Search tips
Search criteria 


Logo of plosonePLoS OneView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS One. 2010; 5(8): e12305.
Published online 2010 August 23. doi:  10.1371/journal.pone.0012305
PMCID: PMC2925899

Identification of a Polycystin-1 Cleavage Product, P100, That Regulates Store Operated Ca2+ Entry through Interactions with STIM1

David Holowka, Editor


Autosomal Dominant Polycystic Kidney Disease (ADPKD) is a genetic disorder resulting in large kidney cysts and eventual kidney failure. Mutations in either the PKD1 or PKD2/TRPP2 genes and their respective protein products, polycystin-1 (PC1) and polycystin-2 (PC2) result in ADPKD. PC2 is known to function as a non-selective cation channel, but PC1's function and the function of PC1 cleavage products are not well understood. Here we identify an endogenous PC1 cleavage product, P100, a 100 kDa fragment found in both wild type and epitope tagged PKD1 knock-in mice. Expression of full length human PC1 (FL PC1) and the resulting P100 and C-Terminal Fragment (CTF) cleavage products in both MDCK and CHO cells significantly reduces the store operated Ca2+ entry (SOCE) resulting from thapsigargin induced store depletion. Exploration into the roles of P100 and CTF in SOCE inhibition reveal that P100, when expressed in Xenopus laevis oocytes, directly inhibits the SOCE currents but CTF does not, nor does P100 when containing the disease causing R4227X mutation. Interestingly, we also found that in PC1 expressing MDCK cells, translocation of the ER Ca2+ sensor protein STIM1 to the cell periphery was significantly altered. In addition, P100 Co-immunoprecipitates with STIM1 but CTF does not. The expression of P100 in CHO cells recapitulates the STIM1 translocation inhibition seen with FL PC1. These data describe a novel polycystin-1 cleavage product, P100, which functions to reduce SOCE via direct inhibition of STIM1 translocation; a function with consequences for ADPKD.


Ca2+ homeostasis plays a vital role in the normal development of tubules in the mammalian nephron [1], [2]. Dysregulation of Ca2+ homeostasis is characteristic in the cyst formation associated with Autosomal Dominant Polycystic Kidney Disease (ADPKD)[3], but how dysregulation leads to cyst production is not well understood. ADPKD results from mutations in the polycystin genes PKD1 and PKD2/TRPP2 and mutations in their respective polycystin proteins, Polycystin 1 (PC1) and Polycystin 2 (PC2), both of which have been implicated as significant regulators of intracellular Ca2+ in renal tubules [4]. PC2 is a member of the transient receptor potential (TRP) family of ion channels [3] and has been demonstrated to be Ca2+ permeant in cilia, plasma, and ER membranes [3], [5], [6]. PC2 is known to regulate ER calcium permeability [7] and modulate IP3R [8] to lower ER Ca2+ stores. PC1's function in Ca2+ homeostasis is far less clear.

Tubular cysts result from a dysfunction in either PC1 or PC2, suggesting a common functional pathway. This idea is supported by evidence that PC1 must bind PC2 in order for PC2 to function as a Ca2+ channel [6]. A PC1, PC2 complex may function as a flow transducer on the primary cilium of epithelial cells [5], wherein flow transduction may be necessary for proper tubule alignment and formation [9]. However a second, less overt relationship may exist between PC1 and PC2, one revolving around a tight regulation of cytosolic and ER Ca2+, where a disruption of any Ca2+ regulator can lead to cyst formation. Normal PC2 expression and the resulting lower ER Ca2+ levels should increase Ca2+ influx and lead to apoptosis and increased cell proliferation [10], but does not. However, mutations or the loss of PC1 results in increased proliferation and apoptosis [2], suggesting that PC1 may be involved in regulating Ca2+ influx. PC1 may also play an important role in regulating cellular Ca2+ responses to stimuli, as PC1 has been reported to alter ATP activated intracellular Ca2+ increases by influencing the rate of Ca2+ reuptake in the ER [11].

ER Ca2+ store depletion is sensed by proteins of the stromal interaction molecule (STIM) family, specifically, STIM1 [12]. STIM1 is found predominantly in the ER membrane, where an EF hand region, located on its C-terminus within the ER lumen, binds ER Ca2+ molecules [12]. When ER stores are depleted, STIM1 re-localizes within the ER membrane to puncta opposite the plasma membrane [12], allowing for STIM1 to physically interact with Orai, a predicted subunit of store operated Ca2+ channels (SOC) [13]. STIM1, therefore, is thought to act as the ER Ca2+ sensor that directly activates the SOC channels to replenish ER Ca2+ levels.

Deciphering the role PC1 plays in Ca2+ homeostasis either at the ER or plasma membranes is further complicated by the cleavage of the PC1 protein and a lack of understanding about PC1 cleavage product localization. The first cleavage occurs constitutively and partially at the juxtamembrane GPS domain, generating a stable N-terminal fragment (NTF), and a C-terminal fragment (CTF) that coexist with uncleaved full-length PC1 [14][16]; the function of both products remains unclear. The second cleavage event previously described for PC1 results in a small C-terminal tail (CTT) fragment [17] that translocates into the nucleus, where it associates with β-catenin to disrupt canonical Wnt signaling [18]. PC1 localization is also controversial. Demonstrating PC1 activity on the cellular and cilia membranes has been the focus of the majority of PC1 work [1][3], however, there exists evidence that PC1 may also occur on the ER membrane [19], [20].

Here we describe a novel PC1 cleavage product, P100. We show that PC1, through its P100 product, inhibits Ca2+ influx at the plasma membrane, and we provide evidence that PC1 interacts with STIM1, preventing its re-localization after store depletion. Our data support the hypothesis that PC1 and P100 regulate store operated calcium entry by interfering with STIM1's ability to activate SOC channels on the plasma membrane.


Analysis of polycystin-1 reveals novel endogenous cleavage product, P100

Using a PC1 C-terminal tail directed antibody (anti-CC-antibody, [16]) (Figure 1A), we detected by Western blot a novel PC1 product of approximately 100 kDa, here termed P100, in the embryo and postnatal mouse, in addition to the previously reported uncleaved full-length (uFL) and C-terminal fragment (CTF) (Figure 1Bi). We found that P100 is also expressed at various developmental stages of postnatal kidneys at levels commensurate to that of CTF: it deceased with the postnatal age and became undetectable at P21 (Figure 1Bii, iii). We detected P100 in the kidney of the Pkd1v/v mice where PC1 cleavage at GPS is disrupted and CTF is thus absent (Figure 1C). We confirmed the authenticity of P100 with the HA-tagged PKD1 knock-in mice (Pkd1HA/HA), which express fully functional PC1 tagged with a 3xHA epitope at the C-terminus [21], and with 5XMyc tagged knock-in mice (Figure S1). We detected P100 in MEF derived from the Pkd1HA/HA mouse by anti-HA after immunoprecipitation or directly in total lysate (Figure 1D). We found that P100 is expressed at different levels in the tissues of the developing mouse and its relative level to CTF also appears to differ among the tissues (Figure 1E).

Figure 1
Biochemical characterization of a novel endogenous polycystin-1 product, P100.

We detected similar PC1 products in a MDCK cell line with inducible Flag-tagged full-length PC1 expression under the control of a tetracycline sensitive promoter (Figure 2A) and in CHO cells (Figure 2C) after transient over-expression of full-length Flag-tagged PC1. This result indicates that P100 is likely generated by proteolytic cleavage at a site that is predicted within the third intracellular loop (Figure 1A) based on the apparent molecular size of P100 and therefore is the portion of PC1 that has sequence similarity to PC2 [22]. The relative amounts of the two cleavage products, CTF and P100 appeared to vary from blot to blot under seemingly similar experimental conditions. We found that 24 hour treatment of MDCK cells with 40nM thapsigargin appeared to reduced the amount of the CTF but not P100 (Figure 2A) whereas 10 µM of ionomycin did not; a result consistent with the hypothesis that ER Ca2+, not general intracellular Ca2+ levels, differentially affects the two cleavage processes.

Figure 2
In vitro biochemical and functional characterization of polycystin-1 cleavage products.

Next we began an investigation into the possible functions of the PC1 cleavage products on Ca2+ homeostasis. It had previously been reported that PC1 inhibited ATP-induced capacitative calcium entry by increasing the rate of Ca2+ uptake to the ER, therefore reducing the stimulus for extracellular Ca2+ entry [11]. We found, however, that after depletion of the ER Ca2+ with thapsigargin in a zero Ca2+ bath, the reintroduction of Ca2+ in the control cells led to an increase in intracellular Ca2+ (Figure 2B) and this increase was significantly larger than in MDCK cells expressing PC1-flag (p<0.001). We confirmed the result in heterogeneous CHO cell populations after transient transfection with full length (FL) PC1-GFP (Figure 2D). Our results suggest that PC1 may also mediate inhibition of the extracellular Ca2+ entry when ER filling is prevented by thapsigargin and raises the possibility that PC1 may modulate SOCE current(s) directly at the cell surface. However, in both MDCK and CHO cells, PC1 was cleaved into CTF and P100. Could the cleavage products themselves be responsible for modulating the SOCE currents?

CTF expression does not inhibit the SOC current

Xenopus laevis oocytes have well characterized Ca2+ activated Cl- currents (CaCC) [23], [24] and both voltage activated Ca2+ channels and store operated Ca2+ currents [24], [25]. We found that Xenopus oocytes, when subjected to a pretreatment with a zero Ca2+ solution containing thapsigargin, displayed large inward currents with complex kinetics (Figure S2). These “check” shaped currents were a combination of a fast transient, Niflumic Acid (NFA) sensitive, Ca2+ activated Cl- current; and a smaller but non deactivating, La3+ sensitive, store operated Ca2+ current (Figure S2). We used these endogenous currents of Xenopus laevis oocytes as an electrophysiological model to examine the role of the PC1 cleavage products in the regulation of SOCE currents. The Xenopus model system combines electrophysiological rigor with a cell type that does not express mammalian PC2, a protein shown to affect PC1 cleavage and expression of PC1 cleavage products [26], allowing a clear picture of any role PC1 cleavage products may have in regulating SOCE. We began with the larger CTF product (Figure 3A). Surprisingly, the expression of CTF in oocytes had no effect on either the transient peak (p<0.49) nor steady state currents (p<0.25) as compared to H2O injected controls (Figure 3B and 3C). To confirm that the lack of SOCE inhibition was not specific to Xenopus oocytes we expressed the CTF construct in CHO cells. In CHO cells first treated with zero Ca2+ ringers and thapsigargin, the reintroduction of extracellular Ca2+ resulted in comparable increases in Ca2+ influx in both the control and CTF expressing cells (Figure S3). These results suggest the CTF is not involved in inhibiting SOC entry. Interestingly, CTF is not further cleaved in Xenopus oocytes or CHO cells into a P100 sized product.

Figure 3
Polycystin-1 product CTF does not inhibit SOCE.

P100 expression inhibits SOC currents

Unlike CTF, the precise cleavage site for P100 is unknown so we created several constructs that start within the third intracellular loop. One of them, starting at V3645, produced a P100-like protein, which co-migrates with the P100 derived from the FL PC1 construct (Figure 2C and E) and can be considered a reasonable approximation of the P100. This construct was used for the subsequent studies of P100 function. In contrast to the larger CTF, P100 when expressed in Xenopus oocytes, had a significant effect on the endogenous currents. In oocytes expressing P100, the check current was dramatically reduced as compared to H20 injected controls (Figure 4A). A comparison of current amplitudes at the transient peak and the steady state revealed P100 expressing cells showed a significant decrease in current amplitude (Figure 4B)(transient peak p<0.01; steady state p<0.01); suggesting both the CaCC current as well as the SOC current are being inhibited.

Figure 4
Polycystin-1 product P100 inhibits SOCE.

We next attempted to discern if P100 expression was affecting the SOCE only (secondarily affecting the CaCC), or affecting both the SOCE and the CaCC directly. Xenopus oocytes have well described voltage activated Ca2+ channels [23] which are responsible for the large outward CaCC currents seen when the cell is depolarized. The voltage gated Ca2+ channels were not activated during the negative pulse used to elicit the “check” currents, but were activated by positive pre-pulses, thereby providing a secondary source of Ca2+ for CaCC activation. Three, two second, +60 mV pre-pulses were delivered repeatedly to cells expressing P100, causing the induction of a check current (Figure 4C) significantly larger than the P100 suppressed current in the same oocytes prior to pre-pulse delivery. Interestingly, the induced current in the P100 oocytes was indistinguishable from the NFA sensitive Cl- current calculated in Figure S2. If compared to currents from H2O injected controls, the transient peak appeared similar, but the induced current dissipated, where as the control reached a steady state. An examination of the current amplitudes during the transient peak revealed the induced current was no different than the control peak (P<0.823)(Figure 4D). In contrast, the current amplitudes at the steady state revealed no induction or increase (p<0.15), but all three were significantly smaller than the control steady state current (p<0.001). These results strongly suggest that the CaCC currents are not being directly affected by the expression of P100, but are being inhibited indirectly, via an inhibition of the SOC current that is necessary for their activation at −120 mV.

To gain insight into whether the SOC current inhibitory effect of P100 may have physiological relevance, we used the mutant P100 expression construct bearing the disease-causing R4227X mutation and tested for the effect of the mutation on SOC current inhibition. The resulting mutant protein, P100 R4227X, lacks the C-terminal 76 amino acids containing the coiled-coil domain required for interacting with PC2 [6]. Expression of P100 R4227X in Xenopus oocytes did not significantly reduce the transient peak (p<0.50) or steady state currents (p<0.44)(Figure 4E and F). The importance of the missing tail region from the P100 R4227X mutant was confirmed by expression of an artificial PC1 product, AESW, containing only the final transmembrane domain and the C-terminal tail in Xenopus oocytes. AESW expressing oocytes displayed an inhibited transient peak (p<0.01) and steady state amplitudes (p<0.01) as compared to controls. Similarly, AESW transient over expression inhibited extracellular Ca2+ entry in thapsigargin treated CHO cells (Figure S3). These results indicate that the C-terminal sequence is required for the SOC inhibition and suggests that this activity of P100 plays a critical role for the physiological function of PC1.

PC1 interferes with STIM1 puncta formation after ER Ca2+ depletion

We hypothesized that PC1, through the actions of its P100 product, may exert its inhibitory effect on SOCE by interfering with STIM1 in the ER, retarding STIM1's ability to transduce a Ca2+ depletion signal to the SOCE channels of the plasma membrane. Functionally, we sought to address this by measuring the amount of STIM1 translocation to the periphery with or without the expression of PC1. We chose to use a MDCK cell line stably expressing mouse PC1, which we compared to empty vector control cells. The MDCK (with or without mPC1) cells were transfected with a YFP-STIM1 construct and photographed in high Ca2+ ringers (5 mM) after 15 minutes exposure to 4 µM thapsigargin (Figure 5A). Similar to a methodology used by Luik et al (2008)[27] the YFP signal of the periphery was compared to the total signal to create a FP/FTotal ratio for the STIM1 fluorescence for before and after exposure to thapsigargin. In cells expressing mPC1, thapsigargin elicited no significant change in the STIM1 fluorescence ratio (p<0.298), suggesting that STIM1 did not translocate after ER store depletion. In the control cells with no mPC1 expression, thapsigargin induced a significant change in the STIM1 ratio (p<0.001). Interestingly, the expression of PC1 also limited the overall STIM1 fluorescence in the high Ca2+ ringer (p<0.001) in addition to the translocation of STIM1.

Figure 5
PC1 inhibits STIM1 translocation after ER Ca2+ depletion.

P100 physically interacts with STIM1

We over expressed STIM1 and P100 in CHO cells and found that P100 and STIM1 could be co-precipitated using an anti-STIM1 antibody, and visualized with the anti-PC1 CT antibody (Figure 6A). Consistent with the lack of SOCE inhibition, CTF was not pulled down with the anti-STIM1 antibody (Figure 6A). CTF and P100 expression was confirmed by immunoprecipitating the same lysate with Flag congregated beads then probing with the anti-PC1 CT antibody (Figure 6A). STIM1 expression was also verified under each condition (Figure 6B). The STIM1/P100 interaction was confirmed by reciprocal co-immunoprecipitation using flag-conjugated beads and visualized with the anti-STIM1 antibody (Figure 6C). The possible functional interaction of P100 and STIM1 was assessed like full length PC1 above. CHO cells were transfected with YFP-STIM1 and either an empty plasmid or P100 and photographed in 5mM Ca2+ ringers and again 10 minutes after exposure to 8 µM thapsigargin (Figure 6E). In CHO cells expressing YFP-Stim1 alone, ten minutes of thapsigargin treatment altered the STIM1 localization from a diffuse ER pattern to dramatic puncta around the periphery of the cell. However, the co-expression of YFP-Stim1 and P100 presents a different localization pattern, with very little of the puncta signal or YFP signal just beneath the plasma membrane. The inhibition of STIM1 re-localization in the presence of the P100 is not total, but does suggest that PC1 regulates Ca2+ entry through the generation of P100.

Figure 6
P100 physically interacts with STIM1.


In this study, we have discovered a previously unrecognized endogenously expressed PC1 product of ~ 100 kDa, P100, in various tissues including the kidney. Importantly, we also detected P100 in cells expressing recombinant PC1 with a full-length PKD1 cDNA expression construct. Together, these data indicate that P100 is most likely derived from proteolytic cleavage within the third intracellular loop and is expected to contain the final 6 transmembrane domains and the C-terminal tail, a segment of PC1 with significant sequence similarity to PC2. Interestingly, P100 is not produced in Xenopus oocytes or in CHO cells expressing only the CTF product, thus P100 cleavage may occur uniquely in the context of full-length PC1. One possible explanation for the differential cleavage of full length PC1 and CTF is that they are distributed in different subcellular locations with differing proteases. P100 is also present in Pkd1V/V kidneys, indicating that P100 cleavage does not require GPS cleavage. Therefore, the full-length PC1 can act as a reservoir for generating CTF/NTF and P100 in vivo. PKD1V/V mice have severely cystic kidneys at postnatal stages, but have no embryonic lethality in contrast to PKD1 knock-out mice [16]. The generation of P100 in Pkd1V/V mice raises the possibility that P100 may help prevent various abnormalities during embryonic development such as cystic expansion of the kidney and pancreas observed in PKD1 knockouts, and therefore may have an important function during embryonic development.

Differential cleavage of full length PC1 and CTF could also be due to specific localization of a regulatory protein. Bertuccio et al (2009)[26] found that cleavage of PC1 into the CTT PC1 product is directly dependent on the expression of PC2. We also looked into the possible role of PC2 on P100 creation and found over expression of PC2 increased the amount of PC1 cleavage products, generally, but not any one specifically (Figure 2C). We also found, unlike Bertuccio et al (2009)[26], that ER Ca2+ levels had a small effect on the amount of PC1 cleavage, again generally, with no change in the CTF to P100 ratio. This could mean that ER Ca2+ levels or PC2 expression may not affect directly the P100 cleavage event, but more likely affect generally the stability of the PC1 products. The nature of the PC1 cleavage responsible for generating P100 is currently unknown.

We have also found that PC1 expression, and specifically P100, leads to an inhibition SOCE, an occurrence hereto unreported. PC1 mediated inhibition of SOCE could lower ER Ca2+ levels and shorten/reduce cytosolic Ca2+ transients [28], conditions known to increase resistance to apoptosis and proliferation [10]. Previously, SOCE inhibition has been directly linked to regulation of apoptosis and proliferation via multiple pathways [29][31]. In addition, many physiological ligands (e.g. ATP) act through the PLC/IP3 pathway to increase the release of Ca2+ form ER stores and raise cytosolic Ca2+. PC1, therefore, may attenuate the extent of net intracellular Ca2+ increases upon exposure to physiological stimuli. Li et al (2009)[20] showed that an ER localized PC1 fragment, QIF38 (identical to our P100), directly associates with IP3R to inhibit Ca2+ release from ER stores upon IP3 stimulation, an action that results in attenuated responses to exogenous ATP application in MDCK cells [20]. These findings taken with our own form a consistent picture of ER localized PC1 products acting to limit transient Ca2+ responses to physiological stimuli. Interestingly, a number of studies using the C-terminal tail of PC1 over expressed as a fusion protein have found the inverse; the expression of C-terminal tail leads to increases in intracellular Ca2+ and SOCE [32], [33]. However, in light of recent findings by Basavanna et al (2007)[34] who showed that the over expression of a PC1 C-terminus fusion protein acted as a dominant negative, these seemingly contrary findings may in fact be supportive of our hypothesis that PC1 expression leads to inhibition of the SOCE.

Can PC1's regulation of SOCE play a role in ADPKD? We found that a disease causing mutation in PC1, R4227X, does not inhibit SOC currents when expressed in Xenopus oocytes. These results suggest dysfunctional SOCE regulation (Figure 7) may disrupt normal Ca2+ homeostasis and therefore play a significant role in ADPKD. The same R4227X mutation also disrupts PC1/PC2 interactions [6] suggesting a role for PC2 in SOCE regulation.

Figure 7
Model of P100 STIM1 interaction in the ER.

Finally, we have demonstrated that expression of PC1 and P100 interferes with STIM1 translocation upon ER Ca2+ depletion. Normally, STIM1 in the absence of ER Ca2+ oligomerizes [35], [36] then secondarily translocates to form puncta at the ER-PM junction [35], [37], [38]. Oligomerization is dependent on the interactions of the EF-SAM regions located in the ER lumen portion of STIM1 [36], but translocation and puncta formation are dependent on the cytosolic polybasic [37], [38] and coil-coiled domains [35], [39]. Therefore, considering the C-terminal coil-coiled domain of P100, it seems most likely P100 interferes with the corresponding cytosolic domains of STIM1 which would predominately alter STIM1 translocation and puncta formation at the ER-PM junction (Figure 7). Further work on the involvement of the STIM1 coil-coiled domains in oligomerization would be necessary to confirm this prediction. Previously, the only reported physiological instances of either SOCE, CRAC, or specifically STIM1 suppression was during cell division, regulated by the phosphorylation of STIM1 [40]. Our data support an additional avenue of SOCE regulation, independent of cell division, a direct inhibition of STIM1 translocation by another protein, PC1. Although STIM1 has been shown to interact with a number of proteins (Orai and TRP channels), the PC1 interactions described here are among the first to describe a protein interaction that inhibits STIM1 function.


Detailed methods can be found in the Supporting Information section (Methods S1).


Whole cell voltage clamp recordings from the Xenopus oocytes were performed at room temperature in standard ND-96 ringers solution (in mM: 96 NaCl, 2 KCl, 1 MgCl2, 1.8 CaCl2, 5 hepes, pH 7.5). To increase the conductance of endogenous SOC currents, oocytes were pretreated with 4 µM thapsigargin (Sigma-Aldrich, USA) for up to 2 hours in the zero Ca2+ bath solution; generally, recordings were begun 3 minutes after the Ca2+ containing ND-96 bath solution was re-introduced to the oocytes. A holding potential of −40 mV was used on all oocytes.

Mammalian Cells and culturing conditions

Stably transfected Madin-Darby canine kidney (MDCK) cells were a generous gift from Gregory G. Germino (NIDDK, Bethesda, MD USA) and cultured with selection agents hygromycin (100 µg/ml) and blasticidin (5 µg/ml).

Plasmids and constructs

The human P100, the P100 R4227X, and the human PC1 fragment AESW constructs were also described previously under the names QIF38, R4227X, and AESW respectively [20]. The human STIM1 constructs, A151 and YFP-STIM1 were a generous gift from Guang Huang and Paul Worley (Johns Hopkins School of Medicine, Department of Neuroscience, Baltimore, MD USA).

Fura 2 Ca2+ imaging and STIM1 images

CHO cells were rinsed with non-supplemented media then loaded with fura 2 (Invitrogen, USA). The cover slips were then bathed in a zero Ca2+ solution (in mM: 120 NaCl, 4.5 KCl, 1 EGTA, 2 MgCl2, 10 hepes, pH 7.4). Images were acquired once every 5 seconds using IPLab Software (BD Biosciences, USA). Thapsigargin (Sigma, USA, 4 µM) was used to deplete ER stores and high Ca2+ ringers (in mM: 120 NaCl, 4.5 KCl, 2 MgCl2, 10 hepes, and 3–5 CaCl2, pH 7.4) was secondarily applied to observe the store depletion activated Ca2+ entry. For STIM1 translocation assays, CHO cells expressing either YFP-STIM1 alone or with the CTF-100 construct began in high Ca2+ ringer then the bath was replaced with the zero Ca2+ ringer and 8 µM thapsigargin. For live images of STIM1 translocation in MDCK cells, MDCK cells stably transfected with either murine PC1 or the blank vector in addition to the YFP-STIM1 construct. 4 µM thapsigargin was used for store depletion. STIM1 translocation analysis was done as described by Luik et al (2008)[27]. All reported means are ± standard error of the mean (SEM).

Supporting Information

Methods S1

Detailed methods.

(0.03 MB DOC)

Figure S1

Biochemical characterization of PC-1 product, P100 in Myc-tagged knock in mouse model. (A) PKD1 alleles and schematic diagram of their corresponding polycystin-1 proteins. PKD1Myc and PKD1ΔCMyc are 5xMyc-tagged Pkd1 knock-in alleles that produce fully functional PC1 protein. The domains in polycystin-1 are shown. The Pkd1ΔCmyc allele produces 5xMyc-tagged truncated polycystin-1 protein with deletion of C-terminal 257 amino acids [21]. (B) Western blot for heterozygous Pkd1myc/+ and Pkd1ΔCmyc/+ and their wild-type littermate embryo (E17) using anti-Myc antibody after immunoprecipitation. The truncated CTFΔCmyc/+ and P100ΔCmyc/+ are detected in the Pkd1ΔCmyc/+ embryo.

(1.73 MB EPS)

Figure S2

SOC and CaCC currents in Xenopus laevis oocytes. (A) Currents elicited from a representative H2O injected control Xenopus laevis oocytes 3–5 days after injection in a ND96 bath solution subjected to a +20mV step protocol from −100 mV to +60 mV from an initial holding potential of −40 mV. (B) Currents elicited from a representative H2O injected control oocyte pretreated with 4 µM thapsigargin in a zero Ca2+ ND96. (C) Summary steady state current/voltage relation from H2O injected control oocytes with (blue circles, n = 21) or without (red triangles, n = 13) thapsigargin/zero Ca2+ ND96 pretreatment. ±SEM; (**p<0.01). (D) Averaged currents in H2O inject control oocytes elicited by a 10 second voltage step to −120 mV from a −40 mV holding potential. For each cell (n = 4) currents were first recorded in zero Ca2+ ND96 (blue trace), then in the normal ND96 (1.8 mM Ca2+)(black trace) and finally in ND96 with 100 µM La3+ (red trace). Inset: mean current amplitudes at the transient peak (1.5 sec from beginning of record) and at the steady state (10 sec from beginning of record). ±SEM; (**p<0.01)(*p<0.05). (E) Averaged currents in H2O inject control oocytes elicited by a 10 second voltage step to −120 mV from a −40 mV holding potential. For each cell (n = 10) currents were recorded before (black trace) and after (red trace) replacing the bath with a low Cl- bath containing 100 µM Niflumic acid (NFA). Currents were recorded from a subset of cells (n = 4) further treated with 100 µM La3+ (blue trace). Subtraction of currents before and after treatment with NFA indicates the waveform of the NFA sensitive, probable Cl- currents (black dotted black trace). Inset: mean current amplitudes at the transient peak and steady state. ±SEM; (**p<0.01)(*p<0.05). (F) Measurements of transient peak current reversal potentials. Current/voltage relation of tail current amplitudes after initial −120 mV step in normal ND96 bath (black squares, n = 9), low Cl-/100 µM NFA bath (red circles, n = 9), or low Cl-/100 µM NFA/100 µM La3+ bath (blue triangles, n = 4). Inset: representative tail current measurements using reversal potential paradigm.

(3.58 MB EPS)

Figure S3

Expression of Polycystin-1 cleavage products have differing effects on store operated Ca2+ influx. Fura 2- AM measurements in CHO cells expressing PC1 cleavage products. Recordings began after cells reached steady state in a zero Ca2+, 4 µM thapsigargin ringers. The bath was then replaced with a high Ca2+ bath and Ca2+ influx through SOC channels is measured. (A) CHO cells transiently transfected with CTF (Red trace, n = 4 coverslips, 36 cells) or empty plasmid control (Black trace, n = 7 coverslips, 58 cells). (B) CHO cells transiently transfected with AESW (Red trace, n = 6 coverslips, 24 cells) or empty plasmid control (Black trace, n = 7 coverslips, 34 cells). ±SEM; (*p<0.05).

(0.82 MB EPS)


We wish to thank Tatia Chay Woodward and the anonymous reviewers for their critical reading of the manuscript.


Competing Interests: The authors have declared that no competing interests exist.

Funding: This work was supported by the National Institute of Diabetes and Digestive and Kidney Diseases (NIDDK) grants DK032753-25A1 (to W.B.G.) and DK062199 (to F.Q.). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Wilson PD. Polycystic kidney disease. N Engl J Med. 2004;350:151–164. [PubMed]
2. Sutters M, Germino GG. Autosomal dominant polycystic kidney disease: molecular genetics and pathophysiology. J Lab Clin Med. 2003;141:91–101. [PubMed]
3. Kottgen M. TRPP2 and autosomal dominant polycystic kidney disease. Biochim Biophys Acta. 2007;1772:836–850. [PubMed]
4. Somlo S, Ehrlich B. Human disease: calcium signaling in polycystic kidney disease. Curr Biol. 2001;11:R356–R360. [PubMed]
5. Nauli SM, Alenghat FJ, Luo Y, Williams E, Vassilev P, et al. Polycystins 1 and 2 mediate mechanosensation in the primary cilium of kidney cells. Nat Genet. 2003;33:129–137. [PubMed]
6. Hanaoka K, Qian F, Boletta A, Bhunia AK, Piontek K, et al. Co-assembly of polycystin-1 and -2 produces unique cation-permeable currents. Nature. 2000;408:990–994. [PubMed]
7. Wegierski T, Steffl D, Kopp C, Tauber R, Buchholz B, et al. TRPP2 channels regulate apoptosis through the Ca2+ concentration in the endoplasmic reticulum. EMBO J. 2009;28:490–499. [PubMed]
8. Li Y, Wright JM, Qian F, Germino GG, Guggino WB. Polycystin 2 interacts with type I inositol 1,4,5-trisphosphate receptor to modulate intracellular Ca2+ signaling. J Biol Chem. 2005;280:41298–41306. [PubMed]
9. Simons M, Walz G. Polycystic kidney disease: cell division without a c(l)ue? Kidney Int. 2006;70:854–864. [PubMed]
10. Orrenius S, Zhivotovsky B, Nicotera P. Regulation of cell death: the calcium-apoptosis link. Nat Rev Mol Cell Biol. 2003;4:552–565. [PubMed]
11. Hooper KM, Boletta A, Germino GG, Hu Q, Ziegelstein RC, et al. Expression of polycystin-1 enhances endoplasmic reticulum calcium uptake and decreases capacitative calcium entry in ATP-stimulated MDCK cells. Am J Physiol Renal Physiol. 2005;289:F521–F530. [PubMed]
12. Hogan PG, Rao A. Dissecting ICRAC, a store-operated calcium current. Trends Biochem Sci. 2007;32:235–245. [PubMed]
13. Prakriya M, Feske S, Gwack Y, Srikanth S, Rao A, et al. Orai1 is an essential pore subunit of the CRAC channel. Nature. 2006;443:230–233. [PubMed]
14. Wei W, Hackmann K, Xu H, Germino G, Qian F. Characterization of cis-autoproteolysis of polycystin-1, the product of human polycystic kidney disease 1 gene. J Biol Chem. 2007;282:21729–21737. [PubMed]
15. Qian F, Boletta A, Bhunia AK, Xu H, Liu L, et al. Cleavage of polycystin-1 requires the receptor for egg jelly domain and is disrupted by human autosomal-dominant polycystic kidney disease 1-associated mutations. Proc Natl Acad Sci U S A. 2002;99:16981–16986. [PubMed]
16. Yu S, Hackmann K, Gao J, He X, Piontek K, et al. Essential role of cleavage of Polycystin-1 at G protein-coupled receptor proteolytic site for kidney tubular structure. Proc Natl Acad Sci U S A. 2007;104:18688–18693. [PubMed]
17. Chauvet V, Tian X, Husson H, Grimm DH, Wang T, et al. Mechanical stimuli induce cleavage and nuclear translocation of the polycystin-1 C terminus. J Clin Invest. 2004;114:1433–1443. [PMC free article] [PubMed]
18. Lal M, Song X, Pluznick JL, Di G, V, Merrick DM, et al. Polycystin-1 C-terminal tail associates with beta-catenin and inhibits canonical Wnt signaling. Hum Mol Genet. 2008;17:3105–3117. [PMC free article] [PubMed]
19. Grimm DH, Cai Y, Chauvet V, Rajendran V, Zeltner R, et al. Polycystin-1 distribution is modulated by polycystin-2 expression in mammalian cells. J Biol Chem. 2003;278:36786–36793. [PubMed]
20. Li Y, Santoso NG, Yu S, Woodward OM, Qian F, et al. Polycystin-1 interacts with inositol 1,4,5-trisphosphate receptor to modulate intracellular Ca2+ signaling with implications for polycystic kidney disease. J Biol Chem. 2009;284:36431–36441. [PMC free article] [PubMed]
21. Wodarczyk C, Rowe I, Chiaravalli M, Pema M, Qian F, et al. A novel mouse model reveals that polycystin-1 deficiency in ependyma and choroid plexus results in dysfunctional cilia and hydrocephalus. PLoS One. 2009;4:e7137. [PMC free article] [PubMed]
22. Mochizuki T, Wu G, Hayashi T, Xenophontos SL, Veldhuisen B, et al. PKD2, a gene for polycystic kidney disease that encodes an integral membrane protein. Science. 1996;272:1339–1342. [PubMed]
23. Barish ME. A transient calcium-dependent chloride current in the immature Xenopus oocyte. J Physiol. 1983;342:309–325. [PubMed]
24. Hartzell HC. Activation of different Cl currents in Xenopus oocytes by Ca liberated from stores and by capacitative Ca influx. J Gen Physiol. 1996;108:157–175. [PMC free article] [PubMed]
25. Yao Y, Tsien RY. Calcium current activated by depletion of calcium stores in Xenopus oocytes. J Gen Physiol. 1997;109:703–715. [PMC free article] [PubMed]
26. Bertuccio CA, Chapin HC, Cai Y, Mistry K, Chauvet V, et al. Polycystin-1 C-terminal cleavage is modulated by polycystin-2 expression. J Biol Chem. 2009;284:21011–21026. [PMC free article] [PubMed]
27. Luik RM, Wang B, Prakriya M, Wu MM, Lewis RS. Oligomerization of STIM1 couples ER calcium depletion to CRAC channel activation. Nature. 2008;454:538–542. [PMC free article] [PubMed]
28. Chiu WT, Tang MJ, Jao HC, Shen MR. Soft substrate up-regulates the interaction of STIM1 with store-operated Ca2+ channels that lead to normal epithelial cell apoptosis. Mol Biol Cell. 2008;19:2220–2230. [PMC free article] [PubMed]
29. Li N, Zheng L, Lin P, Danielpour D, Pan Z, et al. Overexpression of Bax induces down-regulation of store-operated calcium entry in prostate cancer cells. J Cell Physiol. 2008;216:172–179. [PubMed]
30. Vanden AF, Skryma R, Shuba Y, Van CF, Slomianny C, et al. Bcl-2-dependent modulation of Ca(2+) homeostasis and store-operated channels in prostate cancer cells. Cancer Cell. 2002;1:169–179. [PubMed]
31. Vanoverberghe K, Vanden AF, Mariot P, Lepage G, Roudbaraki M, et al. Ca2+ homeostasis and apoptotic resistance of neuroendocrine-differentiated prostate cancer cells. Cell Death Differ. 2004;11:321–330. [PubMed]
32. Wildman SS, Hooper KM, Turner CM, Sham JS, Lakatta EG, et al. The isolated polycystin-1 cytoplasmic COOH terminus prolongs ATP-stimulated Cl- conductance through increased Ca2+ entry. Am J Physiol Renal Physiol. 2003;285:F1168–F1178. [PubMed]
33. Manzati E, Aguiari G, Banzi M, Manzati M, Selvatici R, et al. The cytoplasmic C-terminus of polycystin-1 increases cell proliferation in kidney epithelial cells through serum-activated and Ca(2+)-dependent pathway(s). Exp Cell Res. 2005;304:391–406. [PubMed]
34. Basavanna U, Weber KM, Hu Q, Ziegelstein RC, Germino GG, et al. The isolated polycystin-1 COOH-terminal can activate or block polycystin-1 signaling. Biochem Biophys Res Commun. 2007;359:367–372. [PMC free article] [PubMed]
35. Liou J, Fivaz M, Inoue T, Meyer T. Live-cell imaging reveals sequential oligomerization and local plasma membrane targeting of stromal interaction molecule 1 after Ca2+ store depletion. Proc Natl Acad Sci U S A. 2007;104:9301–9306. [PubMed]
36. Stathopulos PB, Zheng L, Li GY, Plevin MJ, Ikura M. Structural and mechanistic insights into STIM1-mediated initiation of store-operated calcium entry. Cell. 2008;135:110–122. [PubMed]
37. Park CY, Hoover PJ, Mullins FM, Bachhawat P, Covington ED, et al. STIM1 clusters and activates CRAC channels via direct binding of a cytosolic domain to Orai1. Cell. 2009;136:876–890. [PMC free article] [PubMed]
38. Baba Y, Hayashi K, Fujii Y, Mizushima A, Watarai H, et al. Coupling of STIM1 to store-operated Ca2+ entry through its constitutive and inducible movement in the endoplasmic reticulum. Proc Natl Acad Sci U S A. 2006;103:16704–16709. [PubMed]
39. Li Z, Lu J, Xu P, Xie X, Chen L, et al. Mapping the interacting domains of STIM1 and Orai1 in Ca2+ release-activated Ca2+ channel activation. J Biol Chem. 2007;282:29448–29456. [PubMed]
40. Smyth JT, Petranka JG, Boyles RR, DeHaven WI, Fukushima M, et al. Phosphorylation of STIM1 underlies suppression of store-operated calcium entry during mitosis. Nat Cell Biol. 2009;11:1465–1472. [PubMed]

Articles from PLoS ONE are provided here courtesy of Public Library of Science