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Research ArticleCardiovascular
Open Access

KATP Channel Openers Inhibit Lymphatic Contractions and Lymph Flow as a Possible Mechanism of Peripheral Edema

Brittney R. Garner, Amanda J. Stolarz, Daniel Stuckey, Mustafa Sarimollaoglu, Yunmeng Liu, Philip T. Palade, Nancy J. Rusch and Shengyu Mu
Journal of Pharmacology and Experimental Therapeutics January 2021, 376 (1) 40-50; DOI: https://doi.org/10.1124/jpet.120.000121

Abstract

Pharmacological openers of ATP-sensitive potassium (KATP) channels are effective antihypertensive agents, but off-target effects, including severe peripheral edema, limit their clinical usefulness. It is presumed that the arterial dilation induced by KATP channel openers (KCOs) increases capillary pressure to promote filtration edema. However, KATP channels also are expressed by lymphatic muscle cells (LMCs), raising the possibility that KCOs also attenuate lymph flow to increase interstitial fluid. The present study explored the effect of KCOs on lymphatic contractile function and lymph flow. In isolated rat mesenteric lymph vessels (LVs), the prototypic KATP channel opener cromakalim (0.01–3 µmol/l) progressively inhibited rhythmic contractions and calculated intraluminal flow. Minoxidil sulfate and diazoxide (0.01–100 µmol/l) had similar effects at clinically relevant plasma concentrations. High-speed in vivo imaging of the rat mesenteric lymphatic circulation revealed that superfusion of LVs with cromakalim and minoxidil sulfate (0.01–10 µmol/l) maximally decreased lymph flow in vivo by 38.4% and 27.4%, respectively. Real-time polymerase chain reaction and flow cytometry identified the abundant KATP channel subunits in LMCs as the pore-forming Kir6.1/6.2 and regulatory sulfonylurea receptor 2 subunits. Patch-clamp studies detected cromakalim-elicited unitary K+ currents in cell-attached patches of LMCs with a single-channel conductance of 46.4 pS, which is a property consistent with Kir6.1/6.2 tetrameric channels. Addition of minoxidil sulfate and diazoxide elicited unitary currents of similar amplitude. Collectively, our findings indicate that KCOs attenuate lymph flow at clinically relevant plasma concentrations as a potential contributing mechanism to peripheral edema.

SIGNIFICANCE STATEMENT ATP-sensitive potassium (KATP) channel openers (KCOs) are potent antihypertensive medications, but off-target effects, including severe peripheral edema, limit their clinical use. Here, we demonstrate that KCOs impair the rhythmic contractions of lymph vessels and attenuate lymph flow, which may promote edema formation. Our finding that the KATP channels in lymphatic muscle cells may be unique from their counterparts in arterial muscle implies that designing arterial-selective KCOs may avoid activation of lymphatic KATP channels and peripheral edema.

Introduction

ATP-sensitive potassium (KATP) channels are metabolically sensitive ion channels in the plasma membrane that open in response to low intracellular concentrations of ATP and other metabolic challenges. The opening of KATP channels mediates K+ efflux, membrane hyperpolarization, closure of voltage-gated calcium channels, and reduced excitation of many cell types (Mannhold, 2004; Foster and Coetzee, 2016). In arterial smooth muscle cells (SMCs), the pharmacological activation of KATP channels exerts powerful vasodilator and blood pressure–lowering effects. Indeed, pharmacologic KATP channel openers (KCOs) were administered as antihypertensive agents prior to understanding their mechanism of action. Minoxidil was approved in 1971 for the treatment of hypertension (Bryan, 2011), and this was followed by the introduction of diazoxide in 1976 (https://online.lexi.com/lco/action/doc/retrieve/docid/patch_f/6729?cesid=2JtH6XyTRqQ&searchUrl=%2Flco%2Faction%2Fsearch%3Fq%3Ddiazoxide%26t%3Dname%26va%3Ddiazoxide). Although the prototypic KCO, cromakalim, was synthesized from a β-blocker skeleton in the 1980s (Mannhold, 2004), it was not until 1983 that Noma and colleagues discovered the KATP channel in cardiomyocytes (Noma, 1983). Subsequently, new structural families of KCOs were synthesized, but only minoxidil and diazoxide were ever approved for clinical use in the United States. Minoxidil is used for hypertensive emergencies in patients resistant to standard antihypertensive medications. Diazoxide was developed as an antihypertensive medication but has evolved into a valuable drug for treating persistent hyperinsulinism (Welters et al., 2015).

Although the KCOs are potent antihypertensive agents (Nichols et al., 2013; Rubaiy, 2016), they are not drugs of choice to treat chronic hypertension because of potentially severe side effects, including peripheral edema, which manifests as fluid retention and gross swelling of the feet and/or legs (Sica, 2004; Nichols et al., 2013). A common presumption is that peripheral edema results when KCOs preferentially dilate arteries compared with veins, resulting in elevated capillary pressure and movement of intravascular fluid into tissues to establish filtration edema (Sica, 2003; Weir, 2003). Indeed, the molecular composition and pharmacology of KATP channels in arterial SMCs and their response to KCOs are well defined. Arterial KATP channels primarily are composed of four pore-forming Kir6.1 subunits physically associated with four regulatory sulfonylurea receptor (SUR) isoform 2B subunits (Shi et al., 2012; Foster and Coetzee, 2016; Rubaiy, 2016). The SUR2B subunit contains binding domains for KCOs, which when occupied antagonize ATP-mediated pore inhibition as the basis for pharmacological activation of KATP channels and vasodilation (Mannhold, 2004; Foster and Coetzee, 2016).

In contrast with the arterial circulation, only a limited number of studies have described the effect of KCOs on the lymphatic circulation. Interestingly, lymph vessels are composed of “hybrid” lymphatic muscle cells (LMCs), which share functional properties with smooth and striated muscle cells and express smooth, cardiac, and skeletal muscle biomarkers (Muthuchamy et al., 2003). Similar to cardiac myocytes, collecting lymph vessels exhibit rhythmic contractions. In the lymphatic circulation, these contractions “pump” fluid from the extracellular space to the central venous ducts to prevent the formation of edema (Gashev, 2002; Nipper and Dixon, 2011; Choi et al., 2012; Mortimer and Rockson, 2014). In guinea pig mesenteric lymphatics, micromolar concentrations of cromakalim inhibit the rhythmic contractions of collecting lymph vessels (Mathias and von der Weid, 2013), implying that KCOs may impair lymph flow. Similarly, KCOs can abolish the rhythmic contractions of isolated human mesenteric lymph vessels (Telinius et al., 2014). However, whether KCOs inhibit the rhythmic contractions of collecting lymph vessels at clinically achievable plasma concentrations is unclear, and the effect of KCOs on lymph flow in vivo has not been reported to our knowledge. Finally, although transcripts encoding the KATP channel Kir6.1 and SUR2B subunits were reported in guinea pig mesenteric lymph vessels (LVs) (Mathias and von der Weid, 2013), the identity of the protein subunits that coassemble to form KATP channels in LMCs also is unclear.

The goal of the present study was to define the impact of the prototypic KCO, cromakalim, and of clinically relevant concentrations of minoxidil and diazoxide on the rhythmic contractile activity of isolated rat mesenteric LVs and evaluate whether KCOs impair lymph flow in vivo. A final set of studies used flow cytometry and patch-clamp recordings to identify the subunit composition of functional KATP channels in single LMCs. Our findings indicate that the rhythmic contractions of rat mesenteric LVs and lymph flow in vivo are impaired by KCOs at concentrations associated with their therapeutic actions. Furthermore, the KATP channels in LMCs may be structurally distinct from their counterparts in arterial SMCs, implying that differential targeting of arterial versus lymphatic KATP channels by KCOs may represent one strategy to avoid peripheral edema while retaining powerful blood pressure–lowering effects.

Materials and Methods

Animals

Animals used in experiments were housed in the Division of Laboratory Animal Medicine at the University of Arkansas for Medical Sciences. Animal use protocols (numbers 3672 and 3923) were approved by the Institutional Animal Care and Use Committee under the provisions of the National Institutes of Health guidelines. For all ex vivo studies, LVs were obtained from 9- to 13-week-old male Sprague-Dawley rats ordered from Envigo (Indianapolis, IN). Rats were anesthetized using 2.5% isoflurane with pure oxygen at a flow rate of 3 l/min for 5 minutes and then euthanized by decapitation. For the purposes of imaging LVs in vivo, 5–7-week-old male Sprague-Dawley rats from the same vendor were used to minimize mesenteric fat. At the completion of in vivo experiments, rats were exsanguinated via cardiac puncture.

Diameter Measurements

Mesenteric LVs.

After sacrifice, the rat mesentery was dissected free and placed in a beaker of cold physiologic saline solution (PSS) consisting of the following (in millimole per liter): 119 NaCl, 24 NaHCO3, 5.5 glucose, 4.7 KCl, 1.6 CaCl2, 1.17 NaH2PO4, 1.17 MgSO4, and 0.026 EDTA. Subsequently, the mesentery was transferred to a silicone-based dissection tray filled with cold PSS. Mesenteric loops were exposed and stabilized by insect pins to allow the dissection of second-order LVs from connective and adipose tissue. A single LV was then transferred to a Living Systems perfusion chamber (Living Systems Instrumentation, Burlington, VT) containing PSS at 37°C with 7% CO2 bubbling to maintain a pH of 7.4. The LV was cannulated with glass micropipettes (75–100 µm; Living Systems Instrumentation) and perfused with PSS in the distal to proximal direction at an intraluminal pressure of 4 to 5 mm Hg. The vessel was allowed to equilibrate for 45 minutes or until rhythmic contractions were stable. Then concentration-dependent diameter responses to KCOs or corresponding solvent were recorded at a sampling rate of three frames/s using DMTvas edge-detection software (IonOptix Corporation, Westwood, MA). The KCOs included cromakalim (0.01–3 µmol/l; quarter-log units), minoxidil sulfate (0.01–100 µmol/l; half-log units) and diazoxide (0.01–100 µmol/l; half-log units). Origin 9.1 software (OriginLab Corporation, Northampton, MA) was used to analyze the following contractile parameters: end diastolic diameter (EDD), end systolic diameter (ESD), frequency of contraction, and amplitude of contraction. Flow per unit length in a single lymph vessel was calculated using the equation, π/4(EDD2-ESD2)F, as previously described (Stolarz et al., 2019).

High-Speed In Vivo Microscopy

Rats were fasted overnight and anesthetized using 2.5% isoflurane in 1.5 l/min oxygen. A midline abdominal incision was made, and a single loop of mesentery was pulled out and placed in a customized heated (37°C) chamber filled with HEPES-PSS consisting of the following (in millimole per liter): 119 NaCl, 4.7 KCl, 1.17 MgSO4, 1.6 CaCl2, 24 NaHCO3, 0.026 EDTA, 1.17 NaH2PO4, 5.5 glucose, and 5.8 HEPES; pH was titrated to 7.4 using NaOH. A single LV was visualized, and increasing concentrations of cromakalim or minoxidil sulfate (0.01–10 μmol/l; log units) were added to the superfusate bathing the mesentery for 15 minutes at each drug concentration. Customized software developed in collaboration with our institution’s Nanomedicine Center was used to track individual lymph cells in flow as described earlier in detail (Sarimollaoglu et al., 2018; Stolarz et al., 2019). Using these data files, flow velocity and positive volumetric flow were calculated to evaluate the effect of KCOs on lymph flow in vivo.

Real-Time Polymerase Chain Reaction

The entire rat mesentery was pinned in a dissecting tray filled with cold PSS and first- to third-order mesenteric LVs were dissected free during a 2-hour interval and immediately placed in a safe-lock tube containing 600 µl of RNeasy Lysis Buffer solution (Qiagen, Hilden, Germany) and 1% β-mercaptoethanol. After addition of 200 mg of 0.5-mm stainless steel bullets (Next Advance, Troy, NY), the LVs were homogenized at speed 9 in a Next Advance bullet blender (Next Advance) for 2 minutes, and then after a 2-minute interval to allow for cooling, they were homogenized for an additional 2 minutes. Total RNA was isolated using the Qiagen RNeasy Plus Mini Kit according to commercial instructions and stored at −80°C.

Invitrogen’s SuperScript III Reverse Transcriptase kit was used to synthesize cDNA from total RNA. This kit utilizes oligo(dT)20 primer to target only mature mRNAs from total RNA content. Generation of cDNA was performed according to the manufacturer’s protocol. The cDNA was stored at 4°C. Real-time PCR was accomplished using Applied Biosystems TaqMan Universal Master Mix II, with uracil-N-glycosylase and specific TaqMan gene expression primers listed in Supplemental Table 1 (Thermo Fisher, Invitrogen). The primers were designed to anneal to specific gene sequences encoding four different KATP channel subunits: Kir6.1, Kir6.2, SUR1, and SUR2. Additionally, GAPDH served as an amplification control.

Isolation of Lymphatic Muscle Cells

Freshly dissected mesenteric LVs were placed in a glass tube containing 500 µl of initial dissociation solution (solution I) containing the following (in millimole per liter): 145 NaCl, 4 KCl, 1 MgCl2, 10 HEPES, 0.05 CaCl2, 10 glucose, and 0.5 mg/ml bovine serum albumin; pH was adjusted to 7.4 using NaOH. After 10 minutes at room temperature, a glass bulb pipette was used to carefully remove solution I and replace it with 500 µl of new dissociation solution (solution II) containing 3.4 mg papain (3119, 1.7 mg/ml; Worthington) and 2 mg of dithioerythritol stock (D8255, 1 mg/ml; Sigma, St. Louis, MO). The LVs were incubated in this solution for 25–30 minutes at 37°C before a glass bulb pipette was used to carefully remove solution II and replace it with 500 µl of enzyme solution (solution III) containing 1 mg collagenase H (C8051, 0.5 mg/ml; Sigma), 1.4 mg collagenase F (C7926, 0.7 mg/ml; Sigma), and 2 mg trypsin inhibitor (T9128, 1 mg/ml; Sigma). After another 5–7 minutes at 37°C, solution III was similarly removed, and the LVs were removed using a glass bulb pipette and placed in an Eppendorf tube containing 1 ml of the final enzyme solution (solution IV), which contained 10 mg/ml collagenase I (SCR103; Millipore Sigma), 1.5 mg/ml collagenase II (CLS-2; Worthington), and 200 units/ml DNase (J62229; Alfa Aesar). The Eppendorf tube was placed in an incubator (37°C, 5% CO2, Steri-Cycle CO2 Incubator, Model 370, Marietta, OH) and rotated using a MACSmix tube rotator (Miltenyi Biotec, Gladbach, Germany) for 30 minutes. Subsequently, the solution containing the dissociated LVs was spun at 0.5 g for 3 minutes to collect single LMCs. The cells were resuspended in 300 µl of isolation buffer (IB) composed of 0.5% bovine serum albumin and 2 mmol/l EDTA in phosphate-buffered saline and spun down at 0.5 g for 3 minutes. This process was repeated twice more to wash the cells before they were directed to flow cytometry studies.

Flow Cytometry and ImageStream Flow Cytometry

Once the rat mesenteric LMCs were isolated and washed, they were incubated with Kir6.1, Kir6.2, SUR1, or SUR2 primary antibodies (Supplemental Table 1) for 1 hour at room temperature in IB. These antibodies target subunit-specific protein sequences, a claim that we substantiated by searching epitope sequences of antibodies using BLAST (https://blast.ncbi.nlm.nih.gov). The specificities of anti-Kir6.1 and anti-Kir6.2 antibodies also have been validated in cells from Kir6.1−/− and Kir6.2−/− mice (Milovanova et al., 2006). Subsequently, the cells were washed and incubated with goat anti-rabbit IgG secondary antibody Alexa 647 (1:500) and smooth muscle–specific α-actin–FITC (1:100) for 30–45 minutes. Then cells were washed three times with 1 ml of IB and resuspended in 300 µl IB for flow cytometry analysis. The data were collected using an Accari C6 flow cytometer (BD Biosciences, San Jose, CA) and analyzed with FlowJo-V10 software (FlowJo LLC, Ashland, OR) to provide information on the expression of distinct KATP channel subunit proteins in isolated LMCs.

To visually confirm that the antibody signal arose from single LMCs and not contaminating cell types, we also subjected isolated LMCs to imaging flow cytometry. The LMCs were incubated with primary antibodies (Supplemental Table 1) corresponding to Kir6.1 subunit (rabbit anti-rat, 1:50) and Kir6.2 subunit (guinea pig anti-rat, 1:50) for 1–1.5 hours at room temperature in IB. Subsequently, the LMCs were washed and incubated with two secondary antibodies, goat anti-rabbit IgG Cy3 (1:2000) and goat anti-guinea pig Alexa 647 (1:2000), together with smooth muscle–specific α -actin–FITC (1:500) antibody, respectively, for 45 minutes. Then the cells were washed and resuspended in 50 µl of PBS. Finally, the suspensions of LMCs were imaged using an ImageStreamX Mk II Imaging Flow Cytometer (Luminex Corporation, Austin, TX). Images were collected using IDEAS 6.2 software (Luminex Corporation).

Patch-Clamp Electrophysiology

Lymph vessels were subjected to enzymatic isolation as described for flow cytometry, except after incubation in 500 µl of solution III, a drop of solution was visualized on an inverted microscope to ensure initial release of LMCs from LVs. The tube containing the LVs was then placed on ice, and a glass bulb pipette was used to remove solution III and replace it with solution I, which was free of enzymes. Gentle trituration resulted in the further separation of LMCs from residual LV tissue. The resulting suspension of LMCs was transported to a patch-clamp station, and aliquots of LMCs were transferred to a chamber mounted on the stage of an Olympus IMT-2 inverted microscope (Olympus Corporation, Shinjuki City, Tokyo, Japan) and allowed to settle before superfusion with high-K+ bath solution of the following composition (in millimole per liter): 145 KCl, 5 HEPES, 1.8 CaCl2, and 1 MgCl2, titrated to pH 7.4 with KOH. Patch pipettes were pulled from borosilicate glass (number 7052; Garner Glass Co., Claremont, CA), fire-polished to a tip resistance of 5–8 MΩ, and filled with solution consisting of (in millimole per liter): 145 KCl, 5 HEPES, 1.8 CaCl2, and 1 MgCl2, titrated to pH 7.4 with KOH. Slight suction was used to form a high-resistance seal (>5 GΩ) between LMC membranes and the pipette tip to establish the cell-attached recording mode for recording of unitary K+ currents. The patch potential was maintained at −50 mV for 2 minutes to record single-channel K+ currents in drug-free bath solution. Subsequently, the chamber was filled with new bath solution containing 1 μmol/l cromakalim to activate KATP channels. Cromakalim-induced single-channel currents were recorded for 2–4 minutes at −50 mV and then in 10-mV steps using 2-minute increments at patch potentials between −70 and +50 mV. Current signals were amplified by an EPC-7 patch-clamp amplifier (List Medical Electronic, Darmstadt, Germany) connected to a TL-1 DMA Interface driven by pClamp 6.0 software (Axon Instruments, Foster City, CA) running an IBM-compatible computer for data acquisition and digitization. Analog to digital conversion was accomplished at a sampling rate of 5 kHz after signals were passed through an eight-pole Bessel filter with a cutoff frequency of 1 kHz to enable real-time visualization of small current amplitudes. After an average current-voltage relationship was generated by plotting unitary current amplitudes as a function of patch potential using Clampfit 10.3 software (Molecular Devices, San Jose, CA) and GraphPad Prism 7 software (GraphPad Software, San Diego, CA), the average unitary conductance of cromakalim-sensitive channels was calculated at negative patch potentials associated with linearity and then again at positive patch potentials associated with inward rectification. In additional studies, the patch potential was maintained at −50 mV in drug-free bath solution for 2 minutes prior to filling the chamber with solution containing either 0.1 μmol/l minoxidil sulfate or 3 μmol/l diazoxide. Recordings at a patch potential of −50 mV were resumed to determine whether these concentrations of KCOs, which caused half inhibition of calculated flow in cannulated LVs, also activated a similar single-channel current as cromakalim in rat mesenteric LMCs.

Materials

Cromakalim, minoxidil sulfate, and diazoxide were obtained from Sigma-Aldrich. Cromakalim and minoxidil sulfate were dissolved in DMSO and stored as 50 mmol/l aliquots at −20°C. Diazoxide was dissolved in 0.1 mol/l sodium hydroxide and stored as 50 mmol/l aliquots at −20°C. Phenylephrine was dissolved in pure water as 10 mmol/l aliquots and stored at −20°C.

Statistics

Data obtained from control and treated groups were expressed as mean ± S.D. and compared using the unpaired t test or one-way ANOVA as applicable. All differences were judged to be significant at the level of P < 0.05. Sample sizes were determined assuming S.D. equal to 20% of the mean of the control group and a 30% change of the mean in experimental groups with power = 0.8–0.9, α = 0.05, and β = 0.20. Flow cytometry data were repeated in triplicate.

Results

KCOs Inhibit the Rhythmic Contractions of Isolated LVs.

Increasing concentrations of the prototypic KCO, cromakalim, inhibited and ultimately abolished the rhythmic contractions of rat mesenteric LVs (Fig. 1). Addition of the corresponding DMSO solvent did not significantly affect contraction parameters (Fig. 1; Supplemental Table 2). Cromakalim significantly impaired flow through LVs at concentrations higher than 0.18 µmol/l by attenuating the frequency and amplitude of rhythmic contractions (Fig. 3; Table 1). Consistent with the hyperpolarizing effect of KCOs on LMCs that drives the resting membrane potential further from the threshold for action potential firing (Mathias and von der Weid, 2013), contraction frequency was most sensitive to concentration-dependent inhibition by KCOs. In contrast, contraction amplitude failed to show progressive inhibition by increasing concentrations of KCOs. Instead contractions abruptly ceased at a given KCO concentration, which varied slightly between different LVs. This all-or-none response is reflected in the steep negative relationship between KCO concentration and amplitude in Fig. 3 and accounts for the high S.D. values. Cromakalim also increased EDD, an effect predicted to promote flow by increasing filling volume between contractions and thereby stroke volume, but the effect on EDD was mild (≤5%) compared with the profound negative effect of cromakalim on contraction frequency and amplitude. Notably, we implicated KATP channels in cromakalim-induced inhibition of rhythmic contractions by demonstrating that 1 µmol/l glibenclamide, a KATP channel antagonist, caused a rightward shift in the IC50 of cromakalim for contraction frequency and amplitude (Supplemental Fig. 1). We avoided using higher concentrations of glibenclamide, which are known to lose selectivity for KATP channels (Bessadok et al., 2011; Simard et al., 2012).

Fig. 1.
Fig. 1.

Effect of cromakalim on the contractile behavior of isolated rat mesenteric LVs. (A) Increasing concentrations of cromakalim (0.01–3 µmol/l, quarter-log increments) progressively inhibit the rhythmic contractions of isolated mesenteric LVs, ultimately leading to cessation of contractions. (B) No significant changes in LV contractile parameters occurred with increasing concentrations of the DMSO solvent. Images in this figure are representative of n = 6 determinations.

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TABLE 1

Measurements of contraction amplitude, contraction frequency, end diastolic diameter, and intraluminal flow in isolated rat mesenteric lymph vessels in response to three different KCOs

Exposure of LVs to either increasing quarter-log conc. of cromakalim (0.01–3 μmol/l), half-log conc. of minoxidil sulfate, or half-log conc. of diazoxide (0.01–100 μmol/l) progressively increased EDD concurrent with decreases in contraction frequency, amplitude, and calculated flow (*P < 0.05; **P < 0.01; ***P < 0.001;****P < 0.0001, mean ± S.D., n = 6).

Next, we explored the effect of clinically available KCOs on the contractile activity of isolated LVs. Increasing half-log (0.01–100 µmol/l) concentrations of either minoxidil sulfate or diazoxide inhibited the rhythmic contractions of isolated LVs (Fig. 2) but with markedly different potencies. The potency of minoxidil sulfate was comparable to cromakalim (Fig. 3); minoxidil sulfate exhibited IC50 values of 0.35 and 1.82 µmol/l for contraction frequency and amplitude, respectively, compared with cromakalim’s IC50 values of 0.25 and 0.77 µmol/l for the same parameters. Intraluminal flow was attenuated significantly by 0.1 µmol/l minoxidil sulfate, and its IC50 value of 0.47 µmol/l was within the clinically achievable peak plasma concentration of 0.48 µmol/l observed in patient who were chronic hypertensive and administered minoxidil (Lowenthal and Affrime, 1980). This IC50 value also was well within the range of 0.2–1.2 µmol/l reported for therapeutic plasma concentrations (The International Association of Forensic Toxicologists, 2004).

Fig. 2.
Fig. 2.

Effect of clinically available KCOs on the contractile behavior of isolated rat mesenteric LVs. (A) Increasing concentrations of minoxidil sulfate (0.01–100 µmol/l, half-log increments) progressively inhibited the rhythmic contractions of isolated mesenteric LVs, ultimately stopping contractions. (B) Increasing concentrations of diazoxide (0.01–100 µmol/l, half-log increments) progressively inhibited the rhythmic contractions of isolated mesenteric LVs but at higher concentrations than minoxidil sulfate. Images in this figure are representative of n = 6 determinations.

Fig. 3.
Fig. 3.

Profile of KCO effects on rhythmic contractions and intraluminal flow of isolated mesenteric LVs. Increasing concentrations of KCOs: cromakalim (○), minoxidil sulfate (▪), and diazoxide (∆) significantly decreased the amplitude of contraction (A), progressively reduced the frequency of contraction (B), resulted in a small but significant increase in EDD (C), and decreased calculated lymph flow (D). Data are reported as mean ± S.D. analyzed using one-way ANOVA with Holm-Sidak post-test, significance refers to ANOVA. (n = 6, **P < 0.01; ****P < 0.0001).

Diazoxide inhibited rhythmic contractions in rat mesenteric lymph vessels at much higher concentrations compared with cromakalim and minoxidil sulfate (Figs. 2 and 3; Table 1). The inhibition of contraction amplitude by diazoxide was very abrupt, exhibiting an IC50 value of 30.2 µmol/l, which represented a 16.56-fold higher value compared with minoxidil sulfate. Similarly, the IC50 value of 8.3 µmol/l for diazoxide inhibition of contraction frequency was 233.8-fold higher compared with minoxidil sulfate. Diazoxide only inhibited intraluminal flow at concentrations ≥3 µmol/l. However, the therapeutic plasma concentrations of diazoxide reportedly range between 145 and 332 µmol/l (Neary et al., 1973). Thus, the entire concentration range of diazoxide tested in the present study was easily within clinically achievable plasma concentrations.

KCOs Decrease Mesenteric Lymph Flow In Vivo.

Our finding that clinical KCOs inhibit intraluminal flow through isolated lymph vessels at therapeutic plasma concentrations pointed to the importance of determining whether this effect translates to lymph flow in vivo. For these studies, we focused on minoxidil sulfate as the clinical KCO with the highest potency for disrupting rhythmic contractions in isolated LVs. Similar to our in vitro studies, we used cromakalim in parallel studies because this prototypic KCO is regarded as the most selective activator of KATP channels. Superfusion of the mesenteric lymphatic circulation with increasing log concentrations (0.01–10 µmol/l) of cromakalim abruptly inhibited positive volumetric lymph flow in vivo at concentrations ≥0.1 µmol/l (Fig. 4; Table 2). Minoxidil sulfate also exhibited a concentration-dependent inhibition of positive volumetric lymph flow in vivo, exhibiting significant slowing of flow at 1 µmol/l (Fig. 4; Table 2), a concentration corresponding to patient plasma concentrations (Lowenthal and Affrime, 1980; Zarghi et al., 2004, The International Association of Forensic Toxicologists, 2004). Superfusion of a similar solvent concentration of corresponding DMSO did not significantly alter lymph flow.

Fig. 4.
Fig. 4.

Cromakalim and minoxidil sulfate decrease lymph flow in vivo. Bathing the mesentery with HEPES-PSS (□) did not significantly affect lymph flow, although there was a trend of increasing lymph flow during the experiment. Increasing concentrations of cromakalim (▪) and minoxidil sulfate (▪) significantly decreased lymph flow compared with HEPES-PSS controls. Data reported as mean ± S.D. analyzed using one-way ANOVA with Holm-Sidak post-test (n = 5, *P < 0.01; ****P < 0.0001). Significance reported over bars indicates significance compared with baseline. Significance denoted with labels indicates one-way ANOVA significance.

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TABLE 2

Topical superfusion of cromakalim or minoxidil sulfate decreased volumetric lymph flow in rat mesenteric LVs in vivo

Increasing log conc. of cromakalim or minoxidil sulfate (0.01–10 μmol/l) progressively decreased positive volumetric lymph flow compared with the DMSO solvent control (*P < 0.05, mean ± S.D., n = 5).

Rat Mesenteric LMCs Primarily Express Kir6.1, Kir6.2, and SUR2.

Next we considered whether LMCs might express a unique population of KATP channels considering that they represent “hybrid” cells with properties of smooth and striated muscle. In this series of studies, we initially defined subunit transcripts in rat mesenteric LVs using real-time PCR (Table 3). These results indicated the presence of both Kir6.1 and Kir6.2 transcripts. Expression level of the SUR2 transcript was comparable to Kir6.1, whereas the SUR1 transcript was only detected at a high cycle threshold suggesting low expression. The small quantity of RNA obtained from LVs limited our analysis to using validated TaqMan primers to differentiate KATP channel subunits. We did not differentiate between the SUR2A/B splice variants that lack validated TaqMan primers. GAPDH was used as a quality-control amplicon to ensure consistent amplification between different vessel samples (n = 3). However, the cDNA for these studies was obtained from whole lymph vessels, which contain multiple cell types that potentially express variable types of KATP channels. Thus, further studies were performed to define the protein expression of KATP channel subunits in purified populations of LMCs. Isolated LMCs were costained with the smooth muscle marker α-smooth muscle actin (SMA)-FITC and antibodies directed against either the Kir6.1, Kir6.2, SUR1, or SUR2 subunit. LMCs were incubated subsequently with the secondary antibody conjugated to Alexa-Fluor 647 and then subjected to flow cytometry. The α-SMA–FITC stain was used to set the gate that defined the LMC population (Fig. 5A). Next, we used a negative control, which consisted of LMCs incubated with α-SMA–FITC and the Alexa-Fluor 647–conjugated secondary antibody without primary antibodies to control for any nonspecific positive staining of the secondary antibody within the gated region (Fig. 5B). Using these gates, we then measured the Alexa-Fluor 647 signals in the LMC samples incubated with primary antibodies as described above. Flow cytometry detected immunoreactivity corresponding to protein expression of Kir6.1, Kir6.2, and SUR2. In contrast, SUR1 immunoreactivity was not detected on the cell surface (Fig. 5, C–E), supporting data from our gene expression studies that indicated rare SUR1 transcripts (Table 3). In the α-SMA positive-gated cells (Fig. 5B), we found that 37.09% of the cells stained positive for Kir6.1 expression (Fig. 5C), 11.75% stained positive for Kir6.2 expression (Fig. 5D), and 33.14% stained positive for SUR2 expression (Fig. 5F). We did not observe any positive SUR1 staining in the gated region (Fig. 5E). Flow cytometry with ImageStream visually confirmed the fluorescent signals were localized to single LMCs rather than representing artifact or signals from other cell types not fully dissociated from LMCs (Fig. 6). Interestingly, ImageStream results (Fig. 6) also indicated that the Kir6.1 and Kir6.2 subunits are coexpressed on the same LMCs.

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TABLE 3

Cycle thresholds for real-time PCR amplification using TaqMan primers specific for KATP channel subunits in whole-rat mesenteric LVs

Transcripts encoding all four known KATP channel subunits were detected, including the pore-forming Kir6.1 and Kir6.2 subunits and the regulatory SUR1 and SUR2 subunits. However, the SUR1 transcript was extremely sparse. GAPDH was the amplification standard. Data reported as mean ± S.D., n = 3.

Fig. 5.
Fig. 5.

Expression of KATP channel subunits in LMCs. (A) Mesenteric LVs were digested and coincubated with a smooth muscle protein marker, α-SMA–FITC. A gate was set around the cells staining positive for α-SMA. This gate is used in all subsequent panels. (B) Cells selected from the α-SMA positive gate were coincubated with Alexa-647 conjugated secondary antibody only as a negative control. (C) α-SMA positive-gated cells show immunoreactivity corresponding to Kir6.1. (D) α-SMA positive-gated cells also exhibited Kir6.2 immunoreactivity. (E) Immunoreactivity corresponding to SUR1 protein was not detected in α-SMA positive-gated cells. (F) α-SMA positive-gated cells display immunoreactivity for SUR2. FSC, Forward Scatter; SSC, Side Scatter. Images in this figure are representative of n = 3 determinations.

Fig. 6.
Fig. 6.

ImageStream shows costaining corresponding to the pore-forming Kir6.1 and Kir6.2 subunits on the LMC surface. In a single LMC, from left to right: Differential interference contrast (DIC) image shows single LMC morphology. α-SMA–FITC positive staining indicates the cell is an SMC. Kir6.1-Alexa647 blue fluorescence indicates surface expression of Kir6.1, whereas Kir6.2-Cy3 red fluorescence indicates the surface presence of Kir6.2. Images in this figure are representative of n = 50 images.

In follow-up studies, we applied the patch-clamp technique to provide initial information on whether Kir6.1 and/or Kir6.2 subunits coassemble to form the tetrameric structure of functional KATP channels in rat mesenteric LMCs. Earlier studies suggest that homotetrameric KATP channels composed of Kir6.1 and SUR2B subunits exhibit a single-channel conductance of 29.4 pS, whereas homotetrameric Kir6.2 pore structures exhibit a higher single-channel conductance of 60.2 pS in symmetrical K+ recording solutions. Corresponding Kir6.1/6.2 heterotetramers show a hybrid conductance of approximately 47.5 ± 1.6 pS (Cui et al., 2001). Using patch pipettes filled with 145 mmol/l KCl applied to cell-attached patches of LMCs, single-channel currents were rarely detected at a patch potential of −50 mV in drug-free bath solution (Fig. 7A). The negative patch potential of −50 mV was chosen to silence voltage-gated K+ channels, which presumably are expressed in LMCs similar to other types of muscle cells. However, within 5 minutes exposure to 1 µmol/l cromakalim in the bath solution, single-channel currents were detected in the majority (16 of 19) of patches (Fig. 7B), and cromakalim activation was progressive, revealing multiple channels evident as stacked current openings in some patches (unpublished data). In most patches, channel open-state probability continued to increase for the duration of experiments, which generally ended because of loss of the high-resistance seal between 10 and 20 minutes after exposure to drug. This confounding factor prevented us from performing studies to reverse cromakalim-elicited channel activation using KATP channel-specific antagonists. Alternatively, we focused on defining the single-channel conductance of cromakalim-elicited K+ current and the response of cell-attached patches of LMCs to additional KCOs.

Fig. 7.
Fig. 7.

Patch recordings of cromakalim-elicited K+ currents. (A) Cell-attached recording fails to reveal unitary K+ currents at a patch potential of −50 mV. (B) The same recording as in (A) after addition of 1 µmol/l cromakalim reveals channel activity. (C) A plot of single-channel current amplitude as a function of patch potential depicts an avg. unitary conductance of 46.4 pS at negative patch potentials between −70 and −30 mV. Mild inward rectification results in a unitary conductance of 33.6 pS at positive patch potentials (+20 to +50 mV). Filled ovals located at the left of each trace represent the closed state. Data are reported as mean ± S.D. (X,X) = (number cells, number of cell isolations from different animals).

Accordingly, cromakalim-induced unitary currents were recorded in 2-minute intervals at patch potentials (10-mV steps) between −70 and +50 mV, and current amplitude was plotted as a function of patch potential to obtain a current-voltage relationship (Fig. 7C). Because KATP channels show weak inward rectification (i.e., conduct current more readily at negative compared with positive patch potentials), we focused our recordings at negative patch potentials to calculate single-channel conductance between −70 and −30 mV. A single-channel conductance of 46.4 pS was resolved, which is indicative of heterotetrameric KATP channels composed of Kir6.1/6.2 subunits. The lower single-channel conductance of 33.6 pS at positive patch potentials confirmed the presence of weak inward rectification (Fig. 7C), which is a property of KATP channels, including Kir6.1/6.2 heterotetrameric channels that only weakly rectify (Cui et al., 2001; Acevedo et al., 2006; Wu et al., 2007). We presume these apparent functional Kir6.1/6.2 pore-forming structures coassemble with the abundant SUR2 subunits detected by flow cytometry to form functional KATP channels in LMCs.

In a final series of cell-attached patch-clamp studies, LMCs were exposed to 0.1 µmol/l minoxidil sulfate and 3 µmol/l diazoxide to determine whether these concentrations of KCOs, which reduced calculated flow in isolated LVs by ∼50% (Fig. 3D), elicited unitary currents of similar amplitude as cromakalim in the corresponding LMCs, implying targeting of the same KATP channel. Notably, these concentrations of minoxidil sulfate and diazoxide are within the range of clinical plasma concentrations. Similar to our earlier patch-clamp studies in which 1 μmol/l cromakalim elicited an inward current with an amplitude of 2.67 ± 0.12 pA at a patch potential of −50 mV (Fig. 7), 0.1 μmol/l minoxidil sulfate and 3 μmol/l diazoxide also elicited inward currents at a patch potential of −50 mV with average unitary amplitudes of 2.51 ± 0.07 pA and 2.58 ± 0.13 pA, respectively (n = 4 patches each) under the same condition (Fig. 8, C–F). In parallel control studies using the DMSO solvent, no unitary currents were observed during recording periods as long as 20–30 minutes (Fig. 8, A and B). Thus, all three KCOs included in this study shared activation of a channel of similar current amplitude. Interestingly, in a single patch not included in the analysis, minoxidil sulfate elicited a clearly lower-amplitude current (1.6 pA) corresponding to a presumed single-channel conductance of 32 pS. Although only an isolated observation, this finding was consistent with the single-channel conductance of 29.4 pS associated with Kir6.1 homotetrameric KATP channels. Collectively, our patch-clamp findings were consistent with the expression of a preponderance of Kir6.1/6.2 channels in rat mesenteric LMCs with potential inclusion of KATP channels of other pore-forming subunit compositions.

Fig. 8.
Fig. 8.

Cell-attached recordings of K+ currents elicited by minoxidil sulfate and diazoxide. Patch potential was maintained at −50 mV. Recordings failed to reveal unitary K+ currents before (A) or after (B) addition of DMSO solvent. In another LMC initially exposed to control solution (C), the addition of 0.1 µmol/l minoxidil sulfate elicited unitary K+ currents (D). Similarly, recordings in control solution were quiescent (E), whereas the addition of 3 µmol/l diazoxide elicited a current of similar amplitude as minoxidil sulfate (F).

Discussion

The present study provides three new findings that may shed light on the mechanisms by which clinical KCOs cause peripheral edema as an off-target effect. First, minoxidil sulfate and diazoxide in concentrations achieved in plasma samples of patients progressively attenuate and ultimately interrupt the rhythmic contractions of isolated LVs. Inhibition of contraction frequency appears to be the key effect by which KCOs disrupt rhythmic contractions and mitigate intraluminal flow under these conditions. Second, minoxidil sulfate also compromises lymph flow in vivo at clinically relevant concentrations. Third, immune-imaging of KATP channel proteins combined with patch-clamp analysis of cromakalim-elicited K+ currents suggest that functional KATP channels in LMCs represent Kir6.1/6.2 heterotetramers coassembled with SUR2 subunits. In contrast, the predominant KATP channels in arterial SMCs are presumed to be Kir6.1 homotetrameric channels (Mannhold, 2004; Jahangir and Terzic, 2005; Rubaiy, 2016). Thus, the population of KATP channels expressed by LMCs may differ from arterial SMCs, implying an opportunity to design new KCOs that only target arterial KATP channels to avoid disrupting lymphatic contractions and lymph flow.

The primary emphasis of our study was to determine whether the clinical KCOs minoxidil sulfate and diazoxide disrupt lymphatic contractions and lymph flow at concentrations measured in samples of human plasma. However, we also used cromakalim in our study because it has been characterized extensively as a prototypic, first-generation KATP channel–selective agonist (Mannhold, 2004). Earlier studies reported that cromakalim hyperpolarized guinea pig and rat mesenteric LMCs, thereby inhibiting the voltage-dependent Ca2+ influx that mediates the rhythmic contractions of collecting LVs (Von der Weid, 1998; Gashev, 2002; Imtiaz et al., 2007; Dougherty et al., 2008; Davis et al., 2011, 2012; Mathias and von der Weid, 2013; Scallan et al., 2013). Additionally, the use of cromakalim helped ensure congruence between our lymphatic preparation and those of earlier studies. In this regard, our calculated IC50 value of 0.247 µmol/l for cromakalim-induced inhibition of contractile frequency in rat mesenteric lymph vessels closely resembles the IC50 value of 0.126 µmol/l reported in guinea pig mesenteric lymph vessels (Mathias and von der Weid, 2013).

Importantly, the subunit composition of KATP channels primarily determines their biophysical and pharmacological properties, including sensitivity to KCOs. Therefore, we employed a combination of functional and molecular techniques to explore the composition of KATP channels in the lymphatic vasculature. In this regard, four Kir6.1 and/or Kir6.2 subunits coassemble as homotetramers or heterotetramers to form the KATP channel pore, which confers the properties of K+-selectivity and single-channel conductance. Accessory sulfonylurea receptor subunits (SUR1 or SUR2A/B) coassemble in a ratio of 4:4 with the Kir6.x subunits to form the fully functional KATP channel ((Dörschner et al., 1999; Foster and Coetzee, 2016)). Structurally different KCO families bind preferentially to either SUR1 or SUR2 subunits to regulate cell excitability in a tissue-specific manner (Mannhold, 2004; Jahangir and Terzic, 2005; Foster and Coetzee, 2016). Cromakalim, the prototypic KCO, binds to SUR2A and SUR2B (Matsuo et al., 2000; Tricarico et al., 2008; Nichols et al., 2013). In contrast, the preferential binding of minoxidil sulfate, the active metabolite of minoxidil, to SUR2B explains its potent vasodilator and antihypertensive effect because arterial SMCs primarily express Kir6.1/SUR2B complexes (Gopalakrishnan et al., 1993). The different pharmacological profiles of cromakalim and minoxidil sulfate also may relate to different binding sites on the SUR2 subunit for the two KCOs, which is suggested by the fact that glibenclamide noncompetitively antagonizes minoxidil sulfate but competitively antagonizes cromakalim (Wickenden et al., 1991). Finally, diazoxide has been described as a weakly acting KCO (Mannhold, 2004), but it exhibits equal affinity for SUR1 and SUR2B but not SUR2A (Matsuo et al., 2000; Matsuoka et al., 2000). Accordingly, it avidly binds to Kir6.2/SUR1 channels expressed by pancreatic β cells to enact membrane hyperpolarization and inhibition of Ca2+-dependent insulin release, thereby providing a valuable therapeutic for the treatment of persistent hyperinsulinism. Its dual affinity for vascular Kir6.1/SUR2B channels also explains its continued use for the treatment of malignant hypertension (Jahangir and Terzic, 2005).

Notably, clinically achievable plasma concentrations of minoxidil sulfate range between 0.2 and 1.2 µmol/l (The International Association of Forensic Toxicologists, 2004), whereas therapeutic plasma concentrations of diazoxide are many-fold higher and range between 43.3 and 216.7 µmol/l (The International Association of Forensic Toxicologists, 2004). Both KCO medications can cause severe peripheral edema (Mehta et al., 1975; Pettinger and Mitchell, 1988; Herrera et al., 2018). For our ex vivo studies in isolated LVs, the resulting IC50 values for minoxidil sulfate– and diazoxide-induced inhibition of intraluminal flow were well within clinically achievable plasma concentrations. We further explored whether KCOs disrupted lymph flow in vivo. Again, using cromakalim as the KCO prototype, we initially superfused mesenteric loops with progressive concentrations of cromakalim to control the concentration of drug delivered to the lymphatic vasculature. Our in vivo results demonstrate that cromakalim also markedly compromises flow in the intact lymphatic circulation. Additional studies revealed that minoxidil sulfate also reduced lymph flow at concentrations beginning at 1 µmol/l, which is within the range of clinically achievable plasma concentrations for this antihypertensive medication (The International Association of Forensic Toxicologists, 2004). To our knowledge, the latter finding provides the first direct evidence that KCOs can severely compromise lymph flow in vivo. Interestingly, patients with Cantύ syndrome, which is a disease caused by gain-of-function mutations of KATP channels, also exhibit edema similar to patients administered KCOs for extended periods of time (Mehta et al., 1975; Sica, 2004; Harakalova et al., 2012; Nichols et al., 2013; Scallan et al., 2013).

A single earlier report indicated that whole LVs from the guinea pig mesentery primarily express Kir6.1 and SUR2B transcripts similar to vascular SMCs (Newgreen et al., 1990; Mathias and von der Weid, 2013). Here, we used a multifaceted approach to conclude that functional KATP channels in LMCs primarily represent Kir6.1/6.2 complexes coassembled with SUR2. In this regard, pharmacological studies revealed that both cromakalim and minoxidil sulfate mitigate lymphatic contractions, but they show low affinity for the SUR1 subunit, implicating SUR2 as their binding site in LMCs (Davies et al., 2005; Electrophysiology, 2017). Second, our gene amplification studies using RNA extracted from whole LVs revealed Kir6.1 and Kir6.2 transcripts in similar abundance and SUR2 transcript in overwhelming preponderance to SUR1. Third, immune-imaging of purified populations of cell-sorted LMCs confirmed the coexpression of Kir6.1, Kir6.2, and SUR2 proteins on the surface of single LMCs but failed to detect SUR1. Finally, our patch-clamp studies revealed a slope conductance more consistent with hybrid heterodimerized Kir6.1/6.2 channels than with homotetrameric Kir6.1 or 6.2 channels (Cui et al., 2001). Only a single patch revealed a minoxidil-elicited lower-amplitude current more consistent with a Kir6.1 homotetramer structure. Thus, although some structural homogeneity is possible, our collective findings suggest that KATP channels in rat mesenteric LMCs represent Kir6.1/Kir6.2 pore structures coassembled with regulatory SUR2 subunits. In this respect, KATP channels in LMCs may be molecularly unique from their counterparts in the arterial vasculature, which appear to be predominantly Kir6.1 homotetramers coassembled with SUR2.

The present study has several limitations. First, we used the rat mesenteric lymphatic circulation in our study because it is amenable to high-speed optical imaging. However, further studies are needed to ensure our findings translate to other lymphatic circulations, including those of humans. Second, it is possible that the concentrations of KCOs may differ between plasma, interstitial fluid, and lymph after systemic administration. In our study, we assumed that LVs would be exposed to plasma concentrations of KCOs in vivo after systemic administration of these medications, but we failed to find information to help us predict the pattern of KCO partitioning. Finally, instead of infusing the KCOs systemically, we chose to topically apply cromakalim and minoxidil sulfate to determine the effect of KCOs on mesenteric lymph flow in vivo. Topical application ensured tight control of KCO concentration at the level of the LV and guaranteed an absence of KCO-elicited systemic effects that could have confounded interpretation of results. In contrast, systemic administration is potentially fraught with difficulties in data interpretation because of the poorly characterized pharmacokinetic profiles of minoxidil sulfate and diazoxide in rats and the unintended effects of KCOs on blood pressure that could indirectly affect capillary filtration and thereby lymph flow.

In summary, it is assumed that KCOs cause edema by strongly dilating arterioles and increasing capillary pressure to promote fluid movement from the intravascular to the interstitial space (Sica, 2003; Mortimer and Levick, 2004). However, our findings suggest that KCO medications at clinically relevant plasma concentrations also directly disrupt lymphatic contractions and lymph flow as another potential mechanism of edema formation. Finally, our new evidence that KATP channels in rat mesenteric LMCs may predominantly represent Kir6.1/6.2 heterotetramers coassembled with SUR2 implies that LMCs may express KATP channel populations that differ from the predominantly Kir6.1 homotetrameric channels of the arterial circulation. In this regard, the KCOs in clinical practice are known to bind to sulphonylurea receptors to disinhibit arterial Kir6.1 channels and induce vasodilation. However, it is conceivable that the coassembly of Kir6.1 and Kir6.2 subunits in LMCs may provide a novel three-dimensional structure containing binding domains with lower affinity for novel pore-targeting KCOs than their arterial counterparts. In this case, it may be possible to design new KCOs that bind selectively to KATP channels in arterial SMCs to mediate vasodilation but avoid activation of the KATP channels in LMCs to prevent peripheral edema or ameliorate its severity.

Authorship Contributions

Participated in research design: Garner, Rusch, Mu.

Conducted experiments: Garner, Stolarz, Stuckey, Liu.

Contributed new reagents or analytical tools: Sarimolloaglu.

Performed data analysis: Garner, Stolarz, Rusch, Mu.

Wrote or contributed to the writing of the manuscript: Garner, Stolarz, Palade, Rusch, Mu.

Footnotes

    • Received May 21, 2020.
    • Accepted October 8, 2020.

  • This work was supported by National Institutes of Health National Cancer Institute [Grant R21-CA131164] and National Heart, Lung, and Blood Institute [Grant R01-HL146713] as well as the Systems Pharmacology and Toxicology Training Program [Grant T32-GM106999], the Center for Studies of Host Response to Cancer Therapy through Center of Biomedical Research Excellence Award [Grant P20-GM109005]; and the Center for Microbial Pathogenesis and Host Inflammatory Responses [Grant P20-GM103625] through National Institute of General Medical Sciences Centers of Biomedical Research Excellence. The content is solely the responsibility of the authors and does not necessarily represent the official views of NIH.

  • This work has been partially presented in meeting abstracts: Garner BR, Stolarz AJ, Fletcher TW, and Rusch NJ ATP-Sensitive K+ Channels in Smooth Muscle Cells from Rat Mesenteric Lymph Vessels. Poster presentation at Experimental Biology; 2017 April; Chicago, IL; Garner BR, Stolarz AJ, Fletcher TW, Mu S, and Rusch NJ Potassium Channel Openers Inhibit Rhythmic Contractions and Lymph Flow in Rat Mesenteric Lymph Vessels. Poster presentation at North American Vascular Biology Organization’s Vasculata Workshop; 2018 July; St. Louis, MO.

  • https://doi.org/10.1124/jpet.120.000121.

  • ↵Embedded ImageThis article has supplemental material available at jpet.aspetjournals.org.

Abbreviations

EDD
end diastolic diameter
FITC
fluorescein isothiocyanate
IB
isolation buffer
KATP
ATP-sensitive potassium
KCO
KATP channel opener
LV
lymph vessel
LMC
lymphatic muscle cell
PCR
polymerase chain reaction
PSS
physiologic saline solution
SMA
smooth muscle actin
SMC
smooth muscle cell
SUR
sulfonylurea receptor

This is an open access article distributed under the CC BY-NC Attribution 4.0 International license.

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Research ArticleCardiovascular

KATP Channel Openers Inhibit Lymphatic Contractions and Flow

Brittney R. Garner, Amanda J. Stolarz, Daniel Stuckey, Mustafa Sarimollaoglu, Yunmeng Liu, Philip T. Palade, Nancy J. Rusch and Shengyu Mu
Journal of Pharmacology and Experimental Therapeutics January 1, 2021, 376 (1) 40-50; DOI: https://doi.org/10.1124/jpet.120.000121
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