|
|
|
|||||||
|
|||||||||
J. Biol. Chem., Vol. 281, Issue 38, 27669-27673, September 22, 2006
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
Minireview
Transporters on Demand: Intracellular Reservoirs and Cycling of Bile Canalicular ABC Transporters*
1
From the
Unit on Cellular Polarity, Cell Biology and Metabolism Branch, NICHD, National Institutes of Health, Bethesda, Maryland 20892, Departments of Physiology and Medicine, Tufts University School of Medicine, Boston, Massachusetts 02111, and ¶Institute of Anatomy and Cell Biology, University of Wuerzburg, Wuerzburg 97070, Germany
 |
INTRODUCTION |
|---|
TOP
INTRODUCTION
Intracellular Reservoirs of...An important advance in hepatobiliary physiology was the discovery in 1986 that the secretion of major biliary components is ATP-dependent rather than, as had long been accepted, driven by the transcellular electrochemical gradient (1). Studies using canalicular membrane vesicles revealed separate transport processes for bile acids, phospholipids, and non-bile acid organic anions (glutathione, glucuronide, and sulfate conjugates) and cations (mainly drugs) (2). Specific transporters were subsequently identified as ABC2 transporters (3) and included BSEP (ABCB11, bile acids), MDR3 (ABCB4, phospholipid flippase, MDR1 (ABCB, organic cations) (1), MRP2 (ABCC2, non-bile acid organic anions), and ABCG5/8 (sterols) (4). Genetic studies in man and transgenic animals revealed recessively inherited hepatobiliary phenotypes resulting from mutations in specific transporter genes; defects in ABCB11 and MDR3 produced familial intrahepatic cholestasis types 2 and 3, respectively; defects in MRP2 produced the Dubin Johnson syndrome, and defects in ABCG5 or ABCG8 resulted in sitosterolemia.
Attention was then directed to understanding how the transporters traffic to the canalicular plasma membrane. Initial trafficking studies with antibodies recognizing canalicular membrane proteins revealed trafficking to the basolateral plasma membrane followed by transcytosis to the canalicular domain (5). It was then proposed that all canalicular membrane proteins utilized the transcytotic route and that hepatocytes differed from other polarized epithelial cells in lacking a direct vesicular pathway from Golgi to the apical membrane; however, none of these studies examined ABC transporters. Subsequent immunohistochemical analyses revealed restriction of ABC transporters to the bile canaliculus and their absence from the basolateral plasma membrane (6).
|
Intracellular Reservoirs of Canalicular ABC Transporters |
|---|
Bile acid secretion increases in response to the enterohepatic circulation of bile acids and postprandial secretion of peptide hormones that increase cAMP production in hepatocytes. Treatment of rats with taurocholate or cAMP selectively increased canalicular ABC transporters (6). Because these effects occurred within minutes and required an intact microtubular system, intracellular reservoirs of canalicular ABC transporters were postulated from which additional transporters could rapidly be recruited.
The intracellular distribution and trafficking routes of canalicular ABC transporters were identified in pulse-chase studies performed in rats (7, 8) (Fig. 1A). In contrast to other canalicular proteins, newly synthesized ABC transporters were not detected in the basolateral plasma membrane before they reached the bile canaliculus. MDR1 trafficked directly from Golgi to the canalicular membrane; however, BSEP trafficking required an additional hour after passage through the Golgi before appearing in the canalicular membrane. In the intermediate time, BSEP chased through a post-Golgi endosomal fraction suggesting that the transporter was sequestered before apical delivery. These observations were consistent with immunoelectron microscopic demonstration of BSEP in both a subapical compartment and the plasma membrane. Administration of cAMP or taurocholate increased the amounts of MDR1, MDR2, MRP2, and BSEP in the canalicular membrane by 
3-fold, which was unaffected by cycloheximide (6, 8).
These studies confirm that additional ABC transporters in the canalicular membrane result from recruitment from intracellular pools rather than from enhanced transcription or translation. The half-life of MDR1, MDR2, and BSEP is 5 days in rat liver suggesting that ABC transporters cycle between intracellular pools and the bile canalicular membrane before degradation. The intrahepatic reservoir is at least 6-fold greater than the content of ABC transporters in the canalicular membrane. The effects of taurocholate and cAMP summated, indicating either two separate reservoirs of ABC transporters or regulation by two mechanisms from a single pool. Intracellular reservoirs supply additional ABC transporters to the bile canaliculus to cope with increased metabolic demand to secrete bile. Alternatively, the reservoirs may be part of an unidentified bile secretion mechanism because intrahepatic reservoirs of MRP2, which co-localizes with BSEP, secrete MRP2 substrates into intracellular structures (9).
|
ABC Transporter Reservoirs and Recruitment Mechanisms |
|---|
To quantify the distribution of individual canalicular ABC transporters and determine the mechanism and regulation for their transfer to the apical membrane, studies were performed in WIFB9 cells (10), a stable hybrid of rat hepatoma and human fibroblasts that express liver-specific functions and have osmotically sealed bile canaliculi into which fluorescent bile acids and organic cations are secreted (11, 12). HepG2 cells also polarize and have been useful in studies of bile canalicular formation and turnover, particularly involving lipid components (13, 14). Most studies of secretory trafficking utilize MDCK cells, which maintain a polarized phenotype (15, 16); however, differences in trafficking pathways occur between WIFB and MDCK cells.
|
In WIFB cells, confocal imaging of BSEP-YFP and MDR1-YFP revealed localization in the bile canalicular membrane, in tubular-vesicular structures adjacent to the MTOC, and in diffusely distributed carriers (11, 18, 19). Steady-state concentrations of BSEP and MDR1 were
49% in vesicles, 10% adjacent to the MTOC, and 40% in the bile canalicular region. Additional studies revealed selective co-localization of BSEP-YFP with Rab11a, a small GTPase marker of the recycling endosomal compartment. Constitutive BSEP cycling from intracellular compartments and the canalicular membrane was demonstrated by selective photobleaching experiments in WIFB cells infected with adenoviral BSEP-YFP (18) (Fig. 1B). These experiments revealed that BSEP-YFP molecules transiently reside in the canalicular membrane before rapidly exchanging with intracellular BEP-YFP reservoirs. The exchange was inhibited by microtubule disruption.
Cycling of membrane transporters between the plasma membrane and intracellular sites regulates the amount of transporter at the cell surface. Utilizing this mechanism, the plasma membrane permeability for certain substances can be rapidly changed allowing cells to respond to varying physiologic conditions (e.g. substrate concentrations). This mechanism may have broad physiologic importance because cycling pools are described for several plasma membrane transporters including insulin-responsive glucose transporter 4 in rat adipocytes (20), aquaporin 8 water channel in LLC PK1 cells (21), cystic fibrosis transmembrane conductance regulator in duodenal epithelium (22), proton K+-ATPase in gastric parietal cells (23), and Na+-dependent glucose transporter in Caco-2 cells (24).
|
Sorting Pathways for Canalicular Membrane Proteins |
|---|
Because many canalicular proteins are delivered to the apical membrane by transcytosis (e.g. polymeric immunoglobulin A receptor, 5'-nucleotidase) whereas others traffic directly from Golgi through a recycling endosome system (e.g. canalicular ABC transporters), sorting of cargo is required. Based primarily on studies in MDCK cells, the trans-Golgi network is considered to be the major sorting site (16, 17); however, sorting site(s) for carriers containing BSEP and other ABC transporters have not been established.
|
Protein Components of the Trafficking System |
|---|
Cellular Proteins That Bind ABC Transporters—Yeast two-hybrid screens identified HAX-1 and MLC2a as potential binding partners for BSEP, MDR1, and MDR2 (25, 26). RNAi-mediated knockdown of HAX-1 RNAi increased BSEP apical membrane content because of apical membrane retention of BSEP without affecting translation, exocytosis, or the half-life of the transporter. HAX-1 interacts with cortactin, an actin-binding protein involved in clathrin-mediated endocytosis (25). Expression of dominant-negative cortactin doubled the steady-state level of BSEP in the apical membrane. Therefore, HAX-1 and cortactin participate in clathrin-mediated endocytosis of BSEP and possibly other ABC transporters from the apical membrane. In contrast, a non-phosphorylatable dominant-negative MLC2 significantly reduced apical delivery of labeled BSEP (26). Thus, MLC2a is required for apical delivery of newly synthesized BSEP and possibly other ABC transporters to the apical membrane and/or TGN release of ABC transporter vesicles (Fig. 2).
Rab Proteins—Different Rab proteins have been associated with different organelles in MDCK and hepatic cell lines. In hepatocytes, Rab11a co-localizes with vesicles containing ABC transporters before their insertion in the canalicular membrane (19), and Rab4 and -5 facilitate endocytosis and vesicle fusion (27).
Co-localization of Rab11a and apical proteins and the role of Rab11-interacting proteins in endosomal recycling were initially characterized in MDCK cells (17, 28, 29). The Rab GTPase family has been designated a "master regulator of membrane trafficking" (30). Rab11 acts as a molecular switch in which GTP loading and hydrolysis are coupled to recruitment of membrane tethering and docking factors (36) and activation of vesicle-linked motor activity. In the active GTP-bound form, Rab11a binds to downstream effector proteins that localize to recycling endosomes and influences vesicle sorting (30). Rab proteins selectively bind to cytoskeletal components and protein kinases, thereby facilitating discrete steps in membrane transport.
cAMP and Phosphatidylinositol 3-Kinase—Increased hepatocellular cAMP promotes apical surface-directed trafficking of vesicles containing proteins and lipids, suggesting that cAMP controls the relative abundance of canalicular membrane proteins in response to postprandial changes in the enterohepatic circulation and peptide hormone secretion (31, 32). In pulsechase studies in rats, cAMP administration did not affect the rate of transfer of BSEP to the canalicular membrane consistent with exchange with a large intracellular transporter pool (8). In HepG2 cells, inhibition of cAMP-induced dihydroceramide synthesis resulted in intracellular sphingosine accumulation, altered recycling endosome dynamics, and impaired bile canalicular formation (33).
cAMP activates PI 3-kinase in hepatocytes and other cells by different pathways (32). PI 3-kinase inhibition reduced bile secretion in perfused liver and ATP-dependent bile acid transport in canalicular membrane vesicles but had no effect on cAMP-stimulated trafficking of ABC transporters (44, 45). The latter effect was reversed by 3-phosphoinositides but not PI 4,5-trisphosphate (35), suggesting that PI 3-kinase association with the canalicular membrane and 3-phosphoinositide formation are required for BSEP localization and activity. Neither the mechanism nor the specificity of this regulation are known. A decapeptide mimic of the gelsolin binding site on PI bisphosphate activates PI 3-kinase activity and bile acid transport in rat cytomegalovirus and WIFB cells and increased bile secretion in perfused rat liver (11, 35). These observations suggest that 3-phosphoinositides regulate canalicular bile acid secretion. In addition, PI trisphosphate regulates endocytosis of apical resident proteins (36).
The taurocholate-mediated intracellular pool of ABC transporters is also large (6); however, neither its subcellular site nor regulation have been defined. In contrast to the effect of cAMP, taurocholate-stimulated bile acid secretion and recruitment of canalicular ABC transporters were unaffected by inhibition of PI 3-kinase activity (34). Whereas the cAMP-mediated cycling event is similar to that present for other ligands in other cells, the taurocholate pool appears unique to liver.
Cytoskeleton: Microtubules—In WIFB cells, live cell imaging of BSEP-YFP revealed microtubular-dependent oscillatory movement of cargo-containing tubular vesicles along microtubules from the MTOC throughout the cell; however, attachment and fusion occurred only in the canalicular domain (13). In WIFB and MDCK cells, apical trafficking of cargo by transcytotic and direct routes was inhibited by microtubular disruption (12, 19). The source of the tubular carriers is the TGN from which a steady stream of proteins and lipids bud because of the action of dynamin. Cargo proteins transported along these tubules to basolateral or apical plasma membranes have transmembrane domains that mainly partition into lipid regions enriched in sphingolipids and cholesterol ("rafts") (37). Kinesins move the tubules along microtubules. Delivery of canalicular membrane proteins requires an intact microtubule structure that is affected by PAR-1, a kinase for microtubular-associated proteins (38). Inhibition of PAR-1 prevents canalicular formation in WIFB cells (38).
Cytoskeleton: Actin—In hepatocytes and WIFB cells, the actin cytoskeleton is distributed in a ring around the bile canaliculus at the adherens cell junction and also in microvilli (2, 7). How actin participates in BSEP apical trafficking, cycling, and endocytosis is unclear; however, several observations support a role for actin. (i) Rab GTPases interact with the actin cytoskeleton as determined by co-localization studies using GFP Rab11a constructs (19). (ii) Cytochalasin and latrunculin A inhibit bile acid- and cAMP-mediated increases in bile acid secretion in vivo (39) and in WIFB cells (11). (iii) An actin-based complex participates in clathrin-mediated endocytosis of BSEP from the canalicular domain in MDCK cells (25). (iv) In WIFB cells expressing BSEP-YFP, photobleaching of all but the canalicular region resulted in rapid decline of BSEP-YFP fluorescence; cytochalasin D or latrunculin A prevented endocytosis indicating that impaired actin polymerization inhibits cycling of canalicular BSEP-YFP (19). (v) In MDCK cells, blebistatin A, which inhibits MLC kinase, reduced BSEP trafficking to the canalicular membrane (26). In other experiments, latrunculin A modulated basolateral endosomal cycling (40). (vi) The most direct studies implicating actin in targeting or maintaining apical ABC proteins involve mice in which radixin, the dominant ezrin-radixin-moesin protein in liver, was eliminated by targeted mutation (41). The ezrin-radixin-moesin family of proteins cross-links actin filaments and integral membrane proteins. Removal of radixin, which is concentrated in the bile canalicular domain, resulted in progressive dilation of the canaliculus, decreased microvilli, jaundice because of impaired apical trafficking of MRP2, and disappearance of other canalicular ABC transporters.
|
|
Convergence of Trafficking Pathways |
|---|
Immunoelectron microscopy of rat liver organelles revealed that the pIga receptor, a transcytosis marker, and ABC transporters occurred in the same vesicles. In experimental cholestasis in rat liver and WIFB cells, transcytotic and ABC transporters partially co-localized in intracellular organelles (42). In the steady-state transcytosis, markers and ABC transporters localized to Rab11a-positive endosomes in WIFB cells (18). The pIga receptor is a GPI-linked protein that is endocytosed at the basolateral membrane and moves to the early endosome. Before trafficking to the canalicular domain, pIga resides in a morphologically and kinetically distinct subapical compartment (43, 44), which has not yet been shown to contain ABC transporters (Fig. 3). Because pIgA receptors are rapidly degraded (t
= 0.05 day), they are located mainly in the transcytotic and degradation pathways. In contrast, ABC transporters have long half-lives (t =5 days) and are mainly located in the apical recycling pathway; few molecules enter the degradation pathway at any given time (8). Together, these data reveal little evidence for convergence of the transcytotic and apical recycling pathways.
|
|
Fusion of Post-Golgi Transport Intermediates with Apical Membrane |
|---|
Fusion of transport vesicles with the plasma membrane releases cargo, and membrane lipids and proteins redistribute laterally by diffusion within the plasma membrane. Live cell imaging of BSEP-YFP in WIFB cells revealed that intracellular carriers elongated and dissociated as tubular elements from a globular structure adjacent to the MTOC (19). The tubular elements displayed oscillatory movement toward the entire plasma membrane but only fused with the canalicular membrane. Specificity in fusion could be because of specific motor proteins that transport BSEP-containing vesicles to their appropriate membrane domain or to downstream selectivity in membrane fusion. It is likely that attachment to and insertion into the canalicular plasma membrane require downstream signals that are not present in the basolateral plasma membrane. Downstream site(s) for attachment and fusion of cargo-containing vesicles to the canalicular membrane have not been identified; however, specific SNAREs may participate (45). Different forms and subcellular localization of v- and t-SNARES involved in different membrane traffic pathways confer specificity. For example, trafficking of cargo from the TGN to the apical membrane requires SNAP-23 and syntaxin-3, whereas basolateral to apical transcytosis requires SNAP-23 and NSF. In WIFB cells and hepatocytes, syntaxin-3 is restricted to the apical region.
Total internal reflection microscopy of polarized MDCK cells revealed fusion of post-Golgi transport intermediates directly with the basolateral membrane (46); however, similar studies of the apical membrane have not been performed. Antibodies to syntaxin-3 and microtubular inhibitors inhibited fusion. The apical fusion sites appear focally distributed suggesting specific docking requirements (17). The distribution of fusion sites paralleled that of syntaxin-3. Microtubule disruption depolarized syntaxin-3, which suggested that microtubules might organize apical trafficking routes partly through positioning of syntaxin-3. Following cargo delivery into the apical membrane, diffusion is rapid and distribution is limited by tight junctions. Microtubules do not attach directly to the apical membrane but interact with actin microfilaments along which cargo is delivered to or from the apical membrane (46).
|
Apical Endocytosis of ABC Transporters |
|---|
Inaccessibility of the bile canaliculus to micro-sampling restricts studies of apical retrieval mechanisms. The apical surface area would double every 15–20 min if not compensated (37, 47). Loss of canalicular membrane because of the detergent effect of bile acids contributes to apical membrane turnover; however, the major retrieval mechanism is endocytosis and delivery of membrane components to lysosomes and proteasomes. In support of this view, clathrin-coated profiles, SNARES, Rabs, and annexins are located in the apical domain (47). Treatment of hepatocytes or WIFB cells with PI 3-kinase inhibitors resulted in accumulation of apical plasma membrane proteins in lysosomes (47). In wortmannin-treated cells, transcytosing apical proteins traversed the subapical compartment, whereas apically internalized proteins did not (47). Whether the endogenous recycling process in rat liver and WIFB cells for canalicular ABC transporters is entirely clathrin-dependent has not been tested; however, caveoli do not participate (43).
|
Role of ABC Transporter Trafficking in Polarization |
|---|
Sorting and trafficking pathways may be reprogrammed during differentiation and polarization (48). In non-polarized WIFB cells, GPI-linked and single transmembrane domain proteins traffic from Golgi to the entire plasma membrane, whereas canalicular ABC transporters remain in a perinuclear region associated with the MTOC (19, 41). Upon polarization, the apical ABC transporters traffic only to the canalicular domain and transcytotic proteins traffic to the basolateral domain from which they cross to the canalicular membrane. These studies further indicate that trafficking patterns are multiple and relate to differentiation and polarization.
Bile canalicular formation (apical polarization) is essential for biliary secretion and is disrupted in cholestatic disorders. Many components participate in apical polarization and targeting of canalicular membrane components, including ABC transporters; however, their specific interactions are not well defined. In WIFB cells, Rab11a and myosin Vb participate in apical targeting of recycling endosomes. Stable knockdown of Rab11a expression by RNAi or overexpression of a Rab11a-GDP-locked mutant prevented polarization (19). Overexpression of the tail domain of myosin Vb, which competes with full-length myosin Vb for binding to Rab11a, also prevented bile canalicular formation. The absence of Rab11a or myosin Vb caused ABC transporters to remain intracellularly co-localized with transcytotic membrane proteins that were also transported to the plasma membrane. These results suggest that myosin Vb, which binds Rab11a and actin, is required for trafficking endosomes that contain apical ABC transporters to sites that initiate polarization. Myosin Vb may serve as a motor for delivery of endosomal cargo through the actin network in WIFB cells.
Several mechanisms may account for the role of Rab11a and myosin Vb in canalicular biogenesis. In polarized mammalian cells, Rab11a participates in targeting apical proteins to the apical surface (28). In Drosophila, Rab11a participates in morphogenesis (48). Both Rab11a and myosin Vb may be required for directing critical junctional, cytoskeletal, targeting, and other components to the plasma membrane. In their absence, proteins that normally traffic to the canalicular membrane by the transcytosis route are primarily directed to the plasma membrane, whereas ABC transporters that normally traffic by the direct route remain intracellular, and normal turnover of canalicular membrane proteins and lipids results in loss of polarity and inability to polarize. Rab11a- and myosin Vb-positive endosomes constitute a reservoir for proteins that, in concert with unidentified polarization cues, are required for canalicular formation and trafficking of ABC transporters (and perhaps transcytotic membrane proteins) to the canalicular membrane. These endosomes may contain or be linked to specific targeting molecules, such as SNARES, which facilitate membrane targeting and fusion.
|
FOOTNOTES |
|---|
* This minireview will be reprinted in the 2006 Minireview Compendium, which will be available in January, 2007. This work was supported by NIDDK Grant DK 35652 from the National Institutes of Health. Space limitations restricted the choice of references.
The on-line version of this article (available at http://www.jbc.org) contains supplemental Fig. 1.
1 To whom correspondence should be addressed: CBMB, NICHD, National Institutes of Health, Bldg. 32T, Rm. 101, Bethesda, MD 20892. Tel.: 301-402-8394; Fax: 301-402-0078; E-mail: ariasi{at}mail.nih.gov.
2 The abbreviations used are: ABC, ATP-binding cassette; BSEP, bile salt excretory protein; GPI, apoglycophosphoinositol A protein; HAX-1, HS-1-associated protein X-1; MDCK, Madin-Darby canine kidney cells; MDR1 and -3, multidrug-resistant transporters 1 and 3, respectively; MLC2a, non-muscle myosin II regulatory light chain 2a; MRP2, multidrug-resistant-like protein 2; MTOC, microtubular organizing center; NSF, N-ethylmaleimide-sensitive factor; SNARE, soluble NSF attachment protein receptor; SNAP, SNARE attachment protein; TGN, trans-Golgi network; YFP, yellow fluorescent protein; PI, phosphatidylinositol; RNAi, RNA interference.
|
REFERENCES |
|---|
- Kamimoto, Y., Gatmaitan, Z., Hsu, J., and Arias, I. M. (1989) J. Biol. Chem. 264, 11693–11698
[Abstract/Free Full Text] - Ujhazy, P. (2001) in The Liver: Biology and Pathobiology (Arias, I. M., Boyer, J. L., Fausto, N., Chisari, F., and Shafritz, D., eds), Ed. 4, pp. 361–373, Raven Press, Boston
- Dean, M. (2002) The Human ATP-binding Cassette (ABC) Transporter Superfamily, pp. 361–373, NCBI, Bethesda, MD
- Berge, K. E., Tian, H., Graf, G. A., Yu, L., Grishin, N. V., Schultz, J., Kwiterovich, P., Shan, B., Barnes, R., and Hobbs, H. H. (2000) Science 290, 1771–1775
[Abstract/Free Full Text] - Schell, M. J., Maurice, M., Stieger, B., and Hubbard, A. L. (1992) J. Cell Biol. 119, 1173–1182
[Abstract/Free Full Text] - Gatmaitan, Z. C., Nies, A. T., and Arias, I. M. (1997) Am. J. Physiol. 272, G1041–G1049[Medline] [Order article via Infotrieve]
- Kipp, H., Khoursandi, S., Scharlau, D., and Kinne, R. K. (2003) Am. J. Physiol. 285, C737–C749
- Kipp, H., Pichetshote, N., and Arias, I. M. (2001) J. Biol. Chem. 276, 7218–7224
[Abstract/Free Full Text] - Rajagopal, A., and Simon, S. M. (2003) Mol. Biol. Cell 14, 3389–3399
[Abstract/Free Full Text] - Decaens, C., Rodriguez, P., Bouchaud, C., and Cassio, D. (1996) J. Cell Sci. 109, 1623–1635[Abstract]
- Sai, Y., Nies, A. T., and Arias, I. M. (1999) J. Cell Sci. 112, 4535–4545[Abstract]
- Ihrke, G., Neufeld, E. B., Meads, T. Shanks, M. R., Cassio, D., Laurent, M., Schroer, T. A., Pagano, R. E., and Hubbard, A. L. (1993) J. Cell Biol. 123, 1761–1775
[Abstract/Free Full Text] - van IJzendoorn, S. C., Theard, D., Van Der Wouden, J. M., Visser, W., Wojtal, K. A., and Hoekstra, D. (2004) Mol. Biol. Cell 15, 4105–4114
[Abstract/Free Full Text] - Schmitt, M., Kubitz, R., Lizun, S., Wettstein, M., and Haussinger, D. (2001) Hepatology 33, 509–518[CrossRef][Medline] [Order article via Infotrieve]
- Leung, S. M., Ruiz, W. G., and Apodaca, G. (2000) Mol. Biol. Cell 11, 2131–2150
[Abstract/Free Full Text] - Mostov, K., Su, T., and ter Beest, M. (2003) Nat. Cell Biol. 5, 287–293[CrossRef][Medline] [Order article via Infotrieve]
- Rodriguez-Boulan, E., Kreitzer, G., and Musch, A. (2005) Nat. Rev. Mol. Cell Biol. 6, 233–247[CrossRef][Medline] [Order article via Infotrieve]
- Wakabayashi, Y., Lippincott-Schwartz, J., and Arias, I. M. (2004) Mol. Biol. Cell 15, 3485–3496
[Abstract/Free Full Text] - Wakabayashi, Y., Dutt, P., Lippincott-Schwartz, J., and Arias, I. M. (2005) Proc. Natl. Acad. Sci. U. S. A. 102, 15087–15092
[Abstract/Free Full Text] - Kandror, K. V., and Pilch, P. F. (1998) Biochem. J. 331, 829–835[Medline] [Order article via Infotrieve]
- Gradilone, S. A., Garcia, F., Huebert, R. C., Tietz, P. S., Larocca, M. C., Kierbel, A., Carreras, F. I., Larusso, N. F., and Marinelli, R. A. (2003) Hepatology 37, 1435–1441[CrossRef][Medline] [Order article via Infotrieve]
- Kleizen, B., Braakman, I., and de Jonge, H. R. (2000) Eur. J. Cell Biol. 79, 544–556[CrossRef][Medline] [Order article via Infotrieve]
- Hales, C. M., Griner, R., Hobdy-Henderson, K. C., Dorn, M. C., Hardy, D., Kumar, R., Navarre, J., Chan, E. K., Lapierre, L. A., and Goldenring, J. R. (2001) J. Biol. Chem. 276, 39067–39075
[Abstract/Free Full Text] - Vega-Salas, D. E., Salas, P. J., and Rodriguez-Boulan, E. (1988) J. Cell Biol. 107, 1717–1728
[Abstract/Free Full Text] - Ortiz, D. F., Moseley, J., Calderon, G., Swift, A. L., Li, S., and Arias, I. M. (2004) J. Biol. Chem. 279, 32761–32770
[Abstract/Free Full Text] - Chan, W., Calderon, G., Swift, A. L., Moseley, J., Li, S., Hosoya, H., Arias, I. M., and Ortiz, D. F. (2005) J. Biol. Chem. 280, 23741–23747
[Abstract/Free Full Text] - Bananis, E., Murray, J. W., Stockert, R. J., Satir, P., and Wolkoff, A. W. (2003) J. Cell Sci. 116, 2749–2761
[Abstract/Free Full Text] - Fan, G. H., Lapierre, L. A., Goldenring, J. R., Sai, J., and Richmond, A. (2004) Mol. Biol. Cell 15, 2456–2469
[Abstract/Free Full Text] - Hales, C. M., Vaerman, J. P., and Goldenring, J. R. (2002) J. Biol. Chem. 277, 50415–50421
[Abstract/Free Full Text] - Pfeffer, S. R. (2001) Trends Cell Biol. 11, 487–491[CrossRef][Medline] [Order article via Infotrieve]
- Roelofsen, H., Soroka, C. J., Keppler, D., and Boyer, J. L. (1998) J. Cell Sci. 111, 1137–1145[Abstract]
- Kagawa, T., Varticovski, L., Sai, Y., and Arias, I. M. (2002) Am. J. Physiol. 283, C1655–C1666
- van IJzendoorn, S. C., and Hoekstra, D. (2000) Mol. Biol. Cell 11, 1093–1101
[Abstract/Free Full Text] - Misra, S., Ujhazy, P., Gatmaitan, Z., Varticovski, L., and Arias, I. M. (1998) J. Biol. Chem. 273, 26638–26644
[Abstract/Free Full Text] - Misra, S., Ujhazy, P., Varticovski, L., and Arias, I. M. (1999) Proc. Natl. Acad. Sci. U. S. A. 96, 5814–5819
[Abstract/Free Full Text] - Tuma, P. L., Finnegan, C. M., Yi, J. H., and Hubbard, A. L. (1999) J. Cell Biol. 145, 1089–1102
[Abstract/Free Full Text] - Slimane, T. A., Trugnan, G., van IJzendoorn, S. C., and Hoekstra, D. (2003) Mol. Biol. Cell 14, 611–624
[Abstract/Free Full Text] - Cohen, D., Rodriguez-Boulan, E., and Musch, A. (2004) Proc. Natl. Acad. Sci. U. S. A. 101, 13792–13797
[Abstract/Free Full Text] - Misra, S., Varticovski, L., and Arias, I. M. (2003) Am. J. Physiol. 285, G316–G324
- Sheff, D. R., Kroschewski, R., and Mellman, I. (2002) Mol. Biol. Cell 13, 262–275
[Abstract/Free Full Text] - Kikuchi, S., Hata, M., Fukumoto, K., Yamane, Y., Matsui, T., Tamura, A., Yonemura, S., Yamagishi, H., Keppler, D., Tsukita, S., and Tsukita, S. (2002) Nat. Genet. 31, 320–325[CrossRef][Medline] [Order article via Infotrieve]
- Tuma, P. L., and Hubbard, A. L. (2003) Physiol. Rev. 83, 871–932
[Abstract/Free Full Text] - Hoekstra, D., Tyteca, D., and van IJzendoorn, S. C. (2004) J. Cell Sci. 117, 2183–2192
[Abstract/Free Full Text] - Ihrke, G., Martin, G. V., Shanks, M. R., Schrader, M., Schroer, T. A., and Hubbard, A. L. (1998) J. Cell Biol. 141, 115–133
[Abstract/Free Full Text] - Low, S. H., Chapin, S. J., Wimmer, C., Whiteheart, S. W., Komuves, L. G., Mostov, K. E., and Weimbs, T. (1998) J. Cell Biol. 141, 1503–1513
[Abstract/Free Full Text] - Kreitzer, G., Schmoranzer, J., Low, S. H., Li, X., Gan, Y., Weimbs, T., Simon, S. M., and Rodriguez-Boulan, E. (2003) Nat. Cell Biol. 5, 126–136[CrossRef][Medline] [Order article via Infotrieve]
- Hao, M., and Maxfield, F. R. (2000) J. Biol. Chem. 275, 15279–15286
[Abstract/Free Full Text] - Schuck, S., and Simons, K. (2006) J. Cell Biol. 172, 963–965
[Abstract/Free Full Text]
CiteULike 
Complore 
Connotea 
Del.icio.us 
Digg 
Reddit 
Technorati What's this?
This article has been cited by other articles:
|
|
 |
|
  G. Bajaj, Y. Zhang, M. I. Schimerlik, A. M. Hau, J. Yang, T. M. Filtz, C. Kioussi, and J. E. Ishmael N-Methyl-D-aspartate Receptor Subunits Are Non-myosin Targets of Myosin Regulatory Light Chain J. Biol. Chem., January 9, 2009; 284(2): 1252 - 1266. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 T. Kagawa, N. Watanabe, K. Mochizuki, A. Numari, Y. Ikeno, J. Itoh, H. Tanaka, I. M. Arias, and T. Mine Phenotypic differences in PFIC2 and BRIC2 correlate with protein stability of mutant Bsep and impaired taurocholate secretion in MDCK II cells Am J Physiol Gastrointest Liver Physiol, January 1, 2008; 294(1): G58 - G67. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
K. Mochizuki, T. Kagawa, A. Numari, M. J. Harris, J. Itoh, N. Watanabe, T. Mine, and I. M. Arias Two N-linked glycans are required to maintain the transport activity of the bile salt export pump (ABCB11) in MDCK II cells Am J Physiol Gastrointest Liver Physiol, March 1, 2007; 292(3): G818 - G828. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||