We examined gap junction coupling of descending vasa recta (DVR). DVR endothelial cells or pericytes were depolarized to record the associated capacitance transients. Virtually all endothelia and some pericytes exhibited prolonged transients lasting 10–30 ms. Carbenoxolone (100 μM) and 18β-glycyrrhetinic acid (18βGRA; 100 μM) markedly shortened the endothelial transients. Carbenoxolone and heptanol (2 mM) reduced the pericyte capacitance transients when they were prolonged. Lucifer yellow (LY; 2 mM) was dialyzed into the cytoplasm of endothelial cells and pericytes. LY spread diffusely along the endothelial monolayer, whereas in most pericytes, it was confined to a single cell. In some pericytes, complex patterns of LY spreading were observed. DVR cells were depolarized by voltage clamp as fluorescence of bis(1,3-dibarbituric acid)-trimethine oxanol [DiBAC4(3)] was monitored ∼200 μm away. A 40-mV endothelial depolarization was accompanied by a 26.1 ± 5.5-mV change in DiBAC4(3) fluorescence. DiBAC4(3) fluorescence did not change after 18βGRA or when pericytes were depolarized. Similarly, propagated cytoplasmic Ca2+ responses arising from mechanical perturbation of the DVR wall were attenuated by 18βGRA or heptanol. Connexin (Cx) immunostaining showed predominant linear Cx40 and Cx43 in endothelia, whereas Cx37 stained smooth muscle actin-positive pericytes. We conclude that the DVR endothelium is an electrical syncytium and that gap junction coupling in DVR pericytes exists but is less pronounced.
- blood flow
descending vasa recta (DVR) are ∼12- to 18-μm-diameter branches of juxtamedullary efferent arterioles that supply the renal medulla with blood flow. In addition to their role in countercurrent exchange (39), they are surrounded by smooth muscle-like cells (pericytes) that contract and dilate in response to a variety of hormonal and paracrine agents (38, 40). In an ongoing effort to delineate the channel architecture of DVR, we devised methods to patch clamp either the abluminal pericytes or luminal endothelia of explanted vessels (44). Those approaches have been used to define the regulation of membrane potential (37, 59), K+ currents (5), and cation entry pathways (55, 59). As previously described, prolonged, decaying capacitance transients, possibly attributable to cell-to-cell coupling through gap junctions, are sometimes observed upon patch clamp of pericytes of intact explanted vessels. When the goal of the experiment has been to measure single-cell ion currents, study of such cells was abandoned. Similar prolonged capacitance transients are nearly always found when electrical access to DVR endothelial cells has been obtained using whole cell patch-clamp methods (5, 44, 55).
In this study, we tested whether those prolonged transients arise from gap junction coupling in the DVR wall. In both pericytes and endothelium, application of gap junction blockers reduced the time of decay time of the transients from 10 to 30 ms to <1 ms. The fluorescent probe Lucifer yellow (457 Da) was found to diffuse freely from cell to cell in the endothelial monolayer. In contrast, Lucifer yellow was most often sequestered within single pericytes. Depolarizing pulses imposed by voltage clamp were readily conducted along the endothelial monolayer. Similar electrical spreading was not observed from patched pericytes. Cytoplasmic Ca2+ responses ([Ca2+]cyt) that propagated away from a point of mechanical stimulation of the DVR wall were attenuated by gap junction blockade. Finally, immunochemical staining showed predominant expression of connexin (Cx)40 and Cx43 in the endothelium and predominantly Cx37 in pericytes. We conclude that the DVR endothelium is an electrical syncytium. In contrast, open gap junctions between adjacent pericytes or between pericytes and the underlying endothelium exist but are less common.
Isolation of DVR.
Investigations involving animal use were performed according to protocols approved by the Institutional Animal Care and Use Committee of the University of Maryland. Kidneys were harvested from Sprague-Dawley rats (120–200 g; Harlan) that had been anesthetized with an intraperitoneal injection of ketamine (80 mg/kg)-xylazine (10 mg/kg). Tissue slices were stored at 4°C in a physiological saline solution (PSS). For patch clamp of pericytes, wedges of renal medulla were enzymatically digested in Blendzyme 1 (0.27 mg/ml; Roche) in high-glucose DMEM medium (Invitrogen) at 37°C for 45 min. Access to endothelial cells for patch clamp necessitated removal of pericytes from the abluminal surface. This was done, as previously described in detail (44), by drawing the vessel into the mouth of a micropipette that had been heat-polished to ∼6 μm. For those protocols, tissue digestion was performed in a cocktail of collagenase 1A (0.5 mg/ml), protease XIV (0.4 mg/ml), and bovine serum albumin (1.0 mg/ml) in PSS (in mM: 155 NaCl, 5 KCl, 1 MgCl2, 1 CaCl2, 10 HEPES, and 10 glucose, pH 7.4). In all cases, after digestion, medullary tissue was transferred to PSS and held at 4°C. DVR were isolated by microdissection as needed and transferred to an inverted microscope (Nikon TE300) for patch-clamp recording and fluorescent microscopy.
Whole cell patch-clamp recording.
Patch pipettes were made from borosilicate glass (PG52151-4, external diameter 1.5 mm, internal diameter 1.0 mm; World Precision Instruments, Sarasota, FL) with the use of a two-stage vertical pipette puller (Narshige PP-830) and were heat-polished. Whole cell currents were recorded using either the nystatin-perforated patch or ruptured patch configurations as previously described (5, 37, 55). For nystatin-perforated patches or ruptured patches used to dialyze Lucifer yellow into the cell cytoplasm, the electrode solution contained (in mM) 120 K-aspartate, 20 KCl, 10 NaCl, and 10 HEPES, pH 7.2, and nystatin (100 μg/ml with 0.1% DMSO) in ultrapure water. For protocols that focused on measurement of membrane capacitance, membrane currents were minimized with the following electrode solution (in mM): 115 Cs-methanesulfonate, 18 CsCl, 10 NaCl, 2.35 MgATP, 1 CaCl2, 5 EGTA, and 10 HEPES, pH 7.2. The extracellular buffer was PSS, and where required, niflumic acid (100 μM) and tetraethylammonium Cl (TEA; 30 mM) were added to suppress Cl− and K+ currents, respectively. TEA was added to PSS by isosmotic replacement of NaCl. Current recordings were obtained with a CV201AU head stage and Axopatch 200 amplifier (Axon Instruments, Foster City, CA). Cell capacitance (Cm) was measured using 10-mV pulses from a holding potential of −70 mV with the “membrane test” feature of Clampex (Axon Instruments). Such analysis was limited to spontaneously uncoupled cells or cells uncoupled by gap junction blockers.
In some experiments, membrane potential was recorded using the voltage-sensitive fluorescent probe bis(1,3-dibarbituric acid)-trimethine oxanol [DiBAC4(3); 5 μM] according to methods previously described (56). To test whether membrane potential changes are conducted from cell to cell along the DVR wall, we accessed an endothelial cell or pericyte for voltage clamp by using nystatin-perforated patches. The cell was depolarized from −70 to −30 mV while DiBAC4(3) fluorescence was monitored along the vessel wall ∼200 μm away from the site of patch formation. A region of several cells was optically isolated by adjusting a rectangular window of a photon-counting photomultiplier detection assembly (D104B; Photon Technology International). DiBAC4(3) was excited at 485 nm with a DeltaRAM illuminator (Photon Technology International). Fluorescent emission at 530 nm was isolated with a band-pass filter (Omega Optical, Brattleboro, VT). Calibration of DiBAC4(3) has been described previously (27). Briefly, cellular permeability to monovalent cations was equalized by exposure to the ionophore gramicidin D (2 mg/ml). Extracellular Na+ concentration was varied by isosmotic substitution with N-methyl-d-glucamine to yield 2.5, 5, 25, 50, 100, or 150 mM, and the imposed membrane potential was calculated using the Goldman equation. The associated change in DiBAC4(3) fluorescence yielded the corresponding percent change per millivolt (27, 56).
To determine whether gap junctions between cells along the DVR wall facilitate diffusion of molecules, we included the 457-Da fluorescent probe Lucifer yellow (2 mM, excitation 425 nm, emission 540 nm) in the electrode. Ruptured patches were formed on endothelial cells or pericytes, after which membrane currents were recorded to determine whether prolonged capacitance transients were present, indicating cell-to-cell coupling. Subsequently, white light and Lucifer yellow fluorescent images were captured by timed exposure (Spot Cam; Diagnostics Instruments).
To record propagated [Ca2+]cyt transients along the DVR wall, we loaded the Ca2+-sensitive fluorescent probe fluo-4 (Molecular Probes) by incubation of the AM ester (2 μmol/l, 20 min, 37°C). The probe was excited at 485 nm (DeltaRam), and emissions were monitored at 530 nm (B-2E/C filter cube; Nikon), with a ×40 CF fluor oil-immersion objective (1.3 numerical aperture). Fluorescence was monitored by capturing sequential images, once per second, with a low light level charge-coupled device camera with on-chip multiplication gain (Photometrics Cascade 512B; Roper Scientific). A micropipette with a 10-μm orifice was positioned close to the DVR wall at one end of the vessel. At 1-min intervals, pressurization of the pipette from a reservoir was used to puff a stream of buffer onto the vessel wall. Resultant [Ca2+]cyt transients along the vessel wall were quantified within rectangular regions of interest by using ImageMaster software (Photon Technology International).
Immunofluorescent labeling of isolated DVR.
Using methods previously described (5, 33), we performed immunofluorescent labeling to detect expression of Cx37, Cx40, and Cx43 in the DVR wall. Monoclonal antibody directed against α-smooth muscle actin (SMA; 1:500 dilution to 9 μg/ml; Sigma A2547) was used to delineate the pericytes (33, 41). Rabbit polyclonal antibodies directed against Cx37 (1:50 dilution to 20 μg/ml; Alpha Diagnostic International CX37B12-A), Cx40 (1:50 dilution to 20 μg/ml; Chemicon AB1276), and Cx43 (1:100 dilution; Cell Signaling Technology 3512) were used to identify their respective distributions within pericytes and endothelium. Microdissected DVR were transferred onto slides and fixed with 3% paraformaldehyde in 100 mM cacodylate buffer, pH 7.4, and then rinsed three times. Vessels were then permeabilized with 0.1% Triton in PSS buffer for 2 min, blocked with 5% bovine serum albumin in PSS with 0.1% Triton (10 min, room temperature), and exposed to the primary antibody for 1 h at room temperature and then overnight at 4°C. After three washes with PSS containing 0.1% Triton X-100, the vessels were incubated with secondary antibodies conjugated to Alexa Fluor 488 goat anti-rabbit IgG (1:400 dilution to 5 μg/ml; Molecular Probes A-11034) and Alexa Fluor 568 goat anti-mouse IgG (1:400 dilution to 5 μg/ml; Molecular Probes A-11031) for 1 h at room temperature. After several additional washes, coverslips were mounted with Vectorshield (Vector Laboratories, Burlingame, CA). Fluorescent images were obtained using a Zeiss LSM410 scanning confocal microscope with a ×63 oil-immersion objective with a Z-axis 0.5-μm step size. Z-series overlays (SUM images) of the actin and connexin images were generated with ImageJ 1.33 (NIH) to augment the ability to localize connexins to pericytes or endothelium. Nomarski (differential interference contrast) images were obtained of the same vessel for comparison. To verify specificity, negative controls were performed in which primary antibodies were omitted.
Lucifer yellow and DiBAC4(3) were obtained from Molecular Probes. Niflumic acid, 18β-glycyrrhetinic acid (18βGRA), carbenoxolone, heptanol, nystatin, collagenase 1A, protease XIV, and other chemicals were obtained from Sigma (St. Louis, MO). Liberase Blendzyme 1 was obtained from Roche Applied Science. Niflumic acid and 18βGRA were dissolved in DMSO. Reagents were thawed and diluted on the day of the experiment. Excess was discarded daily. Blendzyme was stored in 40-μl aliquots of 4.5 mg/ml in water and diluted into high-glucose DMEM on the day of the experiment.
Data are reported as means ± SE. The significance of differences was evaluated with SigmaStat 3.11 (Systat Software, Point Richmond, CA) using parametric or nonparametric tests as appropriate for the data. Comparisons between two groups were performed with Student's t-test (paired or unpaired, as appropriate) or the rank sum test (nonparametric). Comparisons between multiple groups were performed with repeated-measures ANOVA or repeated-measures ANOVA on ranks (nonparametric). Post hoc comparisons were performed using Tukey's or Holm-Sidak tests. P < 0.05 was used to reject the null hypothesis. Curve fits to data points were performed using the Levenberg-Marquardt algorithm in Clampfit 9.2 (Axon Instruments).
Gap junction coupling in DVR endothelia.
Access to DVR endothelia was achieved by removing pericytes with a micropipette (44). Endothelial whole cell currents, measured with nystatin-perforated patches, always showed large, decaying transients at the beginning of depolarizing or hyperpolarizing pulses (Fig. 1A). We tested whether those transients are due to the large membrane area resulting from cell-to-cell coupling through gap junctions. As shown in Fig. 1A, exposure to the gap junction blocker 18βGRA (100 μM) markedly shortened the transients. To quantify the effect, the transients were recorded by imposing sequential depolarizing pulses from −70 to 0 mV (100-ms duration) at 10-s intervals. During pulsation, the cells were exposed to the gap junction blockers 18βGRA (100 μM) or carbenoxolone (100 μM) or to vehicle (0.1% DMSO). An example is shown in Fig. 1B where sequential transients are superimposed that include baseline and subsequent traces following introduction of carbenoxolone. The marked shortening of the capacitance transients in carbenoxolone favors the interpretation that cell-to-cell coupling predominates in DVR endothelium and is eliminated by gap junction blockade.
In an isolated cell, a fit to the appropriate single-exponential relationship can yield a proper measure of cell membrane capacitance. In contrast, the circuit theory underlying that analysis is inappropriate for calculation of capacitance in gap junction-coupled cells (32, 35). For that reason, we chose to quantify the time course of changes in capacitance transients using the simple method illustrated in Fig. 1C. Custom software was written to determine the time required for membrane current to fall from the maximum that occurs at the beginning of an applied voltage pulse to within 80% of its end-pulse value. A typical application is illustrated in Fig. 1C where only the transients present before (curve 1) and long after exposure to carbenoxolone (curve 2) are shown. The corresponding 80% decay time falls from 7.56 to 0.21 ms. In the case of curve 2, it is appropriate to fit the data to a single exponential to calculate single-cell capacitance (Cm); that yields a value of Cm = 12.2 pF. Using that approach, we quantified the effects of 18βGRA, carbenoxolone, and vehicle (DMSO). Exposure to the gap junction blockers rapidly reduced the decay time of the transients (Fig. 1D). Neither blocker easily reversed upon washout. Sequential pulses in DMSO did not reduce decay time, verifying that 18βGRA and carbenoxolone, and not the repeated depolarizing pulses, closed the endothelial gap junctions.
Spread of Lucifer yellow along the endothelial syncytium.
To obtain further evidence that endothelial cells of DVR are coupled by gap junctions, we formed ruptured patches and included the fluorescent probe Lucifer yellow (457 Da, 2 mM) in the electrode buffer. In such experiments, Lucifer yellow consistently spread between endothelial cells. Examples of white light and fluorescent images, similar to n = 8 vessels, is provided in Fig. 2.
Gap junction coupling in DVR pericytes.
As previously described (5, 55), some DVR pericytes show prolonged capacitance transients that indicate gap junction coupling. Many pericytes, however, do not. Examples of current records are provided in Fig. 3. Figure 3A, a and b, shows whole cell records composed of submillisecond capacitance transients followed by activating currents (pulse protocol defined in inset). We have previously shown that the activating currents are largely carried by Cl− influx through Ca2+-activated Cl− channels (37, 56, 59). Figure 3B, a and b, shows examples of pericyte whole cell records, elicited with the same pulse protocol, in which large-capacitance transients precede the activating currents. To demonstrate that the prolonged transients of such cells are due to gap junction coupling, we sequentially pulsed the pericytes from −70 to 0 mV during introduction of carbenoxolone (100 μM) into the extracellular buffer. As with endothelial cells (Fig. 1, B and D), the decay time of the pericyte transients was reduced to submillisecond time scales typical of single-cell recordings (Fig. 3C, a and b). As in the endothelium, the effects of carbenoxolone in pericytes were not readily reversible.
In a separate series, we examined the effectiveness and reversibility of 1-heptanol as a blocker of pericyte gap junctions. As shown in Fig. 4, A and B, heptanol (2 mM) was very effective; however, it also globally reduced membrane currents, implying nonspecific inhibition of membrane conductance. Unlike 18βGRA and carbenoxolone, the effects of heptanol were readily reversible upon washout. The concentration dependence of heptanol is defined by the experiment shown in Fig. 4C and summarized in Fig. 4D. At concentrations below 2 mM, inhibition of the gap junction-associated transients was incomplete.
Spread of Lucifer yellow from DVR pericytes.
The data shown in Figs. 1–4 are consistent with the interpretation that the endothelium of isolated DVR is always coupled as an electrical syncytium. In contrast, cell-to-cell coupling of pericytes via open gap junctions is inconsistent. Examination of the pattern of spreading of Lucifer yellow from patched pericytes reinforced that notion. Figure 5 shows three examples of pericytes in which currents (top) elicited with the protocol illustrated in Fig. 4A, inset, have capacitance transients whose durations are much less than 1 ms. Corresponding white light and fluorescent images show that Lucifer yellow was confined to the patched cell. In contrast, Fig. 6 shows three examples of pericytes whose current tracings revealed prolonged transients consistent with gap junction coupling. Figure 6A shows a thin rim of Lucifer yellow (white arrowheads), a pattern that is expected for diffusion from cell to cell along the thin abluminal pericyte layer. Figure 6, B and C, shows examples of Lucifer yellow spread that includes transport to the endothelium. The images in Fig. 6, B and C, imply the existence of open myoendothelial gap junctions. Of a total of 27 consecutive pericytes examined by patch clamp and Lucifer yellow imaging, 8 (∼30%) showed evidence of coupling, whereas 19 had only brief capacitance transients without evident spreading of the dye.
Spread of voltage clamp-induced depolarizations.
To further assess the nature of cell-to-cell coupling, we tested whether depolarization of an individual pericyte or endothelial cell by voltage clamp also depolarized adjacent cells along the DVR wall. The method used for the experiment is illustrated in Fig. 7A. With the use of nystatin-perforated patches, an endothelial cell or pericyte was accessed for voltage clamp. The vessel was loaded with the voltage-sensitive fluorescent probe DiBAC4(3), the fluorescence of which, emitted from cells ∼200 μm away from the patch pipette, was measured with a photon-counting photomultiplier detection assembly. As shown in Fig. 7B and summarized in Fig. 7C, depolarization of endothelial cells from −70 to −30 mV consistently and reversibly increased DiBAC4(3) fluorescence, verifying simultaneous depolarization of nearby cells on the DVR wall. The cells within the optical window of the photomultiplier assembly that emitted DiBAC4(3) fluorescence included both pericytes and endothelium. We cannot quantify the relative origins of the signal from the two cell types. The mean increase in fluorescence achieved by the 40-mV depolarization was 9.8 ± 2%, from which a change of 26.1 ± 5.5 mV (n = 11) was computed by DiBAC4(3) calibration. Given that some signal may have been from pericytes that did not respond, the membrane potential change in the endothelium might have been >26.1 mV. Pretreatment with 18βGRA eliminated the change in DiBAC4(3) fluorescence that occurred upon depolarization of an endothelial cell. In contrast to the spread of depolarization from endothelia, identical depolarization of pericytes failed to alter DiBAC4(3) fluorescence (Fig. 7D). Those data, coupled with the results shown in Figs. 1–6, support the interpretation that the DVR endothelium is an electrical syncytium, whereas gap junction coupling in pericytes is inconsistent.
Propagated [Ca2+]cyt responses along the DVR wall.
We have previously shown that the DVR endothelium is mechanosensitive. Stretch of the DVR wall by luminal pressurization induces [Ca2+]cyt responses and NO generation (57). We exploited a variation of that property to demonstrate that [Ca2+]cyt responses can be conducted along the DVR wall. A micropipette with an ∼10-μm orifice was placed adjacent to fluo-4-loaded DVR that were adherent to the bottom of the perfusion chamber. At 1-min intervals, the pipette was briefly pressurized from a reservoir to puff a stream of buffer onto the abluminal surface of the vessel. Quantification of the fluo-4 fluorescence change within rectangular regions of interest (R1–R4, Fig. 8A) demonstrated that a [Ca2+]cyt response was elicited at all points along the vessel axis (Fig. 8B). When this maneuver was performed after introduction of 18βGRA (100 μM) or heptanol (2 mM), the [Ca2+]cyt responses were attenuated (Fig. 8, C and D). The effect of heptanol was more reversible than that of 18βGRA. As shown in Fig. 8A, fluo-4 distributed largely into the endothelium. These data show that endothelial [Ca2+]cyt responses can conduct along the DVR wall in a gap junction-sensitive manner.
Immunostaining for vascular gap junction proteins.
Of the connexin family proteins, Cx37, Cx40, and Cx43 are most frequently observed in the vasculature (8, 15). Double antibody immunofluorescent staining was performed in microdissected DVR to assess their presence and distribution. Counterstaining with antibody directed against SMA was used to identify pericytes (5, 33, 41). Results are shown in the reconstructions in Figs. 9–11. Antibody directed against Cx40 revealed a linear pattern largely confined to the endothelium (Fig. 9). Cx43 staining yielded a similar endothelial pattern; however, punctate staining of pericytes was more obvious (Fig. 10). Immunostaining with antibody against Cx37 yielded a pattern that was distinct from that of Cx40 and Cx43 (Fig. 11). Cx37 colocalized with SMA, implying greater expression in DVR pericytes than in endothelium.
Cell-to-cell communication through gap junctions is common in the microvasculature (4, 8, 10, 14, 15, 31, 53). It is currently understood that this occurs through transcellular channels called connexons that are formed by docking of heximeric connexin hemichannels. Connexons behave as true channels with variable open probability, subconductance states, and, in some cases, ion selectivity (3, 4). Unlike typical ion channels, however, some connexon pores are large enough to conduct diffusion of molecules as large as 1 kDa (4, 14). Homocellular connexons bridge the cytoplasm between adjacent smooth muscle cells or between adjacent endothelial cells. Heterocellular connexons, formed between smooth muscle and endothelium, yield myoendothelial gap junctions (6, 12, 17, 18, 26, 45, 50). Of some 20 connexins coded by the mammalian genome, Cx37, Cx40, Cx43, and Cx45 are found in the vasculature (14), including the microcirculation of the kidney (1, 2, 21–23, 25, 29). The functional roles of connexins are poorly understood, but cell-to-cell transfer of signaling molecules such as cAMP, inositol trisphosphate , and Ca2+, as well as conduction of membrane potential changes and vasodilatory responses, have been described (11, 14, 15, 19, 20, 25). Myoendothelial gap junctions may be responsible for transfer of endothelium-dependent hyperpolarizing factors that limit vasoconstriction (11, 12, 17, 19, 20). Studies in transgenic mice have given some important insights into connexin function (8, 52). Because of cardiac malformation, deletion of Cx43 is lethal, implying an important role for Cx43 in morphogenesis (8, 43). Cx43−/− lethality is corrected when it is replaced by Cx40, but the substitution yields hypotrophic testicles and sterility (42). Separate Cx37 and Cx40 knockouts yield viable offspring except when Cx37 and Cx40 deletions are combined (47). Cx37 knockout mice lack a vascular phenotype, but deletion of Cx40 yields hypertension, irregular vasomotion, and attenuated conduction of vasodilatory responses (8, 9). Interestingly, a recent study correlated Cx40 polymorphisms with male hypertension in humans (16). In contrast to the hypertension associated with Cx40 deletion, targeted deletion of Cx43 from the endothelium using the Cre recombinase approach has been reported to reduce blood pressure (34, 49). In animal models of hypertension, expression of Cx43 has been reported to undergo variable regulation in both the peripheral and renal vasculature (24, 25), and replacement of Cx43 with Cx32 is associated with decreased renin expression and resistance to two kidney-one clip hypertension (23).
The renal medullary microcirculation is arranged as a countercurrent exchanger to accommodate the competing need to supply oxygen and nutrient blood flow while maintaining the corticomedullary gradients of NaCl and urea that enable urinary concentration. One consequence of countercurrent flow is that oxygen is shunted from DVR to ascending vasa recta so that oxygen tension in the medulla is low. A growing body of evidence favors robust release of the paracrine agents, prostaglandins, adenosine, and NO that guard against hypoxic insult by limiting microvessel constriction and by reducing Na+ transport (7, 38, 40). Given the pivotal role of DVR in medullary perfusion, we established methods to study the channel architecture that governs their contraction and dilation (44). Cell culture models of DVR pericytes or endothelium do not exist. For that reason, we have performed electrophysiological studies on DVR explanted from the renal outer medulla by microdissection (37, 44). Isolated DVR are typically ∼13 μm in diameter and 500 μm in length. Formation of gigaohm seals on abluminal pericytes has made study of their channel activity possible. In contrast, study of the endothelium has been limited by cell-to-cell coupling that is manifest during experiments by large time-decaying capacitance transients. Such large-capacitance transients are very frequent in the endothelium, implying syncytial coupling through gap junctions. In contrast, capacitance transients of pericytes are often <1 ms in duration, showing that they are uncoupled from neighboring cells (5, 55).
In this study, we verified that the prolonged capacitance transients that are always observed during patch-clamp studies of the DVR endothelium (Fig. 1), and sometimes during patch-clamp studies of DVR pericytes (Fig. 3), are a result of gap junction coupling. Several lines of investigation support that contention. The decay time of capacitance transients was reduced by application of the known gap junction blockers carbenoxolone, 18βGRA, and heptanol. In pericytes that exhibited prolonged capacitance transients, carbenoxolone and heptanol (Figs. 3 and 4) effectively reduced them. Dialysis of Lucifer yellow into the cytoplasm of an endothelial cell through a ruptured patch was always accompanied by diffuse spreading of the probe to neighboring cells (Fig. 2). In pericytes, the spreading patterns were complex and inconsistent. In uncoupled cells, as judged by short capacitance transients, Lucifer yellow was generally confined to a single cell (Fig. 5). In coupled cells, it sometimes diffused along the abluminal pericyte cell layer and sometimes spread to adjacent endothelium (Fig. 6). Those observations support the conclusion that although cell-to-cell coupling of pericytes is inconsistent, homocellular connexons and myoendothelial junctions do exist. Myoendothelial junctions in the kidney have been previously described (48). To examine cell coupling by an independent method, we measured the spread of a depolarizing pulse along the vessel wall. When the pulse was applied to an endothelial cell, depolarization of adjacent cells was observed and was prevented by gap junction blockade. In contrast, when the patched cell was a pericyte, depolarization did not spread along the DVR wall (Fig. 7).
Examinations of myocyte and endothelial membrane potential responses using impaled electrodes in the murine cremasteric bed, in vivo, suggested poor myoendothelial coupling (46), as we have observed. In contrast, similar studies in feed arterioles of the hamster retractor muscle showed near equivalence of membrane potential, suggesting a high degree of coupling (13). We are uncertain why DVR pericyte cell-to-cell coupling was less robust than that observed in the endothelium, but incomplete myoendothelial coupling has been reported in other microvessel preparations (15, 46). In our study, there was a substantial incidence of coupling in pericytes, but it was less uniform than that in the endothelium (Figs. 5 and 6). This may be related to the isolation of the vessels from the rat, or it may be an intrinsic property of the DVR wall. Technical limitations preclude examination of function in vivo, because the renal cortex overlies the outer medullary vascular bundles from which outer medullar DVR are derived. Warm ischemia time after harvest of the kidney from the rat and before microdissection is limited to only a few minutes, but connexins are known to be rapidly inserted and retrieved from the cell membrane. Similarly, connexins are regulated by many factors such as phosphorylation events, pH, and elevation of [Ca2+]cyt (8, 15, 19, 24, 52). Stimulation by agonists such as endothelin and angiotensin II affects opening of gap junctions so that residual effects of those and other hormones occurring in vivo may be responsible for setting the relative open state of myoendothelial junctions (30, 31).
As with fura-2 (40), fluo-4, loaded into DVR by incubation of the esterified form, yields a predominantly endothelial signal (Fig. 8A). In addition, like luminal pressurization, abluminal wall stretch induced by puffing the abluminal surface of the vessel with a localized buffer stream induces a [Ca2+]cyt response (Fig. 8B) (57). The data in Fig. 8, C and D, show that the responses are attenuated by gap junction blockade with 18βGRA or heptanol. Thus gap junctions can conduct responses along the DVR wall. These data do not show whether the [Ca2+]cyt changes are due to actual diffusion of Ca2+ ion between cells in Ca2+ waves or whether the propagation results from conduction of membrane potential changes that lead to localized Ca2+ signaling events. Much faster image acquisition and faster-acting fluorescent voltage-sensitive probes are likely needed to delineate and quantify those details.
To complement electrophysiological and Lucifer yellow tracer studies, we used immunochemistry with commercial antibodies to detect the presence and distribution of Cx37, Cx40, and Cx43. To aid in localization, we counterstained DVR pericytes with antibody directed against SMA. In our hands, Cx40 and Cx43 yielded a heavy, predominantly linear, staining in an endothelial pattern (Figs. 9 and 10). Lighter, punctate staining of Cx43, but not Cx40, was also observed in the pericytes (Fig. 10). The staining pattern of Cx37 was distinct from that of either Cx40 or Cx43; it was absent from endothelium, predominantly colocalizing with SMA to pericytes. Investigators have frequently reported Cx40 and Cx43 in endothelium as well as smooth muscle. In contrast, Cx37 is most often found in the endothelium (15). Thus our finding of Cx37 expression in pericytes (Fig. 11) is somewhat unusual but not unique (28, 36, 51, 54). As emphasized by Figueroa et al. (15), studies of connexin isoform distribution between endothelia and smooth muscle in both conduit arteries and microvessels have yielded diverse results. That variability may be real; to some degree, it may reflect inherent limitations of immunochemistry.
A number of studies have examined the distribution of connexins in the vasculature of the kidney. Arensbak et al. (1) observed that mRNA for Cx37, Cx40, and Cx43 is present in cultured preglomerular smooth muscle cells of the rat. In contrast, only Cx40 staining was observed by immunofluorescence or immunochemistry in tissue sections. In an extensive survey of the distribution of the same connexins in the mouse, Zhang and Hill (54) found preglomerular endothelial expression of all three isoforms at many sites between the main renal artery and the afferent arteriole. As in our study (Fig. 11), Cx37 was predominant in smooth muscle. In contrast to our findings in the rat (Fig. 10), staining of Cx37 and Cx40, but not Cx43, was observed in the murine outer medullary vascular bundles. That may be attributable to species variation, because a prior study identified robust expression of Cx43 in rat medulla and vascular bundles, similar to our observations (2, 21). Heavy Cx40 expression in juxtaglomerular cells has been described, however, with minimal expression in smooth muscle of afferent and efferent arterioles near the glomerular vascular poles (29). Modulation of renin secretion may be tied to actions of connexins in granular cells of the afferent arteriole (22, 23).
In summary, we have studied gap junction coupling of DVR pericytes and endothelium. Multiple lines of evidence lead to the conclusion that the endothelium is highly coupled by open gap junctions but that similar coupling of pericytes to one another and to the endothelial layer is inconsistent. The surreptitious nature of gap junction coupling in pericytes makes such efforts difficult to perform. It is possible that depolarizing or hyperpolarizing waves are spread between cells to regulate vasomotion in vivo. Because of the overlying renal cortex, these vessels are inaccessible, so that pertinent measurements may be difficult to obtain. If such waves do propagate along the DVR wall, an interesting, related question concerns the existence and location of a putative pacemaker, possibly in the efferent arterioles or juxtamedullary glomerulus. The possibility that the recently described voltage-operated Na+ channels may participate in such a scheme is worthy of consideration (55). Given the ability of DVR gap junctions to conduct Lucifer yellow (457 Da), it seems reasonable to speculate that small signaling molecules such as cAMP, cGMP, Ca2+, NO, and inositol trisphosphate may transfer between cells to modulate vasoconstriction and function as endothelium-dependent hyperpolarizing factors. Superoxide is generated by DVR pericytes (58) and may be conducted across myoendothelial junctions to limit bioavailability of NO. The physiological roles served by connexons in DVR require extensive studies to define.
These studies have been supported by National Institutes of Health Grants R37 DK-42495, R01 DK-67621, and P01 HL-78870.
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