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Journal of Virology, June 2005, p. 7195-7206, Vol. 79, No. 11
0022-538X/05/$08.00+0     doi:10.1128/JVI.79.11.7195-7206.2005
Copyright © 2005, American Society for Microbiology. All Rights Reserved.

Identification and Characterization of the Putative Fusion Peptide of the Severe Acute Respiratory Syndrome-Associated Coronavirus Spike Protein

Bruno Sainz Jr.,1 Joshua M. Rausch,2 William R. Gallaher,3 Robert F. Garry,1 and William C. Wimley2*

Department of Microbiology and Immunology, Program in Molecular Pathogenesis and Immunity,1 Department of Biochemistry, Tulane University Health Sciences Center, New Orleans, Louisiana 70112,2 Department of Microbiology, Immunology and Parasitology, Louisiana State University Health Sciences Center, New Orleans, Louisiana 701123

Received 28 October 2004/ Accepted 5 January 2005


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ABSTRACT
 
Severe acute respiratory syndrome-associated coronavirus (SARS-CoV) is a newly identified member of the family Coronaviridae and poses a serious public health threat. Recent studies indicated that the SARS-CoV viral spike glycoprotein is a class I viral fusion protein. A fusion peptide present at the N-terminal region of class I viral fusion proteins is believed to initiate viral and cell membrane interactions and subsequent fusion. Although the SARS-CoV fusion protein heptad repeats have been well characterized, the fusion peptide has yet to be identified. Based on the conserved features of known viral fusion peptides and using Wimley and White interfacial hydrophobicity plots, we have identified two putative fusion peptides (SARSWW-I and SARSWW-II) at the N terminus of the SARS-CoV S2 subunit. Both peptides are hydrophobic and rich in alanine, glycine, and/or phenylalanine residues and contain a canonical fusion tripeptide along with a central proline residue. Only the SARSWW-I peptide strongly partitioned into the membranes of large unilamellar vesicles (LUV), adopting a ß-sheet structure. Likewise, only SARSWW-I induced the fusion of LUV and caused membrane leakage of vesicle contents at peptide/lipid ratios of 1:50 and 1:100, respectively. The activity of this synthetic peptide appeared to be dependent on its amino acid (aa) sequence, as scrambling the peptide rendered it unable to partition into LUV, assume a defined secondary structure, or induce both fusion and leakage of LUV. Based on the activity of SARSWW-I, we propose that the hydrophobic stretch of 19 aa corresponding to residues 770 to 788 is a fusion peptide of the SARS-CoV S2 subunit.


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INTRODUCTION
 
Severe acute respiratory syndrome (SARS) is a disease characterized by influenza-like symptoms, including fever, cough, dyspnea, and headache. The global outbreak of SARS began in the fall of 2002 in the Guangdong Province of China and gained worldwide attention due to its relative ease of transmission and disease severity. By July 2003, 8,098 probable cases had been reported, resulting in 774 deaths in 29 countries worldwide (33). The etiological agent of SARS was quickly identified as a newly emerged coronavirus (CoV) that is genetically distinct from previously characterized members of the Coronaviridae family (20, 45, 60).

Coronaviruses are large positive-strand RNA viruses with a broad host range (47, 74). Like other enveloped viruses, CoVs enter target cells by fusion between the viral and cellular membranes, a process mediated by the viral spike (S) protein (25). The CoV S protein, as characterized to date, consists of two noncovalently associated subunits, S1 and S2. The S1 subunit of the S glycoprotein mediates receptor binding (12, 82), while the S2 subunit is responsible for driving viral and target cell membrane fusion (83). The S2 subunit is a prototypical class I viral fusion protein containing common structural features (11, 26-28, 92) such as (i) a hydrophobic fusion peptide (50, 51), (ii) a pair of extended {alpha}-helices, specifically 4,3-hydrophobic heptad repeats (HR) (7, 97), and (iii) a cluster of aromatic amino acids proximal to (iv) a hydrophobic transmembrane anchoring domain.

Although the SARS-CoV S protein shares only 20 to 27% amino acid (aa) homology with the S proteins of other CoVs (69), recent studies have confirmed that the putative SARS-CoV S2 subunit is also a class I viral fusion protein. Using computational analysis, Gallaher and Garry (29) first proposed that the portion of the SARS-CoV S protein corresponding to the S2 subunit fit the prototypical model of a class I viral fusion protein based on the presence of two predicted HR regions at the N and C termini of S2 and an aromatic-aa-rich region just prior to the transmembrane anchor domain. Using synthetic peptides analogous to the two HR regions of S2, several groups have demonstrated that SARS-CoV HR1 and HR2 interact with one another to assume a coiled coil conformation (6, 49, 84, 99). Most recently, Xu et al. showed by crystal structure analysis that the SARS-CoV S protein fusion core forms a typical six-helix coiled coil bundle (98), as seen with the murine hepatitis virus (MHV) S protein (97). Furthermore, we have shown that the aromatic-aa-rich region of the SARS-CoV S2 subunit has similar functionality to the aromatic regions of both the human immunodeficiency virus (HIV) transmembrane (TM) glycoprotein (GP) (80) and Ebola virus (EboV) GP2 (71), in that peptides analogous to this aromatic region can induce the permeabilization of lipid vesicles (73). Although the putative fusion peptide of the SARS-CoV S2 subunit has yet to be identified, it has been predicted that the SARS-CoV S fusion peptide lies within the N-terminal region of the S2 portion (residues 851 to 882), preceding HR1 (84).

Like other enveloped viruses encoding class I viral fusion proteins (27, 28), it is presumed that SARS-CoV uses membrane fusion mechanisms for viral entry (98, 99). After binding of the SARS-CoV S1 subunit to the mammalian receptor angiotensin-converting enzyme 2 (ACE2) (48, 85, 95) and/or CD209L (L-SIGN) (44), a conformational change in the S protein results in the exposure of an unidentified hydrophobic fusion peptide within S2. As with other class I viral fusion proteins (27, 28), the fusion peptide is believed to penetrate the target cell membrane, initiating the virion-cell membrane fusion event. Numerous mutagenesis studies of other enveloped viruses encoding class I viral fusion proteins (8, 23, 32, 38, 43, 51), as well as synthetic peptide studies (1, 14, 15, 17, 21, 34, 46, 58, 59, 62, 63, 66, 70), have provided substantial evidence of the role of the fusion peptide in initiating membrane fusion. Following insertion of the fusion peptide into the target cell membrane, HR interactions between residues 916 to 950 of HR1 and residues 1151 to 1185 of HR2 (84) mediate the formation of a six-helix coiled coil bundle (98, 99). The formation of this structure, also known as the trimer of hairpins, is believed to facilitate the apposition of both the viral and target cell membranes, resulting in fusion and subsequent entry of the viral core into the target cell.

Class I viral fusion proteins generally contain one fusion peptide, located (i) internally (27, 34, 38), as seen for avian sarcoma virus (ASV) TM and EboV GP2, or (ii) either at or near the N terminus of the protein, as seen for HIV TM and influenza virus hemagglutinin (HA) (28, 61, 66, 89). Variations in the number of aa and the position within the fusion protein are apparent between fusion peptides of different class I viral fusion proteins; however, distinct features are conserved. In general, fusion peptides are short (16 to 26 residues), hydrophobic sequences (8, 24, 88) that are rich in alanine, glycine, and phenylalanine residues (8, 26, 41). The presence of a canonical fusion tripeptide (YFG or FXG) is highly conserved among the fusion peptides of retroviruses, paramyxoviruses, influenza virus, and filoviruses (21, 26, 64, 70). It is believed that the canonical fusion tripeptide contributes to the functional organization of the fusion peptide itself (64). Lastly, the presence of a proline residue at or near the center of many fusion peptides has been implicated as critical for the interaction of the peptide with the target cell lipid membrane (19, 37, 43, 70). Taken together, the presence of these conserved features and the inherent hydrophobicity of fusion peptide sequences allow for their preferential interaction with lipid membranes.

For the present study, we identified the putative SARS-CoV fusion peptide by using synthetic peptides analogous to regions of the N terminus of the putative S2 subunit. We show here that a 19-aa synthetic peptide corresponding to residues 770 to 788 strongly partitions into the membranes of lipid vesicles and has a high propensity to adopt a ß-sheet secondary structure. Furthermore, we demonstrate that this peptide alone induces membrane fusion of lipid vesicles and causes leakage of vesicle contents in a newly developed vesicle leakage assay. The data presented herein provide evidence of the presence of a putative fusion peptide at the N-terminal region of the SARS-CoV S2 protein and are consistent with previous findings using synthetic peptides to identify and characterize the fusion peptides of HIV gp41 and EboV GP2 (71, 78).


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MATERIALS AND METHODS
 
Peptide synthesis. SARS-CoV fusion (SARSWW-I and SARSWW-II) and SARS-CoV scrambled (SARSWW-I-SCR) peptides were synthesized by a solid-phase methodology using a semiautomated peptide synthesizer and conventional N-alpha-9-fluorenylmethyloxycarbonyl chemistry by Genemed Synthesis, Inc. (San Francisco, Calif.). Peptides were purified by reversed-phase high-performance liquid chromatography, and their purity was confirmed by amino acid analysis and electrospray mass spectrometry. Peptide stock solutions were prepared in dimethyl sulfoxide (DMSO; spectroscopy grade), and their concentrations were determined spectroscopically (SmartSpec 3000; Bio-Rad, Hercules, Calif.).

LUV preparation. Large unilamellar vesicles (LUV) consisting of 1-palmitoyl-2-oleoyl-sn-glycero-3-phosphatidylcholine (POPC) with L-{alpha}-phosphatidylinositol (PI) from bovine livers (Avanti Polar Lipids, Birmingham, Ala.) and/or cholesterol (Sigma, St. Louis, Mo.) were prepared according to the extrusion method of Nayar and coworkers (54, 56). Briefly, lipids were dried from a chloroform solution with a nitrogen gas stream and a high vacuum overnight. Lipid vesicles used for peptide binding assays and fusion assays were resuspended in 5 mM HEPES, 100 mM NaCl, pH 7.4, to bring the concentration to 100 mM total lipid. For circular dichroism (CD) studies, lipid vesicles were resuspended in 10 mM potassium phosphate (PO4), pH 7.0. Samples were subjected to repeated freezing and thawing for 15 cycles, followed by extrusion through 0.1-µm polycarbonate membranes in a Lipex Biomembranes extruder (Vancouver, British Columbia, Canada). For the preparation of terbium (III) chloride hexahydrate (Tb3+) LUV, lipids were resuspended to a 100 mM concentration in 50 mM Tb3+, 100 mM sodium citrate, and 10 mM N-Tris-(hydroxymethyl)methyl-2-amino ethane sulfonic acid (TES), pH 7.2. Gel filtration with Sephadex G-200 was used to remove unencapsulated Tb3+ in a buffer of 10 mM TES and 325 mM NaCl (67). Final lipid concentrations were determined by phosphate analysis (16, 22).

Peptide binding assay. The partitioning of peptides into the lipid bilayer was monitored by the fluorescence enhancement of tryptophan (91). Fluorescence was recorded at excitation and emission wavelengths of 280 and 340 nm, respectively, and with 8-nm bandwidths by use of an SML Aminco 8100 spectrofluorometer (Rochester, N.Y.). Quartz cuvettes with excitation and emission path lengths of 4 and 10 mm, respectively, were used. Measurements were carried out in 5 mM HEPES, 100 mM NaCl, pH 7.4. Peptides were added from stock solutions in DMSO to 250 µl of buffer and mixed by inversion. Likewise, LUV were titrated to a final lipid concentration of 1 mM and then mixed by inversion. Intensity values (I) were adjusted for lipid scattering and normalized to that of the peptide in buffer (Io). Partitioning coefficients were obtained with equation 1, as follows:

(1)
where Kx is a mole fraction partition coefficient that represents the amount of peptide in bilayers as a fraction of the total amount of peptide present in the system, Imax is a variable value for the fluorescence enhancement at complete partitioning determined by fitting the equation to the experimental data, [L] is the concentration of lipid, and [W] is the concentration of water (55.3 M).

Lipid vesicle fusion assay. Experiments to detect membrane fusion were performed by use of a fluorescence resonance energy transfer (FRET) technique for dye-labeled lipids (57, 77). In this assay, the fluorescence of one dye-labeled lipid, the donor, is quenched by the presence of another dye-labeled lipid, the acceptor, as long as they are confined to the same lipid membranes. Fusion with other unlabeled membranes dilutes the dye concentrations, and the quenching of the donor molecule is relaxed. FRET fusion assays employed 25 µM labeled 9:1 POPC:PI LUV with 7-nitro-2,1,3-benzoxadiazol-4-yl (NBD)-1-palmitoyl-2-oleoyl-sn-glycero-3-phosphatidylethanolamine (POPE) and rhodamine (Rho)-POPE (Avanti Polar Lipids) at a concentration of 1% mole fraction of total lipid each. Unlabeled 9:1 POPC:PI LUV were then added to the system to a total lipid concentration of 500 µM. Fluorescence spectra for these samples were recorded from 480 to 750 nm on an SLM Aminco 8100 spectrofluorometer, with excitation at 465 nm, in a 500-µl quartz cuvette. Time trace experiments of 1,000 s were conducted. The ability of peptides to increase NBD fluorescence was examined at peptide:lipid (P:L) ratios of 1:50, 1:25, and 1:10 beginning at 120 s. Prior to and following time trace spectra, the NBD fluorescence at 530 nm was measured to determine the pre- and postpeptide NBD fluorescence. Likewise, the use of 5% Triton X-100 (Sigma) to permeabilize vesicles was used to normalize the NBD fluorescence of the system and to scale the resultant spectra for comparison.

Controls to determine the extent of fusion were prepared as separate LUV solutions representing serial twofold dilutions of dye concentrations within bilayers. LUV were prepared at NBD-Rho-POPE concentrations of 1.0%, 0.5%, 0.25%, 0.125%, and 0.0625% as well as with only 1.0% NBD-POPE or 1% Rho-POPE. These LUV were representative of 1, 3, 7, 15, and an infinite number of fusion events if all vesicles underwent uniform fusion with unlabeled LUV. Stocks of each of these labeled LUV solutions were prepared with unlabeled LUV to a final lipid concentration of 500 µM in proportions such that the overall number of each dye molecule was maintained. The NBD fluorescence of these solutions at 530 nm was determined and used to calculate the extent of membrane fusion observed upon the addition of peptide by the use of equation 2, as follows:

(2)
where F is equal to the NBD fluorescence normalized to the Triton X-100 control.

Lipid vesicle leakage assays. For microwell plate assays, a 200-µl aliquot of vesicle solution containing 500 µM Tb3+ LUV in 10 mM TES, 50 µM 2,6-pyridine dicarboxylic acid (DPA), and 325 mM NaCl, pH 7.2, was pipetted into each well of a plastic 8-by-12-format plate (67). Peptides in DMSO were added to each well at P:L molar ratios of 1:500, 1:250, 1:100, 1:50, and 1:25, the well contents were thoroughly mixed, and the plates were allowed to incubate at room temperature for 2 h. In addition to the peptide-treated wells, DMSO-treated and Triton X-100-treated wells served as negative and positive controls, respectively. After 2 h of incubation, Tb3+/DPA fluorescence was visualized under horizontally mounted short-wave (254 nm) UV sources in a darkroom (67). Plates were photographed and images were recorded with a Nikon Coolpix 995 camera using a 4-s exposure time at 100 speed with a 2.6 aperture and a 540-nm band-pass optical filter between the sample and the lens. For each experimental plate, the Tb3+/DPA fluorescence for the peptide-treated wells was compared to that of wells containing the same amount of untreated vesicles and of wells containing vesicles that had been lysed with the detergent Triton X-100. Color adjustment and contrasting were normalized to negative controls by the use of Adobe Photoshop.

To quantitate the extent of leakage observed in the Tb3+/DPA microwell assay, we added peptides to 500 µM Tb3+ LUV in 10 mM TES, 50 µM DPA, and 325 mM NaCl, pH 7.2, at P:L molar ratios of 1:750, 1:500, 1:250, 1:100, 1:50, and 1:25. The samples were shaken at room temperature for 2 h, and the fluorescence of the samples was recorded at excitation and emission wavelengths of 270 nm and 490 nm, respectively, and with 8-nm bandwidths by use of an SML Aminco 8100 spectrofluorometer. Quartz cuvettes with excitation and emission path lengths of 4 and 10 mm, respectively, were used. The percent leakage of Tb3+ was calculated with equation 3 as follows:

(3)
where Fmax is obtained by adding 25 µl 5% Triton X-100 and Fo is equivalent to the value for DMSO controls.

CD spectroscopy. CD spectra were recorded on a Jasco J-810 spectropolarimeter (Jasco Inc., Easton, Md.), using a 1-mm path length, 1-nm bandwidth, 16-s response time, and a scan speed of 10 nm/min. All CD runs were performed at room temperature with peptides dissolved in 10 mM PO4 buffer at pH 7.0. LUV were added at a lipid concentration of 1 mM from a stock in 10 mM PO4 buffer, pH 7.0. Three successive scans from 190 to 250 nm were collected, and the CD data are expressed as mean residue ellipticities, derived from the formula {Theta} = (deg x cm2)/dmol.

Proteomic computational methods. Methods to derive general models of surface glycoproteins have been described previously (28). Domains with a significant propensity to form transmembrane helices were identified with TMpred (ExPASy; Swiss Institute of Bioinformatics) and Membrane Protein eXplorer (MPeX; Stephen White laboratory [http://blanco.biomol.uci.edu/mpex]). TMpred is based on a statistical analysis of TMbase, a database of naturally occurring transmembrane proteins (40), while MPeX detection of membrane spanning sequences is based on experimentally determined hydrophobicity scales (90, 94). Sequences with a propensity to partition into the lipid bilayer were also identified by MPeX, using interfacial settings.


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RESULTS
 
Identification of putative fusion peptide(s) within the SARS-CoV S2 subunit. The Wimley and White interfacial hydrophobicity (WWIH) scale was used to initially identify regions of the SARS-CoV S2 subunit (N terminus) with a high propensity to partition into lipid membranes. This scale is based on the free energies of transfer ({Delta}G [kcal/mol]) of amino acid sequences from water to bilayer interfaces, taking into consideration the contribution from the peptide bond (94). Although no consensus exists regarding whether the SARS-CoV S protein is proteolytically cleaved into two noncovalently linked subunits (S1 and S2), the presence of a minimum furin cleavage site (R-X-X-R) (9, 55, 68) at residues 758 to 761 (R-N-T-R) suggests that the S glycoprotein may be proteolytically cleaved. The SARS-CoV S protein minimum furin cleavage site is not unlike the furin cleavage sites found in other CoV S proteins, such as the S proteins of MHV strain A59 (R-A-H-R) (52) and the human CoV OC43 (R-R-S-R), which can also be represented as R-X-X-R. Furthermore, recent studies to investigate SARS-CoV S protein processing reported that proteolytic processing of the viral glycoprotein is detectable in vitro (2, 96). As such, our analysis of the SARS-CoV S protein was limited to the putative S2 subunit (residues 762 to 1255).

Due to the salient similarities between the SARS-CoV S protein and the class I fusion proteins of other RNA viruses, we compared the interfacial hydrophobicity plot of the N-terminal region of the SARS-CoV S2 subunit to those of the N-terminal regions of HIV-1 gp41 and EboV GP2. For the N-terminal regions of the HIV-1 and EboV viral fusion proteins (Fig. 1A and B), a distinct region of high interfacial hydrophobicity was identified, corresponding to the experimentally determined fusion peptides of these two viral glycoproteins (1, 27, 34, 43, 59, 61, 64, 70, 79). For the SARS-CoV S2 subunit, however, two regions of high interfacial hydrophobicity were identified. Their positions within the S2 subunit N-terminal region are shown in Fig. 1C. The first region (WW-I), located 9 aa downstream of the minimum furin cleavage site (758R-N-T-R761), corresponds to residues 770MYKTPTLKYFGGFNFSQIL788 and has a predicted interfacial hydrophobicity score of 3.07 kcal/mol (Fig. 1C and Table 1). Its proximity to the presumed extreme N-terminal end of S2 is almost coincident with that of the fusion peptides of HIV-1, influenza virus, and paramyxoviruses. A second region (WW-II), located ~103 aa downstream of the minimum furin cleavage site, corresponds to residues 864ATAGWTFGAGAALQIPFAMQMAY886 and has a predicted interfacial hydrophobicity score of 3.76 kcal/mol (Fig. 1C and Table 1). This region more resembles the EboV GP2 (27) and ASV TM (38, 42) internal fusion peptides due to its distance from the furin cleavage site.



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  		FIG. 1. Interfacial hydrophobicity plots corresponding to sequences of HIV-1 gp41, EboV GP2, and SARS-CoV S2. Interfacial hydrophobicity plots (mean values for a window of 19 residues) were generated by using the WWIH scales for individual residues (94) of HIV-1 strain HXB2 gp41 (amino acids 502 to 600) (A), EboV strain Zaire GP2 (amino acids 520 to 590) (B), and the SARS-CoV strain Urbani S2 subunit (amino acids 763 to 900) (C). The residues corresponding to the known fusion peptides of the HIV (A) and EboV (B) fusion proteins are indicated by black bars and labeled FP. In addition, the two putative SARS-CoV fusion peptides (C) studied in this work are indicated by black bar and are labeled SARSWW-I and SARSWW-II.


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  		TABLE 1. Amino acid sequences and WWIH scores of viral fusion peptides

Sequence analyses of these two putative fusion peptides (SARSWW-I and SARSWW-II) showed several conserved features that are shared with known viral fusion peptides. Both sequences are short, composed of mainly hydrophobic and nonpolar residues, and rich in alanine, glycine, and/or phenylalanine residues. Likewise, a putative canonical tripeptide or dipeptide with a central phenylalanine residue was present in both SARSWW-I and SARSWW-II (Table 1). Interestingly, SARSWW-I shares an identical canonical tripeptide with the EboV GP2 fusion peptide (Table 1). Another typical feature of fusion peptides is the presence of a proline residue at or near the center of the peptide (19, 37, 43, 70). Both SARSWW-I and SARSWW-II contain a proline residue 5 and 2 aa, respectively, from the center of the peptide (Table 1). Based on the WWIH plots (Fig. 1C) and the above conserved features, peptides analogous to these two regions of the S2 subunit were synthesized and examined for the ability to function independently as fusion peptides in the assays presented below.

SARS-CoV fusion peptide interacts with lipid membranes. A fundamental characteristic of viral fusion peptides is their inherent capacity to partition into lipid membranes. Therefore, we first assessed the ability of the two putative SARS-CoV fusion peptides to interact with membranes of LUV composed of POPC, PI, and/or cholesterol (CHOL). The degree to which a peptide partitions into a vesicle membrane can be determined fluorometrically by observing the change in tryptophan fluorescence (F) as a function of increasing lipid concentrations. The fluorescence of tryptophan increases in a low-polarity environment such as the lipid membrane interface. Figure 2 illustrates the tryptophan emission intensities of SARSWW-I and SARSWW-II in the presence of LUV composed of POPC and PI (9:1). Both peptides had similar fluorescence emission spectra in 10 mM HEPES buffer; however, only SARSWW-I showed a significant increase in tryptophan fluorescence accompanied by a negative shift in the maximum ({Delta}{lambda}max = 7 nm) following the addition of 1,000 µM lipid (Fig. 2A). SARSWW-II fluorescence increased only slightly upon the addition of lipid, with a small negative shift in the maximum ({Delta}{lambda}max = 2 nm) (Fig. 2B). Several studies have demonstrated a requirement for Ca2+ or Mg2+ in order for viral fusion peptides to partition into the membranes of lipid vesicles (59, 66, 70, 79). We observed no change in the tryptophan fluorescence of either peptide upon the addition of a divalent cation (5 mM Ca2+) in the presence or absence of lipids. Emission spectra under these conditions were similar to those illustrated in Fig. 2 (data not shown).



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  		FIG. 2. Tryptophan fluorescence emission spectra of SARS-CoV fusion peptides. (A) SARSWW-I; (B) SARSWW-II; (C) SARSWW-I-SCR. The peptides were incubated in 5 mM HEPES buffer alone (solid lines) or after the addition of LUV (dashed lines) composed of POPC and PI (9:1) (1,000 µM). The P:L molar ratio was 1:400.

The normalized tryptophan fluorescence (F/Fo) of the SARS-CoV putative fusion peptides was plotted as a function of increasing lipid concentrations to generate partition coefficients for each LUV tested (Table 2). Figure 3 illustrates a representative peptide-binding curve for SARSWW-I, from which the partition coefficients were derived. The SARSWW-I peptide partitioned strongly into the membranes of all three LUV tested, with an increased preference for LUV containing the anionic lipid PI over LUV composed of only POPC. This result was not surprising, as numerous studies have shown that viral fusion peptides preferentially partition into membranes composed of anionic lipids such as PI or phosphatidylglycerol (59, 70). Consistent with the tryptophan emission spectra (Fig. 2B), the SARSWW-II peptide demonstrated minimal to nondetectable partitioning into LUV compared to the SARSWW-I peptide (Table 2). Although SARSWW-II scored favorably (3.76 kcal/mol) on the WWIH scale, fluorometric partitioning experiments do not easily detect peptide partitioning if the energy of partitioning is smaller than about 5 kcal/mol.


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  		TABLE 2. Partition coefficients of SARS-CoV peptides



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  		FIG. 3. SARSWW-I partitions into membranes of LUV. The graph shows changes in the tryptophan fluorescence of SARSWW-I as a function of increasing concentrations of LUV composed of POPC ({blacksquare}), POPC and PI (9:1) (•), or POPC, PI, and CHOL (6.5:1:2.5) ({circ}). LUV were titrated at concentrations of 100, 250, 500, 750, and 1,000 µM lipid with 2.5 µM peptide. Tryptophan fluorescence values at each lipid titration (F) were normalized to tryptophan fluorescence values in 5 mM HEPES buffer alone (Fo).

SARS-CoV fusion peptide induces fusion of lipid vesicles. By analogy to studies examining the ability of other synthetic viral fusion peptides to induce the fusion of lipid vesicles, the SARS-CoV putative fusion peptide would be expected to have a similar capacity. The induction of lipid membrane mixing by the peptides as a measure of fusogenic potential was measured by use of a FRET technique for dye-labeled lipids, which monitors the increase in NBD fluorescence following the fusion of labeled vesicles with unlabeled vesicles. Therefore, increases in NBD fluorescence are indicative of mixing of membrane lipids. Figure 4 illustrates the results of a time course experiment in which NBD fluorescence was measured pre- and postaddition of the SARS-CoV putative fusion peptides to LUV composed of POPC and PI (9:1). Only after the addition of SARSWW-I, but not SARSWW-II, was there a rapid exponential increase in NBD fluorescence, followed by a plateau at 300 s post-peptide addition (Fig. 4, line b). Although SARSWW-II induced a marginal increase in NBD fluorescence over that of DMSO-treated vesicles (Fig. 4, line c versus line a), the extent and rate of fusion were not comparable to those with SARSWW-I. Likewise, the addition of the divalent cation Ca2+ did not affect the capacity of either peptide tested to induce more or less NBD fluorescence (data not shown). Vesicle aggregation as a result of peptide-mediated fusion of lipid vesicles has been reported for several viral fusion peptides (59, 64, 66). Similar to these reports, we observed an aggregation of LUV after the addition of the SARSWW-I peptide at P:L molar ratios of 1:50 and higher; however, no vesicle aggregation was apparent after the addition of the SARSWW-II peptide at all P:L molar ratios tested (data not shown).



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  		FIG. 4. SARSWW-I induces fusion of LUV. NBD fluorescence was detected by the FRET assay as a function of time. A DMSO control (a), SARSWW-I (b), SARSWW-II (c), or SARSWW-I-SCR (d) (P:L ratio of 1:10) was added to a 500 µM suspension of lipid composed of 25 µM POPC-PI-NBD-POPE-Rho-POPE LUV (8.8:1:0.1:0.1) and 475 µM POPC-PI LUV (9:1). The arrow indicates the time of addition of the peptides.

The experimental results in Table 3 summarize the extents of fusion observed for both SARSWW-I and SARSWW-II by use of the above-described FRET technique. The addition of SARSWW-I to LUV at P:L molar ratios of 1:50, 1:25, and 1:10 resulted in 38, 45, and 59% of the vesicles undergoing one fusion event. In contrast, the addition of SARSWW-II at equal P:L molar ratios resulted in only 11, 14, and 18% of the vesicles undergoing one fusion event. These data indicate that SARSWW-I has the capacity to induce effective mixing of lipid membranes, a function shared by other synthetic viral fusion peptides.


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  		TABLE 3. SARSWW-mediated fusion of LUV

SARS-CoV fusion peptide induces leakage of lipid vesicles. To test the potential of the SARS-CoV fusion peptides to perturb membrane integrity, we used a high-throughput leakage assay. The Tb3+/DPA microwell assay is a sensitive visual screening assay developed to rapidly identify peptides capable of permeabilizing lipid membranes (67). The detection ability of the assay is based on the strong fluorescence emission of the lanthanide metal Tb3+ when it interacts with the aromatic chelator DPA. In the experimental assay, LUV containing encapsulated Tb3+ were added to a solution of 50 µM DPA in buffer. If the membrane integrity is compromised, Tb3+/DPA fluorescence can be visually determined by the detection of bright green fluorescence upon irradiation with UV light. An example plate is shown in Fig. 5A in which both SARSWW-I and SARSWW-II were tested for the potential to permeabilize LUV composed of POPC and PI (9:1) at various P:L molar ratios. The SARSWW-I peptide permeabilized vesicles at P:L ratios as low as 1:250, with extensive leakage detected at P:L ratios of 1:50 and 1:25 (Fig. 5A, row 1). The extent of leakage induced by SARSWW-I at a P:L ratio of 1:25 was comparable to the observed leakage of Triton X-100-solubilized wells (Fig. 5A, row 1 versus row 4). In contrast, leakage induced by the SARSWW-II peptide was minimal compared to that induced by the SARSWW-I- and Triton X-100-treated groups and was only detectable at P:L ratios of 1:25 and 1:50 (Fig. 5A, row 2).



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  		FIG. 5. SARSWW-1 induces leakage of LUV contents. (A) Tb3+/DPA microwell assay. Each well contained 250 µl of 50 µM DPA and 500 µM Tb3+-encapsulated LUV composed of POPC and PI (9:1). The wells were treated with SARSWW-I (1), SARSWW-II (2), SARSWW-I-SCR (3) (P:L molar ratio of 1:500, 1:250, 1:100, 1:50, or 1:25), 20 µl of Triton X-100 (4), or 20 µl of DMSO (5) or were left untreated (6). The plates were incubated for 2 h at room temperature, and membrane permeabilization was determined by visual detection of Tb3+/DPA fluorescence. (B) Time trace analysis of Tb3+ fluorescence after theaddition of a DMSO control (a) or SARSWW-I at a P:L molar ratio of 1:100 (b), 1:50 (c), or 1:25 (d). The arrow indicates the time of addition of the peptides. (C) Extent of leakage from Tb3+-encapsulated LUV. SARSWW-I (•), SARSWW-II ({diamondsuit}), or SARSWW-I-SCR ({circ}) was added to LUV composed of POPC and PI (9:1) at the indicated P:L molar ratios. The samples were incubated at room temperature for 2 h before Tb3+ fluorescence was measured. The percent leakage was determined by using equation 3.

To further characterize the extent of leakage observed in the Tb3+/DPA microwell assay, we measured Tb3+ fluorescence fluorometrically as described in Materials and Methods. A time trace experiment was initially performed to observe the rate of SARSWW-I-induced leakage of Tb3+ encapsulated within LUV at P:L ratios of 1:100, 1:50, and 1:25 (Fig. 5B). Compared to the rate of NBD fluorescence observed in the fusion assay, SARSWW-I induced a slower exponential increase in Tb3+ fluorescence (Fig. 5B). Likewise, the lack of a plateau in Tb3+ fluorescence at 30 min post-peptide addition suggested that leakage was not complete. Therefore, for determination of the full extent of peptide-induced leakage of Tb3+ from LUV, the SARS-CoV fusion peptides were incubated at various P:L molar ratios, and after 2 h of incubation at room temperature, the extent of Tb3+ leakage from lipid vesicles was measured fluorometrically. As with the Tb3+/DPA microwell assay, the SARSWW-I peptide induced Tb3+ leakage from LUV to a greater degree than did SARSWW-II at all P:L molar ratios tested. For example, SARSWW-I induced 20%, 46%, and 65% leakage of vesicle contents at P:L ratios of 1:100, 1:50, and 1:25, respectively. In contrast, the SARSWW-II peptide induced only 4%, 10%, and 15% leakage at the same P:L molar ratios. Taken together, the data presented above indicate that the SARSWW-I peptide efficiently disrupts membrane integrity, as evident by its ability to induce leakage in the Tb3+/DPA assay.

A scrambled SARS-CoV fusion peptide is inactive. The data presented thus far demonstrate that of the two putative fusion peptides tested, only SARSWW-I is active in all three assays. This peptide not only fulfills the compositional requirements of a viral fusion peptide, but it demonstrates functional characteristics that have been identified for isolated fusion peptides of other class I viral fusion proteins (21, 26, 30). Therefore, in order to determine if the capacity of SARSWW-I to partition into lipid membranes and to induce both fusion and permeabilization of lipid vesicles is a property of the specific peptide sequence, we synthesized and tested a scrambled peptide in the aforementioned assays. The resulting scrambled peptide, SARSWW-I-SCR, was identical in polarity, hydrophobicity, and aa composition to SARSWW-I; however, the specific order of aa was arbitrarily rearranged and the canonical tripeptide was intentionally altered (Table 1). The ability of the SARSWW-I-SCR peptide to interact with membranes of LUV composed of POPC, PI, and/or CHOL was first assessed. Upon the addition of 1,000 µM lipid, no enhancement or shift in the maximum was detected, indicating minimal to no partitioning of the peptide into the membranes of the vesicles tested (Fig. 2C and Table 2). In addition, when tested for the ability to induce vesicle fusion, the SARSWW-I-SCR peptide, at a P:L molar ratio of 1:10, showed no significant increase in NBD fluorescence compared to DMSO-treated control samples (Fig. 4, line d versus line a). Again, when tested in the Tb3+/DPA assay, the SARSWW-I-SCR peptide did not induce Tb3+ leakage (Fig. 5A, row 3, and C). The inability of the SARSWW-I-SCR peptide to partition into lipid membranes and to induce both fusion and permeabilization of lipid vesicles suggests that the aa sequence order is vital for the activity of the SARSWW-I peptide.

CD analysis of the SARS-CoV fusion peptide. To examine the potential for the formation of secondary structures upon interactions with lipid membranes, we examined the SARSWW-I peptide by CD spectroscopy. Figure 6 shows representative far-UV CD spectra of both the SARSWW-I and SARSWW-I-SCR peptides in buffer and with LUV. An analysis of SARSWW-I in 10 mM PO4 buffer, pH 7.0, showed a ß-sheet spectrum with a prominent minimum at 218 nm and a tryptophan minimum at 228 nm (93). Likewise, in the presence of 1 mM LUV composed of POPC and PI (9:1), the SARSWW-I peptide again showed a ß-sheet spectrum, although the minimum at 218 nm was shifted to a slightly higher wavelength (Fig. 6A). The lack of a more defined minimum at 218 nm was most likely a result of the scattering effect attributed to the visible vesicle fusion and aggregation at the P:L molar ratios tested. To ensure that the SARSWW-I peptide assumed a well-defined ß-sheet structure upon interaction with lipid vesicles at low peptide concentrations, at which vesicle aggregation was not apparent, we analyzed the 5 µM peptide in buffer and with LUV. A 32-s response time and a scan speed of 5 nm/min were used to obtain a reliable UV CD spectrum. Under these conditions, the SARSWW-I peptide showed a well-defined minimum at 218 nm in the presence of lipid, which is indicative of a transition to a ß-sheet structure in membranes (Fig. 6A, inset). The SARSWW-I-SCR peptide was also examined by CD spectroscopy for the formation of secondary structures in buffer and with LUV (Fig. 6B). This peptide did not partition into lipid membranes or induce membrane fusion or leakage; therefore, we examined whether scrambling the peptide sequence interfered with the formation of the secondary structure required for its function. No defined {alpha}-helical or ß-sheet structure was apparent, as evident by the random coil spectra observed in buffer and upon the addition of LUV (Fig. 6B). These data suggest that the SARS-CoV fusion peptide has a sequence-specific propensity to adopt a ß-sheet structure upon interaction with lipid membranes. In addition, it appears that the inability of the SARSWW-I-SCR peptide to functionally mimic SARSWW-I could be due, in part, to the loss of a defined secondary structure.



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  		FIG. 6. SARSWW-1 adopts a ß-sheet conformation. The graphs show CD spectra (mean residue ellipticities [{Theta}]) of the SARS-CoV fusion peptides (50 µM) SARSWW-I (A) and SARSWW-I-SCR (B) in 10 mM PO4 buffer, pH 7.0, alone (•) or with 1 mM LUV composed of POPC and PI (9:1) ({circ}) at room temperature. Inset, CD spectra of SARSWW-I (5 µM) in 10 mM PO4 buffer, pH 7.0, alone (•) or with 1 mM LUV composed of POPC and PI (9:1) ({circ}) at room temperature. Settings were adjusted to a 32-s response time and a scan speed of 5 nm/min.


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DISCUSSION
 
Dissecting the mechanisms by which the SARS-CoV S protein mediates fusion between the virion envelope and the cellular membrane could significantly contribute to our understanding of SARS-CoV pathobiology and to the design of antiviral drugs and vaccines. Recent studies have determined that the SARS-CoV S fusion protein is a prototypical class I viral fusion protein in that it contains two 4,3-hydrophobic HR regions responsible for the formation of a six-helix bundle, similar to the fusion proteins of EboV (53, 86, 87) and the lentiviruses HIV and simian immunodeficiency virus (10, 13, 53). The formation of this hairpin structure is believed to drive membrane fusion by mediating the juxtaposition of both the viral and cellular membranes. The formation of the six-helix bundle, however, is preceded by the insertion of a hydrophobic fusion peptide located within the N-terminal region of the fusion protein (36). Insertion of the fusion peptide into the target cell membrane facilitates both target cell membrane disruption and the subsequent formation of the six-helix bundle. Although studies by Luo and Weiss have identified putative fusion peptides of MHV (50, 51), no fusion peptide has been identified in the N-terminal region of the SARS-CoV S2 subunit.

Using the characteristics of known viral fusion peptides, including their hydrophobicity and aa composition and the presence of a canonical fusion tripeptide, we identified two putative fusion peptides with high interfacial hydrophobicities in the N-terminal region of the SARS-CoV S2 subunit (Fig. 1 and Table 1). SARSWW-I is located at the extreme N-terminal end of S2, 9 aa downstream of a minimum furin cleavage site. In viral fusion proteins that undergo proteolytic cleavage (e.g., HIV TM and influenza virus HA), fusion peptides are situated at the N-terminal region. Although it has not been conclusively determined whether the SARS-CoV S protein is proteolytically cleaved during maturation, a minimum furin cleavage site is present within the S protein (758R-N-T-R761), and recent studies reported that the SARS-CoV S protein is proteolytically cleaved in vitro (2, 96). Studies examining the conserved furin cleavage sites in other coronaviruses have shown conflicting results regarding whether cleavage is necessary for infectivity and/or cell-cell fusion (reviewed in reference 18). Most recently, de Haan et al. demonstrated that the S protein of MHV strain A59 is proteolytically cleaved; however, the requirements for cleavage during virion-cell and cell-cell fusion differ (18).

The second possible SARS-CoV fusion peptide, SARSWW-II, is similar to the fusion peptides of EboV GP2 (27, 70) and ASV TM (27) and the internal fusion peptides of class II viral fusion proteins (31), as it is located distal to the furin cleavage site but still within the N-terminal region of S2. Despite their different locations within the S2 subunit, both SARSWW-I and SARSWW-II contain several features which are conserved among all known viral fusion peptides. For example, both demonstrated a high interfacial hydrophobicity when analyzed with the WWIH scale (Fig. 1C and Table 1), suggesting an inherent propensity to partition into lipid membranes (94). Similar regions of high interfacial hydrophobicity are apparent in the fusion proteins of HIV and EboV (Fig. 1A and B). Moreover, both SARSWW-I and SARSWW-II are rich in alanine, glycine, and/or phenylalanine residues and contain a canonical fusion tripeptide and a proline residue (Table 1), making both peptides potential fusion peptide candidates. Classifying SARSWW-I and SARSWW-II as internal or N-terminal putative fusion peptides will depend on deciphering whether and where the SARS-CoV S protein is proteolytically cleaved. It is important that while cleavage of the S protein of CoV appears to enhance fusion (35, 81), cleavage is not absolutely required for fusion (4, 5, 39, 75, 76).

Although the transition of the fusion protein core to the six-helix bundle conformation has been shown to mediate fusion by repositioning the cell and viral lipid membranes, the fusion peptide has been implicated as the mediator of the fusion process through its ability to induce the fusion and permeabilization of lipid membranes. We employed biophysical assays to identify which of the two possible SARS-CoV fusion peptides could partition into lipid membranes as well as induce fusion and permeabilization of lipid vesicles. These criteria were chosen based on the experimental approaches used to identify the fusion peptides of several other viral fusion proteins. Only SARSWW-I strongly partitioned into the lipid membranes of all LUV tested (Table 2). While SARSWW-II appeared to weakly bind to LUV composed of POPC and PI (9:1) (Fig. 2B), the calculated partition coefficient was significantly lower than that of SARSWW-I (Table 2). In a FRET fusion assay, we observed a rapid exponential increase in NBD fluorescence following the addition of SARSWW-I, corresponding to 58% of the vesicles undergoing one fusion event at a P:L molar ratio of 1:10. In contrast, SARSWW-II caused a marginal increase in NBD fluorescence, indicative of fewer vesicles (~18%) undergoing membrane fusion events (Fig. 3 and Table 3). Even at a P:L ratio of 1:50, 38% of the vesicles underwent one fusion event in the presence of SARSWW-I, whereas only 11% of vesicles underwent one fusion event in the presence of SARSWW-II. The differences in fusion may correlate with the differing capacities of both peptides to partition into lipid membranes. While other studies have shown a correlation between a cation-mediated preaggregation of vesicles and peptide fusion activity (59, 64, 79), we observed no enhancement of NBD fluorescence for either SARSWW-I or SARSWW-II in the presence of 5 mM Ca2+. Therefore, the peptide-mediated fusion observed was not dependent on a cation-mediated preaggregation of vesicles (data not shown).

When tested in the Tb3+/DPA leakage assay, SARSWW-I induced measurable lipid vesicle permeabilization at all P:L ratios tested, whereas SARSWW-II induced minimal to no observable leakage (Fig. 5). Although both SARSWW-I and SARSWW-II showed similar propensities to interact with lipids based on their high interfacial hydrophobicities (Table 1), not all small hydrophobic peptides, even those with high WWIH scores, are capable of membrane disruption (94). Furthermore, the scrambled peptide of SARSWW-I did not interact with membranes (Fig. 2C and Table 2) and was unable to induce fusion (Fig. 4) or leakage (Fig. 5) of lipid vesicles, indicating that we measured a sequence-specific membrane disruption mediated by SARSWW-I. The SARSWW-I peptide used throughout the aforementioned studies contained an aa substitution at residue 2 (Table 1), where the aromatic aa tyrosine was replaced with tryptophan. The rationale for this conservative aromatic aa replacement was that the intrinsic fluorescence of tryptophan is stronger and thus easier to quantitate spectrofluorometrically than that of tyrosine. To rule out the possibility that the capacity of SARSWW-I to induce both fusion and leakage of lipid vesicles was a consequence of the aromatic aa substitution, we tested an unmodified peptide in both the FRET fusion and Tb3+/DPA leakage assays. As expected, the unmodified peptide exhibited activity identical to that of SARSWW-I in both assays (data not shown).

We also used CD spectroscopy to determine the propensity of the SARSWW-I peptide to adopt a defined secondary structure ({alpha}-helix or ß-sheet) upon interaction with lipid membranes. Studies examining the secondary structures of viral fusion peptides have been conflicting. While numerous studies suggest that a predominantly {alpha}-helical structure is the single fusion-active conformation adopted by viral fusion peptides (reviewed in reference 21), other studies argue that a ß conformation is the active fusion state (1, 17, 65, 72, 80). CD analysis of the SARSWW-I peptide showed a propensity for the formation of a ß-sheet structure in buffer and upon the addition of LUV (Fig. 6A). The formation of a ß-sheet structure was independent of the presence of a cation, which has been shown to be necessary for the fusion peptides of EboV and HIV to assume a defined ß-sheet secondary structure as well as to induce the aggregation and fusion of lipid vesicles (59, 80). The ability of the SARSWW-I peptide to adopt a secondary structure appears to be necessary for the peptide to interact with lipid membranes. Scrambling the peptide resulted in a loss of the ß-sheet conformation (Fig. 6B) and an inability to bind to and interact with LUV. The secondary structure is a strongly driven thermodynamic consequence of membrane partitioning for hydrophobic peptides (90) which can be influenced by the peptide charge, aa organization, peptide-membrane surface density, lipid composition, and monolayer lateral pressure (79). Therefore, assumptions regarding the secondary structures of synthetic peptides are dependent on experimental conditions and are far from reflective of the true propensity of a viral fusion peptide to adopt a defined secondary structure in the context of the full glycoprotein. Nonetheless, CD analysis is a useful tool to study the behavior of these peptides in the context of model lipid membranes. The data presented herein for the SARS-CoV putative fusion peptide are consistent with the idea that the biologically relevant activity of viral fusion peptides is based on the propensity to adopt a defined secondary structure upon interaction with lipid membranes.

The biophysical studies presented above provide evidence that SARSWW-I behaves similarly to the synthetic viral fusion peptides of HIV, EboV, and influenza virus (14, 17, 21, 46, 58, 59, 62, 63, 65, 66, 70), in that the peptide has the capacity to partition into lipid membranes, adopt a well-defined secondary structure, and induce both fusion and permeabilization of lipid vesicles. The nominal P:L molar ratio was ~1:25 for both fusion and leakage assays; however, peptide binding assays demonstrated that at this molar ratio, ~40% of the peptide was actually bound to the lipid membrane under our experimental conditions. This suggests that less peptide is required to induce the observed levels of fusion and leakage. Observations that synthetic peptides corresponding to the fusion peptide domains of class I viral fusion proteins can induce measurable levels of fusion and leakage, separate from the context of the entire glycoprotein, provide support for models of viral fusion in which the fusion peptide and other domains actively facilitate lipid mixing (3, 73). The transition to the six-helix-bundle state may not only facilitate membrane juxtaposition but also function to align the fusion peptide with the aromatic domain and the transmembrane domain. The alignment of these three domains may then form a continuous track of hydrophobic, membrane-interacting surfaces that provide a low-energy (low-barrier) path for lipid flow and subsequent membrane fusion during the transition to or formation of the six-helix-bundle configuration (73).

Lastly, since the SARSWW-II peptide was capable of inducing one-third the amount of fusion and permeabilization of lipid vesicles that the SARSWW-I peptide induced, this less active sequence may work in conjunction with the SARSWW-I peptide or may constitute a second fusion peptide. Although its location within the S2 subunit is consistent with the position of the known internal fusion peptides of ASV and EboV, its inability to partition into lipid membranes (Fig. 2 and Table 2) and to adopt a well-defined secondary structure (data not shown) argues against the latter possibility. Although further mutagenesis studies need to be conducted to further verify the role of the SARSWW-I sequence in vitro, based on the biophysical assays presented above, we propose that residues 770 to 788 constitute the putative fusion peptide of the SARS-CoV S2 subunit. A working schematic of the SARS-CoV class I viral fusion protein, including the putative fusion peptide, the two well-characterized {alpha}-helices (HR1 and HR2), the transmembrane anchor, and other conserved structural domains present among many other class I viral fusion proteins, such as the aromatic domain and stem-loop region, is depicted in Fig. 7.



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  		FIG. 7. Schematic of SARS-CoV S protein. The putative fusion peptide (red) is depicted at aa residues 770 to 788, 9 aa downstream of the minimum furin cleavage site (758R-N-T-R761). The two {alpha}-helical regions, N-helix (HR1, orange) and C-helix (HR2, yellow), are depicted at aa residues 902 to 1011 and 1131 to 1185, respectively. This is consistent with the HR predictions of Tripet et al. (84), Liu et al. (49), and Xu et al. (98). An interhelical domain of approximately 120 aa is depicted between the N- and C-helices. This region is extremely similar to the interhelical region of retrovirus TM proteins and EboV GP2 and has therefore been modeled as a similar disulfide-stabilized apex. Just prior to the transmembrane anchor (indigo) of S2, there is a region enriched in aromatic aa. This region, termed the aromatic domain (green), is highly conserved throughout the Coronaviridae and lies in an identical location to that of the aromatic domains of HIV and EboV. The S1 subunit, which includes the receptor-binding domain, is depicted schematically as a large ellipse, corresponding to the characteristic large globular head groups seen in electron micrographs of SARS-CoV.


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ADDENDUM IN PROOF
 
In a very recent paper, Guillén et al. (J. Guillén, A. J. Pérez-Berná, M. R. Moreno, and J. Villalaín, J. Virol. 79:1743-1752, 2005) describe experiments with overlapping peptides from the SARS-CoV S protein in which they show that peptides corresponding to the pre-TM aromatic domain and the region containing the WW-II segment cause moderate leakage from lipid vesicles at high peptide concentration. Based on this leakage data only, these authors suggest that the WW-II region may contain the S protein fusion peptide. We have observed similar levels of membrane disruption by these two sequences previously (73) and in this work and have also suggested a possible role for the aromatic domain and WW-II region in SARS-CoV S-protein-mediated membrane fusion. However, using direct measurements of binding, fusion, and membrane disruption, we have also shown here that the N-terminal WW-I region of the S2 protein has much more potent fusogenic and membrane disrupting activity than the other two sequences. We suggest that the WW-I sequence may be the primary fusion peptide, perhaps acting together with the WW-II region and the aromatic domain (73). Given the high interfacial hydrophobicity of the WW-I sequence, it is not clear why Guillén et al. observed no activity in their leakage experiments with corresponding peptides. However, none of the peptides they tested were identical in sequence to the WW-1 peptide used in the present study. The most similar peptides (105 and 106 in their series) were shifted 3 or 4 amino acids toward either the N or the C terminus, respectively (J. Villalaín, personal communication), suggesting that sequence details can determine membrane fusion activity of peptides. Our observation that a scrambled WW-I peptide has no activity supports this hypothesis.


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ACKNOWLEDGMENTS
 
This work was supported by the National Institutes of Health (AI054626, AI054238, RR018229, and CA08921 [R.F.G.] and GM60000 [W.C.W.]). Bruno Sainz is a recipient of a National Research Service Award from the National Institutes of Health (AIO543818).


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FOOTNOTES
 
* Corresponding author. Mailing address: Department of Biochemistry, Tulane University Health Sciences Center, 1430 Tulane Avenue, SL-43, New Orleans, LA 70112. Phone: (504) 988-7076. Fax: (504) 988-2739. E-mail: wwimley{at}tulane.edu. Back


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Journal of Virology, June 2005, p. 7195-7206, Vol. 79, No. 11
0022-538X/05/$08.00+0     doi:10.1128/JVI.79.11.7195-7206.2005
Copyright © 2005, American Society for Microbiology. All Rights Reserved.



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