were cut for immunofluorescence. Following deparaffinization and rehydration, antigen retrieval was performed by incubating the sections in a steamer for 20 min in sodium citrate buffer (10 mM Tri-sodium citrate, 0.05% Tween-20, pH 6.0). Sections were then quenched of autofluorescence, blocked and permeabilized, and incubated with anti-PC2 (Santa Cruz Biotechnology), anti-lectin Dolichos biflorus agglutinin (DBA; Vector Laboratories), and anti-VDAC (Cell Signaling) antibodies. Tissues were mounted in ProLong Gold Antifade Mountant (Life Technologies) and imaged with 40× and 100× oil-immersion lenses on a Leica SP8 gated STED Microscope using Leica LAS X software (Heidelberg, Germany). To enable comparison among samples, the same laser power, gain and acquisition settings were used across all slides.

Immunofluorescence

LLC-PK1 and mIMCD3 cells were immunostained as described previously41. Briefly, cells were plated on poly-L-lysine-coated glass coverslips and fixed with 4% paraformaldehyde for 10 minutes at 37 °C. After blocking in 2% BSA and 0.2% Triton X-100, cells were incubated in the same solution with primary antibody for active caspase 3 and PC2 overnight at 4 °C, then incubated in anti-rabbit AlexaFluor 488 (Life Technologies), phalloidin conjugated to tetramethylrhodamine (TRITC; Life Technologies), and anti-mouse AlexaFluor 633 (Life Technologies) for 1 hour before mounting with ProLong Gold antifade mounting reagent with DAPI (Life Technologies). Slides were imaged with a Leica TCS SP5 Confocal Laser Scanning Microscope.

To calculate PC2 and Cleaved Caspase 3 intensity, ImageJ (NIH) was used for image processing. All measurements of fluorescence intensity were calculated using images taken at 10X magnification to ensure unbiased and robust quantification. Individual cells or cell groups were selected as regions of interest (ROIs,) and the fluorescence intensity and area were calculated for each ROI. Intensity was divided by its corresponding area and averaged across each image. Five images were taken per condition and averaged to plot as Intensity/Area.

Human heart RNA-Seq

RNA Sequencing was performed on left ventricular tissue samples from non-failing (NF; n = 8) human donor hearts, and from failing human hearts obtained from patients with ischemic cardiomyopathy (ICM; n = 8) or non-ischemic cardiomyopathy (NICM; n = 8) as described previously48. Data were analyzed using Qlucore Omics Explorer (Lund, Sweden). Normalized Reads Per Kilobase of transcript, per Million mapped reads (RPKM) values were log2 transformed and fold change calculated. Curated lists of genes associated with cellular responses to ER and oxidative stress were collected and cross-referenced from MetaCore (Clarivate Analytics) and Ingenuity Pathway Analysis (Ingenuity Systems, QIAGEN Bioinformatics). The genes were compiled and used to generate an expression heat map of differentially regulated (p < 0.05) ER and oxidative stress-related genes. Linear regression analysis was performed to show significant (p < 0.0001) correlation between PKD2 and NFE2L2 transcripts.

iPSC culture and differentiation

Human induced pluripotent stem cells (iPSC) were acquired from the Coriell Institute (GM23338), as characterized previously102. iPSC colonies were maintained on growth-factor reduced Matrigel (Corning)-coated tissue culture plates in mTeSR1 medium (Stem Cell Technologies). iPSCs were differentiated into iPSC-derived cardiomyocytes (iPSC-CMs) following a sequential protocol of manipulating the WNT pathway103, using 12.5 μM CHIR99021 (Stem Cell Technologies) for 24 hours and 5 μM IWP4 (Tocris Bioscience) for 48 hours on day 3 after the induction of differentiation. Subsequently, the differentiating cultures were maintained in RPMI + B2-insulin until day 11 when spontaneous beating was observed. Media was then changed to RPMI + B27 + insulin for 2 days, followed by 4 days of metabolic selection using DMEM without glucose and 4 mM lactate104. iPSC-CMs were kept in RPMI + B27 + insulin until day 21 after the start of differentiation when they were dissociated and re-plated on a 12-well plate coated with 50 μg/ml fibronectin (bovine, Sigma-Aldrich)105. iPSC-CMs were cultured for a subsequent 2 days in RPMI + B27 + insulin before experiments were performed.

Human glioblastoma project RNA-Seq

The open-source RNA-Seq dataset from The Allen Institute’s human glioblastoma project was used to interrogate the relationship between PKD2 expression in human brain and integrated stress response genes. RNA-Seq was performed on different glioblastoma structures as described62 and the FPKM values log2 normalized before analysis with Qlucore Omics Explorer. Linear regression analysis was performed to show significant (p < 0.0001) correlation between PKD2 and NFE2L2 transcripts.

Creation of stable knockdown cells

Short hairpin RNA (shRNA) against Pkd2 was designed to be specific to the pig sequence. The previously described41,106 PC2 shRNA constructs were put into a psiRNA vector (InvivoGen, San Diego, CA), which was stably transfected into LLC-PK1 cells. Cells were exposed to G418 (2.5 mg/ml) as previously described41,106. LLC-PK1 cells were maintained in Dulbecco’s Modified Eagle Medium (DMEM) supplemented with 10% fetal bovine serum (FBS) and kept at 37 C in 5% CO2.

In vitro stress treatment

Cells were plated on a 6-well plate (Corning) at a density of 400,000 cells per well. The following day, cells were either treated with the commonly used ER-stress inducer Tunicamycin (TM)107 or serum-starved for 24 hours. After treatment, the cells were lysed and collected as described above for Western Blot or stained for Immunofluorescence.

Measurement of cellular stress

To assess the level of cellular stress in both in vivo and in vitro samples, we immunoblotted for several markers whose levels are changed in response to stress: 4-HNE, a reactive short-chain aldehyde formed during lipid peroxidation following oxidative stress108; CHOP, a protein involved in ER-stress mediated apoptosis51; eIF2α, whose phosphorylation (p-EIF2α) is the core event in the integrated stress response pathway50; cleaved caspase 3, a commonly used marker for apoptotic cells109.

mRNA analysis

mRNA was extracted from animal tissue and cultured cells using a RNeasy RNA Isolation Kit (Qiagen, Hilden, Germany) and reverse-transcribed to complementary DNA (cDNA) using Multiscribe Reverse Transcriptase and random primers (Applied Biosystems, Foster City, CA). For real-time quantitative PCR, 20 ng of cDNA was used as transcript template in a reaction with Power SYBR Green Master Mix (Applied Biosystems) on a 7500 Fast Real-Time PCR system (Applied Biosystems). Fold change in Pkd2 (Fwd 5′—CAGAGGGGCTGCTACAGTTT—3′; Rev 5′—TTGAAGAGCTTAATCCAGACCA—3′) and Nfe2l2 (Fwd 5′—AGATGACCATGAGTCGCTTGC—3′; Rev 5′—CCTGATGAGGGGCAGTGAAG—3′) mRNA transcript levels compared to control samples were determined using the 2−(ΔΔCT) method. Actin (Fwd 5′—GTGACGTTGACATCCGTAAAGA—3′; Rev 5′—GCCGGACTCATCGTACTCC—3′) or Gapdh (Fwd 5′—AGGTCGGTGTGAACGGATTTG—3′; Rev 5′—GGGGTCGTTGATGGCAACA—3′) were used as internal control.

CellTiter-Glo assay

Cells were plated at a density of 1000 cells per well on a 96-well plate (Corning) and treated the following day. After 24 hours of treatment, CellTiter-Glo Luminescent Cell Viability assays were carried out according to the manufacturer’s instructions (Promega Corporation). Experiments were performed in triplicates with 10 replicates per experiment.

Statistical analysis

For cell-based experiments, data were calculated from at least three separate preparations. For animal-based experiments, data were calculated from at least three biological replicates. Where appropriate, one-way analysis of variance (ANOVA) with multiple comparisons or non-parametric Mann Whitney U test was applied. Data are presented as (1) mean ± SD, or (2) median with range, as stated in the figure legend. In all experiments, p < 0.05 was considered statistically significant. *p < 0.05, **p < 0.01, ***p < 0.001, and ****p < 0.0001.

Data availability

The data generated, used, and/or analyzed in the current study are available from the corresponding author upon reasonable request.

References

  1. 1.

    Cornec-Le Gall, E. et al. PKD2-Related Autosomal Dominant Polycystic Kidney Disease: Prevalence, Clinical Presentation, Mutation Spectrum, and Prognosis. American Journal of Kidney Diseases 70, 476–485, https://doi.org/10.1053/j.ajkd.2017.01.046 (2017).

  2. 2.

    Uhlen, M. et al. Towards a knowledge-based Human Protein Atlas. Nature biotechnology 28, 1248–1250, https://doi.org/10.1038/nbt1210-1248 (2010).

  3. 3.

    Uhlen, M. et al. Proteomics. Tissue-based map of the human proteome. Science (New York, N.Y.) 347, 1260419, https://doi.org/10.1126/science.1260419 (2015).

  4. 4.

    Thul, P. J. et al. A subcellular map of the human proteome. Science (New York, N.Y.) 356, https://doi.org/10.1126/science.aal3321 (2017).

  5. 5.

    Koulen, P. et al. Polycystin-2 is an intracellular calcium release channel. Nature Cell Biology 4, 191–197, https://doi.org/10.1038/ncb754 (2002).

  6. 6.

    Cantiello, H. F. Regulation of calcium signaling by polycystin-2. American journal of physiology. Renal physiology 286, F1012–1029, https://doi.org/10.1152/ajprenal.00181.2003 (2004).

  7. 7.

    Anyatonwu, G. I. & Ehrlich, B. E. Calcium signaling and polycystin-2. Biochemical and Biophysical Research Communications 322, 1364–1373, https://doi.org/10.1016/j.bbrc.2004.08.043 (2004).

  8. 8.

    Hofer, A. M. Interactions between calcium and cAMP signaling. Current medicinal chemistry 19, 5768–5773 (2012).

  9. 9.

    Torres, V. E. & Harris, P. C. Strategies targeting cAMP signaling in the treatment of polycystic kidney disease. Journal of the American Society of Nephrology: JASN 25, 18–32, https://doi.org/10.1681/asn.2013040398 (2014).

  10. 10.

    Padovano, V. et al. The polycystins are modulated by cellular oxygen-sensing pathways and regulate mitochondrial function. Mol Biol Cell 28, 261–269, https://doi.org/10.1091/mbc.E16-08-0597 (2017).

  11. 11.

    Kuo, I. Y. et al. Polycystin 2 regulates mitochondrial Ca&lt;sup&gt;2 + &lt;/sup&gt; signaling, bioenergetics, and dynamics through mitofusin 2. Science signaling 12, eaat7397, https://doi.org/10.1126/scisignal.aat7397 (2019).

  12. 12.

    Goilav, B. Apoptosis in polycystic kidney disease. Biochimica et biophysica acta 1812, 1272–1280, https://doi.org/10.1016/j.bbadis.2011.01.006 (2011).

  13. 13.

    Wegierski, T. et al. TRPP2 channels regulate apoptosis through the Ca2 + concentration in the endoplasmic reticulum. The EMBO journal 28, 490–499, https://doi.org/10.1038/emboj.2008.307 (2009).

  14. 14.

    Grantham, J. J. Lillian Jean Kaplan International Prize for advancement in the understanding of polycystic kidney disease. Understanding polycystic kidney disease: a systems biology approach. Kidney international 64, 1157–1162, https://doi.org/10.1046/j.1523-1755.2003.00242.x (2003).

  15. 15.

    Calvet, J. P. Strategies to Inhibit Cyst Formation in ADPKD. Clinical Journal of the American Society of Nephrology 3, 1205, https://doi.org/10.2215/CJN.05651207 (2008).

  16. 16.

    Rowe, I. et al. Defective glucose metabolism in polycystic kidney disease identifies a new therapeutic strategy. Nature medicine 19, 488–493, https://doi.org/10.1038/nm.3092 (2013).

  17. 17.

    Riwanto, M. et al. Inhibition of Aerobic Glycolysis Attenuates Disease Progression in Polycystic Kidney Disease. PloS one 11, e0146654, https://doi.org/10.1371/journal.pone.0146654 (2016).

  18. 18.

    Menezes, L. F., Lin, C. C., Zhou, F. & Germino, G. G. Fatty Acid Oxidation is Impaired in An Orthologous Mouse Model of Autosomal Dominant Polycystic Kidney Disease. EBioMedicine 5, 183–192, https://doi.org/10.1016/j.ebiom.2016.01.027 (2016).

  19. 19.

    Roveri, A. et al. Effect of hydrogen peroxide on calcium homeostasis in smooth muscle cells. Archives of Biochemistry and Biophysics 297, 265–270, https://doi.org/10.1016/0003-9861(92)90671-I (1992).

  20. 20.

    Renard, D. C., Seitz, M. B. & Thomas, A. P. Oxidized glutathione causes sensitization of calcium release to inositol 1,4,5-trisphosphate in permeabilized hepatocytes. Biochemical Journal 284, 507, https://doi.org/10.1042/bj2840507 (1992).

  21. 21.

    Rooney, T. A., Renard, D. C., Sass, E. J. & Thomas, A. P. Oscillatory cytosolic calcium waves independent of stimulated inositol 1,4,5-trisphosphate formation in hepatocytes. Journal of Biological Chemistry 266, 12272–12282 (1991).

  22. 22.

    Wang, H. & Joseph, J. A. Mechanisms of hydrogen peroxide-induced calcium dysregulation in PC12 cells. Free Radical Biology and Medicine 28, 1222–1231, https://doi.org/10.1016/S0891-5849(00)00241-0 (2000).

  23. 23.

    Ermak, G. & Davies, K. J. Calcium and oxidative stress: from cell signaling to cell death. Molecular immunology 38, 713–721 (2002).

  24. 24.

    Chauveau, D., Fakhouri, F. & GrÜNfeld, J.-P. Liver Involvement in Autosomal-Dominant Polycystic Kidney Disease. Journal of the American Society of Nephrology 11, 1767 (2000).

  25. 25.

    Kim, J. A. et al. Pancreatic Cysts in Autosomal Dominant Polycystic Kidney Disease: Prevalence and Association with PKD2 Gene Mutations. Radiology 280, 762–770, https://doi.org/10.1148/radiol.2016151650 (2016).

  26. 26.

    Chang, M. Y. & Ong, A. C. M. Autosomal Dominant Polycystic Kidney Disease: Recent Advances in Pathogenesis and Treatment. Nephron Physiology 108, p1–p7, https://doi.org/10.1159/000112495 (2008).

  27. 27.

    Vlak, M. H., Algra, A., Brandenburg, R. & Rinkel, G. J. Prevalence of unruptured intracranial aneurysms, with emphasis on sex, age, comorbidity, country, and time period: a systematic review and meta-analysis. The Lancet. Neurology 10, 626–636, https://doi.org/10.1016/s1474-4422(11)70109-0 (2011).

  28. 28.

    Ecder, T. Cardiovascular complications in autosomal dominant polycystic kidney disease. Current hypertension reviews 9, 2–11 (2013).

  29. 29.

    Yu, T.-M. et al. Risk of cancer in patients with polycystic kidney disease: a propensity-score matched analysis of a nationwide, population-based cohort study. The Lancet Oncology 17, 1419–1425, https://doi.org/10.1016/S1470-2045(16)30250-9 (2016).

  30. 30.

    Sun, K., Xu, D. & Mei, C. The association between autosomal dominant polycystic kidney disease and cancer. International urology and nephrology 51, 93–100, https://doi.org/10.1007/s11255-018-1951-5 (2019).

  31. 31.

    Prasad, S., McDaid, J. P., Tam, F. W. K., Haylor, J. L. & Ong, A. C. M. Pkd2 Dosage Influences Cellular Repair Responses following Ischemia-Reperfusion Injury. The American Journal of Pathology 175, 1493–1503, https://doi.org/10.2353/ajpath.2009.090227 (2009).

  32. 32.

    Pennekamp, P. et al. The ion channel polycystin-2 is required for left-right axis determination in mice. Current biology: CB 12, 938–943 (2002).

  33. 33.

    Markowitz, G. S. et al. Polycystin-2 expression is developmentally regulated. American Journal of Physiology-Renal Physiology 277, F17–F25, https://doi.org/10.1152/ajprenal.1999.277.1.F17 (1999).

  34. 34.

    Bisgrove, B. W., Snarr, B. S., Emrazian, A. & Yost, H. J. Polaris and Polycystin-2 in dorsal forerunner cells and Kupffer’s vesicle are required for specification of the zebrafish left-right axis. Developmental biology 287, 274–288, https://doi.org/10.1016/j.ydbio.2005.08.047 (2005).

  35. 35.

    Zhao, Y. Polycystin-2 expression is increased following experimental ischaemic renal injury. 17, 2138–2144, https://doi.org/10.1093/ndt/17.12.2138 (2002).

  36. 36.

    Giehl, E. et al. Polycystin 2-dependent cardio-protective mechanisms revealed by cardiac stress. Pflugers Archiv: European journal of physiology 469, 1507–1517, https://doi.org/10.1007/s00424-017-2042-7 (2017).

  37. 37.

    Lu, J. et al. Polycystin-2 Plays an Essential Role in Glucose Starvation-Induced Autophagy in Human Embryonic Stem Cell-Derived Cardiomyocytes. STEM CELLS 36, 501–513, https://doi.org/10.1002/stem.2764 (2018).

  38. 38.

    Gargalionis, A. N. et al. Polycystin-1 and polycystin-2 are involved in the acquisition of aggressive phenotypes in colorectal cancer. International Journal of Cancer 136, 1515–1527, https://doi.org/10.1002/ijc.29140 (2015).

  39. 39.

    Li, Y., Wright, J. M., Qian, F., Germino, G. G. & Guggino, W. B. Polycystin 2 Interacts with Type I Inositol 1,4,5-Trisphosphate Receptor to Modulate Intracellular Ca2 + Signaling. Journal of Biological Chemistry 280, 41298–41306, https://doi.org/10.1074/jbc.M510082200 (2005).

  40. 40.

    Sammels, E. et al. Polycystin-2 activation by inositol 1,4,5-trisphosphate-induced Ca 2 + release requires its direct association with the inositol 1,4,5-trisphosphate receptor in a signaling microdomain. 285, jbc.M109.090662, https://doi.org/10.1074/jbc.m109.090662 (2010).

  41. 41.

    Kuo, I. Y. et al. Cyst formation following disruption of intracellular calcium signaling. Proceedings of the National Academy of Sciences 111, 14283, https://doi.org/10.1073/pnas.1412323111 (2014).

  42. 42.

    Young, E. W. & Humes, H. D. Calcium and acute renal failure. Mineral and electrolyte metabolism 17, 106–111 (1991).

  43. 43.

    Spirli, C. et al. Altered store operated calcium entry increases cyclic 3’,5’-adenosine monophosphate production and extracellular signal-regulated kinases 1 and 2 phosphorylation in polycystin-2-defective cholangiocytes. Hepatology (Baltimore, Md.) 55, 856–868, https://doi.org/10.1002/hep.24723 (2012).

  44. 44.

    Noeman, S. A., Hamooda, H. E. & Baalash, A. A. Biochemical study of oxidative stress markers in the liver, kidney and heart of high fat diet induced obesity in rats. Diabetol Metab Syndr 3, 17–17, https://doi.org/10.1186/1758-5996-3-17 (2011).

  45. 45.

    Fick, G. M., Johnson, A. M., Hammond, W. S. & Gabow, P. A. Causes of death in autosomal dominant polycystic kidney disease. Journal of the American Society of Nephrology: JASN 5, 2048–2056 (1995).

  46. 46.

    Orskov, B., Sorensen, V. R., Feldt-Rasmussen, B. & Strandgaard, S. Changes in causes of death and risk of cancer in Danish patients with autosomal dominant polycystic kidney disease and end-stage renal disease. Nephrology, dialysis, transplantation: official publication of the European Dialysis and Transplant Association - European Renal Association 27, 1607–1613, https://doi.org/10.1093/ndt/gfr467 (2012).

  47. 47.

    Yang, K. C., Ku, Y. C., Lovett, M. & Nerbonne, J. M. Combined deep microRNA and mRNA sequencing identifies protective transcriptomal signature of enhanced PI3Kalpha signaling in cardiac hypertrophy. Journal of molecular and cellular cardiology 53, 101–112, https://doi.org/10.1016/j.yjmcc.2012.04.012 (2012).

  48. 48.

    Yang, K. C. et al. Deep RNA sequencing reveals dynamic regulation of myocardial noncoding RNAs in failing human heart and remodeling with mechanical circulatory support. Circulation 129, 1009–1021, https://doi.org/10.1161/circulationaha.113.003863 (2014).

  49. 49.

    Wang, C. et al. Inhibiting the integrated stress response pathway prevents aberrant chondrocyte differentiation thereby alleviating chondrodysplasia. eLife 7, e37673, https://doi.org/10.7554/eLife.37673 (2018).

  50. 50.

    Pakos-Zebrucka, K. et al. The integrated stress response. EMBO Rep 17, 1374–1395, https://doi.org/10.15252/embr.201642195 (2016).

  51. 51.

    Harding, H. P. et al. Regulated Translation Initiation Controls Stress-Induced Gene Expression in Mammalian Cells. Molecular Cell 6, 1099–1108, https://doi.org/10.1016/S1097-2765(00)00108-8 (2000).

  52. 52.

    Bhandary, B., Marahatta, A., Kim, H.-R. & Chae, H.-J. An involvement of oxidative stress in endoplasmic reticulum stress and its associated diseases. Int J Mol Sci 14, 434–456, https://doi.org/10.3390/ijms14010434 (2012).

  53. 53.

    Zeeshan, H. M., Lee, G. H., Kim, H. R. & Chae, H. J. Endoplasmic Reticulum Stress and Associated ROS. Int J Mol Sci 17, 327, https://doi.org/10.3390/ijms17030327 (2016).

  54. 54.

    Alam, J. et al. Nrf2, a Cap’n’Collar transcription factor, regulates induction of the heme oxygenase-1 gene. J Biol Chem 274, 26071–26078, https://doi.org/10.1074/jbc.274.37.26071 (1999).

  55. 55.

    Kensler, T. W., Wakabayashi, N. & Biswal, S. Cell survival responses to environmental stresses via the Keap1-Nrf2-ARE pathway. Annual review of pharmacology and toxicology 47, 89–116, https://doi.org/10.1146/annurev.pharmtox.46.120604.141046 (2007).

  56. 56.

    Kobayashi, A. et al. Oxidative and electrophilic stresses activate Nrf2 through inhibition of ubiquitination activity of Keap1. Molecular and cellular biology 26, 221–229, https://doi.org/10.1128/mcb.26.1.221-229.2006 (2006).

  57. 57.

    He, C. H. et al. Identification of Activating Transcription Factor 4 (ATF4) as an Nrf2-interacting Protein: IMPLICATION FOR HEME OXYGENASE-1 GENE REGULATION. Journal of Biological Chemistry 276, 20858–20865, https://doi.org/10.1074/jbc.M101198200 (2001).

  58. 58.

    Hofherr, A., Wagner, C., Fedeles, S., Somlo, S. & Köttgen, M. N-glycosylation determines the abundance of the transient receptor potential channel TRPP2. The Journal of biological chemistry 289, 14854–14867, https://doi.org/10.1074/jbc.M114.562264 (2014).

  59. 59.

    Gluck, M. R., Jayatilleke, E., Shaw, S., Rowan, A. J. & Haroutunian, V. CNS oxidative stress associated with the kainic acid rodent model of experimental epilepsy. Epilepsy research 39, 63–71 (2000).

  60. 60.

    Evans, M. C., Griffiths, T. & Meldrum, B. S. Kainic acid seizures and the reversibility of calcium loading in vulnerable neurons in the hippocampus. Neuropathology and applied neurobiology 10, 285–302 (1984).

  61. 61.

    Ben-Ari, Y. & Cossart, R. Kainate, a double agent that generates seizures: two decades of progress. Trends in neurosciences 23, 580–587 (2000).

  62. 62.

    Puchalski, R. B. et al. An anatomic transcriptional atlas of human glioblastoma. Science (New York, N.Y.) 360, 660, https://doi.org/10.1126/science.aaf2666 (2018).

  63. 63.

    Zhang, Y. et al. Tauroursodeoxycholic acid (TUDCA) alleviates endoplasmic reticulum stress of nuclear donor cells under serum starvation. PloS one 13, e0196785, https://doi.org/10.1371/journal.pone.0196785 (2018).

  64. 64.

    Zhang, Y. et al. Inhibition of Starvation-Triggered Endoplasmic Reticulum Stress, Autophagy, and Apoptosis in ARPE-19 Cells by Taurine through Modulating the Expression of Calpain-1 and Calpain-2. Int J Mol Sci 18, 2146, https://doi.org/10.3390/ijms18102146 (2017).

  65. 65.

    Pandey, S., Lopez, C. & Jammu, A. Oxidative stress and activation of proteasome protease during serum deprivation-induced apoptosis in rat hepatoma cells; inhibition of cell death by melatonin. Apoptosis: an international journal on programmed cell death 8, 497–508 (2003).

  66. 66.

    Teske, B. F. et al. The eIF2 kinase PERK and the integrated stress response facilitate activation of ATF6 during endoplasmic reticulum stress. Molecular biology of the cell 22, 4390–4405, https://doi.org/10.1091/mbc.E11-06-0510 (2011).

  67. 67.

    Qian, Q. et al. Pkd2 haploinsufficiency alters intracellular calcium regulation in vascular smooth muscle cells. Human Molecular Genetics 12, 1875–1880, https://doi.org/10.1093/hmg/ddg190 (2003).

  68. 68.

    Brookes, Z. L. S. et al. Pkd2 mesenteric vessels exhibit a primary defect in endothelium-dependent vasodilatation restored by rosiglitazone. Am J Physiol Heart Circ Physiol 304, H33–H41, https://doi.org/10.1152/ajpheart.01102.2011 (2013).

  69. 69.

    Chang, M. Y. et al. Haploinsufficiency of Pkd2 is associated with increased tubular cell proliferation and interstitial fibrosis in two murine Pkd2 models. Nephrology Dialysis Transplantation 21, 2078–2084, https://doi.org/10.1093/ndt/gfl150 (2006).

  70. 70.

    Zhang, D. D. Mechanistic Studies of the Nrf2-Keap1 Signaling Pathway. Drug Metabolism Reviews 38, 769–789, https://doi.org/10.1080/03602530600971974 (2006).

  71. 71.

    Park, J. H. et al. Cloning and characterization of the murine pkd2 promoter. Genomics 66, 305–312, https://doi.org/10.1006/geno.2000.6197 (2000).

  72. 72.

    Rodova, M., Islam, M. R., Maser, R. L. & Calvet, J. P. The polycystic kidney disease-1 promoter is a target of the beta-catenin/T-cell factor pathway. J Biol Chem 277, 29577–29583, https://doi.org/10.1074/jbc.M203570200 (2002).

  73. 73.

    Ecder, T. et al. Caspases, Bcl-2 proteins and apoptosis in autosomal-dominant polycystic kidney disease. Kidney international 61, 1220–1230, https://doi.org/10.1046/j.1523-1755.2002.00250.x (2002).

  74. 74.

    Edelstein, C. L. What is the role of tubular epithelial cell apoptosis in polycystic kidney disease (PKD)? Cell cycle (Georgetown, Tex.) 4, 1550–1554, https://doi.org/10.4161/cc.4.11.2185 (2005).

  75. 75.

    Bai, C.-X. et al. Formation of a new receptor-operated channel by heteromeric assembly of TRPP2 and TRPC1 subunits. EMBO reports 9, 472–479, https://doi.org/10.1038/embor.2008.29 (2008).

  76. 76.

    Palsamy, P. & Subramanian, S. Resveratrol protects diabetic kidney by attenuating hyperglycemia-mediated oxidative stress and renal inflammatory cytokines via Nrf2-Keap1 signaling. Biochimica et biophysica acta 1812, 719–731, https://doi.org/10.1016/j.bbadis.2011.03.008 (2011).

  77. 77.

    Moradi, H. & Vaziri, N. D. Effect of resveratrol on progression of polycystic kidney disease: a case of cautious optimism. Nephrology Dialysis Transplantation 31, 1755–1758, https://doi.org/10.1093/ndt/gfw097 (2016).

  78. 78.

    Wu, M. et al. Resveratrol delays polycystic kidney disease progression through attenuation of nuclear factor kappaB-induced inflammation. Nephrology, dialysis, transplantation: official publication of the European Dialysis and Transplant Association - European Renal Association 31, 1826–1834, https://doi.org/10.1093/ndt/gfw058 (2016).

  79. 79.

    Scheff, R. T., Zuckerman, G., Harter, H., Delmez, J. & Koehler, R. Diverticular disease in patients with chronic renal failure due to polycystic kidney disease. Annals of internal medicine 92, 202–204, https://doi.org/10.7326/0003-4819-92-2-202 (1980).

  80. 80.

    Sharp, C. K., Zeligman, B. E., Johnson, A. M., Duley, I. & Gabow, P. A. Evaluation of colonic diverticular disease in autosomal dominant polycystic kidney disease without end-stage renal disease. American journal of kidney diseases: the official journal of the National Kidney Foundation 34, 863–868, https://doi.org/10.1016/s0272-6386(99)70043-0 (1999).

  81. 81.

    Morris-Stiff, G., Coles, G., Moore, R., Jurewicz, A. & Lord, R. Abdominal wall hernia in autosomal dominant polycystic kidney disease. The British journal of surgery 84, 615–617 (1997).

  82. 82.

    Modi, K. B., Grant, A. C., Garret, A. & Rodger, R. S. Indirect inguinal hernia in CAPD patients with polycystic kidney disease. Advances in peritoneal dialysis. Conference on Peritoneal Dialysis 5, 84–86 (1989).

  83. 83.

    Fick, G. M. & Gabow, P. A. Hereditary and acquired cystic disease of the kidney. Kidney Int 46, 951–964, https://doi.org/10.1038/ki.1994.354 (1994).

  84. 84.

    Bae, K. T. et al. Magnetic resonance imaging evaluation of hepatic cysts in early autosomal-dominant polycystic kidney disease: the Consortium for Radiologic Imaging Studies of Polycystic Kidney Disease cohort. Clinical journal of the American Society of Nephrology: CJASN 1, 64–69, https://doi.org/10.2215/cjn.00080605 (2006).

  85. 85.

    Alpern, M. B., Dorfman, R. E., Gross, B. H., Gottlieb, C. A. & Sandler, M. A. Seminal vesicle cysts: association with adult polycystic kidney disease. Radiology 180, 79–80, https://doi.org/10.1148/radiology.180.1.2052727 (1991).

  86. 86.

    Danaci, M. et al. The prevalence of seminal vesicle cysts in autosomal dominant polycystic kidney disease. Nephrology, dialysis, transplantation: official publication of the European Dialysis and Transplant Association - European Renal Association 13, 2825–2828, https://doi.org/10.1093/ndt/13.11.2825 (1998).

  87. 87.

    Kuo, I. Y., Duong, S. L., Nguyen, L. & Ehrlich, B. E. Decreased Polycystin 2 Levels Result in Non-Renal Cardiac Dysfunction with Aging. PloS one 11, e0153632, https://doi.org/10.1371/journal.pone.0153632 (2016).

  88. 88.

    Cai, Y. et al. Identification and Characterization of Polycystin-2, the PKD2 Gene Product. Journal of Biological Chemistry 274, 28557–28565, https://doi.org/10.1074/jbc.274.40.28557 (1999).

  89. 89.

    Yoder, B. K., Hou, X. & Guay-Woodford, L. M. The Polycystic Kidney Disease Proteins, Polycystin-1, Polycystin-2, Polaris, and Cystin, Are Co-Localized in Renal Cilia. Journal of the American Society of Nephrology 13, 2508, https://doi.org/10.1097/01.ASN.0000029587.47950.25 (2002).

  90. 90.

    Kottgen, M. et al. TRPP2 and TRPV4 form a polymodal sensory channel complex. The Journal of cell biology 182, 437–447, https://doi.org/10.1083/jcb.200805124 (2008).

  91. 91.

    Walker, R. V. et al. Ciliary exclusion of Polycystin-2 promotes kidney cystogenesis in an autosomal dominant polycystic kidney disease model. Nature. Communications 10, 4072, https://doi.org/10.1038/s41467-019-12067-y (2019).

  92. 92.

    Luo, Y., Vassilev, P. M., Li, X., Kawanabe, Y. & Zhou, J. Native Polycystin 2 Functions as a Plasma Membrane Ca&lt;sup&gt;2 + &lt;/sup&gt;-Permeable Cation Channel in Renal Epithelia. Molecular and cellular biology 23, 2600, https://doi.org/10.1128/MCB.23.7.2600-2607.2003 (2003).

  93. 93.

    Scheffers, M. S. et al. Distinct subcellular expression of endogenous polycystin-2 in the plasma membrane and Golgi apparatus of MDCK cells. Human Molecular Genetics 11, 59–67, https://doi.org/10.1093/hmg/11.1.59 (2002).

  94. 94.

    Santoso, N. G., Cebotaru, L. & Guggino, W. B. Polycystin-1, 2, and STIM1 interact with IP(3)R to modulate ER Ca release through the PI3K/Akt pathway. Cellular physiology and biochemistry: international journal of experimental cellular physiology, biochemistry, and pharmacology 27, 715–726, https://doi.org/10.1159/000330080 (2011).

  95. 95.

    Anyatonwu, G. I., Estrada, M., Tian, X., Somlo, S. & Ehrlich, B. E. Regulation of ryanodine receptor-dependent calcium signaling by polycystin-2. Proceedings of the National Academy of Sciences of the United States of America 104, 6454–6459, https://doi.org/10.1073/pnas.0610324104 (2007).

  96. 96.

    Tsiokas, L. et al. Specific association of the gene product of PKD2 with the TRPC1 channel. Proceedings of the National Academy of Sciences of the United States of America 96, 3934–3939, https://doi.org/10.1073/pnas.96.7.3934 (1999).

  97. 97.

    Montalbetti, N., Cantero, M. R., Dalghi, M. G. & Cantiello, H. F. Reactive oxygen species inhibit polycystin-2 (TRPP2) cation channel activity in term human syncytiotrophoblast. Placenta 29, 510–518, https://doi.org/10.1016/j.placenta.2008.02.015 (2008).

  98. 98.

    Kale, S. et al. Bone marrow stem cells contribute to repair of the ischemically injured renal tubule. The Journal of Clinical Investigation 112, 42–49, https://doi.org/10.1172/JCI17856 (2003).

  99. 99.

    Baculis, B. C. et al. Prolonged seizure activity causes caspase dependent cleavage and dysfunction of G-protein activated inwardly rectifying potassium channels. Scientific Reports 7, 12313, https://doi.org/10.1038/s41598-017-12508-y (2017).

  100. 100.

    Racine, R. J. Modification of seizure activity by electrical stimulation. II. Motor seizure. Electroencephalography and clinical neurophysiology 32, 281–294 (1972).

  101. 101.

    Boehringer, R. et al. Chronic Loss of CA2 Transmission Leads to Hippocampal Hyperexcitability. Neuron 94, 642–655.e649, https://doi.org/10.1016/j.neuron.2017.04.014 (2017).

  102. 102.

    Cohn, R. et al. A Contraction Stress Model of Hypertrophic Cardiomyopathy due to Sarcomere Mutations. Stem cell reports 12, 71–83, https://doi.org/10.1016/j.stemcr.2018.11.015 (2019).

  103. 103.

    Lian, X. et al. Directed cardiomyocyte differentiation from human pluripotent stem cells by modulating Wnt/beta-catenin signaling under fully defined conditions. Nature protocols 8, 162–175, https://doi.org/10.1038/nprot.2012.150 (2013).

  104. 104.

    Tohyama, S. et al. Distinct metabolic flow enables large-scale purification of mouse and human pluripotent stem cell-derived cardiomyocytes. Cell stem cell 12, 127–137, https://doi.org/10.1016/j.stem.2012.09.013 (2013).

  105. 105.

    Edwards, S. L. et al. A Multiwell Cardiac μGMEA Platform for Action Potential Recordings from Human iPSC-Derived Cardiomyocyte Constructs. Stem cell reports 11, 522–536, https://doi.org/10.1016/j.stemcr.2018.06.016 (2018).

  106. 106.

    DesRochers, T. M., Kuo, I. Y., Kimmerling, E. P., Ehrlich, B. E. & Kaplan, D. L. The effects of mycoplasma contamination upon the ability to form bioengineered 3D kidney cysts. PloS one 10, e0120097, https://doi.org/10.1371/journal.pone.0120097 (2015).

  107. 107.

    Oslowski, C. M. & Urano, F. In Methods in Enzymology Vol. 490 (ed P. Michael Conn) 71-92 (Academic Press, 2011).

  108. 108.

    Uchida, K. 4-Hydroxy-2-nonenal: a product and mediator of oxidative stress. Progress in Lipid Research 42, 318–343, https://doi.org/10.1016/S0163-7827(03)00014-6 (2003).

  109. 109.

    Brentnall, M., Rodriguez-Menocal, L., De Guevara, R. L., Cepero, E. & Boise, L. H. Caspase-9, caspase-3 and caspase-7 have distinct roles during intrinsic apoptosis. BMC Cell Biology 14, 32, https://doi.org/10.1186/1471-2121-14-32 (2013).

Download references

Acknowledgements

We thank Qi Wang and Dr. Xiaoyong Yang for kindly providing liver cDNA samples from ND- and HFD-fed mice. We thank Dr. Bentley Lim, Eunice Cho (Yale University), and Dr. Olga Buzovetsky (The Rockefeller University) for helpful discussions and edits. We thank Esther Giehl (Charité – Universitätsmedizin Berlin) for the contribution of saline- and ISO-treated murine hearts. Federal and NIH grant support is acknowledged: 5P01DK057751 and P30DK090744 (B.E.E.), F31DK118836 (A.L.B.), 1R01NS083402 and 1R01NS097610 (H.J.C.), T32GM007205 (L.R.S.), and GM007324. We acknowledge the use of the Yale Center for Cellular and Molecular Imaging (NIH grants 5P30DK034989 and OD020142). L.R.S. was supported by a P.D. Soros Fellowship for New Americans. WT and PC2 KO mIMCD-3 cells were created by members of the George M. O’Brien Kidney Center at Yale (P30 DK079310). T.T.F. was supported by a scholarship from the German Academic Scholarship Foundation.

Author information

A.L.B. and B.E.E. conceived the project. A.L.B., T.T.F., J.F.W., and H.J.C. conducted experiments and analyzed data. A.M., L.R.S., P.C.W., E.K.J., G.M., L.G.C., S.G.C., J.M.N., H.J.C., and M.E.R. contributed reagents. A.L.B. drafted and edited the manuscript. B.E.E. and T.T.F. edited the manuscript. All authors agreed to the final manuscript.

Correspondence to Barbara E. Ehrlich.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Brill, A.L., Fischer, T.T., Walters, J.M. et al. Polycystin 2 is increased in disease to protect against stress-induced cell death. Sci Rep 10, 386 (2020). https://doi.org/10.1038/s41598-019-57286-x

Download citation

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.