N. Montalbetti and Q. Li contributed equally to this work.
Corresponding author H. F. Cantiello: Renal Unit, Massachusetts General Hospital East, Building 149, 13th Street, Charlestown, MA 02129, USA. Email: email@example.com
Polycystin-2 (PC2), encoded by PKD2, which is one of the genes whose mutations cause polycystic kidney disease, is abundantly produced in the apical domain of the syncytiotrophoblast (hST) of term human placenta. PC2, a TRP-type (TRPP2) non-selective cation channel, is present in primary cilia of renal epithelial cells, a microtubule-based ancillary structure with sensory function. The hST has abundant cytoskeletal structures, and actin filament dynamics regulate PC2 channel function in this epithelium. However, it is expected that the apical hST excludes microtubular structures. Here, we demonstrated by Western blot and immunocytochemical analyses that hST apical vesicles indeed contain microtubule structural components, including tubulin isoforms, acetylated α-tubulin, and the kinesin motor proteins KIF3A and KIF3B. PC2 and tubulin were substantially colocalized in hST vesicles. Treatment of hST vesicles with either the microtubular disrupter colchicine (15 μm) or the microtubular stabilizer paclitaxel (taxol, 15 μm) resulted in distinct patterns of microtubular re-organization and PC2 redistribution. We also observed that changes in microtubular dynamics regulate PC2 channel function. Addition of colchicine rapidly inhibited PC2 channel activity in lipid-bilayer reconstituted hST membranes. Addition of either tubulin and GTP, or taxol, however, stimulated PC2 channel activity in control hST membranes. Interestingly, we found that the kinesin motor protein KIF3A was capable of increasing PC2 channel activity in hST. We believe that the data are the first to provide a direct demonstration of a microtubular interaction with PC2 in the hST. This interaction thus plays an important regulatory role in the control of ion transport in the human placenta.
Microtubules are long cylindrical polymers composed of hetero-dimeric units of α and β tubulins. Microtubules are implicated in vesicular trafficking, the regulation of cell cycle, cell motility and morphology. Microtubular organization is essential for the assembly and organization of mitotic spindles, centriole and organelles emerging from such structures, including cilia and flagella. Previous evidence has suggested a complementary regulatory role of microtubules and actin filaments in channel function. Johnson and Byerly originally determined that cytoskeletal modifying agents alter Ca2+ channel activity in Lymnaea (Johnson & Byerly, 1993) and rat hippocampal pyramidal neurons (Johnson & Byerly, 1994). In those studies it was concluded that drugs which stabilize (taxol and phalloidin) and destabilize (colchicine and cytochalasin B) the actin and microtubular cytoskeletons altered the development of and recovery from Ca2+-dependent inactivation of Ca2+ currents. More recent studies have shown a direct interaction between TRP channels, such as the vanilloid receptor (TRPV1), and β-tubulin, which is one of the key elements in microtubular formation (Goswami et al. 2004).
A microtubular connection to PC2 function in hST is, heretofore, unknown. However, recent evidence suggests potential links between PC2 and microtubular structures. Various forms of cystic kidney disease not directly linked to mutations in the PKD2 gene have been associated with microtubular-associated ciliary proteins (Morgan et al. 1998; Murcia et al. 2000; Pazour et al. 2002; Yoder et al. 2002b; Hou et al. 2002). For example, the cpk gene, whose mutations cause renal cystic disease, encodes cystin (Hou et al. 2002), a novel protein which is expressed and colocalizes with polaris in primary cilia of renal epithelial cells. Treatment of homozygous cpk/cpk mice with taxol (Woo et al. 1997) dramatically moderated progression of the disease. The Tg737 gene mutated in the orpk PKD mice encodes another ciliary protein, polaris, which localizes to the ciliary basal body and the microtubular axoneme (Yoder et al. 2002b). orpk mice display shortened cilia, left-right symmetry defects (Murcia et al. 2000), and increased ciliary PC2 expression (Pazour et al. 2002). A closer microtubular connection to PC2 was provided by Rundle et al. (2004) who found that mDial/Drf1 interacts with PC2 in a cell-cycle-dependent manner. mDia1/Drf1 is a member of the RhoA GTPase-binding formin homology protein families, which participate in cytoskeletal organization, cytokinesis and signal transduction. Interestingly, PC2 is functional in primary cilia of renal epithelial cells (Raychowdhury et al. 2005). More recently, we determined that microtubular dynamics indeed regulate PC2 channel function in primary cilia. We observed that acute addition of the microtubular disrupter colchicine rapidly abolished, while addition of the microtubular stabilizer paclitaxel increased, ciliary PC2 channel activity in isolated ciliary membranes from LLC-PK1 epithelial cells reconstituted in a lipid bilayer system (Li et al. 2006). We further observed that PC2 colocalizes, structurally associates, and functionally interacts with the microtubule-dependent motor kinesin-2 subunit KIF3A, a protein involved in anterograde cargo transport in cilia and flagella (Marszalek et al. 1999; Takeda et al. 1999; Lin et al. 2003). Thus, microtubular organization regulates PC2 function in microtubular-containing organelles.
Therefore, herein, we explored whether microtubules are present in hST apical membranes, and further hypothesized that colocalization of PC2 with microtubules may be potentially important in regulating PC2 function in the human placenta. We determined that the apical domain of hST contains various tubulin isoforms, structured microtubules, and kinesin motor protein subunits. We further determined that PC2 colocalizes with microtubules in this preparation, and observed that microtubular formation activates, while disruption of microtubules inhibits, PC2 channel activity in hST. Interestingly, the kinesin-2 motor subunits KIF3A and KIF3B were also found in hST vesicles, and addition of exogenous KIF3A activated the PC2 channel in this membrane preparation. Thus, a microtubule–PC2 interaction acts as a novel regulatory mechanism of hST PC2 channel function.
Human placenta membrane preparation
Human placenta syncytiotrophoblast (hST) apical membrane vesicles were obtained as previously reported (González-Perrett et al. 2001; Montalbetti et al. 2005b). Term human placentas were obtained within 20 min of normal vaginal delivery under strict institutional guidelines, and immediately processed (González-Perrett et al. 2001). The placentas were obtained from the Instituto Médico de Obstetricia SA, TTE General J. D. Perón 2247, Buenos Aires, Argentina, C1040AAI. Briefly, villous tissue was fragmented, washed with non-buffered NaCl saline (150 mm), and minced into small pieces. The fragmented tissue was stirred for 1 h in 1.5 vols of a solution containing 10 mm Hepes, adjusted to pH 7.4 with KOH, and also containing 0.1 mm EGTA, a protease inhibitor cocktail (González-Perrett et al. 2001), and 250 mm sucrose. The tissue preparation was filtered and centrifuged for 10 min at 1000 g. The supernatant was again centrifuged for 10 min at 14 500 g and for 90 min at 23 400 g. The final pellet was resuspended in a buffer solution containing 10 mm Hepes-KOH, pH 7.4, 250 mm sucrose, and 20 mm KCl. The hST apical membrane preparation was aliquoted and stored at –20°C until the time of the experiment. At least six different hST membrane preparations (i.e. individual donors) were used for the electrophysiological studies in this report.
Immunochemistry and reagents
Specific PC2 labelling in hST apical membranes was conducted with anti-PC2 mouse monoclonal (1A11) and goat polyclonal G-20 antibodies, as reported (Li et al. 2005). Other primary antibodies included rabbit anti-KIF3A polyclonal and mouse antiacetylated α-tubulin monoclonal (Sigma-Aldrich, Oakville, ON, Canada) antibodies. Secondary antibodies used for immunofluorescence included goat antimouse IgG fluorescein isothiocyanate and goat antirabbit IgG-rhodamine (Chemicon International, Temecula, CA, USA). Goat antimouse and -rabbit IgG-horseradish peroxidase (HRP; Chemicon International), were used for Western blot analysis (WB). Tubulin (Cytoskeleton, Denver, CO, USA) was prepared in buffer containing (mm): 2.0 Tris-HCl, 0.5 ATP, 0.2 CaCl2 and 0.5 β-mercaptoethanol, pH 8.0. At the time of the experiment, GTP (0.5 mm) was added to the solution from a stock solution (100 mm). Colchicine (Sigma-Aldrich) was dissolved in water and used at concentrations ranging from 1 to 15 μm in ‘trans’ buffer solution (see below). Paclitaxel (taxol, 1 mg ml−1; Sigma-Aldrich) was used at a 15 μm final concentration. The hST vesicles were placed in Eppendorf tubes (1.5 ml total volume), diluted in 10% mouse and/or rabbit sera in PBS, and incubated for 30 min to prevent non-specific binding of antibodies. A PBS buffer containing 2% BSA was used for antibody dilution and washing. Vesicles were treated with primary antibodies for 1 h, rinsed (×3) by centrifugation, and incubated with the secondary antibody for 45 min. This procedure was followed by another wash (×3) with PBS. Pelleted vesicles were transferred to glass slides, mounted with Vectashield mounting medium (Vector Laboratories, Burlingame, CA, USA), and visualized with a Zeiss 510 confocal laser scanning microscopy with argon 488 nm and helium–neon 543 nm lasers (Zeiss, Weesp, the Netherlands). Composite images were created using Adobe Photoshop 5.5.
KIF3A constructs and protein preparation
PolyHis-tagged KIF3A C terminus (aa 403–702) was purified from Escherichia coli cultures, and the full-length KIF3A (aa 1–702) was obtained from MDCK cells, as described (Li et al. 2006).
The hST apical membranes were subjected to 8% SDS-PAGE electrophoresis and transferred to a nitrocellulose membrane (Amersham, Baie d'Urfe, Canada). The membrane was then blocked with 3% skim milk powder in PBS supplemented with 0.1% Tween-20, which was incubated with the primary antibody and an HRP-coupled secondary antibody, and visualized with enhanced chemiluminescence (Amersham).
Ion channel reconstitution
hST vesicles were used in the lipid bilayer reconstitution experiments, as previously reported (González-Perrett et al. 2001). Briefly, lipid bilayers were formed with a mixture of synthetic phospholipids (Avanti Polar Lipids, Birmingham, AL, USA) in n-decane (Sigma-Aldrich). The lipid mixture contained 1-palmitoyl-2-oleoyl phosphatidylcholine and phosphatidyl-ethanolamine in a 7:3 ratio. The lipid solution (∼20–25 mg ml−1) in n-decane was spread in the aperture of a polystyrene cuvette (CP13-150) of a bilayer chamber (model BCH-13; Warner Instruments, Hamden, CT, USA). Both sides of the lipid bilayer were bathed with a solution containing 10 mm MOPS-KOH, and 10 mm MES-KOH, pH 7.40, and 10–15 μm Ca2+. The final K+ concentration in the solution was approximately 15 mm. KCl was further added to the cis compartment, to reach a final concentration of 150 K+.
Data acquisition and analysis
Electrical signals were obtained with a PC501A patch-clamp amplifier (Warner Instruments) with a 10 GΩ feedback resistor. Output (voltage) signals were low-pass filtered at 700 Hz (−3 dB) with an eight-pole Bessel-type filter (Frequency Devices, Haverhill, MA, USA). Single-channel current tracings were further filtered for display purposes only. Unless otherwise stated, pCLAMP version 5.5.1 (Axon Instruments, Union City, CA, USA) was used for data acquisition and analysis, and Sigmaplot Version 2.0 (Jandel Scientific, Corte Madera, CA, USA) for statistical analysis and graphics. Multiple single-channel currents were expressed as mean currents (I) where I=NiPo was obtained as previously reported (Montalbetti et al. 2005b). In this equation, N is the total number of active channels, i is the average single channel current for the channel species (i.e. PC2), and Po is the open probability of the open channel, at a given holding potential. Statistical significance was obtained by an unpaired Student's test comparison of sample groups of similar size. Averaged data are expressed as the mean ±s.e.m. (n) under each condition, where n represents the total number of experiments analysed and s.e.m. is the standard error of the mean. Statistical significance was accepted at P < 0.05 as calculated by a paired Student's test (Snedecor & Cochran, 1973).
Presence of microtubular components in hST membrane vesicles
To assess whether microtubular organization affects PC2 channel function, we first determined the presence of tubulin isoforms and endogenous microtubular structures in hST vesicles by Western blot and immunofluorescence analyses (Figs. 1 and 2). Indeed, Western blot analysis (Fig. 1) confirmed the presence of PC2, as reported (Li et al. 2005), and several tubulin isoforms in the preparation, including α-, β- and γ-tubulins, as well as the post-translationally modified acetylated tubulin heavily localized in such organelles as primary cilia. Immunofluorescence analysis of control hST vesicles (Fig. 2A) showed strong colocalization of PC2 and microtubules, although not all microtubules were decorated (Fig. 2B) with the channel protein. Some membrane-apposed microtubules distinctly displayed a complete absence of PC2 (Fig. 2A). A comparison between control and colchicine-treated vesicles (15 μm, 24 h, at 4°C) indicated that despite the fact that protein content remained largely the same, the drug affected tubulin–PC2 colocalization in the vesicles. Interestingly, however, microtubular stabilization with paclitaxel (15 μm), clearly displayed longer and PC2-decorated microtubules (Fig. 2B).
Effect of colchicine on PC2 channel activity
To assess a regulatory role of endogenous microtubules on PC2 channel function in hST, apical vesicles were first reconstituted in a lipid bilayer system. Experiments were conducted in the presence of a K+ chemical gradient, with 150 mm and 15 mm in the cis and trans compartments, respectively. Data were chosen for analysis from tracings where spontaneous single channel activity was observed at the beginning of the experiment (Fig. 3A). Currents were highly cation selective (Fig. 3B) and further characterized as those previously observed as mediated by PC2 (González-Perrett et al. 2001). In 17 out of 19 experiments, addition of colchicine (15 μm) to the cis compartment completely inhibited PC2-mediated K+ currents (Fig. 3A–C). Colchicine decreased channel activity from 6.0 ± 3.3 to 0.40 ± 0.30 pA (n= 5, P < 0.01) within 30 s after exposure to the drug (Fig. 3C). In the presence of colchicine, further addition of GTP and tubulin had no effect on channel re-activation (from 0.40 ± 0.30–0.30 ± 0.10, n= 3, P > 0.4). In contrast to the inhibitory effect of the microtubule depolymerizing agent colchicine, addition of the microtubular stabilizer paclitaxel (taxol, 15 μm) to the cis chamber stimulated channel activity (Fig. 4). As expected, PC2 channel activity was completely inhibited by the addition of amiloride to the trans chamber (Fig. 4).
Effect of tubulin and GTP on PC2
To further assess the nature of the microtubular regulation of PC2 channel activity, K+ currents were monitored in control hST vesicles. Contrary to the inhibitory effect of colchicine (Fig. 3) and similar to the stimulatory effect of taxol (Fig. 4), addition of polymerizing concentrations of tubulin (5 mg ml−1) and GTP (500 μm) to the cis compartment increased cation channel activity of spontaneously inactivated PC2 in eight out of nine experiments (Fig. 5A). The mean channel current increased by fivefold, from 1.5 ± 1.2 to 9.1 ± 5.2 pA (n= 6, P < 0.03). It is interesting to note, however, that addition of tubulin plus GTP to the purified PC2 channel protein had no stimulatory effect (reported elsewhere, Li et al. 2006), suggestive of the presence of regulatory proteins mediating this interaction.
Presence of kinesin-2 motor subunits in hST and their regulatory role in PC2 channel function
The above findings indicate that while a structural/functional interaction between microtubules and PC2 exists in apical hST vesicles, intermediate, perhaps microtubule-associated, proteins are likely to mediate this linkage. Indeed a number of proteins have been found associated with the microtubule-containing axoneme of primary cilia, and possibly colocalize with PC2 (Yoder et al. 2002a). The kinesin-2 complex, composed of motor subunits KIF3A and KIF3B and the non-motor subunit KAP3, is involved in ATP-dependent anterograde-directed vesicular transport along axonemal microtubules. Interestingly, KIF3A colocalized with PC2 in primary cilia of renal epithelial cells (Li et al. 2006), and directly associated with the carboxy terminus of PC2, which provides a molecular link between microtubular structures and the channel protein. To confirm this structural interaction, we conducted a Western blot analysis of hST apical vesicles and found that both KIF3A and KIF3B are present in the hST apical vesicles (Fig. 6A). Addition of KIF3A chimera (GST-gusion protein) or purified KIF3A either from bacteria or MDCK cells (data not shown) activated (Fig. 6B) or increased PC2 channel in reconstituted hST apical vesicles (n= 5).
In the present study, we demonstrated that PC2 colocalizes with, and is regulated by, microtubular structures in the human syncytiotrophoblast. PC2 is a TRP channel that is abundantly expressed in the hST, and is likely to represent the most relevant component of apical transport of Ca2+ into the fetus. To date, several Ca2+-permeable cation channels have been identified in the term placenta (Belkacemi et al. 2005), including L-type Ca2+ channels (Robidoux et al. 2000; Moreau et al. 2003; Bernucci et al. 2006), several TRP channels, including TRPP2 (polycystin-2) (González-Perrett et al. 2001), TRPC1–6 (Clarson et al. 2003; Niger et al. 2004), TRPV5–6 (ECaC, CaT1) (Bernucci et al. 2006), and the purinergic receptors P2X4, P2X7, P2Y2 and P2Y6 (Roberts et al. 2006a,b). Clarson et al. (2003) detected the presence of message and protein encoding the canonical TRP channels TRPC3 and TRPC4 in both apical and basal membranes of the hST. However, no electrophysiological information was available to confirm channel phenotypes. More recently, Riquelme's group addressed the issue of the presence of various Ca2+ permeable cation channels, including L-type Ca2+ channels, in the basal membrane of term hST (Bernucci et al. 2006). This exhaustive study confirmed the presence of various Ca2+-permeable channels by using a number of techniques, including electrophysiology (Bernucci et al. 2006). As L-type Ca2+ channels are regulated by voltage changes, namely dynamic shifts in the resting potential of the syncytial epithelium, it is likely that this pathway relates to Ca2+ signalling by placental epithelial cells (Cronier et al. 1999).
We originally observed that the gene product of PKD2, implicated in autosomal dominant polycystic kidney disease (ADPKD), is the most abundant Ca2+-permeable non-selective cation channel in the apical domain of term hST (González-Perrett et al. 2001). PC2 belongs to the superfamily of TRP channel proteins (Montell et al. 2002a,b), has a 1:1 cation perm-selectivity ratio for monovalent cations, and a slight preference for divalent cations, ranging from ∼1.5–5:1. This is likely to depend on the experimental conditions under which PC2 was studied (González-Perrett et al. 2001; Vassilev et al. 2001; Koulen et al. 2002; Luo et al. 2003; see Cantiello, 2004 for discussion). Based on its abundance in the apical hST, its single-channel conductance (130–150 pS), and weak self-inhibition by cytoplasmic Ca2+, PC2 can be considered an important contributor to the apical entry step in the transepithelial movement of Ca2+. Ca2+-transporting TRP channels, quintessentially considered as Ca2+-transporting elements in absorption epithelia, include ECaC1 and CaT1, now known as TRPV5 and TRPV6, respectively (Peng et al. 2003a,b). TRPV5 and 6, originally identified as the Ca2+-transporting mechanism in intestine (Peng et al. 1999), and the kidney (Hoenderop et al. 2000), respectively, have been identified in both apical and basal membranes of the hST (Moreau et al. 2002, 2003). At least two parameters in the channel properties of PC2, as compared with ECaC1 and CaT1, make it most relevant in terms of its potential capabilities as a Ca2+-entry pathway in the human placenta. First, PC2 has a much larger monovalent cation single-channel conductance (Nilius et al. 2000). Second, compared with other TRP channels, PC2 presents a much weaker self-inhibition by Ca2+. Thus, PC2 is an important electrodiffusional pathway for Ca2+ transport from the maternal side of the human placenta in late gestation. PC2 is also implicated in signalling mechanisms, in particular those associated with volume flow in epithelial cells (Nauli et al. 2003), and osmotic signals in the hST (Montalbetti et al. 2005a).
How PC2-mediated Ca2+ transport relates to placentation, and the functional properties of the chorionic place, remains to be defined. Concerning its potential role in cell signalling, PC2 has been implicated in cell division and replication (Aguiari et al. 2004). PC2 is also involved in the developmental pattern of branching in epithelial cells (Grimm et al. 2006). Thus, PC2 may play an important role in placental development. The chorionic villous tree, deriving from the chorionic plate, is an intricate structure, which continuously grows by branching during gestation in a process requiring a dynamic cytoskeleton (Demir et al. 1997). All major cytoskeletal components (Truman & Ford, 1986), including actin filaments (Beham et al. 1988; Parast & Otey, 2000), intermediate filaments (Clark & Damjanov, 1985; Hesse et al. 2000; de Souza & Katz, 2001), and microtubules (Smith et al. 1977; Douglas & King, 1993) are present in the developing placenta. Both the basal and microvillous hST plasma membranes exhibit structural and functional differences, reflecting specific transport and regulatory mechanisms controlled by the maternal and fetal sides of the placental interface, respectively. These differences are not only reflected in the specific segregation of particular Ca2+-transport mechanisms (Moreau et al. 2002, 2003; Clarson et al. 2003; Bernucci et al. 2006), but also depend on the selective expression and location of specific cytoskeletal components. The apical hST cytoskeleton, containing the ‘syncytioskeletal layer’ (Ockleford et al. 1981), expresses the actin bundling protein α-actinin (Booth & Vanderpuye, 1983), which is excluded from the basal membrane cytoskeleton (Vanderpuye et al. 1986). The cytoskeletal anchoring protein EBP50 colocalizes with ezrin and actin only in the apical microvilli of epithelial ST (Berryman et al. 1995; Reczek et al. 1997). The actin cytoskeleton also plays a relevant role in the regulation of PC2 channel function in the term placenta, such that actin filamental dynamics control its function and interaction with actin-associated proteins (Li et al. 2005; Montalbetti et al. 2005b). In this regard, the interactions of PC2 with the actin cytoskeleton may provide a functional unit implicated in signal transduction (Cantiello et al. 2004), which plays a role in osmotic sensing, and thus probably the hydro-electrolytic homeostasis in the human placenta (Montalbetti et al. 2005a). However, apical microvilli are thought to exclude microtubules (Ockleford et al. 1981). This localization not only plays a structural role, but microtubular disruption has been implicated in chorionic differentiation (Douglas & King, 1993). In that study, addition of the microtubular destabilizer colchicine prevented human cytotrophoblast cell differentiation and the process of syncytiation. Microtubular stability has also been implicated in normal fertilization (Wu et al. 1996), and transport in trophoblast-derived cells (Ellinger et al. 1999).
F-actin and microtubular cytoskeletal networks are thought to fulfil separate and independent cellular roles. Highly dynamic actin networks are implicated in cell spreading, motility, and contraction, while the more stable microtubule cytoskeleton is best known for its importance in cell division and organelle trafficking. In the present report, we speculated and confirmed that a functional role(s) of the microtubular cytoskeleton exists in the control of PC2 function, which may have important implications for the control of Ca2+ transport in the human placenta. Our findings indicate that manoeuvres that stabilize microtubules, such as addition of taxol, increase, while addition of colchicine to disassemble microtubules inhibit, endogenous PC2 channel activity in hST membranes. These data suggest a dynamic role of microtubular formation in the activation and regulation of PC2. This was confirmed by addition of exogenous tubulin and GTP, which was also stimulatory. Recent findings from our laboratory indicated, however, that this interaction is not a direct binding of tubulin to the PC2 channel (Li et al. 2006), as the same experiment conducted with purified PC2 channel was unresponsive to the addition of tubulin and GTP (Li et al. 2006). This information suggested the necessity of intermediate protein(s) to mediate the microtubular regulation of PC2. Our data also indicate that, in similar fashion to our findings in ciliary membranes (Li et al. 2006), the kinesin motor protein KIF3A is present in hST, and acts as a mediator protein linking PC2 and the microtubular cytoskeleton. This evidence further suggests a regulatory mechanism that requires microtubule-associated proteins, such as the kinesin-2 in the regulation of PC2. This is particularly relevant in the context of cell trafficking of PC2 by microtubular structures. The data in Fig. 2 indicate that PC2 decorates specific microtubules within the hST vesicles. This is consistent with the possibility that the microtubular connection helps target the channel protein for delivery to specific cell domains. However, a microtubular interaction with PC2 may also be indicative of a novel more universal targeting and signalling mechanism. This hypothesis stems from recent advances in renal and other cystic diseases. Renal polycystic kidney diseases have recently been linked to ciliary dysfunction and microtubular proteins (Morgan et al. 1998; Murcia et al. 2000; Hou et al. 2002; Pazour et al. 2002; Yoder et al. 2002b), including genetic disorders such as autosomal dominant and recessive forms of cystic disease. Dysfunctional ciliary proteins, namely proteins, which preferentially segregate to the primary cilia of epithelial cells, include cystin (Hou et al. 2002) and polaris. These proteins localize to the ciliary basal body and the microtubular axoneme (Yoder et al. 2002b), and produce genetically recessive forms of polycystic kidney disease. PC1 and PC2, also present in primary cilia (Nauli et al. 2003), conform the two main contributors to autosomal dominant polycystic kidney disease. An early observation for a microtubular connection with cystic disease arose by the finding that treatment of homozygous cpk/cpk mice with the microtubular stabilizer paclitaxel (Woo et al. 1997) moderates progression of renal cystic disease, suggesting that the ability to promote microtubule assembly controls cyst formation in mouse kidney. orpk mice, with a dysfunctional polaris, display shortened cilia and left–right asymmetry defects (Murcia et al. 2000) and increased PC2 in cilia (Pazour et al. 2002), in addition to PKD. Primary cilia are clearly implicated in the transduction of signals associated with capacitative Ca2+ entry (Praetorius & Spring, 2001; Praetorius et al. 2003) in renal epithelial cells. Thus, the fact that the PC2 channel interacts with cystin, polaris and ciliary tubulin in primary cilia of renal epithelial cells, strongly suggests that microtubular organization is likely to be a regulator of PC2 function.
In summary, the data from this report and our previous studies (Li et al. 2005; Montalbetti et al. 2005b) suggest a strong complementarity in the cytoskeletal regulation of PC2. The cytoskeletal regulation of PC2 in hST may play two roles: first, as a potential key element in the control of branching and invasion in the developing placenta; and second, fulfilling the fetal needs for Ca2+ intake of late gestational placenta.
H.F.C. was funded by the Polycystic Kidney Disease Foundation. The Canadian Institutes of Health Research and the Kidney Foundation of Canada supported X.-Z.C. and his group. X.-Z.C. is an Alberta Heritage Foundation for Medical Research Scholar. Q.L. is a recipient of the Polycystic Kidney Disease Foundation.