Articles in PresS. Am J Physiol Renal Physiol (January 28, 2015). doi:10.1152/ajprenal.00376.2014
MS#: F-00376-2014R1, Revised Manuscript 1
MS#: F-00376-2014R1, Revised Manuscript
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Am J Physiol Renal Physiol
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Extracellular pH affects phosphorylation and intracellular trafficking of AQP2 in inner medullary collecting duct cells
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Hyo-Jung Choi1,2, Hyun Jun Jung1, and Tae-Hwan Kwon1,2
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Department of Biochemistry and Cell Biology, 2BK21 Plus KNU Biomedical Convergence Program, Department of Biomedical Science, School of Medicine, Kyungpook National University, Taegu, Korea
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Running title: Extracellular pH affects dDAVP-induced AQP2 trafficking
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Correspondence: Tae-Hwan Kwon, MD, PhD, Department of Biochemistry and Cell Biology, School of Medicine, Kyungpook National University, Dongin-dong 101, Taegu 700-422, South Korea. Tel: +82 53 420 4825; Fax: +82 53 422 1466. E-mail:
[email protected] 30 31 32 33 34 35 36 37 38 1
Copyright © 2015 by the American Physiological Society.
MS#: F-00376-2014R1, Revised Manuscript
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Abstract
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Kidney collecting duct cells are continuously exposed to the changes of extracellular pH
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(pHe). We aimed to study the effects of altered pHe on dDAVP-induced phosphorylation
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(S256, S261, S264, and S269) and apical targeting of AQP2 in rat kidney inner medullary
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collecting duct (IMCD) cells. When freshly prepared IMCD tubule suspensions exposed to
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HEPES buffer with pH 5.4, 6.4, 7.4, or 8.4 for 1 h were stimulated with dDAVP (10-10 M, 3
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min), AQP2 phosphorylation at S256, S264, and S269 was significantly attenuated in acidic
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conditions. Next, IMCD cells primary cultured in the transwell chambers were exposed to
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transepithelial pH gradient for 1 h (apical pH 6.4, 7.4 or 8.4 vs. basolateral pH 7.4 and vice
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versa). Immunocytochemistry and cell surface biotinylation assay revealed that exposure to
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either apical pH 6.4 or basolateral pH 6.4 for 1 h was associated with decreased dDAVP (10-9
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M, 15 min, basolateral)-induced apical targeting of AQP2 and surface expression of AQP2.
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Fluorescence resonance energy transfer analysis revealed that dDAVP (10-9 M)-induced
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increase of PKA activity was significantly attenuated when LLC-PK1 cells were exposed to
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pHe 6.4, compared to pHe 7.4 and 8.4. In contrast, forskolin (10-7 M)-induced PKA activation
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and dDAVP (10-9 M)-induced increase of intracellular Ca2+ were not affected. Taken together,
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dDAVP-induced phosphorylation and apical targeting of AQP2 are attenuated in IMCD cells
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under acidic pHe, likely via an inhibition of V2R-G-protein-cAMP-PKA action.
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Key words: Acidosis, Collecting duct, FRET, Vasopressin, V2R receptor.
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Introduction
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Renal tubular epithelial cells, including the kidney collecting duct cells, are
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continuously exposed to the changes of microenvironment, e.g., luminal fluid shear stress,
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transepithelial osmotic gradient, and changes of luminal or interstitial pH. We previously
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demonstrated the effects of altered luminal fluid shear stress (FSS) on the translocation of
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aquaporin-2 (AQP2) and the reorganization of actin cytoskeleton (F-actin) in the kidney inner
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medullary collecting duct (IMCD) cells (14). Immunocytochemistry demonstrated that
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exposure to luminal FSS per se in the microfluidic chamber induced depolymerization of F-
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actin associated with increased apical targeting of AQP2, even in the absence of vasopressin
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stimulation. This finding suggests that changes of microenvironment, including extracellular
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pH, could be importantly involved in the apical targeting of AQP2.
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Aquaporins (AQPs) are a family of membrane proteins that transport water molecules
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through biomembranes (18, 21, 31). AQP2 is the water-selective channel protein that plays a
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key role in arginine vasopressin (AVP)-mediated water reabsorption in the collecting ducts (2,
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20, 21, 27, 30, 31, 41). Vasopressin V2-receptor (V2R)-mediated cAMP/PKA signaling has
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been shown to be a principal signaling pathway for both AQP2 trafficking and protein
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expression via activation of Gsα-mediated adenylyl cyclase activity (7, 16, 30, 41, 42).
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However, despite the well-known effects of AVP stimulation, the concurrent effects of
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changes in luminal or interstitial microenvironment in vivo, e.g., pH, on the phosphorylation
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and apical targeting of AQP2 in the collecting duct cells, are not well understood. Urine pH
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can vary between 4.6 and 8.0, depending on the amount of urinary net acid excretion. A
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recent clinical study demonstrated that almost 60% of patients with stones had a urine pH less
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than 6, a figure consistent with that found in the general population (3). It has been
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demonstrated that the affinity of vasopressin for V2R was significantly lower under the 3
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condition of acidic pH, compared to that at neutral pH in LLC-FLAG-V2R cells (44).
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Moreover, rats with metabolic acidosis were associated with significantly decreased urinary
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excretion of AQP2, whereas renal AQP2 mRNA and protein expressions were increased (28).
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In addition, it has been demonstrated that urine alkalinization promoted the excretion of
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urinary exosomal AQP2 independent of vasopressin stimulation in rats (9).
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Therefore, we hypothesized that changes in the extracellular pH (pHe) could affect the
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intracellular pH (pHi) of the collecting duct cells, resulting in altered response of AQP2
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phosphorylation (S256, S261, S264, S269) and apical targeting of AQP2 to vasopressin
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stimulation. Firstly, dDAVP-induced AQP2 phosphorylation (S256) was examined in IMCD
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tubule suspensions exposed to pH 5.4, pH 6.4, pH 7.4 and pH 8.4, respectively. To study the
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selective effects of apical or basolateral pH on the dDAVP-induced intracellular trafficking of
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AQP2 in the collecting duct cells, IMCD cells of rat kidneys were primary cultured in the
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transwell chamber system. The effects of acidic (pH 6.4), neutral (pH 7.4), or alkaline (pH
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8.4) conditions in the apical or basolateral side of the cells were examined on the dDAVP-
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induced intracellular trafficking and cell surface expression of AQP2. Moreover, for further
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elucidating the underlying signaling mechanisms, fluorescence resonance energy transfer
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(FRET) analysis was exploited and time-lapse changes of AVP- or forskolin-induced PKA
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activity and intracellular Ca2+ dynamics were monitored in LLC-PK1 cells exposed to acidic
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(pH 6.4), neutral (pH 7.4), or alkaline (pH 8.4) microenvironment.
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Materials and Methods
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Primary culture of IMCD cells of rat kidney. The animal protocols were approved by the
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Animal Care and Use Committee of the Kyungpook National University, Korea (KNU 2012-
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10). Primary cultures enriched in IMCD cells were prepared from pathogen-free male
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Sprague-Dawley rats (200 - 250 g, Charles River, Seongnam, Korea), as previously described
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in detail (6, 23, 24). Briefly, rats were anesthetized under enflurane inhalation, and kidneys
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were rapidly removed. After isolating IMCD cell suspension, cells were seeded either on the
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collagen-coated 35-mm glass-base dish (Asahi Techno Glass, Tokyo, Japan) for intracellular
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pH measurement or on the semi-permeable filters of transwell system (0.4 µm pore size,
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Transwell® Permeable Supports, catalog no. 3450, Corning) for cell surface biotinylation
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assay. IMCD cells were fed every 48 h and were grown in hypertonic culture medium (640
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mOsm/KgH2O) supplemented with 10% fetal bovine serum at 37C in 5% CO2, 95% air
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atmosphere for 3 days, and then in fetal bovine serum-free culture medium for additional 1
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day before the experiment at day 5. The culture medium was Dulbecco's modified Eagle's
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medium/F12 without phenol red, containing 80 mM urea, 130 mM NaCl, 10 mM HEPES, 2
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mM L-glutamine, penicillin/streptomycin 10,000 units/ml, 50 nM hydrocortisone, 5 pM
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3,3,5-triiodo-thyronine, 1 nM sodium selenate, 5 mg/L transferrin, and 10% fetal bovine
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serum (pH 7.4, 640 mOsm/KgH2O).
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IMCD tubule suspensions. Fresh inner medullary collecting duct (IMCD) tubules were
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prepared from rat kidneys, as previously described (5, 35). Rats were anesthetized under
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enflurane inhalation. Kidney inner medulla was dissected, minced, and digested in IMCD
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suspension buffer (250 mM sucrose, 10 mM triethanolamine, pH 7.4) containing collagenase
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B (3 mg/ml) and hyaluronidase (2 mg/ml). Then, IMCD suspension was continuously 5
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agitated in a warm water bath at 37°C for 90 min. Thereafter, IMCD tubule suspension was
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centrifuged at 60 g for 30 sec to separate the IMCD-enriched fraction (pellet) and the non-
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IMCD fraction (supernatant). IMCD-enriched fraction was collected and washed twice with
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ice-cold IMCD suspension buffer. For the experiments, IMCD tubule suspensions were
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exposed to the HEPES-buffered saline solution (162.5 mM NaCl, 2.5 mM Na2HPO4, 4 mM
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KCl, 25 mM HEPES, 2 mM CaCl2, 1.2 mM MgSO4, and 5.5 mM glucose) with different pH
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(pH 5.4, 6.4, 7.4 or 8.4) for 1 h, which was established by adding HCl (for pH 5.4) or NaOH
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(for pH 6.4, 7.4, and 8.4) (43). dDAVP stimulation (10-10 M) was done during the last 3 min
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(Fig. 1A).
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Semiquantitative immunoblotting. SDS-PAGE was performed on 12% polyacrylamide gels,
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as previously described (34). Primary antibodies used were anti-AQP2 (H7661AP, 1:2,000)
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(15, 23), anti-phosphorylated AQP2 at S256 (K0307AP, 1:3,000) (34), anti-phosphorylated
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AQP2 at S261, S264 and S269 (Phosphosolutions, 1:1,000), and anti-β-actin (Sigma,
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1:100,000).
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Immunofluorescence microscopy of primary cultured IMCD cells. IMCD cells were grown
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to confluence in each transwell chamber (0.4 µm pore size, Transwell® Permeable Supports,
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catalog no. 3460, Corning) for 4 days. At day 5, IMCD cells were subjected to transepithelial
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pH gradient for 1 h (pH 6.4, 7.4 or 8.4 at the apical side vs. pH 7.4 at the basolateral side and
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vise versa) at 37°C. dDAVP stimulation (10-9 M, 15 min, basolateral side only) was done
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during the last 15 min and then fixed with 3% paraformaldehyde in PBS, pH 7.4 for 20 min at
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room temperature. After fixation, cells were washed twice in PBS and permeabilized with
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0.3% Triton X-100 in PBS at room temperature for 15 min. Cells were washed, the labeled
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with anti-AQP2 (H7661AP, 1:200) antibody and nucleus was stained with DAPI. The AQP2 6
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localization was determined using laser confocal microscopy (Zeiss LSM 5 EXCITER, Jena,
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Germany), and an X63 (NA 1.4) objective lens (Zeiss) was used. Digital images were
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collected and analyzed using the Zeiss Aim Image Examiner program.
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Cell surface biotinylation assays. IMCD cells were primary cultured for 4 days on semi-
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permeable filters of transwell system (0.4 µm pore size, catalog no. 3450, Transwell®
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Permeable Supports, Corning Incorporated, MA). At day 5, they were exposed to
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transepithelial pH gradient for 1 h (apical pH 6.4, 7.4 or 8.4 vs. basolateral pH 7.4 and vice
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versa) at 37°C. Then, the cells were washed three times with ice-cold PBS-CM (10 mM PBS
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containing 1 mM CaCl2 and 0.1 mM MgCl2, pH 7.5) and incubated at 4˚C for 45 min in ice-
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cold biotinylation buffer (10 mM triethanolamine, 2 mM CaCl2, 125 mM NaCl, pH 8.9)
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containing 1 mg/ml sulfosuccinimidyl 2-(biotinamido)-ethyl-1,3-dithiopropionate (Sulfo-
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NHS-SS-biotin, Thermo Scientific, Rockford, IL) on the apical side. Cells were washed once
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with quenching buffer (50 mM Tris-HCl in PBS-CM, pH 8.0) followed by washing twice
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with PBS-CM. Lysis buffer (1% triton X-100, 150 mM NaCl, 5 mM EDTA, 50 mM Tris-HCl,
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pH 7.5, 1.15 mM PMSF, 0.4 μg/ml leupeptin, 0.1 mg/ml pefabloc, 0.1 μM okadaic acid, 1
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mM Na3VO4, 25 mM NaF) was added and the lysates were sonicated 2 × 6 pluses at 20% of
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amplitude. The lysates were centrifuged at 10,000 g for 5 min at 4˚C. The supernatant was
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transferred to columns where Neutravidin agarose resin (200 μl) was previously loaded
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(Thermo Scientific, Rockford, IL) and incubated for 60 min at RT with end-over-end mixing.
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After 4 times washing with PBS containing protease inhibitors, 1 × sample buffer containing
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DTT was added to the column and incubated for 60 min at RT. Samples were heated at 65˚C
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for 10 min.
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Intracellular pH measurement. Intracellular pH (pHi) was measured using the pH-sensitive 7
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fluorescent
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(BCECF-AM, Molecular Probes). BCECF-AM is converted to the membrane-impermeant
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fluorescent dye BCECF by intracellular esterases. Primary cultured IMCD cells of rat kidney
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were seeded and cultured on the collagen-coated 35-mm glass-base dish (Asahi Techno Glass,
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Tokyo, Japan) in hypertonic culture media (pH 7.4 and 640 mOsm/kgH2O) for 4 days. On
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day 5, cells were incubated with non-serum IMCD culture media (Dulbecco's modified
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Eagle's medium/F12 without phenol red, 80 mM urea, 130 mM NaCl, penicillin/streptomycin
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10,000 units/ml) containing 2 µM BCECF-AM at 37C in 5% CO2-95% air for 30 min. The
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cells were washed twice in PBS and changed to non-serum IMCD culture media (pH 7.4) for
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10 min at 37C incubator before the experiments. IMCD cells were mounted in the chamber
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on the temperature-controlled stage of Nikon Ti-E inverted microscope (Nikon, Tokyo,
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Japan). The cells were continuously perfused with a Na+-free solution with different pH
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values (pH 6.4, 7.4, and 8.4, see below) for 60 min by six-channel system (VC-2, Warner
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Instruments, Hamden, CT) and perfusate was collected by the peristaltic pump (EYELA MP3,
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Tokyo, Japan).
dye,
(2,7)-biscarboxyethyl-5(6)-carboxyfluorescein
acetoxymethyl
ester
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The pHi was measured using the dual-excitation fluorescence ratio method. The
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fluorescence was monitored at 530 nm with excitation wavelengths of 440 nm (a wavelength
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at which the fluorescence is relatively pH insensitive) and 490 nm (at which the fluorescence
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is very pH sensitive). The pHi was time-lapse obtained by the Nikon Ti-E inverted
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microscope (Nikon, Tokyo, Japan) equipped with Cascade 512B (EMCCD) camera (Roper
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Scientific, Trenton, NJ) and excitation and emission filter wheels (MAC5000, Ludl Electronic
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Products, Hawthorne, NY). All systems were controlled by MetaMorph software (Universal
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Imaging, Downingtown, PA). Fluorescent images were acquired sequentially through CFP
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filter channels. Images were acquired by using the 4 x 4 binning mode and 200-ms exposure
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time. A X60 (NA 1.4, Nikon, Tokyo, Japan) objective lens was used for the measurements. 8
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The 490/440 nm ratio was created by MetaMorph software. The data were obtained from five
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independent experiments in both groups, respectively.
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The pHi was calculated by the nigericin calibration technique (3). IMCD cells were
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exposed to a Na+-free solution (0 mM Na+, 105 mM K+, 0 mM NH4+, 49 mM NMDG+, 5 mM
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Mg2+, 0 mM Ca2+, 6.3 mM Cl-, 106.4 mM Aspartate-, 0.4 mM H2PO4-, 1.6 mM HPO42-, 17.8
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mM HEPES-, 0 mM HCO3-, 5 mM SO42-, 10 mM EGTA2-, 5.5 mM glucose, 5 mM alanine,
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14.4 mM HEPES) with different pH values (6.4, 7.4, and 8.4) by adding KOH, containing 10
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µM of the K+-H+ exchanger nigericin. When the [K+] was equal between the intracellular and
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extracellular compartments, pHi and pHe should be the same with nigericin (490/440 nm
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ratio = 1.0, pH = 7.0) (3). Therefore the data were normalized to make the ratio at pH 7.0
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equal to unity. Raw data of intensity at each excitation wavelength were corrected for
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background-corrected fluorescence intensity prior to calculation of the ratios. The ratios of
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background-corrected emission intensities (490/440 nm ratio) were transformed into pH
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values as pH = log [(Rn-Rn(min))/(Rn(max)-Rn)] + pKa, where Rn was the background-
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substracted ratio normalized to pH 7.0, Rn(min) and Rn(max) are the minimum and maximum
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obtainable values for the normalized ratio and pKa is the –log of the dissociation constant of
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the fluorophore (1, 3).
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Fluorescence resonance energy transfer imaging for PKA activity. LLC-PK1 cells stably
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transfected with AKAR3EV (PKA fluorescence resonance energy transfer (FRET)-based
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indicator) were cultured on a collagen-coated 35-mm glass-base dish (Asahi Techno Glass,
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Tokyo, Japan). The plasmid for PKA FRET-based indicator (AKAR3EV) was kindly
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provided by Prof. M. Matsuda (Kyoto University, Kyoto, Japan). AKAR3EV was composed
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of the FHA1 (ligand domain), yellow fluorescent protein (YFP), sensor domain of PKA
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(LRRATLVD), and cyan fluorescent protein (CFP) (17). In this probe design, the sensor 9
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domain changes its conformation upon perception of the PKA signal (17). This sensitized
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sensor domain interacts with the ligand domain, thereby inducing a global change of the
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biosensor conformation and concomitant increase of FRET efficiency from the donor to the
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acceptor. With this AKAR3EV probe, the activity of PKA was time-lapse obtained by Nikon
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Ti-E inverted microscope (Nikon, Tokyo, Japan) equipped with a Cascade 512B (EMCCD)
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camera (Roper Scientific, Trenton, NJ) and excitation and emission filter wheels (MAC5000,
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Ludl Electronic Products, Hawthorne, NY). All systems were controlled by MetaMorph
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software (Universal Imaging, Downingtown, PA). Fluorescent images were acquired every 15
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sec sequentially through CFP and FRET filter channels. Images were acquired by using the 4
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x 4 binning mode and 200-ms exposure time. The FRET/CFP ratio was created with
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MetaMorph software, and the value was normalized to 1 at the starting time point in both
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groups. The data were obtained from five independent experiments in both groups,
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respectively.
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Fluorescence resonance energy transfer imaging for intracellular calcium dynamics. Two
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days after the transient transfection of YC3.60 (calcium FRET-based indicator) (29), LLC-
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PK1 cells in Dulbecco’s Modified Eagle Medium (phenol red-free) were subjected to time-
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lapse imaging. LLC-PK1 cells transiently transfected with YC3.60 were cultured on a
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collagen-coated 35-mm glass-base dish (Asahi Techno Glass, Tokyo, Japan). The plasmid for
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calcium FRET-based indicator (YC3.60) was also provided by Prof. M. Matsuda (Kyoto
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University, Kyoto, Japan). YC3.60 was composed of the calmodulin (CaM), enhanced yellow
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fluorescent protein (EYFP), a glycylglycine linker, the CaM-binding peptide of myosin light-
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chain kinase (M13), and an enhanced cyan fluorescent protein (ECFP) (29). Ca2+ ion binding
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to CaM moiety initiates an intramolecular interaction between the CaM and the M13 domains,
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which causing the chimeric protein to shift from a spread form to a more compact form, 10
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therefore increasing the efficiency of FRET from the CFP to the YFP (29). With this YC3.60
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indicator, the changes of intracellular Ca2+ levels were time-lapse obtained by Nikon Ti-E
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inverted microscope (Nikon, Tokyo, Japan). Images were acquired every 15 sec by using the
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4 x 4 binning mode and 200-ms exposure time. The FRET/CFP ratio was created with
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MetaMorph software, and the value was normalized to 1 at the starting time point in all
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groups. The data were obtained from eight independent experiments in both groups,
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respectively.
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Statistical analyses. Values were presented as means ± standard errors. Data were analyzed
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by one-way analysis of variance (ANOVA) followed by Bonferroni’s multiple comparison
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test. Multiple comparisons tests were only applied when a significant difference was
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determined in the ANOVA, P