AJP - Heart Fuel your research with LabChart
HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     

Am J Physiol Heart Circ Physiol 291: H2047-H2056, 2006. First published June 30, 2006; doi:10.1152/ajpheart.00484.2006
0363-6135/06 $8.00
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
291/5/H2047    most recent
00484.2006v1
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in ISI Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via ISI Web of Science (15)
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Haddock, R. E.
Right arrow Articles by Hill, C. E.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Haddock, R. E.
Right arrow Articles by Hill, C. E.

Endothelial coordination of cerebral vasomotion via myoendothelial gap junctions containing connexins 37 and 40

Rebecca E. Haddock,1,2 T. Hilton Grayson,1 Therese D. Brackenbury,1 Kate R. Meaney,1 Craig B. Neylon,3 Shaun L. Sandow,2,* and Caryl E. Hill1,*

1Division of Neuroscience, John Curtin School of Medical Research, Australian National University, Canberra; 2Department of Physiology and Pharmacology, School of Medical Sciences, University of New South Wales, Sydney; and 3Department of Anatomy and Cell Biology and Centre for Neuroscience, University of Melbourne, Parkville, Australia

Submitted 11 May 2006 ; accepted in final form 26 June 2006


   ABSTRACT
TOP
 ABSTRACT
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Control of cerebral vasculature differs from that of systemic vessels outside the blood-brain barrier. The hypothesis that the endothelium modulates vasomotion via direct myoendothelial coupling was investigated in a small vessel of the cerebral circulation. In the primary branch of the rat basilar artery, membrane potential, diameter, and calcium dynamics associated with vasomotion were examined using selective inhibitors of endothelial function in intact and endothelium-denuded arteries. Vessel anatomy, protein, and mRNA expression were studied using conventional electron microscopy high-resolution ultrastructural and confocal immunohistochemistry and quantitative PCR. Membrane potential oscillations were present in both endothelial cells and smooth muscle cells (SMCs), and these preceded rhythmical contractions during which adjacent SMC intracellular calcium concentration ([Ca2+]i) waves were synchronized. Endothelium removal abolished vasomotion and desynchronized adjacent smooth muscle cell [Ca2+]i waves. NG-nitro-L-arginine methyl ester (10 µM) did not mimic this effect, and dibutyryl cGMP (300 µM) failed to resynchronize [Ca2+]i waves in endothelium-denuded arteries. Combined charybdotoxin and apamin abolished vasomotion and depolarized and constricted vessels, even in absence of endothelium. Separately, 37,43Gap27 and 40Gap27 abolished vasomotion. Extensive myoendothelial gap junctions (3 per endothelial cell) composed of connexins 37 and 40 connected the endothelial cell and SMC layers. Synchronized vasomotion in rat basilar artery is endothelium dependent, with [Ca2+]i waves generated within SMCs being coordinated by electrical coupling via myoendothelial gap junctions.

connexin; electron microscopy; endothelial function; potassium channel; membrane potential

VASOMOTION is an intrinsic feature of many arteries and arterioles under normal and pathological conditions and may contribute to regulation of blood flow and pressure (1, 14). Both spontaneous and agonist-induced vasomotion occur when oscillations in the concentration of intracellular calcium ([Ca2+]i) become synchronized among adjacent smooth muscle cells, giving rise to global oscillations in [Ca2+]i across the vessel wall (13, 15, 26, 27, 33, 41, 47–49).

There is clear heterogeneity in the mechanisms that underlie vasomotion, and specifically whether the endothelium plays a mandatory or modulatory role. In the rat iris arteriole, rabbit ear, and superior mesenteric artery, vasomotion is reported to be endothelium independent (3, 18, 39), whereas in the rat mesenteric, rabbit femoral artery, and hamster aorta, vasomotion is suggested to be endothelium dependent, as shown by its abolition with endothelium denudation (12, 21, 34, 38, 40).

Endothelium-dependent effects on vasomotion have been attributed to the vasodilatory factors nitric oxide (NO) and endothelium-derived hyperpolarizing factor (EDHF). In some studies, endothelial cells play an essential role in synchronizing the activity of smooth muscle cells through the release of NO, with endothelium denudation desynchronizing adjacent smooth muscle cell [Ca2+]i oscillations, NO inhibition abolishing vasomotion, and exogenous cGMP activating vasomotion (11, 30, 41). In contrast, in other studies, NO has an apparent inhibitory effect on vasomotion (17, 18, 20, 34, 38, 48, 51, 52). Loss of vasomotion and desynchronization of smooth muscle cell [Ca2+]i oscillations, which mimic endothelium removal, have also been reported in rat mesenteric artery after incubation in the classical EDHF and calcium-activated potassium channel (KCa) blockers apamin and charybdotoxin, thus implying a role for EDHF in vasomotion (8, 34, 38).

Cerebral artery vasomotion occurs in vivo and in vitro (9, 13) and may be integral for regulation of cerebral blood flow. The physiological control of the cerebral circulation differs in many respects from that of other systemic vessels, and mechanisms reliant on changes in membrane voltage play a critical role (7). Thus the hypothesis that the endothelium modulates spontaneous vasomotion of cerebral vessels by direct electrical coupling, rather than by the release of diffusible vasodilators, was investigated in the rat basilar artery.


   MATERIALS AND METHODS
TOP
 ABSTRACT
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
The investigation was conducted under protocols approved by the Animal Experimentation and Ethics Committees of the Australian National University and the University of New South Wales.

Electrophysiology. Male Wistar rats (14–17 days postnatal) were anesthetized with ether and killed by decapitation before removal of the brain into cold dissection buffer containing (in mM) 3 MOPS, 1.2 NaH2PO4, 4.6 glucose, 2 pyruvate, 0.02 NaEDTA, 0.15 albumin, 145 NaCl, 4.7 KCl, 2 CaCl2, and 1.2 MgSO4. The basilar artery and its side branches, in a segment of pial membrane, were pinned via the pia to Sylgard in the base of a recording chamber to secure vessels for electrode impalement and superfused with Krebs solution (3 ml/min, 33–34°C), as described previously (13). Electrophysiological studies were conducted on the primary and secondary branches of the basilar artery. In some vessels the endothelium was removed by rubbing the intimal surface with a tungsten wire before electrical recordings. Endothelial cell damage was confirmed by the absence of vasodilation to acetylcholine (10 µM), while the integrity of the smooth muscle cells was determined by the presence of relaxation to the smooth muscle cell-dependent vasodilator and NO donor S-nitroso-N-acetylpenicillamine (SNAP; 10 µM).

Preparations were equilibrated for 20 min or until spontaneous activity was constant in frequency and amplitude. This spontaneous activity indicated that the in vitro preparations used in the present study mimicked those in vivo, where similar myogenic activity has been previously described in this vascular bed (9). Vessel diameter was continuously monitored using video microscopy (Hanamatsu Performance Vidicon camera) and Diamtrak edge detection program (36); vascular cells were impaled with sharp microelectrodes (120–220 M{Omega}; Flaming Brown micropipette puller, Sutter Instrument) filled with propidium iodide (0.2% in 0.5 M KCl) to confirm cellular identity. Membrane potentials were defined as the most negative values recorded. Records were amplified with an Axoclamp 2B (Axon Instruments). Simultaneous changes in membrane potential and vessel diameter in the region where the cell was impaled were stored for analysis using pClamp software (Axon Instruments).

In some preparations with either intact or damaged endothelium, short segments were cut to 1.3 ± 0.1 mm (n = 28) in length using a microsurgical knife (Sharpoint) to determine input resistance by injection of hyperpolarizing current pulses (0.1–1.0 nA, duration 30–45 s). In these studies, microelectrodes were dipped in silicone, and the fluid level of the organ bath was reduced to a minimum to reduce electrode tip capacitance. Recordings were made in discontinuous current-clamp mode with switching frequencies of 200–500 Hz, and the electrode capacitance was compensated by monitoring the head-stage voltage to ensure that the settling of tip capacitance did not distort the voltage recording.

Changes in [Ca2+]i. Measurement of [Ca2+]i in smooth muscle cells was made after incubation in the ratiometric fluorescent dye fura-2 AM, as described previously (13). To facilitate loading, a section of the pia was removed from over the vessel, resulting in an apparently smaller diameter than that of vessels used for electrophysiology. Changes in [Ca2+]i in the arterial wall were measured with a photometry system (TILL Photonics; pClamp 8 software), while changes in individual smooth muscle cell [Ca2+]i were measured with an intensified cooled CCD (Princeton Instruments; Axon Imaging Workbench, Axon Instruments). Simultaneous measurements of vessel diameter and [Ca2+]i were made by illuminating the preparation with infrared light (775 nm; Hanamatsu Performance Vidicon camera). Measurements of [Ca2+]i were made before and after incubation for 20 min in drugs. Electrophysiological and calcium data were obtained from different preparations.

Quantitative PCR and mRNA expression. The basilar artery and its branches were removed from the meninges and immersed in RNAlater (Ambion). Three samples, each containing vessels from 12 animals, were snap frozen in liquid nitrogen, homogenized, and processed using the RNeasy Mini Kit (Qiagen), including 20 min incubation with DNase, according to the manufacturer's instructions. mRNA was reverse transcribed to cDNA (42°C 1 h, 50°C 1 h, 90°C, 10 min) by using oligo(dT) primers (500 ng/µl, Invitrogen) and Superscript II (200 U/µl, Invitrogen). Reactions from which reverse transcriptase or RNA was omitted were run in parallel to control for contaminating DNA.

Quantitative PCR was used to determine absolute copy numbers of connexins (Cxs) 37, 40, and 43, as previously described (40; ABI Prism 7700 Sequence Detection System). Each experiment included duplicate control reactions containing the corresponding untranscribed RNA sample and water. Expression of all genes was determined in every sample, and the integrity of each PCR reaction checked by using dissociation curve analysis.

For each gene, the absolute mRNA concentration was determined, and to correct for variations in efficiency, the concentration of mRNA was normalized to the number of copies of 18S rRNA, expressed as copies per 106 copies of 18S rRNA.

Immunohistochemistry. Rats were anesthetized (44 mg/kg ketamine and 8 mg/kg xylazine, intraperitoneally) and perfused (60 mmHg) with clearance solution (0.1% NaNO3, 5 U/ml heparin, 0.1% BSA), followed by 2% paraformaldehyde in 0.1 M sodium phosphate buffer. Arteries were removed, stripped of meninges, cut along the longitudinal plane, and pinned out as a flat sheet, intima uppermost. Vessels were preincubated in 2% BSA, 0.2% Triton X-100 in PBS at 22°C (1 h), and further incubated in primary antibody [1:100 for Cx37, Cx40, Cx43, incubation at 37°C for 2 h; 1:2,000 for IK1 (SK4) channels, incubation at 4°C for 48 h] in the same solution. Secondary antibodies were incubated for 1 h at 22°C (Cy3 conjugated anti-rabbit or anti-goat immunoglobulins, 1:100; Jackson Immunoresearch Laboratories) in 0.01% Triton X-100 in PBS, and vessels were mounted in buffered glycerol. IK1 (SK4) antibodies were raised in rabbits against amino acids 2–17 of rat (37) and antibodies against rat Cx37 and Cx40 raised in sheep (42, 44). A characterized commercial anti-rat Cx43 (Zymed) antibody raised in rabbit was also used. Specificity of the IK1 (IK38/6), Cx37, Cx40, and Cx43 antibodies has been determined previously by Western blot and immunolabeling of transfected cells (37, 42, 44).

Image series were taken at 1-µm intervals from the luminal surface of the endothelium through the internal elastic lamina and into the muscle (TCS 4D confocal microscope, Leica Instruments). Sequential images were recombined to create a single image incorporating all of the smooth muscle cell or endothelial cell labeling, above or below the focus of the internal elastic lamina, respectively (ScanWare, Leica). Individual sections within the internal elastic lamina near the inner smooth muscle cell membrane were recombined with the same sections viewed at 488-nm excitation to show the autofluorescent internal elastic lamina. Samples were prepared from four different animals.

Serial section and immunoelectron microscopy. Rats were anesthetized (as above or 3 g/kg urethane ip), cleared, and perfusion fixed in 3% glutaraldehyde in 0.1 M sodium cacodylate, with 35 mM betaine, 0.2 mM CaCl2, and 0.15 M sucrose, pH 7.4, and short segments of artery were processed for electron microscopy (46). Serial transverse sections were cut over ~5 µm of vessel length (n = 6 animals). The vessel circumference was estimated from low-magnification micrographs (x2,500), as the length of the internal elastic lamina. The number of smooth muscle cell profiles was determined as the average along four linear plots 90° apart, from the outer edge of the internal elastic lamina to the adventitia. To detect myoendothelial gap junctions, the internal elastic lamina in each serial section was examined at x10,000, and all myoendothelial gap junctions were photographed at high magnification (x20,000 to x40,000) and identified according to their characteristic pentalaminar membrane structure (35, 46). The number of myoendothelial gap junctions per endothelial cell was determined from the surface area of the arterial segment at the level of the internal elastic lamina, the surface area of endothelial cells, and the number of myoendothelial gap junctions present in this region. Endothelial cell size was determined from immunohistochemical preparations, as described previously (43).

For high-resolution antigen localization studies, segments of basilar artery from four rats were frozen at high pressure (BAL TEC, HPM 010 or Leica EM HPF; ~2,100 bar), freeze-substituted (Leica, AFS; –90°C) in 0.1% uranyl acetate in acetone over 4 days, infiltrated, and embedded in LR gold at –25°C polymerized under UV light. Individual serial thin transverse sections were mounted on Formvar- and carbon-coated slot grids and incubated in 1% normal donkey serum/BSA, 0.2% Tween-20 in PBS (30 min), followed by rabbit anti-rat Cx37 (ADI), rabbit anti-mouse Cx40 (Chemicon), rabbit anti-rat Cx43 (Zymed) or mouse anti-smooth muscle {alpha}-actin (Sigma) in blocking buffer (18 h at 37°C or 4°C), and followed by 5 nm colloidal gold-conjugated secondary antibody (1:40; British Biocell; 2 h) in 0.01% Tween-20. Specificity of Cx antibodies has been previously demonstrated by using Western blotting and immunohistochemistry on tissues and transfected cells (42, 44). Sections were treated with 1% glutaraldehyde in PBS and stained conventionally.

Drugs and solutions. The following drugs were obtained commercially: apamin, charybdotoxin, ACh, and SNAP (Sigma Chemical), NG-nitro-L-arginine methyl ester (L-NAME; Sapphire Bioscience), fura-2 AM and pluronic acid (Molecular Probes), N2,2'-O-dibutyryl-cGMP sodium salt (DBcGMP, Alexis Biochemicals). Charybdotoxin was dissolved in PBS containing 0.1% BSA. Cx-mimetic peptides 40Gap27 and 37,43Gap27 (SRPTEKNVFIV, SRPTEKTIFII, respectively) were synthesized by the Australian Cancer Research Foundation Biomolecular Resource Facility, John Curtin School of Medical Research; purity >97%. All other drugs were made up as x1,000 stock solutions in distilled water and diluted into Krebs solution.

Analysis of results. Frequency of depolarizations or contractions in both control and drug solutions was determined over 5 min, while the amplitude was the average of 15 consecutive responses. Changes in [Ca2+]i are expressed as the ratio of the fluorescence emission recorded in response to 340 nm and 380 nm (F340/380) excitation, whereby the F340/380 in control is defined as 100%. Results are means ± SE of n preparations where each preparation was from a different rat. Data analysis and graphs were prepared with GraphPad Prism (GraphPad Software). Results were analyzed for statistical significance (P < 0.05) by using paired or unpaired t-tests as appropriate.


   RESULTS
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Rhythmic activity in dye-identified cells. Microelectrode recordings from a propidium iodide-identified endothelial cell (Fig. 1A) and smooth muscle cell (Fig. 1B) showed that during spontaneous vasomotion, rhythmical depolarizations were present in both cell types, and these preceded rhythmical contractions (Fig. 1, C and D, respectively). No difference was observed in the resting membrane potential between the two cell types when impalements were made in the same preparation (endothelial cell –45 mV; smooth muscle cell –45 mV, n = 1). A single recording was made from an identified endothelial cell in a total of 32 stable impalements in intact vessels.


Figure 1
View larger version (69K):
[in this window]
[in a new window]
  		Fig. 1. Rhythmical activity in propidium iodide identified endothelial cells (A) and smooth muscle cells (SMCs; B), with dashed line (A and B) indicating vessel edge. Longitudinal vessel axis, left to right. Membrane potential oscillations were recorded in both endothelial cells (C) and smooth muscle cells (D) and preceded peak contractions, with dashed vertical line indicating the same temporal point. Arrows point to cell nuclei. Bar, 20 µm.

 
Endothelium removal. Endothelium removal tended to depolarize smooth muscle cell membrane potential (+endothelium: –42.2 ± 0.9 mV, n = 20, –endothelium: –39.9 ± 0.7 mV, n = 20, unpaired t-test; P > 0.05), and rhythmical depolarizations were decreased in amplitude (+endothelium: 6.3 ± 0.7 mV, n = 20; –endothelium: 3.6 ± 0.2 mV, n = 20; P < 0.05, unpaired t-test) and increased in frequency (Fig. 2A; +endothelium: 16.2 ± 1.0 min–1, n = 20; –endothelium: 31.2 ± 1.7 min–1; n = 20; P < 0.05, unpaired t-test). Endothelium denudation led to loss of coordinated rhythmical contractions (Fig. 2, A and B) without significant effect on vascular tone (+endothelium: 45.9 ± 2.2 µm, n = 53; –endothelium: 50.7 ± 2.8 µm, n = 40, unpaired t-test), although measurements were made in different vessels.


Figure 2
View larger version (21K):
[in this window]
[in a new window]
  		Fig. 2. Influence of the endothelium on rhythmical activity. Rhythmical depolarizations and contractions (A) and calcium oscillations and contractions in the arterial wall (B) and in individual SMCs (C; n = 6 cells), recorded from either endothelium-intact (+endothelium; left) or different endothelium-denuded (–endothelium; right) preparations. Upward deflection indicates increased intracellular Ca2+ concentration ([Ca2+]i). Basal SMC [Ca2+]i levels in endothelium-intact preparations and endothelium-denuded preparations were 0.64 F340/380 and 0.52 F340/380, respectively, where F340/380 is the ratio of the fluorescence emission recorded in response to 340 nm and 380 nm excitation.

 
Calcium oscillations were smaller and irregular with endothelium removal, although no significant change in basal calcium levels occurred (Fig. 2B; +endothelium: 0.53 ± 0.026 F340/380, n = 33; –endothelium: 0.53 ± 0.017 F340/380, n = 20, unpaired t-test). Smooth muscle cell imaging showed that oscillations in [Ca2+]i were still present in individual cells, but these were asynchronous with neighboring cells (Fig. 2C).

Application of hyperpolarizing current pulses to short arterial segments showed that smooth muscle cell input resistance was significantly greater in endothelium-denuded vessels (+endothelium: 5.2 ± 0.9 M{Omega}, n = 12; –endothelium: 11.7 ± 0.9 M{Omega}, n = 16; P < 0.05, unpaired t-test).

Confirmation of endothelium removal and integrity of smooth muscle cells. In endothelium-intact preparations, ACh (10 µM) hyperpolarized the smooth muscle (control: –42.2 ± 0.9 mV; ACh: –51.7 ± 1.7 mV; n = 20; P < 0.05, paired t-test), decreased basal calcium levels in the arterial wall (ACh: 89.9 ± 0.1% of control F340/380; n = 33, P < 0.05, paired t-test), abolished vasomotion, and caused the vessel to relax (control: 45.9 ± 2.2 µm; ACh: 50.0 ± 2.2 µm; n = 53; P < 0.05, paired t-test). In contrast, in endothelium-denuded preparations, ACh had no significant effect on smooth muscle cell membrane potential (control: –39.9 ± 0.8 mV; ACh: –39.0 ± 1.0 mV; n = 20, P > 0.05, paired t-test), basal calcium levels in the arterial wall were increased (ACh: 109.5 ± 0.5% of control F340/380, n = 20, P < 0.05, paired t-test), and a small but significant constriction was observed (control: 50.7 ± 2.8 µm; ACh: 49.9 ± 2.8 µm; n = 40; P < 0.05, paired t-test). These results confirmed successful removal of the endothelium because vasodilation following the addition of ACh was abolished (P < 0.05, unpaired t-test). ACh-induced vasoconstriction in endothelium-denuded vessels confirmed the integrity of the smooth muscle because similar responses have been described in the cerebral, coronary, mesenteric, and renal circulation under conditions in which the endothelium has either been removed or has been shown to be dysfunctional (10, 28).

In endothelium-intact preparations, the effects of SNAP on membrane potential (SNAP: –52.0 ± 1.3 mV, n = 20, paired t-test), basal calcium levels (SNAP: 91.1 ± 0.3% of control F340/380, n = 33, paired t-test), or vessel diameter (SNAP: 50.2 ± 2.2 µm, n = 53, paired t-test) were indistinguishable from ACh. In endothelium-denuded preparations, SNAP hyperpolarized the smooth muscle cells (SNAP: –51.1 ± 1.2 mV; n = 20; P < 0.05, paired t-test), decreased basal calcium levels in the arterial wall (SNAP: 91.0 ± 1.7% of control F340/380; n = 20; P < 0.05, paired t-test), and caused a significant relaxation (SNAP: 53.8 ± 2.8 µm; n = 40; P < 0.05, paired t-test). These effects were indistinguishable from those of SNAP in intact preparations, providing further confirmation of the integrity of the smooth muscle cells.

Role of NO. Endothelium denudation did not mimic inhibition of NO synthase with L-NAME (10 µM; Fig. 3). L-NAME increased the frequency (control: 15.4 ± 0.7 min–1; L-NAME: 19.6 ± 0.9 min–1; n = 8; P < 0.05, paired t-test; Fig. 3A) and amplitude of rhythmical depolarizations (control: 5.3 ± 1.1 mV; L-NAME: 9.4 ± 1.0 mV; n = 4; P < 0.05, paired t-test; Fig. 3A), contractions (control: 3.3 ± 0.4% resting vessel diameter; L-NAME: 5.8 ± 0.5% resting vessel diameter; n = 8; P < 0.05, paired t-test; Fig. 3, A and B), arterial wall [Ca2+]i oscillations (L-NAME: 153.0 ± 3.3% of amplitude of control F340/380 oscillation; n = 4; P < 0.05, paired t-test; Fig. 3B) and individual smooth muscle cell [Ca2+]i (Fig. 3C). L-NAME decreased vessel diameter (control: 46.9 ± 3.9 µm; L-NAME: 44.9 ± 3.5 µm; n = 8; P < 0.05, paired t-test; Fig. 3, A and B), without significant effect on membrane potential (control: –40.5 ± 0.5 mV; L-NAME: –39.5 ± 2.5 mV; n = 4, paired t-test; compare in Fig. 3A) or arterial wall basal calcium levels (L-NAME: 104 ± 2.9% of control F340/380, n = 4, paired t-test; Fig. 3B). Moreover, in endothelium-denuded preparations in which vasomotion was disrupted and oscillations in [Ca2+]i in adjacent smooth muscle cells were asynchronous, addition of DBcGMP (300 µM) did not restore rhythmicity (Fig. 4).


Figure 3
View larger version (24K):
[in this window]
[in a new window]
  		Fig. 3. Effect of nitric oxide synthase (NOS) inhibition on spontaneous activity. The NOS inhibitor NG-nitro-L-arginine methyl ester (L-NAME; 10 µM) increased the frequency and amplitude of rhythmical depolarizations (A) and contractions (A and B) and intracellular Ca2+ concentration ([Ca2+]i) oscillations in the arterial wall (B). Oscillations in individual SMC [Ca2+]i were more synchronized (C). Upward deflection indicates increased [Ca2+]i. The representative control basal calcium level in the arterial wall was 0.73 F340/380. Dashed horizontal lines are a visual aid at the same comparative point for comparing left and right column data.

 

Figure 4
View larger version (24K):
[in this window]
[in a new window]
  		Fig. 4. Effect of DBcGMP (300 µM) on rhythmical activity in the absence of the endothelium. In endothelium-denuded preparations, incubation in DBcGMP (300 µM) had no significant effect on rhythmical depolarization and SMC membrane potential (A, top) or small contractions and vessel diameter (A, bottom). Basal calcium levels and the small irregular calcium oscillations observed in the arterial wall were also not different from control (B). Calcium oscillations in adjacent SMCs remained unsynchronized (C; n = 6 cells). Upward deflection indicates increased [Ca2+]i. The basal arterial wall [Ca2+]i level in control was 0.44 F340/380. Dashed horizontal lines are a visual aid at the same comparative point for comparing left and right column data.

 
Role of EDHF. Apamin (0.5 µM) and charybdotoxin (60 nM) caused smooth muscle cell depolarization (control: –44.6 ± 3.5 mV; apamin + charybdotoxin: –27.8 ± 2.2 mV; n = 4; P < 0.05, paired t-test; Fig. 5A), vessel constriction (control: 65.8 ± 5.6 µm; apamin + charybdotoxin: 52.3 ± 5.2 µm; n = 4; P < 0.05, paired t-test), and the development of irregular uncoordinated contractions (Fig. 5, A and B). Rhythmical depolarizations were increased in frequency (control: 21.5 ± 3.5 min–1; apamin + charybdotoxin: 43.5 ± 8.4 min–1; n = 4; P < 0.05, paired t-test) and amplitude (control: 2.7 ± 0.5 mV; apamin + charybdotoxin: 8.8 ± 2.2 mV; n = 4; P < 0.05, paired t-test; Fig. 5A). Oscillations in [Ca2+]i in the arterial wall became irregular (Fig. 5B), and in adjacent smooth muscle cells, oscillations in [Ca2+]i were reduced in amplitude (P < 0.05) and unsynchronized (Fig. 5C). Similar results on vessel tone (–endothelium: 64.2 ± 3.1 µm; apamin + charybdotoxin: 52.8 ± 4.8 µm; n = 4; P < 0.05, paired t-test), resting membrane potential (–endothelium: –37.2 ± 1.1 mV; apamin + charybdotoxin: –27.5 ± 0.6 mV; n = 4; P < 0.05, paired t-test), and rhythmical depolarization frequency (–endothelium: 31.0 ± 1.2 min–1; apamin + charybdotoxin: 51.0 ± 3.5 min–1; n = 4; P < 0.05, paired t-test) and amplitude (–endothelium: 4.2 ± 0.3 mV; apamin + charybdotoxin: 10.2 ± 0.8 mV; n = 4; P < 0.05, paired t-test) were found in endothelium-denuded preparations, suggesting that the effect of the toxins was on smooth muscle cell KCa.


Figure 5
View larger version (40K):
[in this window]
[in a new window]
  		Fig. 5. Effect of combined apamin (0.5 µM) and charybdotoxin (60 nM) (Apa/ChTx) on basilar artery vasomotion and conventional immunohistochemistry of IK1 (SK4) expression. Small-conductance (SKCa) and intermediate/large-conductance Ca2+-activated potassium channel (I/BKCa) inhibition with apamin and charybdotoxin (ChTx) increased rhythmical depolarization frequency and amplitude and depolarized membrane potential (A). Arterial wall [Ca2+]i oscillations became irregular (B); rhythmic contractions were reduced, and vessel movement became irregular (A and B). [Ca2+]i oscillations recorded in individual adjacent SMCs became asynchronous (C; n = 6 cells). Upward deflection indicates increased [Ca2+]i. The representative basal calcium level in control is 0.44 F340/380. Dashed horizontal lines are a visual aid at the same comparative point for comparing left and right column data. Whole mount IK1 (SK4) localization, indicative of IKCa, was found in smooth muscle (D, left) and endothelial cells (EC; D, right). Smooth muscle and endothelial images are of the same field of view but from different focal planes. No staining was found when the primary antibody was omitted from the incubation solution (insets). Longitudinal vessel axis runs left to right. Bar, 25 µm.

 
Because apamin and charybdotoxin block small (SKCa)-, intermediate (IKCa)-, and large-conductance KCa (BKCa), and voltage-gated potassium (Kv) channels, and our previous electrophysiological studies showed similar effects with IKCa inhibition, but no effect of individual inhibition of either SKCa, BKCa, or Kv (13), the distribution of IKCa protein was investigated using immunohistochemistry. Localization of IK1 (SK4), indicative of IKCa, was found in both smooth muscle and endothelial cells (Fig. 5D, left and right, respectively), while staining was absent when the primary antibody was omitted (Fig. 5, insets).

Effect of gap junction uncouplers. 37,43Gap27 (100 µM; n = 12) abolished rhythmical depolarizations, contractions (Fig. 6A), and oscillations in [Ca2+]i in the arterial wall and in individual smooth muscle cells (Fig. 6, B and C, respectively). Smooth muscle cells hyperpolarized (control: –42.8 ± 2.3 mV; 37,43Gap27: –54.3 ± 2.8 mV; n = 4; P < 0.05, paired t-test), and the vessels relaxed (control: 37.6 ± 4.6 µm; 37,43Gap27: 41.8 ± 4.8 µm; n = 12; P < 0.05, paired t-test).


Figure 6
View larger version (20K):
[in this window]
[in a new window]
  		Fig. 6. Effect of 37,43Gap27 on rhythmical activity. 37,43Gap27 (100 µM) hyperpolarized SMCs and abolished rhythmical depolarizations, contractions (A), and [Ca2+]i oscillations (B) in the arterial wall. Basal [Ca2+]i was reduced and the vessel relaxed. [Ca2+]i oscillations in individual SMCs were abolished (C; n = 6 cells). Upward deflection indicates increased [Ca2+]i. Basal [Ca2+]i in the arterial wall was 0.64 F340/380. Dashed horizontal lines are a visual aid at the same comparative point for comparing left and right column data.

 
40Gap27 (100 µM) also abolished vasomotion but did not hyperpolarize or significantly relax the arteries (Fig. 7, A and B; control: –38.7 ± 1.9 mV; 40Gap27: –39.4 ± 1.3 mV; n = 4; control: 31.9 ± 3.5 µm; 40Gap27: 32.7 ± 4.3 µm; n = 8). Rhythmical depolarizations and individual smooth muscle cell [Ca2+]i oscillations were significantly reduced in amplitude (P < 0.05, paired t-test) and were no longer synchronized (Fig. 7, A and C).


Figure 7
View larger version (23K):
[in this window]
[in a new window]
  		Fig. 7. Effect of 40Gap27 on rhythmical activity. 40Gap27 (100 µM) abolished vasomotion, reduced rhythmical depolarizations (A), and abolished [Ca2+]i oscillations in the arterial wall (B). [Ca2+]i oscillations in adjacent SMCs were reduced in amplitude and asynchronous (C; n = 6 cells). Basal [Ca2+]i in the arterial wall was 0.48 F340/380. Dashed horizontal lines are a visual aid at the same comparative point for comparing left and right column data.

 
Connexins and endothelial and myoendothelial gap junctions. Uniform punctate Cx37 was detected by immunohistochemistry in the media (Fig. 8A). In contrast, Cx40 was absent, and Cx43 was only detected in the cytoplasm of occasional smooth muscle cells (Fig. 8, B and C, respectively). Cx37, Cx40, and Cx43 were detected at adjacent endothelial cell borders (Fig. 8, D–I and K–M). Pentalaminar membrane, characteristic of gap junctions, was present between adjacent endothelial cells (Fig. 8, J and N).


Figure 8
View larger version (143K):
[in this window]
[in a new window]
  		Fig. 8. Conventional and high-resolution immunohistochemistry of endothelial connexin expression. Whole mounts were labeled with antibodies against connexin 37 (Cx37) (A and D), Cx40 (B and E), and Cx43 (C and F), and gray-scale confocal stack images inverted to black on white. Cx37 (A) was weakly expressed in the smooth muscle, while Cx40 (B) and Cx43 (C) were not uniformly detected; cells expressing Cx43 throughout the cytoplasm were detected at low frequency within the SMC layers (C, arrow). Cx37, Cx40, and Cx43 (D–F, respectively) were expressed at the junctions between endothelial cells. The longitudinal axis of the arteries runs left to right. High-resolution ultrastructural immunohistochemistry confirmed the expression of Cx 37, Cx40, and Cx43 conjugated to 5-nm gold (white arrowheads in K–M) at adjacent endothelial borders (black arrows in G, H, and I). Conventional electron microscopy confirmed the presence of the pentalaminar structure between adjacent endothelial cells (white arrows, J), characteristic of gap junction ultrastructure (J and N) (32, 35, 46). Boxes in G–J correspond to the same region at high magnification in K–N, for each respective pair of vertical panels (G and K; H and L; I and M; J and N, respectively). Bar: A–F, 25 µm; G–J, 100 nm, K–N, 50 nm.

 
Confocal imaging of Cx37- and Cx40-labeled tissue at the internal elastic lamina-smooth muscle cell interface suggested the presence of Cx37 and Cx40 but not Cx43 at these sites (Fig. 9, A–D). High-resolution ultrastructural labeling confirmed this distribution of myoendothelial Cxs (Fig. 10).


Figure 9
View larger version (124K):
[in this window]
[in a new window]
  		Fig. 9. Conventional immunohistochemistry of myoendothelial connexin expression. Confocal identification of whole mounts stained with Cx37 (A and B) and Cx40 (C and D) antibody. Single confocal images at the internal elastic lamina (IEL)-SMC interface showed punctate labeling, which, when overlayed with IEL autofluorescence, corresponded with IEL holes shown as dark spots (B and D, for Cx37 and Cx40, respectively; examples with arrows). Cx43 was not observed at this location (data not shown). Bar: A–D, 20 µm.

 

Figure 10
View larger version (166K):
[in this window]
[in a new window]
  		Fig. 10. High-resolution immunohistochemistry of myoendothelial connexin expression. High-pressure frozen, freeze-substituted vessels showed good preservation with no shrinkage around the IEL (A) compared with tissue prepared with conventional ultrastructural methods (B and C). Schwann cells (sc) surrounded perivascular varicosities (v) containing synaptic vesicles (A, inset). Myoendothelial gap junctions (MEGJs) showed pentalaminar membrane in conventional (B and C; asterisk and inset between arrows in C) and high-pressure frozen tissue (D–F, between arrows). Pentalaminar EC-EC gap junctions (C, between arrowheads; F, left inset) were found close to MEGJs. Gold-conjugated antibodies against Cx37 and Cx40 were localized to MEGJs (D and inset; F and right inset). Incubation of the adjacent serial section to that labeled with Cx40-gold in the absence of antibody showed no gold labeling (E and E, inset). Cx43 was not observed at MEGJs. Bar: A–F and A, inset, 1 µm; C–F, inset, 50 nm.

 
The media of the main side branch of the basilar artery consisted of two to three smooth muscle cell layers (2.4 ± 0.2, n = 6, Fig. 10, A and B). Serial sections through 5-µm-long vessel segments contained myoendothelial gap junctions (Fig. 10, B–F) and homocellular endothelial cell gap junctions (Fig. 8, J and N). All myoendothelial gap junctions were characterized by the presence of pentalaminar membrane structures between endothelial cells and smooth muscle cells (Fig. 8, C–F, inset). Myoendothelial gap junction density was 3.2 ± 0.9 per endothelial cell (n = 6; mean endothelial cell size 388 ± 18.6 µm2, n = 6).

The ultrastructural integrity of the vessel wall was well maintained in tissue prepared for high-resolution antigen studies (Fig. 10, A and D–F), with pentalaminar membrane, characteristic of gap junctions, found between adjacent endothelial cells. No subendothelial or sub-smooth muscle space adjacent to the internal elastic lamina was present, in contrast to conventionally prepared tissue (Fig. 10A; compare with Fig. 10, B and C, respectively). Controls conducted on serial sections that were exposed to either primary antibody preincubated in antigenic peptide or to secondary antibody alone showed no specific gold label (Fig. 10E, inset).

As in conventionally prepared tissue (Fig. 10, B and C), endothelial cell-derived projections were found to abut smooth muscle cells (Fig. 10, D–F). At these points of close association, small regions of pentalaminar membrane were present, and Cx37- and Cx40-conjugated gold label, but not Cx43-conjugated gold, was localized (Fig. 10, D and F). These sites were typical of myoendothelial gap junctions found in arteries using conventional ultrastructural methods (compare with Fig. 10, B and C).

mRNA for Cx37, Cx40, and Cx43 was detected in the basilar artery, with Cx37 expression being 20- and 60-fold higher than Cx40 and Cx43, respectively (Cx mRNA expression: Cx37, 38,381 ± 5,534; Cx40, 2,218 ± 605; Cx43, 607 ± 115, as normalized mRNA copy number/106 copies of 18S rRNA; n = 3 RNA samples).


   DISCUSSION
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
In the primary branch of the rat basilar artery, the present data show that the endothelium plays an essential role in initiating vasomotion by synchronizing [Ca2+]i oscillations among adjacent smooth muscle cells. This effect is not mediated by either NO or EDHF but rather by coupling of the endothelium and smooth muscle by myoendothelial gap junctions consisting of Cx37 and Cx40. These junctions enable electrical coupling between the two cell layers and facilitate the synchronization of vasomotor activity along the vessel length.

A similar loss of vasomotion and desynchronization of adjacent smooth muscle cell [Ca2+]i oscillations has been reported in rat mesenteric artery after endothelial denudation. This was attributed to loss of endothelium-derived NO and failure to activate a cGMP-dependent depolarizing current essential for the initiation of agonist-induced vasomotion in this vessel (11, 41). In contrast, in the present study, incubation with the NO synthase inhibitor L-NAME augmented vasomotion of the basilar artery and improved the synchronization of [Ca2+]i oscillations in individual smooth muscle cells, consistent with previous studies of cerebral artery vasomotion (5, 17, 24). Furthermore, a cGMP-activated depolarizing current is unlikely to be important for initiating vasomotion in the basilar artery because the smooth muscle membrane potential was not altered by endothelium removal or inhibition of NO. In addition, application of DBcGMP to endothelium-denuded preparations failed to resynchronize adjacent smooth muscle cell [Ca2+]i oscillations or restore vasomotion.

EDHF was also not responsible for the initiation of vasomotion in the basilar artery. While incubation with apamin and charybdotoxin did result in loss of regular contractions and appearance of asynchronous smooth muscle cell [Ca2+]i oscillations, these effects were accompanied by significant depolarization and constriction, an effect similar to that found previously after individual inhibition of IKCa but not BKCa, SKCa, or Kv (13). Because apamin and charybdotoxin produced the same effect in the absence of the endothelium, an action at IKCa in the smooth muscle is likely, and, indeed, IKCa is present in the media of the basilar artery, as shown in the present study, and in other cerebral vessels (35). Thus the loss of basilar artery vasomotion after KCa inhibition can be attributed simply to an increase in smooth muscle cell [Ca2+]i after membrane depolarization, leading to augmented vasoconstriction and a reduction in the amplitude and synchronization of oscillatory behavior of smooth muscle cells. The modeling of Koenigsberger et al. (23) suggests that when [Ca2+]i is low or high, smooth muscle cells may be in a steady state, while between these extremes they may exhibit calcium oscillations. Thus any effect that results in an increase in mean calcium levels may reduce or abolish oscillatory behavior by movement toward a more stable state. In the present study, this effect followed closure of smooth muscle IKCa, rather than release of EDHF from the endothelium.

The electrophysiological demonstration of increased smooth muscle cell input resistance in endothelium-denuded preparations and similar voltage oscillations in dye-identified endothelial and smooth muscle cells provide evidence that the two cell layers of the basilar artery are electrically coupled. The anatomic data confirm the presence of extensive myoendothelial gap junctions composed of Cx37 and Cx40. At the mRNA level, Cx37 was the predominant Cx expressed in the basilar artery, with these latter data being consistent with the extensive Cx37 protein expression among endothelial cells and weak Cx37 expression in smooth muscle cells in this and previous studies (19). The absence of Cx40 and Cx43 in smooth muscle, but presence of both Cxs in the endothelium (19), suggests that there may be greater potential for intimal than medial coupling in the basilar artery. Interestingly, at the ultrastructural level in the media of muscular arteries, gap junctions are sparse and small (45, 46), implying that the potential for control of the synchronization of smooth muscle cells within the media alone is limited.

The data of the present study suggest that cell coupling through the endothelium might play a critical role in the generation of basilar artery vasomotion by synchronizing smooth muscle cell activity. While previous studies have pointed to the involvement of gap junctions in vasomotion in a number of vascular beds through the use of putative gap junction blockers, such as heptanol, octanol, and 18beta-glycyrrhetinic acid (2, 22, 31, 48), these inhibitors have been shown to exert additional nonspecific effects (3, 4, 16, 31, 50, 53). Peptides mimicking segments of the amino acid sequence of the extracellular loops of Cx proteins have also been used to examine the gap junctional dependence of vasomotion in rabbit superior mesenteric artery (3). The involvement of gap junctions in basilar artery vasomotion was examined in a similar manner using the Cx-mimetic peptides 37,43Gap27 and 40Gap27, with both peptides abolishing vasomotion and 40Gap27 desynchronizing adjacent smooth muscle cell [Ca2+]i oscillations, in a similar manner to endothelium removal. However, the peptides also reduced [Ca2+]i oscillations in smooth muscle cells, and 37,43Gap27 hyperpolarized the membrane, effects not readily explained by an action on gap junctions alone.

The apparent nonjunctional effects of 37,43Gap27 and 40Gap27 in the basilar branch are similar to nonjunctional effects of heptanol and glycyrrhetinic acid in rat mesenteric artery (31). Interestingly, hyperpolarization, relaxation, and decreased wall [Ca2+]i in pressurized mesenteric and cerebral arteries incubated in 37,43Gap27 or glycyrrhetinic acid were attributed to heterogeneous responses of individual smooth muscle cells to exogenous stimuli, cell coupling thus facilitating a uniform response throughout the muscle (6, 25). Nonspecific effects were discounted due to the failure of gap junction antagonists to affect agonist- or depolarization-induced vasoconstriction (6, 25), although an effect on hemichannels cannot be ruled out (29). Unfortunately, other than the technically difficult method of pinocytically loading endothelial cells with Cx antibodies (32), no other selective antagonists for gap junctions are currently available.

It should be noted that the arteries used in the present study were stretched and pinned to the bottom of the recording chamber. These conditions enabled us to continuously monitor activity in the same cell over extended periods of time despite the oscillating vessel diameter and changes in tension after drug additions. However, caution should be exercised when extrapolating our results to the in vivo state because the arterial segments were not intraluminally perfused. Nevertheless, even under these conditions, the vessels exhibited spontaneous vasomotion as described in vivo (9), and the smooth muscle cell membrane potentials in our vessels were depolarized to a similar extent as pressurized vessels in vitro (6).

The present data support the concept that there is considerable heterogeneity in the mechanisms that underlie vasomotion in different segments of the vasculature. While the endothelium is essential for vasomotion in both the mesenteric and basilar artery, in the former the role of the endothelium is to produce vasodilatory factors to synchronize smooth muscle cell activity (34, 38, 41). In contrast, in the basilar artery these factors do not initiate vasomotion, but rather the endothelium facilitates current spread along the vascular wall by indirectly coupling smooth muscle cells through myoendothelial gap junctions composed of Cx37 and Cx40. Thus the endothelium acts to coordinate voltage changes in individual smooth muscle cells and synchronize calcium fluxes through voltage-dependent calcium channels, which are responsible for the coordination of smooth muscle cell [Ca2+]i oscillations (13).


   ACKNOWLEDGMENTS
 
This work was supported by grants from the National Heart Foundation of Australia and National Health and Medical Research Council (NHMRC) to C. E. Hill and T. H. Grayson. S. L. Sandow was supported by an NHMRC RD Wright Fellowship.


   FOOTNOTES
 

Address for reprint requests and other correspondence: C. E. Hill, Div. of Neuroscience, John Curtin School of Medical Research, Australian National Univ., Canberra, 2601 ACT Australia (e-mail: caryl.hill{at}anu.edu.au)

The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.

* S. L. Sandow and C. E. Hill contributed equally to this study. Back


   REFERENCES
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Aalkjaer C and Nilsson H. Vasomotion: cellular background for the oscillator and for the synchronization of smooth muscle cells. Br J Pharmacol 144: 605–616, 2005.[CrossRef][ISI][Medline]
  2. Bonnet S, Hyvelin JM, Bonnet P, Marthan R, and Savineau JP. Chronic hypoxia-induced spontaneous and rhythmic contractions in the rat main pulmonary artery. Am J Physiol Lung Cell Mol Physiol 281: L183–L192, 2001.[Abstract/Free Full Text]
  3. Chaytor AT, Evans WH, and Griffith TM. Peptides homologous to extracellular loop motifs of connexin 43 reversibly abolish contractile activity in rabbit arteries. J Physiol 503: 99–110, 1997.[Abstract/Free Full Text]
  4. Coleman HA, Tare M, and Parkington HC. K+ currents underlying the action of endothelium-derived hyperpolarizing factor in guinea-pig and human blood vessels. J Physiol 531: 359–373, 2001.[Abstract/Free Full Text]
  5. Dirnagl U, Lindhauer U, and Villringer A. Nitric oxide synthase blockade enhances vasomotion in the cerebral microcirculation of anesthetized rats. Microvasc Res 45: 318–323, 1993.[CrossRef][ISI][Medline]
  6. Earley S, Resta TC, and Walker BR. Disruption of smooth muscle gap junctions attenuates myogenic vasoconstriction of mesenteric resistance arteries. Am J Physiol Heart Circ Physiol 287: H2677–H2686, 2004.[Abstract/Free Full Text]
  7. Faraci FM and Heistad DD. Regulation of the cerebral circulation: role of endothelium and potassium channels. Physiol Rev 78: 53–97, 1998.[Abstract/Free Full Text]
  8. Faraci FM, Lynch C, and Lamping KG. Responses of cerebral arterioles to ADP: eNOS-dependent and eNOS-independent mechanisms. Am J Physiol Heart Circ Physiol 287: H2871–H2876, 2004.[Abstract/Free Full Text]
  9. Fujii K, Heistad DD, and Faraci FM. Ionic mechanisms in spontaneous vasomotion of the rat basilar artery in vivo. J Physiol 430: 389–398, 1990.[Abstract/Free Full Text]
  10. Ge ZD, Zhang DX, Chen YF, Yi FX, Zou AP, Campbell WB, and Li PL. Cyclic ADP-ribose contributes to contraction and Ca2+ release by M1 muscarinic receptor activation in coronary arterial smooth muscle. J Vasc Res 40: 28–36, 2003.[CrossRef][ISI][Medline]
  11. Gustafsson H. Vasomotion and underlying mechanisms in small arteries. An in vitro study of rat blood vessels. Acta Physiol Scand 614: 1–44, 1993.
  12. Gustafsson H, Mulvany MJ, and Nilsson H. Rhythmic contractions of isolated small arteries from rat: influence of the endothelium. Acta Physiol Scand 148: 153–163, 1993.[ISI][Medline]
  13. Haddock RE and Hill CE. Differential activation of ion channels by inositol 1,4,5-trisphosphate (IP3)- and ryanodine-sensitive calcium stores in rat basilar artery vasomotion. J Physiol 545: 615–627, 2002.[Abstract/Free Full Text]
  14. Haddock RE and Hill CE. Rhythmicity in arterial smooth muscle. J Physiol 566: 645–656, 2005.[Abstract/Free Full Text]
  15. Haddock RE, Hirst GD, and Hill CE. Voltage independence of vasomotion in isolated irideal arterioles of the rat. J Physiol 540: 219–229, 2002.[Abstract/Free Full Text]
  16. Hashitani H and Suzuki H. K+ channels which contribute to the acetylcholine-induced hyperpolarization in smooth muscle of the guinea-pig submucosal arteriole. J Physiol 501: 319–329, 1997.[Abstract/Free Full Text]
  17. Hempelmann RG, Pradel RH, Mehdom HM, and Ziegler A. Contractions induced by NO synthase inhibition in isolated rat basilar artery: role of the endothelium and endogenous vasoconstrictors. Neurol Res 20: 63–72, 1998.[ISI][Medline]
  18. Hill CE, Eade J, and Sandow SL. Mechanisms underlying spontaneous rhythmical contractions in irideal arterioles of the rat. J Physiol 521: 507–516, 1999.[Abstract/Free Full Text]
  19. Hill CE, Rummery N, Hickey H, and Sandow SL. Heterogeneity in the distribution of vascular gap junctions and connexins: implications for function. Clin Exp Pharmacol Physiol 29: 620–625, 2002.[CrossRef][ISI][Medline]
  20. Huang Y and Cheung KK. Endothelium-dependant rhythmic contractions induced by cyclopiazonic acid in rat mesenteric artery. Eur J Pharmacol 332: 167–172, 1997.[CrossRef][ISI][Medline]
  21. Jackson WF. Oscillations in active tension in hamster aortas: role of the endothelium. Blood Vessels 25: 144–156, 1988.[ISI][Medline]
  22. Jackson WF, Mulsch A, and Busse R. Rhythmic smooth muscle activity in hamster aortas is mediated by continuous release of NO from the endothelium. Am J Physiol Heart Circ Physiol 260: H248–H253, 1991.[Abstract/Free Full Text]
  23. Koenigsberger M, Sauser R, Beny JL, and Meister JJ. Role of the endothelium on arterial vasomotion. Biophys J 88: 3845–3854, 2005.[CrossRef][ISI][Medline]
  24. Lacza Z, Herman P, Gorlach C, Hortobagyi T, Sandor P, Wahl M, and Benyo Z. NO synthase blockade induces chaotic cerebral vasomotion via activation of thromboxane receptors. Stroke 32: 2609–2614, 2001.[Abstract/Free Full Text]
  25. Lagaud G, Karicheti V, Knot HJ, Christ GJ, and Laher I. Inhibitors of gap junctions attenuate myogenic tone in cerebral arteries. Am J Physiol Heart Circ Physiol 283: H2177–H2186, 2002.[Abstract/Free Full Text]
  26. Lamboley M, Schuster A, Beny JL, and Meister JJ. Recruitment of smooth muscle cells and arterial vasomotion. Am J Physiol Heart Circ Physiol 285: H562–H569, 2003.[Abstract/Free Full Text]
  27. Lamont C and Weir WG. Different roles of ryanodine receptors and inositol (1,4,5)-trisphosphate receptors in adrenergically stimulated contractions of small arteries. Am J Physiol Heart Circ Physiol 287: H617–H625, 2004.[Abstract/Free Full Text]
  28. Ludmer PL, Selwyn AP, Shook TL, Wayne RR, Mudge GH, Alexander RW, and Ganz P. Paradoxical vasoconstriction induced by acetylcholine in atherosclerotic coronary arteries. N Engl J Med 315: 1046–1051, 1986.[Abstract]
  29. Martin PE and Evans WH. Incorporation of connexins into plasma membranes and gap junctions. Cardiovasc Res 62: 378–387, 2004.[Abstract/Free Full Text]
  30. Matchkov VV, Aalkjaer C, and Nilsson H. A cyclic GMP-dependent calcium-activated chloride current in smooth-muscle cells from rat mesenteric resistance arteries. J Gen Physiol 123: 121–134, 2004.[Abstract/Free Full Text]
  31. Matchkov VV, Rahman A, Peng H, Nilsson H, and Aalkjaer C. Junctional and nonjunctional effects of heptanol and glycyrrhetinic acid derivates in rat mesenteric small arteries. Br J Pharmacol 142: 961–972, 2004.[CrossRef][ISI][Medline]
  32. Mather S, Dora KA, Sandow SL, Winter P, and Garland CJ. Rapid endothelial cell-selective loading of connexin 40 antibody blocks EDHF dilation in rat small mesenteric arteries. Circ Res 97: 399–407, 2005.[Abstract/Free Full Text]
  33. Mauban JR, Lamont C, Balke CW, and Weir WG. Adrenergic stimulation of rat resistance arteries affects Ca2+ sparks, Ca2+ waves, and Ca2+ oscillations. Am J Physiol Heart Circ Physiol 280: H2399–H2405, 2001.[Abstract/Free Full Text]
  34. Mauban JR and Weir WG. Essential role of EDHF in the initiation and maintenance of adrenergic vasomotion in rat mesenteric arteries. Am J Physiol Heart Circ Physiol 287: H608–H616, 2004.[Abstract/Free Full Text]
  35. McNeish AJ, Sandow SL, Neylon CB, Chen MX, Dora KA, and Garland CJ. Evidence for involvement of both IKCa and SKCa channels in hyperpolarizing responses of the rat middle cerebral artery. Stroke 37: 1277–1282, 2006.[Abstract/Free Full Text]
  36. Neild TO. Measurement of arteriole diameter changes by analysis of television images. Blood Vessels 26: 48–52, 1989.[ISI][Medline]
  37. Neylon CB, Nurgali K, Humme B, Robbins HL, Moore S, Chen MX, and Furness JB. Intermediate-conductance calcium-activated potassium channels in enteric neurones of the mouse: pharmacological, molecular and immunochemical evidence for their role in mediating the slow afterhyperpolarization. J Neurochem 90: 1414–1422, 2004.[CrossRef][ISI][Medline]
  38. Okazaki K, Seki S, Kanaya N, Hattori J, Tohse N, and Namiki A. Role of endothelium-derived hyperpolarizing factor in phenylephrine-induced oscillatory vasomotion in rat small mesenteric artery. Anaesthesiology 98: 1164–1171, 2003.[CrossRef][ISI][Medline]
  39. Omote M and Mizusawa H. Effects of cyclopiazonic acid on phenylephrine-induced contractions in the rabbit ear artery. Br J Pharmacol 111: 233–237, 1994.[ISI][Medline]
  40. Omote M and Mizusawa H. Endothelium-dependant rhythmic contractions induced by cyclopiazonic acid, a sarcoplasmic reticulum inhibitor, in the rabbit femoral artery. Acta Physiol Scand 154: 113–119, 1995.[ISI][Medline]
  41. Peng H, Matchkov V, Ivarsen A, Aalkjaer C, and Nilsson H. Hypothesis for the initiation of vasomotion. Circ Res 88: 810–815, 2001.[Abstract/Free Full Text]
  42. Rummery N, Hickey H, McGurk G, and Hill CE. Connexin 37 is the major connexin expressed in the media of the caudal artery. Arterioscler Thromb Vasc Biol 22: 1427–1432, 2002.[Abstract/Free Full Text]
  43. Rummery N, McKenzie K, Whitworth JA, and Hill CE. Decreased endothelial size and connexin expression in rat caudal arteries during hypertension. J Hypertens 20: 247–253, 2002.[CrossRef][ISI][Medline]
  44. Rummery NM, Grayson TH, and Hill CE. Angiotensin-converting enzyme inhibition restores endothelial but not medial connexin expression in hypertensive rats. J Hypertens 23: 317–328, 2005.[CrossRef][ISI][Medline]
  45. Sandow SL, Bramich NJ, Bandi HP, Rummery N, and Hill CE. Structure, function and EDHF in the caudal artery of the SHR and WKY Rat. Arterioscler Thromb Vasc Biol 23: 822–828, 2003.[Abstract/Free Full Text]
  46. Sandow SL, Goto K, Rummery N, and Hill CE. Developmental changes in myoendothelial gap junctions in the rat saphenous artery. J Physiol 556: 875–886, 2004.[Abstract/Free Full Text]
  47. Schuster A, Oishi H, Beny JL, Stergiopulos N, and Meister JJ. Simultaneous arterial calcium dynamics and diameter measurements: application to myoendothelial communication. Am J Physiol Heart Circ Physiol 280: H1088–H1096, 2001.[Abstract/Free Full Text]
  48. Sell M, Boldt W, and Markwardt F. Desynchronising effect of the endothelium on intracellular Ca2+ concentration dynamics in vascular smooth muscle cells of rat mesenteric arteries. Cell Calcium 32: 105–120, 2002.[CrossRef][ISI][Medline]
  49. Shaw L, O'Neill SC, Jones CJP, Austin C, and Taggart MJ. Comparison of U46619-, endothelin-1- or phenylephrine-induced changes in cellular Ca2+ profiles and Ca2+ sensitization of constriction of pressurized rat resistance arteries. Br J Pharmacol 141: 678–688, 2004.[CrossRef][ISI][Medline]
  50. Tare M, Coleman HA, and Parkington HC. Glycyrrhetinic derivatives inhibit hyperpolarization in endothelial cells of guinea pig and rat arteries. Am J Physiol Heart Circ Physiol 282: H335–H341, 2002.[Abstract/Free Full Text]
  51. Tsai ML, Watts SW, Loch-Caruso R, and Webb RC. The role of gap junctional communication in contractile oscillations in arteries from normotensive and hypertensive rats. J Hypertens 13: 1123–1133, 1995.[ISI][Medline]
  52. Watts SW, Tsai ML, Loch-Caruso R, and Webb RC. Gap junctional communication and vascular smooth muscle reactivity: Use of tetraethylammonium chloride. J Vasc Res 31: 307–313, 1994.[ISI][Medline]
  53. Yamamoto Y, Fukuta H, Nakahira Y, and Suzuki H. Blockade by 18beta-glycyrrhetinic acid of intercellular electrical coupling in guinea-pig arterioles. J Physiol 511: 501–508, 1998.[Abstract/Free Full Text]



This article has been cited by other articles:


Home page
 J. Cell Sci.Home page
B. E. Isakson
Localized expression of an Ins(1,4,5)P3 receptor at the myoendothelial junction selectively regulates heterocellular Ca2+ communication
J. Cell Sci., November 1, 2008; 121(21): 3664 - 3673.
[Abstract] [Full Text] [PDF]

Home page
 Am. J. Physiol. Heart Circ. Physiol.Home page
B. E. Isakson, A. K. Best, and B. R. Duling
Incidence of protein on actin bridges between endothelium and smooth muscle in arterioles demonstrates heterogeneous connexin expression and phosphorylation
Am J Physiol Heart Circ Physiol, June 1, 2008; 294(6): H2898 - H2904.
[Abstract] [Full Text] [PDF]

Home page
 Am. J. Physiol. Regul. Integr. Comp. Physiol.Home page
T. Takenaka, T. Inoue, Y. Kanno, H. Okada, C. E. Hill, and H. Suzuki
Connexins 37 and 40 transduce purinergic signals mediating renal autoregulation
Am J Physiol Regulatory Integrative Comp Physiol, January 1, 2008; 294(1): R1 - R11.
[Abstract] [Full Text] [PDF]

Home page