Search tips
Search criteria 


Logo of jbcThe Journal of Biological Chemistry
J Biol Chem. 2016 March 18; 291(12): 6559–6568.
Published online 2016 January 27. doi:  10.1074/jbc.M115.712760
PMCID: PMC4813582

Rab8b Regulates Transport of West Nile Virus Particles from Recycling Endosomes*


West Nile virus (WNV) particles assemble at and bud into the endoplasmic reticulum (ER) and are secreted from infected cells through the secretory pathway. However, the host factor related to these steps is not fully understood. Rab proteins, belonging to the Ras superfamily, play essential roles in regulating many aspects of vesicular trafficking. In this study, we sought to determine which Rab proteins are involved in intracellular trafficking of nascent WNV particles. RNAi analysis revealed that Rab8b plays a role in WNV particle release. We found that Rab8 and WNV antigen were colocalized in WNV-infected human neuroblastoma cells, and that WNV infection enhanced Rab8 expression in the cells. In addition, the amount of WNV particles in the supernatant of Rab8b-deficient cells was significantly decreased compared with that of wild-type cells. We also demonstrated that WNV particles accumulated in the recycling endosomes in WNV-infected cells. In summary, these results suggest that Rab8b is involved in trafficking of WNV particles from recycling endosomes to the plasma membrane.

Keywords: flavivirus, infection, Rab, transport, vesicles


Viruses have many strategies to exploit the host cellular machinery and evade recognition of host defenses for their replication. They utilize host machinery to promote their entry, replication, and release.

West Nile virus (WNV)2 is an enveloped, single-stranded, positive-sense RNA virus belonging to the Flaviviridae family. In nature, WNV circulates between mosquitoes and birds, and humans and other mammals are incidental hosts (1). In humans, WNV causes a febrile illness, with a subset of patients progressing to severe neurological disease (2). WNV enters host cells through unknown cell surface receptor-mediated endocytosis and is transported to endosomes (3), followed by endosomal membrane fusion and delivery of the infectious RNA genome into the cytoplasm (4, 5). The viral genome is translated as a single polyprotein that is cleaved by host and viral proteases into three structural (C, prM, and E) and seven nonstructural (NS1, NS2A, NS2B, NS3, NS4A, NS4B, and NS5) proteins (4, 5). The structural proteins are components of viral particles and the nonstructural proteins form the replication complex that is essential for replication of viral RNA (6, 7). The viral particles assemble and bud into the ER to form immature particles (8). Viral particle maturation takes place in the Golgi and acidic compartments during transport through the host secretory pathway, and mature particles are released by exocytosis (9, 10). The release of WNV particles through the secretory pathway is well documented; however, little is known about detailed trafficking pathways and related host factors used to deliver the newly formed viral particles to the plasma membrane.

Members of the Rab family of small GTPases regulate intracellular membrane traffic. More than 60 known Rab proteins are localized to each different intracellular organelle on both the endocytic and exocytic pathways of eukaryotic cells (11). Rab proteins recruit and interact with effector proteins, either directly or indirectly, to target vesicles to the appropriate sites on acceptor membranes (12). Several Rab proteins are involved in the life cycles of various enveloped viruses, including WNV (13, 14). WNV replication is hampered in cells transfected with siRNA of Rab5, suggesting that a Rab5-dependent endocytosis pathway is important for WNV entry (14). Thus, many Rab proteins seem to be involved in WNV infection, but their role in secretion of WNV particles is not well elucidated.

Advances in genomics and RNAi methods have led to genome-wide screening to identify the cellular genes that affect viral replication (15, 16). There are several reports of WNV virus-like particles (VLPs), which are produced by complementation of replicon RNA with WNV structural genes expressed in trans (17), for the screening of siRNA or compound libraries (18, 19). In this study, we performed siRNA-based screen silencing of Rab proteins related to vesicle transport from the ER to the plasma membrane to elucidate the mechanisms of WNV particle release. We found that Rab8b is important for WNV particle release and defective Rab8b results in accumulation of WNV particles in recycling endosomes.

Experimental Procedures

Cells and Virus

HEK-293T cells were grown in high-glucose DMEM (Sigma) supplemented with 10% heat-inactivated FBS. Vero cells were grown in minimal essential medium (MEM; Nissui, Tokyo, Japan) supplemented with 10% heat-inactivated FBS and 2 mm l-glutamine (Sigma). SH-SY5Y cells were grown in DMEM/Nutrient Mixture F-12 Ham (Sigma) supplemented with 10% heat-inactivated FBS. WT, Rab8b KO, and Rab8a+b double knock-out (DKO) mouse embryonic fibroblasts (MEFs) were grown in DMEM supplemented with 10% heat-inactivated FBS and 2 mm l-glutamine (Sigma) as described previously (20). The WNV 6-LP strain, previously established by plaque purification of the WNV NY99–6922 strain isolated from mosquitoes in 1999 (21, 22), was kindly provided by Dr. Takashima (Hokkaido University, Japan). All experiments with WNV were performed at the Biosafety Level 3 facility at Hokkaido University in accordance with institutional guidelines. The influenza A virus (IFV) strain, A/Aichi/2/1968 (H3N2) was kindly provided by Dr. A. Takada (Hokkaido University, Japan).

Antibodies and Plasmids

Rabbit anti-Japanese encephalitis virus serum was produced as described previously (23, 24). Antibodies were purchased as follows: mouse anti-Rab8, anti-GM130, and anti-Rab11 monoclonal antibodies (BD Transduction Laboratories, San Diego, CA); mouse anti-WNV E protein and anti-actin monoclonal antibodies (Merck Millipore, Billerica, MA); rabbit anti-Rab5 polyclonal antibody and anti-Rab11 monoclonal antibody (Cell Signaling Technology, Beverly, MA); mouse anti-Rab11a monoclonal antibody, and rabbit anti-Lamp1 and anti-TGN46 polyclonal antibodies (Abcam, Cambridge, MA). Plasmid pCXSN-Rab8b was constructed by subcloning PCR-amplified Rab8b from total RNA of Neuro 2a cells into pCXSN, which was created by removing the myc-tag from pCMV-myc (Clontech) and adding XhoI, SalI, and NotI recognition site (25). WNV structural protein-expressing plasmid (pCXSN-CME) was constructed as described previously (26, 27). The WNV replicon cDNA constructs, pWNIIrep-REN and pWNIIrep-GFP, were generously provided by Dr. Robert W. Doms (17). A lentiviral vector pFU-pGK puro was generously provided by Dr. Kamitani (Osaka University, Japan), and the packaging plasmids (pCAF-HIVgp and pCMV-VSV-G-RSV-Rev) were generously provided by Dr. Miyoshi (Riken, Tsukuba, Japan).

VLP Release Assay

The validated siRNAs that target 18 Rab genes were purchased from Qiagen (Valencia, CA). HEK 293T cells were transfected with each siRNA by HiPerfect Transfection Reagent (Qiagen). At 48 h, siRNA-transfected cells were transfected with WNV structural-protein-expressing plasmid (pCXSN-CME) and WNV replicon cDNA construct (pWNIIrep-REN) that encode WNV nonstructural protein genes, and Renilla luciferase gene that is expressed instead of structural proteins (17), using Lipofectamine 2000 (Life Technologies, Rockville, MD). VLPs were released in culture supernatants and were unable to produce progeny particles because of a lack of structural protein genes in the replicon. Culture supernatants were harvested at 24 h, and plasmid-transfected cells were lysed and measured for luciferase activity (transfection-associated luciferase activity) using the Dual Glo luciferase assay substrate (Promega, Madison, WI). Equal volumes of the harvested supernatants were used to infect Vero cells. VLP-infected cells were lysed and measured for luciferase activity (VLP-associated luciferase activity) at 60-h post-infection (hpi). VLP release was calculated as ratio of luciferase activity of lysates of Vero cells/luciferase activity of 293T cells transfected with plasmids. The data were expressed as mean ± S.D. The Steel test was used for comparison. A value of p < 0.05 was considered statistically significant.


For immunoblotting, cells were lysed in SDS-PAGE sample buffer supplemented with Complete Protease Inhibitor Mixture (Roche Diagnostics, Indianapolis, IN). Cell lysates were fractionated by SDS-PAGE, and separated proteins were transferred to a PVDF filter (Merck Millipore). The filter was incubated with each antibody, and the immune complexes were detected with HRP-conjugated secondary antibodies (BIOSOURCE International, Camarillo, CA) and Immobilon Western HRP-Substrate (Merck Millipore). The chemiluminescence signals were visualized with the VersaDoc 5000MP (Bio-Rad), and obtained images were analyzed using Quantity One software (Bio-Rad).


WNV-infected and mock-infected cells were fixed with 4% paraformaldehyde (PFA) for 10 min, before washing with PBS. The cells were permeabilized in 0.1% saponin or 0.1% Triton X-100 for 5 min, blocked with 1% BSA-PBS, and stained with indicated antibodies in 1% BSA-PBS overnight at 4 °C. The immune complexes were visualized by incubating with Alexa-Fluor-488-, Alexa-Fluor-594- or Alexa-Fluor-647-conjugated secondary antibodies (Life Technologies). The cells were observed using a Zeiss 780 LSM confocal microscope (Carl Zeiss, Jena, Germany). For analysis of fluorescence intensity of viral antigen and number of GFP-expressing cells, the cells were observed using an IN Cell Analyzer 2000 (GE Healthcare, Uppsala, Sweden), and obtained images were analyzed using IN Cell developer Toolbox software (GE Healthcare). For continuous transferrin internalization, WNV-infected cells were washed with Opit-MEM (Life Technologies) and incubated in Opti-MEM with 25 μg/ml Alexa-Fluor-488-conjugated transferrin (Life Technologies) for 30 min at 37 °C. Cells were washed twice with cold PBS and fixed with 4% PFA for 10 min. The signal of transferrin was observed using a Zeiss 780 LSM confocal microscope. Colocalization was analyzed using ZEN 2011 software (Carl Zeiss), and relative colocalization ratios were used as an indicator of colocalization as previously described (28). The ratio of the pixel number of colocalized viral proteins and each organelle marker to the whole pixel number was quantified by the confocal software ZEN 2011 and was represented by a bar graph. For quantification of colocalization, five cells from at least two independent experiments were used in each condition. The data were expressed as mean ± S.D. Student's t test was used for comparison of obtained data.

Plaque Assay

Diluted culture supernatants from infected cells were inoculated into monolayers of Vero cells. After 1 h incubation at 37 °C with rocking, the inocula were removed, and overlay medium (MEM containing 5% FBS and 1.25% methyl cellulose) was added and incubated for 4 days. Plaques were visualized with a 1% crystal violet solution in 70% ethanol.


For quantification of viral particle release, the culture supernatants were collected at 48 hpi and ultracentrifuged at 50,000 × g (SW28 rotor, Beckman Coulter, Brea, CA) at 20 °C for 2 h. The pellets were dissolved by PBS and analyzed by immunoblotting after addition of SDS-PAGE sample buffer.

Influenza Virus Inoculation Experiment

WT and Rab8b KO MEFs were infected with IFV at 1 plaque-forming unit (Pfu)/cell and were cultured for 48 h. The supernatants of IFV-infected MEFs were collected and incubated with 0.0005% acetylated trypsin (Sigma) at 37 °C for 30 min. The incubated supernatants were transferred to MDCK cells. After 1-h incubation at 37 °C with rocking, the inocula were removed, and MEM containing 0.8% Bacto agar and 0.0005% acetylated trypsin was added and incubated for 2 days. Plaques were visualized with a 0.1% crystal violet solution in formalin.

Rab11a and 11b Knockdown (KD)

The fragment was amplified by PCR, and subcloned into the pFU6-pGK puro vector, and the resulting plasmid was named pFU6-pGK puro shRab11a. 293T cells were transfected with pFU6-pGK puro shRab11a and the packaging plasmids using Polyethylenimine Max (Polysciences, Warrington, PA). After 48 h, psuedotyped lentivirus bearing shRNA of Rab11a gene was harvested from the supernatant. WT and Rab8b KO MEFs were infected with the pseudotyped lentivirus and selected with puromycin for 1 week, and the resulting cells were named Rab11a KD WT MEFs and Rab11a KD Rab8b KO MEFs. For KD of Rab11b, the validated siRNA that targeted Rab11b gene was purchased from Qiagen. WT, Rab8b KO, Rab11a KD WT and Rab11a KD Rab8b KO MEFs were transfected with siRNA by Lipofectamine RNAi MAX (Life Technologies). At 24 h, siRNA-transfected cells were infected with WNV (1 Pfu/cell). Culture supernatants were harvested at 24 and 48 h and viral titer was measured by plaque assay.

Electron Microscopy

For ultrathin sections, WT and Rab8b KO MEFs infected with WNV at 1 Pfu/cell were cultured for 48 h and were scraped off the plate, pelleted by centrifugation at 500 × g at 3 min, and fixed for 20 min with 2.5% glutaraldehyde in 0.1 m cacodylate buffer (pH 7.4). Small pieces of the fixed pellet were washed with cacodylate buffer, post-fixed with 2% osmium tetroxide in the cacodylate buffer for 1 h at 4 °C, dehydrated with a graded series of acetone, embedded in Epon 812 Resin mixture (TAAB Laboratories Equipment, Berks, UK), and polymerized at 60 °C for 2 days. Ultrathin sections were stained with uranyl acetate and lead citrate and examined with a Hitachi H-7650 electron microscope (Tokyo, Japan).


Rab8b Involved in WNV Particle Release

We performed siRNA-based screening for silencing 18 Rab genes that are related to the vesicle transport from the ER to the plasma membrane to identify the Rab proteins associated with the later stages of WNV infection. We conducted a Renilla-luciferase-based virus assembly and release assay (Fig. 1A) as described previously (19). The gene-silenced 293T cells were co-transfected with plasmids expressing structural proteins (C, prM, and E) and a subgenomic replicon that expressed the WNV nonstructural proteins and Renilla luciferase, resulted in the production of infectious VLPs in the culture fluid. Culture fluid was harvested at 24-h post-transfection and cells were lysed and subjected to measurement of luciferase activity. To quantify the VLPs in the transfected culture fluid, Vero cells were inoculated with the harvested culture fluid, and then the luciferase activity of the Vero cells was measured at 60 hpi. Viral particle release was represented as ratio of luciferase activity of lysates of Vero cells/luciferase activity of 293T cells transfected with plasmids and replicon (Fig. 1A). The siRNA screen revealed that KD of Rab8b significantly decreased VLP release efficiency and KD of Rab27a significantly increased VLP release efficiency compared with control siRNA-transfected cells (Fig. 1B).

siRNA screen for WNV particle release. A, strategy of siRNA screening. siRNAs were introduced into 293T cells, and these cells were transfected with plasmids expressing WNV structural proteins (C, prM, and E) and replicon. Vero cells were inoculated with ...

KD of Rab8b inhibited secretion of WNV VLPs, and we further analyzed the role of Rab8b in WNV-infected cells. We examined the expression levels of Rab8 in WNV-infected human neuroblastoma SH-SY5Y cells. At 48 hpi, Rab8 expression level was increased in WNV-infected cells compared with mock-infected cells (Fig. 2, A and B). We performed immunocytochemical analysis of Rab8 and the viral antigen in WNV-infected SH-SY5Y cells. Immunopositive signals of Rab8 and the viral antigen were colocalized in the cytoplasm near the plasma membrane of WNV-infected cells (Fig. 2C, Rab8, arrowheads). WNV-infected SH-SY5Y cells were also examined by immunocytochemistry using antibodies against the viral antigen and various makers of endosomes, Golgi, and other organelles. The viral antigen was colocalized with Rab11, a marker of recycling endosomes, at the perinuclear region (Fig. 2C, Rab11, arrowheads). We could not observe clear colocalization of the viral antigen and other organelle markers in SH-SH5Y cells (Rab5, Lamp1, GM130, and TGN46). Rab8 is localized to recycling endosomes and plays a role in vesicle transport to plasma membrane (11, 29). Therefore, these results suggest that Rab8 plays an important role in release of WNV particles; probably from recycling endosomes to the plasma membrane.

Rab8 expression and localization are controlled by WNV infection. A, Rab8 expression levels in WNV-infected cells. SH-SY5Y cells were mock-infected (Mock) or infected with WNV (1 Pfu/cell). Cells were harvested at 48 hpi and analyzed by immunoblotting ...

WNV Antigens Accumulate in Rab8b-deficient Cells

To investigate the role of Rab8b in transport of WNV particles, Rab8b WT, Rab8b-deficient (Rab8b KO), and Rab8a and Rab8b (Rab8a+b)-deficient (DKO) MEFs were infected with WNV. We confirmed the expression levels of Rab8 in Rab8b KO and DKO MEFs by immunoblotting using an antibody, which recognized both Rab8a and Rab8b. The signal of Rab8a was observed in Rab8b KO MEFs and no signal of Rab8 was observed in DKO MEFs (Fig. 3A). We examined the efficiency of WNV replication among these cells. The viral titers in the culture supernatants from Rab8b KO and DKO MEFs were significantly lower than those of WT MEFs (Fig. 3B). This result is consistent with the observation that release of WNV-VLPs was significantly decreased by KD of Rab8b, but not KD of Rab8a (Fig. 1B). Although the expression level of E protein in the culture supernatant from Rab8b KO MEFs was decreased compared with that from WT MEFs, the intracellular expression level of E protein in Rab8b KO MEFs was increased compared with that in WT MEFs (Fig. 3C). To examine whether re-expression of Rab8b in Rab8b KO MEFs rescued reduction of WNV replication, we complemented Rab8b KO MEFs with Rab8b. The Rab8b-complemented Rab8b KO MEFs were infected with WNV and the viral titer of the culture supernatants from the cells were examined. The signal intensity of Rab8a+b was increased in the Rab8b-transfected Rab8b KO MEFs compared that of mock-transfected Rab8b KO MEFs (Fig. 3D). The viral titers in the culture supernatants from Rab8b-transfected Rab8b KO MEFs were significantly higher compared with those from mock-transfected Rab8b KO MEFs at 48 hpi (Fig. 3E).

Viral protein is accumulated in cytoplasm in Rab8b KO MEFs. A, Rab8 expression levels in WT, Rab8 KO or DKO MEFs. WT, Rab8b KO, or DKO MEFs were analyzed by immunoblotting for Rab8 and actin. B, viral titer in culture supernatants. WT, Rab8b KO and DKO ...

We examined the intracellular localization of E protein in WNV-infected WT and Rab8b KO MEFs. Confocal microscopic analysis revealed that E protein was present in the cytoplasm in a diffuse pattern in WT MEFs (Fig. 3F). However, the localization of E protein in Rab8b KO MEFs was distinct from that in WT MEFs, and it formed speckled spots in the cytoplasm (Fig. 3F). We also analyzed the fluorescence intensity of E protein in WNV-infected WT and Rab8b KO MEFs. The intensity of viral antigen in Rab8b KO MEFs was significantly higher than that in WT MEFs (Fig. 3G). These results suggest that Rab8b deficiency was associated with impaired release of viral proteins into the extracellular space and with accumulated viral proteins in the intracellular space.

To examine whether Rab8b affected the entry step of WNV infection, WT and Rab8b KO MEFs were infected with VLPs that possessed GFP-expressing WNV replicon RNA (17, 26). VLPs are unable to produce progeny particles because of a lack of structural protein genes in the replicon (26). GFP positivity was analyzed by fluorescent microscopy and there were no significant difference of GFP positivity between WT and Rab8b KO MEFs (Fig. 3H). This result suggests that the Rab8b plays a role in post-entry steps in WNV infection.

To examine whether the reduction of viral titer in the supernatant of Rab8b-deficient cells was specific for WNV infection, the viral titers of the supernatants from IFV-infected WT and Rab8b KO MEFs were examined. IFV buds at the plasma membrane (30). Unlike WNV infection, there was no significant difference in the viral titers of the supernatants form WT and Rab8b KO MEFs (Fig. 3I).

WNV Antigens Accumulate in Recycling Endosomes in Rab8b-deficient Cells

In order to identify the organelle with accumulated viral protein, we analyzed the localization of viral protein and organelle markers in WT or Rab8b KO MEFs. The viral protein was partially colocalized with Rab11 and Rab8 in WT MEFs (Fig. 4A, upper columns, arrowheads). In contrast, the viral protein was accumulated in a speckled pattern and was markedly colocalized with Rab11 in Rab8b KO MEFs. The viral protein was colocalized with Rab8 in Rab8b KO MEFs (Fig. 4A, lower columns, arrowheads). Rab8a was expressed in Rab8b KO MEFs, therefore, this result indicates that the viral protein was localized at the Rab8a compartment. We also observed the colocalization of the viral protein and TGN46; a marker of the trans-Golgi at low frequency in WT MEFs. We also quantified the relative colocalization ratio of the viral protein and each organelle marker in WT and Rab8b KO MEFs. Compared with WT MEFs, the relative colocalization ratio of Rab11 was significantly higher in Rab8b KO MEFs (Fig. 4B). We further examined whether viral antigen accumulates in recycling endosomes in Rab8b KO MEFs. We incubated WT and Rab8b KO MEFs with Alexa-Fluor-488-conjugated transferrin, which accumulates recycling endosomes at 30 min after entry into the cells (31). Transferrin was mainly localized in the perinuclear region in mock-infected WT MEFs, whereas transferrin in mock-infected Rab8b KO MEFs was diffusely recognized in the cytoplasm (Fig. 4C). These results suggest that intracellular localization of recycling endosomes in MEFs is affected by knock-out of Rab8b. Some viral protein was colocalized with internalized transferrin near the plasma membrane of WT MEFs (Fig. 4C, arrowheads), whereas the viral protein was highly colocalized with internalized transferrin in Rab8b KO MEFs (Fig. 4C, arrowheads). The viral antigen was colocalized with markers of recycling endosomes in both WT and Rab8b KO MEFs and the relative colocalization ratio was significantly higher in Rab8b KO MEFs. This suggests that WNV commonly passes through the Rab11-positive recycling endosomes for their infection and that Rab8b plays a role in transport of WNV particles from recycling endosomes.

Viral protein is accumulated in recycling endosomes in Rab8b KO MEFs. A, intracellular localization of viral protein. WT or Rab8b KO MEFs were infected with WNV (1 Pfu/cell). Cells were harvested at 48 hpi and stained with viral protein (red) and organelle ...

Recycling Endosomes Are Important for WNV Replication

We found that a large amount of viral protein was accumulated in recycling endosomes in Rab8b KO MEFs compared with WT MEFs (Fig. 4). To elucidate whether recycling endosomes are important for WNV transport, we examined the effect of both Rab11a and 11b depletion in WNV-inoculated WT and Rab8b KO MEFs. For depletion of Rab11a, we constructed recombinant lentivirus carrying shRNA. After lentivirus infection, Rab11 expression levels in both WT and Rab8b KO MEFs were decreased compared with control cells (Fig. 5A). Furthermore, Rab11b was depleted by siRNA specific for Rab11b in these cells. At 48 h post-transfection, expression of Rab11 was markedly decreased (Fig. 5A). WT, Rab11a+b KD WT, Rab8b KO, and Rab11a+b KD Rab8b KO MEFs were infected with WNV, and viral titers of the culture supernatants were examined. The viral titers of the supernatants from the Rab11a+b downregulated WT or Rab8b KO MEFs were significantly lower than those of the supernatants from the WT or Rab8b KO MEFs, respectively (Fig. 5B). These results suggest that intracellular trafficking through the Rab11-positive recycling endosomes is important for WNV replication.

Rab11 plays an important role for WNV replication. A, Rab11 expression levels in Rab11 KD cells. WT or Rab8b KO MEFs were infected with recombinant lentivirus carrying shRNA against mouse Rab11a expression cassette (Rab11a KD). shRNA transduced MEFs were ...

WNV Particles Accumulate in Vesicles in Rab8b-deficient Cells

Transmission electron microscopy using Epon-embedded WNV-infected WT and Rab8b KO MEFs fixed at 48 hpi revealed many vesicular membrane structures (Ve in Fig. 6, B and E), which are the viral genome replication site observed in flavivirus infection (32), and viral particles (Vi in Fig. 6, B and E) in the proximity of the nucleus in both cells (Fig. 6, A, B, D, E). The vesicles containing a few virus particles that were located distant from the viral replication site were observed in WT MEFs (Fig. 6C, white arrowheads). A large number of vesicles that contained many virus particles were observed in Rab8b KO MEFs (Fig. 6F, white arrowheads). The vesicular membrane structures were not observed in the vesicles, suggesting that these vesicles are a transport compartment and are not the replication site. These results suggest that viral particles are accumulated in the vesicles in the cytoplasm of Rab8b KO MEFs.

Ultrastructural analysis of WNV-infected WT or Rab8b KO MEFs. Ultrathin sections of WNV-infected, Epon-embedded WT or Rab8b MEFs fixed at 48 hpi are shown in (A–C) or (D–F), respectively. The red and white-boxed areas in A are shown at ...


In the present study, we showed that Rab8b was involved in regulation of the release of WNV particles from host cells. Rab8b deficiency resulted in accumulation of viral particles in the vesicles that were stained with recycling endosome markers at the cell periphery.

Rab8 participates in vesicular transport from the Golgi to the plasma membrane, particularly in transport from recycling endosomes to the plasma membrane (33, 34). The two closely related proteins, Rab8a and Rab8b, which are encoded by different genes, are included in Rab8 (20). There are two possibilities about the function of Rab8b in WNV infection. First, viral particles are wrapped by Rab8b-positive vesicles and transported from recycling endosomes to the plasma membrane. Second, Rab8b-positive vesicles carry important molecules for viral transport from recycling endosomes. WNV antigen was colocalized with Rab8 and Rab11 in WNV-infected SH-SY5Y cells, suggesting that Rab8 plays a role in transport of vesicles containing WNV particles from recycling endosomes to the plasma membrane. The viral antigen and Rab8 double-positive sites were diffusely recognized in the cytoplasm, whereas the viral antigen and Rab11 double-positive sites were mainly recognized in the perinuclear region. The difference in intracellular localization of the viral antigen and organelle marker double-positive sites suggests that the viral antigen and Rab8 double-positive compartment is probably transport vesicles, but not recycling endosomes. Deficiency of Rab8b results in accumulation of viral particles in the recycling endosomes, supporting a model in which WNV particles bud from the recycling endosomes and are transported to the plasma membrane by Rab8b.

Dengue virus and Hantavirus exploit Rab8-related regulatory mechanisms for viral particle release (35,37). These viral particles, including WNV, assemble and bud into intracellular organelles, such as the ER or Golgi apparatus, and are transported by vesicular trafficking to the plasma membrane (10, 37). In contrast, the release of IFV, which has a different release mechanism from that of WNV, was not affected by Rab8b deficiency. Rab8 may have common roles in release of viral particles that have budded in the intracellular organelles. Regarding WNV particle release, an apparent contradiction was observed in previous findings that WNV particles were released from the apical surface (38), or released from the basolateral side (27, 39). A large number of intracellular sorting mechanisms occurring in virus-infected cells have been proposed. Rab8a is associated with apical transport, while Rab8b functions in basolateral transport (20, 29, 40). In our current study, KD of Rab8a had no significant effect on the release of viral particles, whereas KD of Rab8b inhibited particle release. These results suggest that WNV particles are released from the basolateral side.

Following maturation of WNV particles in the trans-Golgi network, viral particles are sorted into secretory vesicles and are transported to the plasma membrane (9, 10). Rab11a-positive recycling endosomes sort some vesicles to define the directions during exocytosis (41, 42). Hepatitis C virus particles are localized in recycling endosomes transiently and the recycling endosomes serve as a sorting station (43). We found that WNV particles colocalized with Rab11- and transferrin-positive recycling endosomes in infected cells. This result suggests that the transit of vesicles containing viral particles to recycling endosomes is a general mechanism for the release of Flaviviridae viruses. Moreover, we noticed that Rab11- and transferrin-positive recycling endosomes were localized near the plasma membrane in Rab8b KO cells. Endogenous recycling endosomes are distributed throughout the cytoplasm, and relatively concentrated in the perinuclear region (42). However, in Rab11 interaction factors, such as Sec15 or Exo70, KD cells, Rab11-positive recycling endosomes are found near the plasma membrane (42). Our results suggest that Rab8b interacts with Rab11 during secretion of WNV particles. Although WNV replication was significantly decreased by co-depletion of Rab11a and Rab11b, down-regulation of Rab11a or Rab11b showed no significant difference in the release of viral particles. These results suggest that there is functional redundancy between Rab11a and Rab11b in the particle release pathway.

Rab27a and Rab27b are regulatory factors of secretion of exosomes (44), and Rab27a dysfunction is related to the cause of human immunodeficiency (45). Interferon-α-stimulated cells induce exosomes that can carry antiviral molecules (46). Increase of VLP release in Rab27a KD cells might be related to inhibition of release of exosomes carrying antiviral molecules. This phenomenon needs to be clarified.

In conclusion, this study provides new information about the release pathway of WNV particles that egress from cells, depending on the function of Rab8b, through recycling endosomes. As demonstrated by the influenza virus inhibitors, the understanding about the processes of viral particle release and budding will provide important information for development of therapeutic strategies. Further investigation of the detailed mechanism of transport and release of the viral particles is necessary.

Author Contributions

S. K., T. S., and H. S. conceived and designed the study. S. K., T. S., A. K., and W. P. performed the experiments and data analysis. S. K., K. Y., H. K., Y. O., and H. S. wrote the paper. T. I. and A. H. provided critical reagents.


We thank Dr. Takashima for providing the WNV NY99 6-LP strain; Dr. Doms for the WNV replicon cDNA construct pWNIIrep-GFP; Dr. Kamitani for providing the pFU-pGK puro; Dr. Miyoshi for providing the lentiviral packaging plasmids (pCAG-HIVgp and pCMV-VSV-G-RSV-Rev) and all members of the Sawa Laboratory for helpful discussion. We are especially grateful for the experimental assistance and advice of Dr. Yamasaki, Dr. Muramatsu, and Mr. Maruyama.

*This study was supported in part by JSPS KAKENHI Grant Number 15K19069 and grants from the Ministry of Education, Culture, Sports, Science and Technology of Japan (MEXT); the Ministry of Health, Labour, and Welfare of Japan; and the Japan Initiative for Global Research Network on Infectious Diseases (J-GRID); as well as by the Grant from MEXT for Joint Research Program of the Research Center for Zoonosis Control, Hokkaido University. The authors declare that they have no conflicts of interest with the contents of this article.

2The abbreviations used are:

West Nile virus
endoplasmic reticulum
hours post-infection
influenza A virus
mouse embryonic fibroblast
minimal essential medium
plaque-forming unit
virus-like particle.


1. Hayes E. B., Sejvar J. J., Zaki S. R., Lanciotti R. S., Bode A. V., and Campbell G. L. (2005) Virology, pathology, and clinical manifestations of West Nile virus disease. Emerg. Infect Dis. 11, 1174–1179 [PMC free article] [PubMed]
2. Guarner J., Shieh W. J., Hunter S., Paddock C. D., Morken T., Campbell G. L., Marfin A. A., and Zaki S. R. (2004) Clinicopathologic study and laboratory diagnosis of 23 cases with West Nile virus encephalomyelitis. Hum. Pathol. 35, 983–990 [PubMed]
3. Brinton M. A. (2002) The molecular biology of West Nile Virus: a new invader of the western hemisphere. Annu. Rev. Microbiol. 56, 371–402 [PubMed]
4. Samuel M. A., and Diamond M. S. (2006) Pathogenesis of West Nile Virus infection: a balance between virulence, innate and adaptive immunity, and viral evasion. J. Virol. 80, 9349–9360 [PMC free article] [PubMed]
5. Suthar M. S., Diamond M. S., and Gale M. (2013) West Nile virus infection and immunity. Nat. Rev. Microbiol. 11, 115–128 [PubMed]
6. Fernandez-Garcia M. D., Mazzon M., Jacobs M., and Amara A. (2009) Pathogenesis of flavivirus infections: using and abusing the host cell. Cell Host Microbe 5, 318–328 [PubMed]
7. Gillespie L. K., Hoenen A., Morgan G., and Mackenzie J. M. (2010) The endoplasmic reticulum provides the membrane platform for biogenesis of the flavivirus replication complex. J. Virol. 84, 10438–10447 [PMC free article] [PubMed]
8. Murray C. L., Jones C. T., and Rice C. M. (2008) Architects of assembly: roles of Flaviviridae non-structural proteins in virion morphogenesis. Nat. Rev. Microbiol. 6, 699–708 [PMC free article] [PubMed]
9. Mackenzie J. M., and Westaway E. G. (2001) Assembly and maturation of the flavivirus Kunjin virus appear to occur in the rough endoplasmic reticulum and along the secretory pathway, respectively. J. Virol. 75, 10787–10799 [PMC free article] [PubMed]
10. Mukhopadhyay S., Kuhn R. J., and Rossmann M. G. (2005) A structural perspective of the flavivirus life cycle. Nat. Rev. Microbiol. 3, 13–22 [PubMed]
11. Henry L., and Sheff D. R. (2008) Rab8 regulates basolateral secretory, but not recycling, traffic at the recycling endosome. Mol. Biol. Cell 19, 2059–2068 [PMC free article] [PubMed]
12. Chen S., Liang M. C., Chia J. N., Ngsee J. K., and Ting A. E. (2001) Rab8b and its interacting partner TRIP8b are involved in regulated secretion in AtT20 cells. J. Biol. Chem. 276, 13209–13216 [PubMed]
13. Guichard A., Nizet V., and Bier E. (2014) RAB11-mediated trafficking in host-pathogen interactions. Nat. Rev. Microbiol. 12, 624–634 [PMC free article] [PubMed]
14. Krishnan M. N., Sukumaran B., Pal U., Agaisse H., Murray J. L., Hodge T. W., and Fikrig E. (2007) Rab 5 is required for the cellular entry of dengue and West Nile viruses. J. Virol. 81, 4881–4885 [PMC free article] [PubMed]
15. Krishnan M. N., Ng A., Sukumaran B., Gilfoy F. D., Uchil P. D., Sultana H., Brass A. L., Adametz R., Tsui M., Qian F., Montgomery R. R., Lev S., Mason P. W., Koski R. A., Elledge S. J., Xavier R. J., Agaisse H., and Fikrig E. (2008) RNA interference screen for human genes associated with West Nile virus infection. Nature 455, 242–245 [PMC free article] [PubMed]
16. Ooi Y. S., Stiles K. M., Liu C. Y., Taylor G. M., and Kielian M. (2013) Genome-wide RNAi screen identifies novel host proteins required for alphavirus entry. PLoS Pathog. 9, e1003835. [PMC free article] [PubMed]
17. Pierson T. C., Sánchez M. D., Puffer B. A., Ahmed A. A., Geiss B. J., Valentine L. E., Altamura L. A., Diamond M. S., and Doms R. W. (2006) A rapid and quantitative assay for measuring antibody-mediated neutralization of West Nile virus infection. Virology 346, 53–65 [PubMed]
18. Puig-Basagoiti F., Deas T. S., Ren P., Tilgner M., Ferguson D. M., and Shi P. Y. (2005) High-throughput assays using a luciferase-expressing replicon, virus-like particles, and full-length virus for West Nile virus drug discovery. Antimicrob. Agents Chemother. 49, 4980–4988 [PMC free article] [PubMed]
19. Garg H., Lee R. T., Tek N. O., Maurer-Stroh S., and Joshi A. (2013) Identification of conserved motifs in the West Nile virus envelope essential for particle secretion. BMC Microbiol. 13, 197. [PMC free article] [PubMed]
20. Sato T., Iwano T., Kunii M., Matsuda S., Mizuguchi R., Jung Y., Hagiwara H., Yoshihara Y., Yuzaki M., Harada R., and Harada A. (2014) Rab8a and Rab8b are essential for several apical transport pathways but insufficient for ciliogenesis. J. Cell Sci. 127, 422–431 [PMC free article] [PubMed]
21. Shirato K., Kimura T., Mizutani T., Kariwa H., and Takashima I. (2004) Different chemokine expression in lethal and non-lethal murine West Nile virus infection. J. Med. Virol. 74, 507–513 [PubMed]
22. Shirato K., Miyoshi H., Goto A., Ako Y., Ueki T., Kariwa H., and Takashima I. (2004) Viral envelope protein glycosylation is a molecular determinant of the neuroinvasiveness of the New York strain of West Nile virus. J. Gen. Virol. 85, 3637–3645 [PubMed]
23. Kimura T., Kimura-Kuroda J., Nagashima K., and Yasui K. (1994) Analysis of virus-cell binding characteristics on the determination of Japanese encephalitis virus susceptibility. Arch. Virol. 139, 239–251 [PubMed]
24. Kobayashi S., Orba Y., Yamaguchi H., Kimura T., and Sawa H. (2012) Accumulation of ubiquitinated proteins is related to West Nile virus-induced neuronal apoptosis. Neuropathology 32, 398–405 [PubMed]
25. Kobayashi S., Suzuki T., Igarashi M., Orba Y., Ohtake N., Nagakawa K., Niikura K., Kimura T., Kasamatsu H., and Sawa H. (2013) Cysteine residues in the major capsid protein, Vp1, of the JC virus are important for protein stability and oligomer formation. PLoS ONE 8, e76668. [PMC free article] [PubMed]
26. Kobayashi S., Orba Y., Yamaguchi H., Takahashi K., Sasaki M., Hasebe R., Kimura T., and Sawa H. (2014) Autophagy inhibits viral genome replication and gene expression stages in West Nile virus infection. Virus Res. 191, 83–91 [PubMed]
27. Hasebe R., Suzuki T., Makino Y., Igarashi M., Yamanouchi S., Maeda A., Horiuchi M., Sawa H., and Kimura T. (2010) Transcellular transport of West Nile virus-like particles across human endothelial cells depends on residues 156 and 159 of envelope protein. BMC Microbiol. 10, 165. [PMC free article] [PubMed]
28. de Kreuk B. J., Anthony E. C., Geerts D., and Hordijk P. L. (2012) The F-BAR protein PACSIN2 regulates epidermal growth factor receptor internalization. J. Biol. Chem. 287, 43438–43453 [PMC free article] [PubMed]
29. Ang A. L., Fölsch H., Koivisto U. M., Pypaert M., and Mellman I. (2003) The Rab8 GTPase selectively regulates AP-1B-dependent basolateral transport in polarized Madin-Darby canine kidney cells. J. Cell Biol. 163, 339–350 [PMC free article] [PubMed]
30. Noda T., Sagara H., Yen A., Takada A., Kida H., Cheng R. H., and Kawaoka Y. (2006) Architecture of ribonucleoprotein complexes in influenza A virus particles. Nature 439, 490–492 [PubMed]
31. Ullrich O., Reinsch S., Urbé S., Zerial M., and Parton R. G. (1996) Rab11 regulates recycling through the pericentriolar recycling endosome. J. Cell Biol. 135, 913–924 [PMC free article] [PubMed]
32. Welsch S., Miller S., Romero-Brey I., Merz A., Bleck C. K., Walther P., Fuller S. D., Antony C., Krijnse-Locker J., and Bartenschlager R. (2009) Composition and three-dimensional architecture of the dengue virus replication and assembly sites. Cell Host Microbe 5, 365–375 [PubMed]
33. Knödler A., Feng S., Zhang J., Zhang X., Das A., Peränen J., and Guo W. (2010) Coordination of Rab8 and Rab11 in primary ciliogenesis. Proc. Natl. Acad. Sci. U.S.A. 107, 6346–6351 [PubMed]
34. Das A., and Guo W. (2011) Rabs and the exocyst in ciliogenesis, tubulogenesis and beyond. Trends Cell Biol. 21, 383–386 [PMC free article] [PubMed]
35. Xu X. F., Chen Z. T., Zhang J. L., Chen W., Wang J. L., Tian Y. P., Gao N., and An J. (2008) Rab8, a vesicular traffic regulator, is involved in dengue virus infection in HepG2 cells. Intervirology 51, 182–188 [PubMed]
36. Xu X. F., Chen Z. T., Gao N., Zhang J. L., and An J. (2009) Myosin Vc, a member of the actin motor family associated with Rab8, is involved in the release of DV2 from HepG2 cells. Intervirology 52, 258–265 [PubMed]
37. Rowe R. K., Suszko J. W., and Pekosz A. (2008) Roles for the recycling endosome, Rab8, and Rab11 in hantavirus release from epithelial cells. Virology 382, 239–249 [PMC free article] [PubMed]
38. Chu J. J., and Ng M. L. (2002) Infection of polarized epithelial cells with flavivirus West Nile: polarized entry and egress of virus occur through the apical surface. J. Gen. Virol. 83, 2427–2435 [PubMed]
39. Verma S., Lo Y., Chapagain M., Lum S., Kumar M., Gurjav U., Luo H., Nakatsuka A., and Nerurkar V. R. (2009) West Nile virus infection modulates human brain microvascular endothelial cells tight junction proteins and cell adhesion molecules: Transmigration across the in vitro blood-brain barrier. Virology 385, 425–433 [PMC free article] [PubMed]
40. Sato T., Mushiake S., Kato Y., Sato K., Sato M., Takeda N., Ozono K., Miki K., Kubo Y., Tsuji A., Harada R., and Harada A. (2007) The Rab8 GTPase regulates apical protein localization in intestinal cells. Nature 448, 366–369 [PubMed]
41. Yu S., Nie Y., Knowles B., Sakamori R., Stypulkowski E., Patel C., Das S., Douard V., Ferraris R. P., Bonder E. M., Goldenring J. R., Ip Y. T., and Gao N. (2014) TLR sorting by Rab11 endosomes maintains intestinal epithelial-microbial homeostasis. EMBO J. 33, 1882–1895 [PMC free article] [PubMed]
42. Takahashi S., Kubo K., Waguri S., Yabashi A., Shin H. W., Katoh Y., and Nakayama K. (2012) Rab11 regulates exocytosis of recycling vesicles at the plasma membrane. J. Cell Sci. 125, 4049–4057 [PubMed]
43. Coller K. E., Heaton N. S., Berger K. L., Cooper J. D., Saunders J. L., and Randall G. (2012) Molecular determinants and dynamics of hepatitis C virus secretion. PLoS Pathog. 8, e1002466. [PMC free article] [PubMed]
44. Ostrowski M., Carmo N. B., Krumeich S., Fanget I., Raposo G., Savina A., Moita C. F., Schauer K., Hume A. N., Freitas R. P., Goud B., Benaroch P., Hacohen N., Fukuda M., Desnos C., Seabra M. C., Darchen F., Amigorena S., Moita L. F., and Thery C. (2010) Rab27a and Rab27b control different steps of the exosome secretion pathway. Nat. Cell Biol. 12, 19–30; sup pp 11–13 [PubMed]
45. Fukuda M. (2005) Versatile role of Rab27 in membrane trafficking: focus on the Rab27 effector families. J. Biochem. 137, 9–16 [PubMed]
46. Li J., Liu K., Liu Y., Xu Y., Zhang F., Yang H., Liu J., Pan T., Chen J., Wu M., Zhou X., and Yuan Z. (2013) Exosomes mediate the cell-to-cell transmission of IFN-α-induced antiviral activity. Nat. Immunol. 14, 793–803 [PubMed]

Articles from The Journal of Biological Chemistry are provided here courtesy of American Society for Biochemistry and Molecular Biology