Stimulation of Na+/K+-ATPase activity in alveolar epithelial cells by cAMP involves its recruitment from intracellular compartments to the plasma membrane. Here, we studied the role of the actin molecular motor myosin-V in this process. We provide evidence that, in alveolar epithelial cells, cAMP promotes Na+/K+-ATPase recruitment to the plasma membrane by increasing the average speed of Na+/K+-ATPase-containing vesicles moving to the cell periphery. We found that three isoforms of myosin-V are expressed in alveolar epithelial cells; however, only myosin-Va and Vc colocalized with the Na+/K+-ATPase in intracellular membrane fractions. Overexpression of dominant-negative myosin-Va or knockdown with specific shRNA increased the average speed and distance traveled by the Na+/K+-ATPase-containing vesicles, as well as the Na+/K+-ATPase activity and protein abundance at the plasma membrane to similar levels as those observed with cAMP stimulation. These data show that myosin-Va has a role in restraining Na+/K+-ATPase-containing vesicles within intracellular pools and that this restrain is released after stimulation by cAMP allowing the recruitment of the Na+/K+-ATPase to the plasma membrane and thus increased activity.
The Na+/K+-ATPase is an essential enzyme that generates the Na+ and K+ gradients required for maintaining membrane potentials, cell volume, and secondary transport of other solutes, such as transcellular transport in the intestine, kidneys and lungs (Gadsby, 2007; Jorgensen et al., 2003; Sznajder et al., 2002). In the lungs, the Na+/K+-ATPase located at the basolateral plasma membrane drives the vectorial Na+ transport across the alveolar epithelium necessary to keep the alveoli free of edema (Mutlu and Sznajder, 2005; Sznajder et al., 2002). Alveolar fluid reabsorption is increased after stimulation of Na+/K+-ATPase activity by G-protein-coupled-receptor (GPCR) agonists that activate the second messenger cAMP (Frank et al., 2000; Litvan et al., 2006; Saldias et al., 1998). cAMP increases the Na+/K+-ATPase function in alveolar epithelial cells by promoting its recruitment from intracellular vesicle pools into the plasma membrane (Bertorello et al., 1999; Lecuona et al., 2003).
Trafficking of vesicles from intracellular pools to the plasma membrane typically involves their transport along microtubules and actin filaments (Soldati and Schliwa, 2006). To accomplish this task, cells utilize molecular motors. Actin-based molecular motors constitute a superfamily of proteins, called myosins (Berg et al., 2001; Richards and Cavalier-Smith, 2005). They use the energy from cycles of ATP binding, hydrolysis, and product release to perform mechanical work along actin filaments (De La Cruz and Ostap, 2004). Within the myosin family, a major actin molecular motor involved in intracellular trafficking is myosin-V, which is involved in the transport of vesicles and organelles in several cell types (Langford, 2002; Mermall et al., 1998). Three genes encoding myosin-V (myosin-Va, Vb and Vc) have been described with specific distribution in different tissues (Espreafico et al., 1992; Rodriguez and Cheney, 2002; Zhao et al., 1996). Myosin-Va has been shown to be involved in the transport of many vesicular carriers, including dense core secretory vesicles (Ivarsson et al., 2005; Varadi et al., 2005), melanosomes (Wu et al., 1998; Wu et al., 1997) and GLUT4-containing vesicles (Yoshizaki et al., 2007), and a role for myosin-Va in tethering vesicles to the actin cytoskeleton has also been suggested (Wu et al., 1998).
We generated an alveolar epithelial cell line that expresses the Na+/K+-ATPase α1-subunit tagged with GFP and, using these cells, we reported that GPCR agonist stimulation increases the directional movement of ATPase-containing vesicles (Bertorello et al., 2003). In the present study, we investigated the role of myosin-V in the recruitment of the Na+/K+-ATPase to the plasma membrane. We provide evidence that myosin-Va has a role in restraining Na+/K+-ATPase-containing vesicles in the intracellular pool; furthermore, the inhibition of myosin-Va by overexpression of a dominant-negative mutant or knockdown with shRNA results in increased traffic and insertion of the Na+/K+-ATPase into the plasma membrane, which is not sensitive to further stimulation.
cAMP increases Na+/K+-ATPase localization at the plasma membrane and the distance traveled by the Na+/K+-ATPase-containing vesicles in A549-GFPα1 cells
To establish whether the A549-GFPα1 cells are a good model to study the effects of cAMP on the Na+/K+-ATPase traffic, we incubated the cells for 10 minutes with 50 μM of the adenylyl cyclase activator forskolin (FSK) at 37°C. As shown in Fig. 1, incubation with FSK increased Na+/K+-ATPase activity (Fig. 1A) as well as the Na+/K+-ATPase protein abundance at the plasma membrane (Fig. 1B), suggesting that in response to FSK the Na+/K+-ATPase is recruited to the plasma membrane from intracellular pools as previously described (Bertorello et al., 1999; Lecuona et al., 2003).
Live imaging of A549-GFPα1 cells showed that, after incubation with FSK for 1 minute, the average speed of the GFP-containing vesicles moving towards the cell periphery increased by ∼80% (Fig. 1C,D) (control, 0.08±0.03 μm/second; FSK, 0.15±0.04 μm/second; P<0.05).
Myosin-Va and myosin-Vc colocalize with the Na+/K+-ATPase in intracellular compartments
To study whether myosin-V has a role in Na+/K+-ATPase trafficking, we determined its expression in A549 cells. We found that the three isoforms of myosin-V (a, b and c) were detected at the mRNA level (Fig. 2A) and at the protein level (Fig. 2B). As shown in Fig. 2C,D, the three myosin-V isoforms distributed equally in fraction 6 of a broad sucrose gradient in which the Na+/K+-ATPase peaks, although the overall distribution of each isoform varied across different fractions.
To elucidate which myosin-V isoform has a role in the traffic of Na+/K+-ATPase, we isolated the intracellular fraction enriched in the cAMP-responsive Na+/K+-ATPase vesicles (Fig. 3A) (Bertorello et al., 1999). This fraction was loaded on a broad sucrose gradient (2 M to 0.5 M) and analyzed for distribution of the Na+/K+-ATPase and myosin-V isoforms. Fig. 3B shows that Na+/K+-ATPase present in the intracellular compartment distributed mainly in fractions 4 to 7. Myosin-Va and myosin-Vc co-distributed in the same fractions, whereas myosin-Vb was not detectable.
Myosin-Va is a negative regulator of the long-range movement of Na+/K+-ATPase-containing vesicles
To determine whether myosin-Va and/or myosin-Vc have a role in cAMP-induced Na+/K+-ATPase traffic, we analyzed by live-cell imaging A549-GFPα1 cells transiently transfected with dominant-negative (DN) myosin-Va (DN-Va) or with DN myosin-Vc (DN-Vc) containing an m-cherry tag. As shown in Fig. 4A,B, expression of m-cherry-DN-Va increased the basal motility of GFP-containing vesicles, motility that was not further increased by FSK. m-Cherry-DN-Vc did not have any effect on the baseline motility nor did it prevent cAMP-mediated stimulation (Fig. 4C,D). These data suggest a role for myosin-Va in the regulation of the basal motility of the GFP-containing vesicles (but not for myosin-Vc) and were confirmed in experiments using shRNA against myosin-Va and myosin-Vc (Fig. 5). We found increased basal motility of GFP-containing vesicles in cells transfected with the shRNA against myosin-Va (Fig. 5A,C) and no change in motility in the cells where myosin-Vc was knocked down (Fig. 5B,C). Knockdown of myosin-Va and myosin-Vc using these shRNA was ∼65% (Fig. 5D).
To study the role of myosin-Va in the recruitment of Na+/K+-ATPase-containing vesicles, we generated A549-GFPα1 cells clones permanently transfected with DN-Va or DN-Vc tagged with V5 (Fig. 6A). Cells were incubated with 50 μM FSK for 10 minutes, which increased the Na+/K+-ATPase activity (Fig. 6B) and protein abundance at the plasma membrane (Fig. 6C) in control cells and cells expressing DN-Vc. However, DN-Va cells had increased baseline levels of Na+/K+-ATPase activity and protein abundance at the plasma membrane and treatment with FSK did not result in further stimulation (Fig. 6B,C). These data are in agreement with the colocalization of the GFP-containing vesicles and myosin-Va observed by immunofluorescence (Fig. 7).
Taken together, these data suggest that myosin-Va has a restraining role on Na+/K+-ATPase-containing vesicles and that this restraint is released upon FSK stimulation. These observations are consistent with the finding that disruption of the microtubule network prevented Na+/K+-ATPase traffic (Fig. 8A,C), whereas depolymerization of the actin cytoskeleton increased it (Fig. 8B,C).
Short-term regulation of Na+/K+-ATPase activity can result from its traffic between intracellular compartments and the plasma membrane (Bertorello and Sznajder, 2005; Clausen, 2003; Dunbar and Caplan, 2001; Therien and Blostein, 2000). β-adrenergic receptor agonists have been shown to upregulate the Na+/K+-ATPase function via cAMP by promoting its recruitment from intracellular compartments into the plasma membrane in alveolar epithelial cells, which results in increased Na+ transport and enhanced lung edema clearance (Bertorello et al., 1999; Lecuona et al., 2003; Saldias et al., 1998). Recruitment of Na+/K+-ATPase-containing vesicles into the plasma membrane is known to involve both microtubules and the actin network (Bertorello et al., 2003; Bertorello et al., 1999; Saldias et al., 1998). Here, we provide the first evidence for the role of an actin-based motor, myosin-Va, in the modulation of the microtubule-dependent movement of the Na+/K+-ATPase in alveolar epithelial cells.
We have generated a human alveolar epithelial cell line that expresses GFP-tagged Na+/K+-ATPase α1-subunit. This cell line has been utilized for the study of trafficking of the Na+/K+-ATPase-containing vesicles (Bertorello et al., 2003). These cells responded to stimulation by cAMP by increasing Na+/K+-ATPase protein abundance and activity at the plasma membrane, in parallel with an increase in the distance traveled (see Fig. 1).
We focused on the role of the myosin-V family of molecular motors, because there is much evidence implicating them in organelle movement (Mermall et al., 1998). Moreover, the presence of myosin-V has been described in organelles that associate with both microtubules and actin (Kuznetsov et al., 1992; Rogers and Gelfand, 1998). We analyzed the presence of the three myosin-V motors, myosin-Va, myosin-Vb and myosin-Vc (Espreafico et al., 1992; Rodriguez and Cheney, 2002; Zhao et al., 1996), and found that the three isoforms were expressed both at the mRNA and at the protein levels, although only myosin-Va and myosin-Vc were found in the intracellular compartment from which the Na+/K+-ATPase moves towards the plasma membrane upon stimulation by cAMP (Bertorello et al., 1999). These findings were somewhat surprising because myosin-Vb has been shown to be involved in the traffic of proteins known to be stimulated by cAMP, such as aquaporin-2 in renal cells (Nedvetsky et al., 2007).
A powerful tool to study the role of myosin-V in the traffic of organelles/vesicles is the overexpression of its tail domain, which competes for binding to the cargo, but lacks the actin-interacting head and thus, acts as a dominant-negative inhibitor (Rodriguez and Cheney, 2002; Rogers et al., 1999). This technique has been useful to study myosin-Va in the traffic of intracellular organelles and vesicles, such as secretory granules in PC12 cells (Rudolf et al., 2003), small synaptic vesicles (Prekeris and Terrian, 1997) and melanosomes (Rogers et al., 1999; Wu et al., 1997). Time-lapse imaging of live cells showed that in basal conditions, the movement of Na+/K+-ATPase-containing vesicles followed a `random walk' pattern in agreement with a previous report (Bertorello et al., 2003). More significantly, we found that cAMP increased the average speed of the vesicles moving towards the cell periphery in control non-transfected cells and in cells transfected with DN-Vc. Cells expressing DN-Va experienced rapid microtubule-dependent vesicle movement to the periphery, independently of cAMP, similar to that observed in melanocytes lacking myosin-Va (Wu et al., 1998). Since a dominant-negative strategy has its pitfalls, such as non-specific effects on related proteins (Roos et al., 1999), we confirmed the role of myosin-Va in the regulation of the basal movement of the Na+/K+-ATPase by specifically knocking down the protein using an shRNA strategy.
Myosin-Va has a role in different aspects of the traffic of several vesicular carriers (Desnos et al., 2007; Eichler et al., 2006). It has been shown to be important in retaining these vesicular carriers (melanosomes, secretory granules) in the F-actin-rich cortex (Rudolf et al., 2003; Wu et al., 1998), and recently a role in fusion and exocytosis has also been reported via the interaction of myosin-Va with syntaxin-1A (Watanabe et al., 2005). Our data suggest that under basal conditions, microtubule-dependent transport of Na+/K+-ATPase-containing vesicles is restrained by myosin-Va. Experiments in cells overexpressing the DN-Va revealed increased Na+/K+-ATPase traffic and insertion into the plasma membrane that was similar to the effects of treating the cells with GPCR agonists.
Intracellular transport is a complex process, driven by at least three types of motors: kinesins and dyneins involved in bidirectional transport along microtubules and myosins that move along actin filaments (King, 2000; Mermall et al., 1998; Woehlke and Schliwa, 2000). Recent work suggests that switching between the two types of cytoskeletal tracks is based on a continuous `tug-of-war' between the two transport systems, where microtubule motors and myosins are simultaneously active on the same organelle and the choice of tracks is determined by competition between these motors (Gross et al., 2002).
Phosphorylation of myosin-Va has been reported to regulate its function (Karcher et al., 2001; Yoshizaki et al., 2007). Interestingly, phosphorylation at Ser1650 by CaMKII releases myosin-Va from melanosomes (Karcher et al., 2001). The consensus sequence for CaMKII (R-x-x-S/T) is very similar to the sequence for PKA (the main effector of cAMP) (Gronborg et al., 2002; O'Flaherty et al., 2004; Taylor et al., 2008), raising the possibility for phosphorylation of this residue in our system, which warrants further studies.
Accordingly, we provide the first evidence that myosin-Va regulates traffic of Na+/K+-ATPase containing-vesicles and that it has a key role in holding the Na+/K+-ATPase-containing vesicles in basal conditions, restraining its recruitment to the plasma membrane; this restraint is released upon stimulation with cAMP agonists.
Materials and Methods
All cell culture reagents were from Mediatech (Herndon, VA). 86Rb+ was purchased from Perkin Elmer (Billerica, MA). Ouabain was purchased from ICN Biomedicals (Aurora, OH). Percoll was from Amersham Biosciences (Uppsala, Sweden). Forskolin, nocodazole and cytochalasin D were from Calbiochem (La Jolla, CA). Restriction enzymes were purchased from Promega (Madison, WI). Rhodamine phalloidin was from Molecular Probes (Eugene, OR). Normal goat serum was purchased from Jackson ImmunoResearch Laboratories (West Grove, PA). Antibody against α-tubulin and all other chemicals were purchased from Sigma (St Louis, MO). Mouse anti-GFP (B-2), rabbit anti-E-cadherin, rabbit anti-Rab5a, rabbit anti-Rab7, and Protein A/G PLUS-Agarose were purchased from Santa Cruz Biotechnology (Santa Cruz, CA). Monoclonal anti-V5 antibody and secondary goat-anti-mouse Alexa Fluor 488 and 568 were from Invitrogen (Carlsbad, CA). Secondary goat anti-mouse-HRP and goat anti-rabbit-HRP were from Bio-Rad (Hercules, CA). Antibody against myosin-Va has been previously described (Rogers et al., 1999). Antibody against myosin-Vb was a gift from Alaa El-Husseini (University of British Columbia, Vancouver, Canada) and antibody against myosin-Vc was a gift from Richard Cheney (University of North Carolina at Chapel Hill, NC).
Human A549 (ATCC CCL 185) and HeLa cells (ATCC CCL 2) were grown in Dulbecco's modified Eagle's medium (DMEM) supplemented with 10% fetal bovine serum, 100 U/ml penicillin, 100 μg/ml streptomycin and 20 mM HEPES. A549 cells expressing the GFP-rat Na+/K+-ATPase-α1-subunit (A549-GFPα1) (Bertorello et al., 2003) were grown in the same conditions as above but 3 μM ouabain was added to the medium to suppress the endogenous Na+/K+-ATPase α1-subunit. Cells were incubated in a humidified atmosphere of 5% CO2, 95% air at 37°C.
The assay was run at 37°C in a reciprocating bath at 100 r.p.m. Cells were pre-incubated in serum-free DMEM, containing HEPES with or without 5 μM ouabain and 50 μM FSK for 5 minutes. Then, the medium was removed and fresh medium containing 1 μCi/ml 86Rb+, with or without 5 μM ouabain and 50 μM FSK was added. Following incubation for 5 minutes, uptake was terminated by aspirating the assay medium and washing the plates in 150 mM MgCl2 (4°C). Cells were air-dried and extracted with 0.1% NaOH. 86Rb+ influx was quantified by liquid scintillation counting. Initial influx, expressed as micromoles of K+/μg of protein per minute, was calculated as: Influx = (c.p.m./μg protein/5)/SAex, where SAex is the specific activity of the extracellular phase (c.p.m./μmol K+). The ouabain-inhibitable fraction of the Na+/K+-ATPase was measured as 86Rb+ uptake in the presence of 5 μM ouabain.
Preparation of basolateral membranes
A549-GFPα1 cells were incubated for 10 minutes with 50 μM FSK at 37°C, washed twice with ice-cold phosphate-buffered saline (PBS), and basolateral membranes were purified according to Hammond and Verroust by using a 16% Percoll gradient (Hammond et al., 1994).
Western blot analysis
Protein was quantified by Bradford assay (Bradford, 1976) (Bio-Rad) and resolved in 10% SDS-PAGE. Thereafter, proteins were transferred onto nitrocellulose membranes (Optitran, Schleider & Schuell, Keene, NH) using a semi-dry transfer apparatus (Bio-Rad). Incubation with specific antibodies was performed overnight at 4°C. Blots were developed with a chemiluminescence detection kit (PerkinElmer Life Sciences, Boston, MA) used as recommended by the manufacturer. The bands were scanned and quantified by ImageJ 1.41a (National Institutes of Health, USA).
Time-lapse epifluorescent microscopy of A549-GFPα1 cells was performed using a Nikon TE2000 (Nikon Instruments, Melville, NY) equipped with an environmental control system chamber (FCS2 system, Bioptechs, Butler, PA) and a Planapo ×60/1.4 NA objective (Nikon Instruments, Melville, NY). During imaging, the chamber was perfused with DMEM saturated with gas mixture containing 5% CO2 and 21% O2. Images were acquired every second with an exposure time of 0.5 seconds and collected with a Cascade EMCCD camera with on-chip multiplication gain (Photometrics, Tucson, AZ) driven by MetaMorph Software v6.5 (Molecular Devices, Downingtown, PA). To decrease phototoxic effects, a 0.25 neutral density filter was used. In some experiments, during imaging process cells were treated with 5 μM FSK by addition of the drug into the perfusion medium.
Vesicle trajectories were obtained by single-particle tracking using Metamorph software v6.5. 20 vesicles from five different experiments were randomly selected among those which showed plus-end-directed displacement (vesicles that display movement towards the cell periphery) and that were able to be measured for up to 120 frames. Their uninterrupted movement was analyzed one by one for each condition.
The trajectories were analyzed in the following way. For each trajectory we obtained the contour length of the trajectory as a function of time, and they showed a linear dependence. Thus, we performed a linear fit for each trajectory and found that the coefficient of determination R2, was close to unity in all cases. supplementary material Table S1 shows the values of the slopes obtained from the linear regressions as well as the R2 values for the control and FSK-treated cases. All other analysis are in supplementary material Tables S2-S6. The straight lines plotted in the figures were obtained by using the average slope in the construction of the lines, i.e. the displacement = contour length = slope × (t+a). For the control cases, we take a=0 and for the treated vesicles the origin corresponds to the last point of the control contour length.
In order to assure that the differences between the slopes were statistically significant, a two-sample t-test was performed for each system of interest. The resulting P-values can be found in supplementary material Tables S1-S6.
Reverse transcriptase-polymerase chain reaction (RT-PCR)
The reverse transcriptase (RT) reaction was performed using the Superscript first-strand synthesis system for RT-PCR by Invitrogen (Carlsbad, CA) following the manufacturer's instructions. 1 μg total RNA (RNeasy, Qiagen, Santa Clarita, CA) was converted into cDNA after denaturing at 70°C for 15 minutes, by incubation with a buffer containing oligo-dT primers, the RT enzyme and deoxynucleoside triphosphate (dNTP) mix for 50 minutes at 42°C. The RT enzyme was then inactivated by incubation at 70°C for 15 minutes. The resultant cDNAs were amplified by polymerase chain reaction (PCR) using myosin-V-specific primers (supplementary material Table S7), then analyzed by 1.5% agarose gel electrophoresis. Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as a positive control.
Cells were washed twice with ice-cold phosphate-buffered saline (PBS), and lysed in modified RIPA buffer (50 mM Tris-HCl, pH 8, 150 mM NaCl, 1% NP-40 and 1% sodium deoxycholate, 1 mM phenylmethylsulfonyl fluoride (PMSF), 100 μg/ml N-tosyl-L-phenylalanine chloromethyl ketone (TPCK), 10 μg/ml leupeptin), and centrifuged 10 minutes at 20,000 g. Supernatant was considered the cell lysate.
Sucrose gradient fractionation
A549-GFPα1 cells were placed on ice, washed twice with ice-cold PBS, scraped off the plate and collected by centrifugation. Pellet was resuspended in subcellular fractionation buffer (0.3 M sucrose, 5 mM EDTA 10 mM Tris-HCl, pH 7.4, 1 mM PMSF, 100 μg/ml TPCK, 10 μg/ml leupeptin) and subcellular fractionation by sucrose gradient was performed as previously described (Rose et al., 2003). Briefly, cells were gently homogenized by using a Dounce homogenizer, and the samples were subjected to a 5 minute centrifugation (4°C, 500 g). Supernatant was centrifuged at 100,000 g and pellet was resuspended in homogenization buffer and loaded on top of a sucrose gradient. Gradient consisted of seven 0.5 ml steps with sucrose concentration increasing from 0.5 M to 1.7 M, plus 1 ml of 2 M sucrose cushion at the bottom. Gradient was centrifuged at 200,000 g for 1 hour and 30 minutes and eight different fractions were collected from the interfaces between the sucrose steps. In some experiments, intracellular compartments obtained as described below were subjected to sucrose gradient fractionation. Briefly, intracellular fractions were centrifuged for 1 hour at 200,000 g, the pellet was resuspended in subcellular fractionation buffer and loaded on top of a sucrose gradient as described above.
Preparation of intracellular compartments
A549-GFPα1 cells were incubated for 10 minutes with 50 μM FSK at 37°C, placed on ice, washed twice with ice-cold PBS, scraped in PBS, centrifuged and resuspended in homogenization buffer (250 mM sucrose, 3 mM imidazole, 2 mM EGTA, 1 mM PMSF, 100 μg/ml TPCK, and 10 μg/ml leupeptin, pH 7.4). Cells were gently homogenized (15-20 strokes) using a Dounce homogenizer, and the samples were subjected to a 5 minute centrifugation (4°C, 500 g). Intracellular compartments were fractionated on a flotation gradient as described (Bertorello et al., 1999; Ridge et al., 2002) by using essentially the technique of Gorvel and colleagues (Gorvel et al., 1991).
Construction of m-cherry-tagged myosin-Va short tail (MST) and m-cherry-tagged myosin-Vc tail (DN-Vc)
pcDNA3-m-cherry-MST contains the C-terminal 601 amino acids of the mouse myosin-Va gene fused to the C-terminus of the m-cherry tag (Shaner et al., 2004). The following PCR primers were used to amplify the m-cherry DNA from the construct pm-cherry-C1: 5′-TTTAAGCTTATGGTGAGCAAGGG-3′ and 5′-TTTTTGGATCCTCTTGTACAGCTC-3′. The PCR product was digested with HindIII and BamHI, and cloned into the vector pcDNA3-Myc-MST (Rogers et al., 1999). To construct lenti-m-cherry-DN-Vc, the following PCR primers were used: 5′-AAAGGATCCATGGTGAGCAAGGGCGAGGA-3′ and 5′-GCTGGATCCTTCTTGTACAGCTCGTCCATGGC-3′ to amplify the m-cherry tag. The PCR product was digested with BamHI, and cloned into the lenti-DN-Vc (described below).
Small-hairpin RNA against myosin-Va and myosin-Vc
shRNAs against myosin-Va and myosin-Vc were generated using the m-cherry version of the pG-SUPER vector (Brummelkamp et al., 2002; Kojima et al., 2004) (a gift from Shin Kojima, Northwestern University, Chicago, IL). This vector co-expresses m-cherry fluorescent protein (under the SRα promoter) and shRNA, (under the human H1 promoter) simultaneously so that the knockdown of the target proteins could be analyzed at the level of individual cells as well as by western blot. The targeting sequences were as follows: MyoVa (NM_000259), 5′-TAAGATGCTACCAGAACTA-3′ and MyoVc (NM_018728), 5′-GGACATACATCGAGTTCTA-3′.
A549-GFPα1 cells were grown on 40 mm round coverslips (Bioptech; Butler, PA) at a density of 1×104 cells per coverslip. m-cherry-MST and m-cherry-DN-Vc were transfected using jetPEI™ (Polyplus transfection; Illkirch, France) as indicated by the manufacturers. Cells were used 24 hours after transfection. Plasmids containing shRNAs constructs were transfected using Lipofectamine LTX (Invitrogen) following recommended protocols. Cells were harvested after 72 hours.
Generation of stable cell lines expressing the myosin-Va and myosin-Vc tails
The myosin tail domains (the last 909 amino acids for myosin-Va and the last 835 amino acids for myosin-Vc) were amplified from A549 cells using sequence specific primers (Myosin-Va, 5′-CACCATGGAGAAACTAACCAATCTG-3′ and 5′-GACCCGTGAAATAAAGCCAGG-3′; Myosin-Vc, 5′-CACCATGGTGGAGAAGCTGACTAGCCTG-3′ and 5′-TAACCTATTCAGAAAGCCTAG-3′. The gel-purified product was then used in TOPO cloning reaction (pLenti6/V5 D-TOPO, Invitrogen). Lentivirus was packaged in 293FT cells (Invitrogen). The supernatant containing the virus was harvested and used directly to infect A549-GFPα1 cells. Stable clones expressing myosin-Va tail (DN-Va) and Myosin-Vc tail (DN-Vc) were selected by adding 4 μg/ml Blastacidin (Invitrogen; Carlsbad, CA). Expression of the constructs in the permanent clones was analyzed by western blotting using an antibody against the V5 tag (Fig. 5A).
A549-GFPα1 cells were fixed for 10 minutes in 3.7% formaldehyde, permeabilized with 0.1% Triton X-100 and blocked in 1 μg/μl normal goat serum with 2% BSA. Myosin-Va was visualized by using an anti-myosin-Va antibody (1:75) and a secondary antibody labeled with Alexa Fluor 568 (1:300). GFP was directly visualized. Cellular distribution of Na+/K+-ATPase-GFPα1 and myosin-Va was analyzed by direct fluorescence using a Zeiss LSM 510 laser-scanning confocal microscope (objective Plan Apochromat, ×63/1.4 NA oil-immersion lens). Cross-sections were generated with a 0.2 μm motor step. Contrast and brightness settings were adjusted so that all pixels were in the linear range. Colocalization was established using the LSM 510 Meta software.
For microtubule staining, cells were fixed for 5 minutes in cold methanol (–20°C) and 15 minutes in 3.7% formaldehyde (4°C); for F-actin staining, cells were fixed 10 minutes in 3.7% formaldehyde at room temperature. After fixation, cells were permeabilized and blocked as described above. Microtubules were visualized by using an anti-α-tubulin antibody (1:100) and a secondary antibody labeled with Alexa Fluor 488 (1:200). Actin was visualized by incubating with Rhodamine-phalloidin (1:60). Images were collected using a Nikon TE2000 epifluorescent microscope and a ×60/1.40 NA Planapo lens (Nikon Instruments, Melville, NY) using a Cascade II EMCCD (Photometrics, Tucson, AZ).
Data are represented as means ± s.e.m. Comparisons between two groups of values were evaluated by Student's t-test. Results were considered significant when P<0.05.
Supplementary material available online at http://jcs.biologists.org/cgi/content/full/122/21/3915/DC1
The authors acknowledge Kui Zhu for the generation of dominant-negative Va and Vc, and Alejandro Bertorello for the GFPα1 plasmid. This research was partially supported by NIH grants HL48129, HL71643, HL076139, GM52111 and RB1-2506-PU-03. D.G. is a recipient of a National Science Foundation Graduate Research Fellowship. Deposited in PMC for release after 12 months.
- Accepted August 3, 2009.
- © The Company of Biologists Limited 2009