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© The Rockefeller University Press,
0021-9525/1997//37 $5.00
The Journal of Cell Biology, Volume 139, Number 1,
, 1997 37-47
Article |
Nef-mediated Clathrin-coated Pit Formation
Division of Infectious Diseases, Hôpital Cantonal Universitaire, University of Geneva 4, Switzerland 1211; and Infectious Disease Laboratory, The Salk Institute for Biological Studies, La Jolla, California 92037
The sequence of events leading to clathrin-coated pit (CCP) nucleation on the cell surface and to the incorporation of receptors into these endocytic structures is still imperfectly understood. In particular, the question remains as to whether receptor tails initiate the assembly of the coat proteins or whether receptors migrate into preformed CCP. This question was approached through a dissection of the mechanisms implemented by Nef, an early protein of human and simian immunodeficiency virus (HIV and SIV, respectively), to accelerate the endocytosis of cluster of differentiation antigen type 4 (CD4), the major receptor for these viruses. Results collected showed that: (a) Nef promotes CD4 internalization via an increased association of CD4 with CCP; (b) the Nef-mediated increase of CD4 association with CCP is related to a doubling of the plasma membrane area occupied by clathrin-coated structures; (c) this increased CCP number at the plasma membrane has functional consequences preferentially on CD4 uptake and does not significantly affect transferrin receptor internalization or fluid-phase endocytosis; (d) the presence of a CD4 cytoplasmic tail including a critical dileucine motif is required to induce CCP formation via Nef; and (e) when directly anchored to the cytoplasmic side of the plasma membrane, Nef itself can promote CCP formation. Taken together, these observations lead us to propose that CD4 can promote CCP generation via the connector molecule Nef. In this model, Nef interacts on one side with CD4 through a dileucine-based motif present on CD4 cytoplasmic tail and on the other side with components of clathrin-coated surface domain (i.e., adaptins). These Nef-generated complexes would then initiate the nucleation of CCP.
Abbreviations used in this paper: AP, adaptor protein; CCP, clathrin-coated pit(s); CD4, cluster of differentiation antigen type 4; Tf-R, transferrin receptor.
RECEPTOR-MEDIATED endocytosis provides a mechanism through which cells selectively capture nutrients and building blocks from the extracellular medium, transduce extracellular signals, and remove signaling receptors from their surface, thereby modulating their sensitivity to external stimuli (Cohen and Fava, 1985; van Deurs et al., 1989; Rodman et al., 1990; Watts and Marsh, 1992; Carpentier, 1994; Feger et al., 1994). Elucidating the molecular mechanisms governing receptor-mediated endocytosis is, therefore, important to unravel how cell growth and maintenance are controlled. Endocytosis of signaling receptors (i.e., the insulin receptor, the EGF receptor, etc.) occurs in response to ligand binding while endocytosis of transport protein receptors (i.e., the transferrin receptor, the LDL receptor, etc.) is constitutive (Cohen and Fava, 1985; Hanover et al., 1985; Hopkins et al., 1985; Watts, 1985; Carpentier et al., 1992; Sorkin and Carpenter, 1993). In both cases the entry of the receptors inside the cell is mediated by plasma membrane invaginated domains decorated on their cytoplasmic side with clathrin: the clathrin-coated pits (CCP)1 (Goldstein et al., 1985; van Deurs et al., 1989; Rodman et al., 1990; Watts and Marsh, 1992). One single CCP can be responsible for the concomitant uptake of both signaling and transport protein receptors (Maxfield et al., 1978; Carpentier et al., 1982).
The development of cell-free assays, analogous to those which have allowed a breakthrough in our understanding of how transport vesicles bud and fuse along the biosynthetic pathway (Orci et al., 1989; Rothman and Orci, 1992), has recently permitted the dissection of key mechanisms governing and controlling the formation of clathrin-coated vesicles from CCP (Lin et al., 1991; Schmid and Smythe, 1991; Schmid, 1993). At the same time, the combination of mutational, biochemical, and morphological studies has revealed that the association of receptors with CCP relies on a mutual recognition between particular CCP components (adaptins) and specific amino acid sequences present in receptor cytoplasmic tails (Trowbridge, 1991; Paccaud et al., 1993; Ohno et al., 1995). These conceptual advances contrast with the lack of information regarding another key event in receptor-mediated endocytosis, namely the triggering and control of CCP formation. In this respect the question remains open as to whether receptors designed to be internalized induce CCP formation or whether receptors are segregated in preformed CCP. According to one model, CCP components first assemble at the plasma membrane and, in a second step, receptors migrate into these structures to be internalized (Fire et al., 1991; Katzir et al., 1994; Sako and Kusumi, 1994; Lazarovits et al., 1996). This concept is supported by the absence of increase in CCP density in the proximity of stimulated Fc receptors (Fc
RI) (Santini and Keen, 1996). By contrast, the second model postulates that the assembly of CCP components is initiated by receptors themselves. Along this line, ligand-induced clustering of IgM receptors was shown to lead to clathrin recruitment at the plasma membrane (Salisbury et al., 1980), and overexpression of transferrin receptors caused an increase in clathrin coating at the plasma membrane (Iacopetta et al., 1988; Miller et al., 1991). Likewise, clathrin-coated vesicle formation at the Golgi membranes was demonstrated to be modulated by expression levels of mannose 6-phosphate receptor as long as the cytoplasmic tail is unaltered (Le Borgne and Hoflack, 1997).
The present study was aimed at exploring the process of CCP formation through the study of Nef, an early protein of primate lentiviruses which downregulates the surface expression of CD4 (Garcia and Miller, 1991; Anderson et al., 1993; Mariani and Skowronski, 1993) by inducing its accelerated internalization followed by lysosomal degradation (Aiken et al., 1994; Rhee and Marsh, 1994). Previous work indicated that 20 membrane-proximal residues of the CD4 cytoplasmic domain are sufficient to confer Nef responsiveness to a heterologous molecule, and that within this region a dileucine-based motif plays a critical role (Aiken et al., 1994; Salghetti et al., 1995). Furthermore, the study of chimeric integral membrane proteins containing Nef as their cytoplasmic domain revealed that, in this context, Nef can act in cis to induce the rapid endocytosis of these fusion molecules via clathrin-coated pits (Mangasarian et al., 1997). Taken together, these data support a model where Nef downregulates CD4 by acting as a connector between this receptor and the endocytic apparatus. Here, the mechanisms of Nef-induced CD4 endocytosis were further investigated. This led to the observation that the viral protein triggers the formation of CD4– enriched CCP. This effect required that Nef be tethered to the plasma membrane either by coexpression with CD4, or as part of a chimeric integral membrane protein. These results strongly suggest that receptors can trigger the formation of CCP at the cell plasma membrane.
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MATERIALS AND METHODS |
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 TopAbstract MATERIALS AND METHODS RESULTSDISCUSSIONREFERENCES |
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globulins, goat anti– mouse IgG (whole molecule) gold conjugate (10 nm), histidinol, and Hepes were purchased from Sigma Chemical Co. (St Louis, MO). RPMI 1640 culture medium and fetal calf serum (FCS) were purchased from GIBCO BRL (Paisley, Scotland). Purified mouse anti–human CD4 (RPA-T4) was obtained from PharMingen (San Diego, CA); purified mouse anti–human CD4 (Leu3a) and purified mouse anti–human CD71 (anti–human transferrin receptor, clone B3/25) were obtained from Boehringer Mannheim (Mannheim, Germany); and monoclonal mouse anticlathrin (directed against the 180-kD heavy chain) was a gift of R.G.W. Anderson. Iodo-Beads as iodination reagent were purchased from Pierce Chemical Co. (Rockford, IL) and 125I from Amersham International (Little Chalmont, England). Other chemicals were of analytical grade and were obtained from Fluka AG (Buchs, Switzerland) or Sigma Chemical Co. Experiments were performed in PBS or a medium containing (micrometers) 138 NaCl, 6 KCl, 1 MgCl2, 20 glucose, and 20 Hepes, pH 7.4 (medium 1).
DNA Constructions
The HIV1-Nef allele and the retroviral vectors LXSN and LNefSN, used in these experiments, were described previously (Aiken et al., 1994). CD4 mutants and CD4–Nef chimera (44Nef) were created by ligating DNA fragments generated by PCR (Mangasarian et al., 1997). The constructs were verified by DNA sequence analysis. CD4 mutants and 44Nef chimera were expressed from the cytomegalovirus (CMV) immediate early promoter, in the pCMX plasmid vector (Umesono et al., 1991).
Cell Lines, Cultures, and Transfections
CEM and Namalwa cell lines expressing Nef were created using the retroviral vectors LNefSN and LXSN as previously described (Aiken et al., 1994). Stably transfected cells were next cultivated in RPMI 1640 medium supplemented with 10% FCS and selected in the presence of 1 mg/ml G418. The Epstein-Barr virus (EBV)-transformed Namalwa human B cell line was maintained in RPMI 1640 medium supplemented with 10% FCS. For the establishment of cell populations stably producing CD4 and derivatives, Namalwa cells were coelectroporated with a mixture comprising a CMV-based plasmid expressing one of these proteins and pSV2-His, at a 1:10 ratio, using a total of 50 µg of DNA for 5 x 106 cells at 250 V and a capacitance of 960 µF. Cells were then selected in histidine-deficient medium containing 1 mM histidinol (Sigma Chemical Co.) (Mangasarian et al., 1997).
Antibody and Holo-transferrin Iodination
Iodination of purified mouse anti–human CD4 antibodies (RPA-T4) and iron-saturated holo-transferrin was performed using Iodo-Beads according to the manufacturer's instructions (Markwell, 1982). Briefly, Iodo-Beads were washed and preloaded with 
0.5–1 mCi of Na125I in PBS for 5 min at room temperature. Free-carrier mouse anti–human CD4 antibodies (50 µg, 330 pmol) or holo-transferrin (100 µg, 1.23 nmol) were added to the beads and incubation was continued for 15 min at room temperature. Iodination was stopped by removing the beads from the mixture reaction and free 125I was discarded by passing the solution through a gel filtration sephadex G-25 column (Pharmacia Biotech, Inc., Piscataway, NJ). Iodinated protein was stored at 4°C in PBS + BSA 1%. Specific activity was comprised between 2–3 µCi/µg of protein and 3–4 µCi/µg of protein for 125I–anti-CD4 and 125I–holo-transferrin, respectively.
Acid Wash Assay
Internalization was assayed using the acid wash technique as previously described (Iacopetta et al., 1986; Pelchen Matthews et al., 1989; Pelchen Matthews et al., 1991; Aiken and Trono, 1995). Briefly, cells (10–20 x 106) were washed and incubated for 2 h at 4°C with 125I–RPA-T4 (0.02–0.04 µCi/106 cells, i.e., 7–20 ng/106 cells) or 125I-transferrin (0.01–0.02 µCi/106 cells, i.e., 3–7 ng/106 cells) in 0.5 ml cold PBS/BSA 1%. Cells were next washed twice by centrifugation (200 g, 5 min) to remove unbound radiolabeled molecules and then incubated at 37°C to allow endocytosis. Cells were washed twice in their corresponding buffer at low pH (pH 2) to remove surface-bound radiolabeled antibodies or ligands. Percentage of 125I–anti-CD4/125I-transferrin internalization was expressed as the ratio of acid wash–resistant radioactivity to total radioactivity associated with cells at neutral pH. Counting was performed in a Beckman 5,500 counter (Fullerton, CA). The iodinated anti–CD4 antibody binding at 4°C was maximal after 90 min of incubation. The nonspecific binding ranged between 3–5% of the total recovered radioactivity. The sequential washes with buffer at pH 2 detached more than 95% of the surface-bound antibodies after a 2-h incubation at 4°C.
Fluid-Phase Endocytosis Assay
Duplicates of 15 x 106 cells were incubated for different periods of time at 37°C in the presence of Lucifer yellow (1.5 mg/ml in Ca2+- and Mg2+-free medium 1). At the end of each incubation period, the endocytic process was stopped by cooling the cells at 4°C. Cells were next washed four times in ice-cold Ca2+- and Mg2+-free medium and lysed with 0.1% Triton X-100 (Krischer et al., 1993). Cell-associated fluorescence was measured in a Perkin-Elmer LS-3 fluorimeter (excitation 415 nm, emission 535 nm; Perkin-Elmer Corp., Norwalk CT). Finally, fluorescence value was reported to protein content of each sample. Protein determination was performed with the Pierce kit using bicinchonic acid.
Autoradiography
CEM T cells were incubated for 2 h at 4°C with 125I–anti-CD4 (0.2–0.3 µCi/106 cells, i.e., 100 ng/106 cells) in PBS/BSA 1%. After antibody binding, cells were washed twice by centrifugation (200 g, 5 min) to remove antibody excess, and warmed for various periods of time at 37°C to allow endocytosis. Cells were then fixed, dehydrated, and processed for electron microscope autoradiography; labeling was quantitated as previously described (Carpentier et al., 1978, 1981, 1992; Fan et al., 1982). Three experiments were performed. For each incubation time analyzed, three Epon blocks were prepared, and sections were cut from each block. For each time point studied and for each cell line, 950–1,150 grains were analyzed from cells judged to be morphologically well preserved. Autoradiographic grains within a distance of ±250 nm from the plasma membrane were considered associated with the cell surface; grains overlying the cytoplasm and >250 nm from the plasma membrane were considered internalized. Grains associated with the plasma membrane were considered associated with CCP if their centers were <250 nm from these surface domains. Indeed, assuming a half distance of 80–100 nm (Salpeter et al., 1977), the radioactive source responsible for each autoradiographic grain has a >80% chance of being contained within this distance of 250 nm around each grain. The center of the grains was determined by overlaying them with a circle of 250-nm radius. This approach has been extensively used and validated in previous studies (Salpeter et al., 1977; Carpentier et al., 1978, 1981, 1992; Fan et al., 1982).
CD4 Immunogold Labeling on EM Thin Sections and Isolated Plasma Membranes
CEM T cells were incubated 2 h at 4°C with anti-CD4 antibodies (Leu3a, 40 ng/106 cells) in cold PBS/BSA 1%. After antibody binding, cells were washed twice by centrifugation (200 g, 5 min) in cold PBS to remove antibody excess and incubated a second time with an anti–mouse IgG coupled with 10-nm colloidal gold particles for 2 h at 4°C. (Antibodies were used at a dilution of 1:15 for a cell suspension of 5 x 107 cell/ml of PBS/BSA 1%.) Unbound secondary antibody was removed by washing twice with cold PBS, and then cells were warmed for various periods of time at 37°C to allow endocytosis. For conventional EM analysis, cells were then fixed, dehydrated, and processed for EM as described previously (Carpentier et al., 1991). Thin sections were examined in an electron microscope (model EM 300; Philips Electron Optics, Eindhoven, The Netherlands), and gold particles were quantitatively analyzed on cells considered well preserved. Gold particles were considered associated with clathrin-coated structures when they were observed immediately adjacent (at a distance <20 nm) to the clathrin coat or totally enclosed in clathrin-coated pits/vesicles. Two experiments were performed. For each incubation time analyzed, two Epon blocks were prepared, and sections were cut from each block. For each time point studied and for each cell line, 700–2,250 gold particles were analyzed from cells judged to be morphologically well preserved. For morphological analysis of isolated plasma membranes, adherent membranes were prepared as described above and gold particles were visualized by transparency. The ratio of gold-labeled CCP/total number of CCP observed was quantitated. A total of 416 and 199 CCP were considered for control and Nef-expressing cells, respectively.
Quantitative Determination of Clathrin-coated Plasma Membrane
Quantitative determination of clathrin-coated plasma membrane CCP and clathrin lattices on the inner face of the plasma membrane were visualized as described by Sanan and Anderson (1991) with minor modifications. Briefly, formvar-coated EM nickel grids were treated with 1 mg/ml of poly-L-lysine for 1 h at 4°C. Cells (106/ml) in cold PBS were then allowed to sediment on the air-dried grids for 1 h at 4°C. Cells adherent to poly-L-lysine–coated grids were next washed with cold PBS, incubated 30 min with cold PBS/BSA 1%, and washed twice again with cold PBS. Adherent isolated plasma membranes were obtained by incubating the grids with the adherent cells in hypotonic (0.65x) PBS for 30 s and then by sonicating the cells at a weak power. This procedure disrupts the cells but allows a large portion of plasma membranes, with conserved internal structures such as clathrin-coated membranes and cytoskeleton elements, to stay adherent to the poly-L-lysine–coated grids. Adherent membranes were next washed with cold PBS and fixed for 15 min at 4°C followed by 15 min at room temperature with 4% glutaraldehyde in PBS. Adherent membranes were subsequently fixed in 2% osmium tetroxide in PBS for 8 min, 30 s at room temperature, washed three times for 5 min with PBS buffer, incubated with 1% aqueous tannic acid for 10 min, washed twice for 5 min in distilled water, incubated with 1% uranyl acetate for 10 min, and finally washed twice for 1 min with distilled water before air-drying. Membranes considered well conserved were then randomly photographed on an electron microscope (model EM 301; Philips Electron Optics). Eventually, the extent of membrane surfaces (%) decorated by clathrin was quantitated on electron micrographs using a Leica Quantimet 500 + (Vienna, Austria).
Concomitant Labeling of CD4 and Transferrin Receptors on EM Thin Sections
Cells in ice-cold PBS/BSA 1% (107/ml) were successively (a) incubated with anti–transferrin receptor antibodies (0.5 µg/106 cells, 90 min at 4°C), (b) washed and incubated a second time with an anti–mouse IgG coupled with 10-nm colloidal gold particles (antibodies diluted 1:15 in 20 x 106 cells/ml, 90 min at 4°C), (c) washed and saturated with nonspecific globulins (100 µg/106cells, 30 min at 4°C), and (d) washed and incubated a third time with 125I–anti-CD4 antibodies (100 ng/106 cells, 90 min at 4°C). Eventually, cells were washed twice with ice-cold PBS and warmed for 5 min at 37°C to allow the recruitment of tagged receptors into CCP and their endocytosis. Cells were then fixed for 30 min at room temperature with 2.5% glutaraldehyde in phosphate buffer, dehydrated, and processed for EM as described previously (Carpentier et al., 1991). Thin sections were examined in an electron microscope (model EM 301; Philips Electron Optics) Finally, association of autoradiographic grains (CD4 labeling) and gold particles (transferrin receptors labeling) with CCP present at the plasma membrane was quantitatively analyzed on cells considered well preserved. Autoradiographic grains located on the plasma membrane were considered associated with CCP if their centers were <250 nm from these surface domains. Gold particles were considered associated with CCP when they were observed immediately adjacent.
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RESULTS |
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3% of plasma membrane–bound CD4 was found associated with CCP in control cells. This value slightly increased with time and temperature to reach 5% after 30 min of incubation at 37°C. By contrast, in cells expressing Nef, the association of 125I–anti-CD4 with CCP peaked after 5 min of incubation at 37°C and plateaued at 8% (Fig. 2 B). CD4 association with CCP was alternatively determined by EM immunogold labeling visualized on ultrathin sections. This method allows a more precise localization of anti-CD4 on the cell surface and a better definition of its association with specialized membrane domains such as CCP (Fig. 1 C). Similar conclusions to the one reached using 125I–anti-CD4 as a ligand were collected through immunogold labeling: in the presence of Nef at 37°C, anti-CD4 association with CCP increased at each time point studied by a factor between two and three (Fig. 2 C). The amount of cell surface 125I–anti-CD4 internalized, in both control and Nef-expressing cells, was closely related to the propensity of CD4 to associate with CCP, as shown by the linear relationship (R = 0.76) connecting the two events (Fig. 2 D). Thus, in the presence of Nef, the stimulated rate of CD4 internalization was related, at least in part, to an increased association of the receptor with CCP.
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chain, ICAM-1, CD38, CD69, the transferrin receptor (Tf-R), and a CD4–LDL receptor fusion protein (Benson et al., 1993; Schwartz et al., 1993; Aiken et al., 1994), indicating that the Nef effect on endocytosis is at least partly receptor specific. To verify this point in our experimental conditions, 125I–transferrin uptake was analyzed. The transferrin receptor is a carrier of cargo molecules concentrated in CCP and constitutively internalized through these structures (Hanover et al., 1985; Watts, 1985). Nef expression only moderately affected the uptake of radiolabeled-transferrin, thus confirming the lack of a general effect of Nef on receptor-mediated endocytosis (Fig. 5 A). Similarly, the uptake of a fluid-phase marker (Lucifer yellow) remained unaffected by Nef (Fig. 5 B).
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7% (Table I). The increase in the number of CCP labeled with both markers showed that additional CCP appearing in Nef-expressing cells do not incorporate exclusively CD4 but may trap, to a low extent, other receptors. This low amount of receptors other than CD4 present in additionally formed CCP is possibly responsible for the small increase in transferrin internalization observed in Nef-expressing cells (Fig. 5 A). The number of unlabeled CCP was also significantly increased by Nef expression. Given that the analysis was performed on thin sections, which does not allow visualization of the entire clathrin-coated pits, and that 125I–anti-CD4 binding was not saturating, results collected led to an underestimation of CD4 potentially present in these structures and to an overestimation of unlabeled CCP. This was verified in the course of an immunogold CD4 labeling detected on adherent plasma membranes preparations (Fig. 3 C). After 5 min of incubation at 37°C of CEM lymphocytes surface- labeled with anti-CD4 immunocomplexes, 13% of the total CCP counted on the adherent membranes incorporated the immunogold probe (data not shown) as compared with the 6.6% observed in the case of 125I–anti-CD4 binding (see above). As compared to the increase in the total number of clathrin-coated pits, these values remain low, which leaves the possibility open that some of the newly formed CCP are not functional, although the preferential Nef- induced formation of CCP versus flat clathrin lattices is in favor of the functionality of the generated structures. Moreover, Nef might generate additional CCP in CEM lymphocytes incorporating some unidentified receptors, the endocytosis of which could also be increased by the viral protein. Of note, in CEM T lymphocytes as well as in Namalwa B lymphocytes, little Nef-induced MHCI downregulation was observed (data not shown). Together, these morphological analyses strongly suggest that at least part of the Nef-induced CCP preferentially contain CD4.
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LL). As previously described (Aiken et al., 1994), this mutation completely abolished Nef-induced CD4 accelerated endocytosis (Fig. 8). The quantitative morphological analysis of CCP present at the plasma membrane of established cell lines coexpressing Nef together with either wild-type or dileucine-mutated CD4 was consistent with the internalization kinetics of these molecules. The amount of CCP decorating the plasma membrane was thus similar in cells expressing either of these proteins. However, Nef induced the formation of CCP only when coexpressed with wild-type CD4, not with the CD4LL mutant (Fig. 7). Together, these data demonstrate that the generation of new CCP capable of triggering CD4 internalization not only required Nef, but also a receptor cytoplasmic tail capable of a functional interaction with the viral protein.
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DISCUSSION |
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TopAbstractMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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The CD4 specificity of Nef-induced endocytosis is supported not only by the observation that the uptake of transferrin receptors was only weakly stimulated by Nef, but also by the results of immunocytochemical experiments carried out at the EM level, revealing a clear contrast between the percentage of clathrin-coated pits labeled with CD4 or with transferrin receptor in cells expressing Nef. These observations are in agreement with previously published results showing that the surface expression of receptors including CD8, CD29, CD45RO, interleukin-2 receptor ( chain), ICAM-1, CD38, CD69, HLA-DR, and a CD4-LDL receptor fusion protein are unaffected by Nef (Benson et al., 1993; Schwartz et al., 1993; Aiken et al., 1994). The only known exception is the MHCI molecule, the internalization of which is also stimulated by Nef, although less efficiently than that of CD4 (Schwartz et al., 1996). Nef also did not affect fluid-phase endocytosis in our experimental conditions. This latter observation supports the recent proposal that the total uptake of membrane and fluids is not strictly regulated by the clathrin- dependent endocytic pathway but might involve alternative mechanisms (Hansen et al., 1993; Cupers et al., 1994; Eker et al., 1994; Damke et al., 1995). The receptor-dependent formation of CD4-specific CCP could appear to contradict previous observations showing that CCP are relatively nonspecific structures capable of concentrating receptors of diverse nature (Dickson et al., 1981; Willingham et al., 1981; Carpentier et al., 1982). It is likely, however, that the selectivity of the observed phenomenon reflects a specific interaction between Nef and CD4 (Harris and Neil, 1994; Greenway et al., 1995; Grzesiek et al., 1996; Rossi et al., 1996). As Nef might interact with other receptors such as MHCI, it may appear surprising that the Nef-dependent CCP formation observed here required the presence of CD4, at least if Nef-induced CD4 and MHCI endocytosis proceed through similar mechanisms. However, levels of MHCI were found to be minimally affected by Nef expression in Namalwa cells (data not shown).
The relative receptor specificity of the clathrin-coated structures induced by Nef could be interpreted as evidence for the initiation by receptors of the de novo formation of CCP, or alternatively could mean that CD4 is preferentially segregated in preformed Nef-induced CCP. The second possibility can be ruled out since, except in nonphysiological conditions where Nef is constitutively attached to the plasma membrane as part of a chimeric integral membrane protein, the viral protein alone is not able to induce CCP formation. Concomitant expression of CD4 is indeed necessary for this process; furthermore, there is a strict requirement for the preservation, within the CD4 cytoplasmic tail, of a dileucine-based motif previously identified as critical for CD4 response to Nef (Aiken et al., 1994).
These observations demonstrate that, at least in some circumstances, receptor tails can initiate coat protein assembly. This conclusion contrasts with that of previous studies in which a series of transport protein receptors showed a surface mobility consistent with random movements and occasional encounters with CCP (Fire et al., 1991; Ghosh and Webb, 1994; Katzir et al., 1994; Sako and Kusumi, 1994; Lazarovits et al., 1996). Along the same line, the relocalization and aggregation of FcRIs induced by multivalent antigens was not found to be accompanied by any change in the distribution of adaptor protein 2 (AP2) or clathrin (Santini and Keen, 1996). However, our findings are in agreement with other studies showing: (a) clathrin recruitment at the plasma membrane subsequent to ligand-induced clustering of IgM receptors in lymphoblastoid cells (Salisbury et al., 1980); and (b) a correlation between the number of surface Tf-Rs and CCP in transfected cells (Iacopetta et al., 1988; Miller et al., 1991). The present work adds another dimension to these results, by providing direct evidence for a causal relationship between the presence of receptors and the formation of CCP.
Since both CD4 and Nef are required for the induction of CCP, what are their respective contributions to this phenomenon? Results presented show that both CD4 and Nef are required for the induction of CCP, and that Nef artificially tethered to the membrane as the cytoplasmic tail of a transmembrane fusion protein is capable of producing the same effect. These observations imply that Nef targeting to the plasma membrane, either through a direct physical interaction with CD4 (or the CD4/p56lck complex), or alternatively through part of a chimeric integral protein, is the primary requirement to induce CCP generation. This targeting may either permit the interaction of the viral protein with other proteins involved in signal transduction pathways leading to CCP generation, or allow a direct participation of the viral protein in CCP formation. Clathrin coat assembly is a multistep process in which a pivotal role is played by AP (Smythe and Warren, 1991; Schmid, 1992; Robinson, 1994). These heterotetrameric proteins participate in at least three crucial stages of clathrin-coated pit formation where Nef might act: (a) they must be recruited onto the right membrane, probably through binding to specific adaptor receptors (Mahaffey et al., 1990); (b) they next are activated to make them competent (possibly as part of complexes with other molecules) to bind clathrin triskelions (Peeler et al., 1993); and (c) they initiate the nucleation process leading to clathrin assembly into lattices (Keen et al., 1991; Gallusser and Kirchhausen, 1993). Several studies have provided evidence for a direct interaction of Nef with signal-transducing molecules such as protein tyrosine kinases of the src family (p56lck, hck) (Saksela et al., 1995; Collette et al., 1996), serine/threonine protein kinases (Sawai et al., 1995), protein kinase C (Bandres et al., 1994), or protein phosphatidylinositol 3-kinase (Graziani et al., 1996), all molecules which may participate in the triggering and/or regulation of endocytotic processes. Via these effects on signal transduction pathways Nef might, therefore, interfere with CD4 endocytosis. However, Nef-induced CD4 downregulation is generally dissociated from the effects of the viral protein on signal transduction pathways (Aiken and Trono, 1995; Chowers et al., 1995; Saksela et al., 1995), suggesting that mechanisms implemented by Nef to induce the formation of CCP are not related to perturbation of signal transduction and might rather involve a more direct participation of the viral protein. Several observations support this alternative: (a) Nef is capable of physical interaction with CD4 and this interaction requires the integrity of a dileucine motif present in CD4 cytoplasmic tail; (b) Nef-induced CD4 endocytosis is specific and is not dependent on CD4 alteration; (c) the chimeric molecule CD4–Nef is internalized efficiently through CCP, suggesting that Nef contains the determinants required to associate with CCP components (Mangasarian et al., 1997); and (d) Nef is capable of physical interactions through different domains with both CD4 and adaptins (Piguet, V., M. Foti, A. Mangasarian, D. Lew, K.-H. Krause, D. Trono, and J.-L. Carpentier, manuscript in preparation). Thus, although we cannot exclude that CCP generation is related to Nef-induced signaling cascades, data collected favor a model where Nef plays the role of a connector between specific recognition signals present in receptor tails (e.g., CD4) and adaptins. They also suggest that the CD4–Nef complex participates together with adaptins in the nucleation process, perhaps via the Nef-mediated activation of adaptins. A third model would be that Nef itself behaves as an adaptin. We do not favor this possibility since it would imply that Nef, which has no structural analogy with adaptins, not only plays all the diverse and complex functions of these molecules, but in addition can generate CCP morphologically identical to those requiring adaptins.
Nef might mimic endogenous molecules capable, in physiological conditions, to link various receptors bearing dileucine-based motifs (or other motifs) to components of the endocytic machinery, and sometimes to induce the formation of CCP. Along this line, if a possible direct interaction of dileucine motifs with adaptins has recently been reported, this concept is not accepted by others (Ohno et al., 1995; Heilker et al., 1996). It is noteworthy that several cellular proteins appear to function as connectors between cell surface receptors and CCP. β-arrestin has thus been demonstrated to act as a clathrin adaptor facilitating the endocytosis of the β2-adrenergic receptor (Ferguson et al., 1996; Goodman et al., 1996), while the Eps15 and Shc proteins are thought to participate in connecting the EGF receptor tyrosine kinase with CCP (Okabayashi et al., 1996; Van Delft et al., 1997). However, no data is available to suggest that these proteins can induce the formation of CCP.
Taken together, the present results demonstrate that CCP nucleation can be receptor driven and support the following ordered sequence of events leading to the nucleation process in these conditions: (1) receptors recruit endogenous helper molecules (here mimicked by Nef) via specific domain(s) of their cytoplasmic tail (e.g., dileucine-based domains); (2) the recruitment of these partner molecules on the cytoplasmic side of the plasma membrane renders possible their interaction with molecules capable of initiating clathrin assembly (i.e., AP2); and (3) after activation of these assembly proteins, the clathrin coat nucleation is generated. According to the model proposed, the internalization capacity of surface receptors might be modulated by factors affecting the expression or the affinity of these hypothetical endogenous connectors for their respective receptor tails. The participation of such connector molecules in the endocytosis of some receptors might be alternative (or complementary) to the recently documented mechanism implicating the direct binding of receptor cytoplasmic tails to AP-2 (Sorkin and Carpenter, 1993; Ohno et al., 1995; Heilker et al., 1996).
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Acknowledgments |
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This work was supported by the Fonds National Suisse pour la Recherche Scientifique, grants 31-36063.92 and 31-42409.95, National Institutes of Health (NIH) Fogarty International Center award R03 TW 00531 (to D. Trono and J.-L. Carpentier), a grant from the Fondation Centre de Recherches medicales Carlos et Elsie de Reuter (to J.-L. Carpentier), and NIH award R37 AI34306 (to D. Trono).
Submitted: 9 May 1997
Revised: 9 July 1997
Address all correspondence to Jean-Louis Carpentier, Department of Morphology, Centre Médical Universitaire, 1, rue Michel-Servet, 1211 Geneva 4, Switzerland. Tel.: 41.22.7025201. Fax: 41.22.7025260. E-mail: Jean-LouisCarpentier{at}medecine.unige.ch
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