- Open Access
Dynamics and restriction of murine leukemia virus cores in mitotic and interphase cells
© Elis et al. 2015
- Received: 16 June 2015
- Accepted: 22 October 2015
- Published: 14 November 2015
Murine leukemia viruses (MLVs) naturally infect unsynchronized T and B lymphocytes, thus, the incoming virus encounters both interphase and mitotic cells. While it is well accepted that MLV requires cell division to complete its replication cycle, it is not known if ab initio infection of mitotic cells can result in productive infection. This question is highly relevant since the milieu of mitotic cells is markedly different from this of interphase cells; e.g. lacking radial microtubule network and intact nuclear envelope. To follow MLV infection in mitotic and interphase cells in real-time, we employed our recently developed infectious MLV particles with labeled cores, cellular models expressing fluorescence markers of different intracellular compartments and protocols for reversible mitotic arrest of MLV-susceptible cells.
Multi-wavelength live cell imaging was employed to simultaneously visualize GFP-labeled MLV cores, DiD-labeled viral or cellular membranes, and fluorescently-labeled microtubules or chromosomes. Cells were imaged either at interphase or upon mitotic arrest with microtubule poisons. Analysis of virus localization and trajectories revealed entry by endocytosis at interphase and mitosis, and correlation between viral mobility parameters and presence or absence of polymerized interphase microtubules. The success of infection of viruses that entered cells in mitosis was evidenced by their ability to reverse transcribe, their targeting to condensed chromosomes in the absence of radial microtubule network, and gene expression upon exit from mitosis. Comparison of infection by N, B or NB -tropic viruses in interphase and mitotic human cells revealed reduced restriction of the N-tropic virus, for infection initiated in mitosis.
The milieu of the mitotic cells supports all necessary requirements for early stages of MLV infection. Such milieu is suboptimal for restriction of N-tropic viruses, most likely by TRIM5α.
- Mitotic Cell
- Murine Leukemia Virus
- Mean Square Displacement
- U2OS Cell
- Interphase Cell
After entry into the cytoplasm of the infected cell, the retroviral core that harbors the reverse-transcribed DNA genome has to reach the chromosomes in order for integration to occur. The interactions of the core with cellular components along this route are not fully known. Microtubule-directed movements toward the nucleus were documented for HIV-1 cores [1, 2] and the involvement of the kinesin-1 adaptor protein—FEZ1—in this process has recently been demonstrated . In addition, dynein and kinesin motors were implicated in the enhancement of HIV uncoating along these movements . The importance of the microtubule network for viral trafficking and retroviral infection is further apparent by the HIV-induced formation of stable microtubules that enhances infection .
After traversing the cytoplasm, HIV-1 cores are thought to enter the nucleus through their interaction with nuclear pore proteins [6–11]. Unlike HIV-1, the murine leukemia virus (MLV) shows high tropism for dividing cells [12, 13] and its infection is thought to be dependent on the nuclear envelope (NE) breakdown during mitosis [12, 14]. Indeed, our previous microscopic analyses demonstrated that immediately upon the start of NE breakdown, MLV cores enter the nucleus and dock onto mitotic chromosomes . In addition, exit from mitosis is required for integration of this virus . Taken together, these requirements establish the need for passage through cell-cycle for MLV productive infection.
MLVs naturally infect T and B lymphocytes [16, 17]. Considerable portion of such lymphocytes—freshly isolated from lymph nodes of neonatal or adult mice—are cycling (~4–7 % for CD4+ cells and ~13–15 % for B220+ cells; ). This raises the question if this subpopulation of cells is equally susceptible to infection as interphase cells. This question is particularly relevant as the cellular milieu of mitotic cells is substantially different from this of interphase cells. Specifically, mitosis induces structural and functional alterations to the endocytic machinery, radial microtubule network, the presence or absence of intact NE and chromatin organization (reviewed in [19–21]), all potentially relevant to early and late stages of MLV infection. Moreover, cellular restriction factors that restrict HIV infection were shown to interact with and to be dependent on subset of these cellular features [22, 23]. Yet, most MLV infections were tested in unsynchronized cells (i.e. mainly interphase cells) and even in synchronized cells, the steps of MLV infection were not evaluated in the context of mitotic cells.
Here we used a p12-based system to label MLV cores for their detection at early steps of infection in interphase and mitotic cells. This system is based on the generation of MLV particles harboring cores that only portion of their p12 molecules are labeled with GFP. This results in labeled cores, which retain their infectious potential . Using this system, we show that the mitotic cellular context affects the dynamics and restriction of MLV cores.
MLV enters through the endocytic pathway in both interphase and mitotic cells
Virion-containing supernatants were incubated with unsynchronized or nocodazole-arrested U/R/EMTB-mCherry cells. These cells originated from U/R cells (U2OS human osteosarcoma cells that express the MLV receptor ), which also express the EMTB-mCherry fusion protein (composed of two mCherry repeats fused to the N-terminus of the microtubule binding-domain of ensconsin; EMTB ). The infected cultures were visualized by live-cell imaging during the first 2 h of infection, after which the cells were washed and re-visualized 24 h postinfection. The labeling of different viral components (membrane vs. cores) allows for analysis of entry. Specifically, the double-labeling (GFP+DiD+) is indicative of enveloped particles before fusion. Conversely, singly-labeled particles (GFP+DiD−) represent two classes, either particles that were not labeled with DiD or post-fusion cores. In interphase cells, as early as 5 min after exposure of the cells to the labeled virions, the majority of particles decorated the cell contour, suggesting plasma membrane localization, while minor portion of the labeled particles already localized to the cell interior. A measurable portion of membrane-attached particles were double-labeled (GFP+DiD+) (Fig. 1a; yellow dots) and the proportion of double labeled particles was similar for the particles attached to the glass or to the plasma membrane, suggesting that the DiD labeling does not affect cell attachment of particles.
At 75 min postinfection, the distribution and dynamics of labeled particles differed from those observed at 5 min. Namely, a greatly increased number of particles were intracellular (localizing to the area occupied by stained microtubules, pseudocolored in blue; compare Fig. 1b–a) and motile (Fig. 1c and Additional file 1: Mov. S1). Within the cell, the portion of GFP+DiD+ relative to all GFP-labeled puncta was 30 % (Fig. 1b, c). The notion that these double-labeled particles represent incoming virions engulfed in endocytic compartments is supported by their retention of DiD label (marking viral lipid envelopes) and the movement of subset of these particles along microtubules (marked with EMTB-mCherry; Fig. 1c, empty arrowheads and Additional file 1: Mov. S1 and Additional file 2: Mov. S2; and see below movement analyses). Such GFP+DiD+ particles presented saltatory movement, which was heterogeneous in terms of path length, velocity and confinement (Methods; Microscopy). Cytoplasmic GFP+ complexes that were not labeled with DiD (GFP+DiD−) were also observed (Fig. 1b, c); a portion of these likely represent MLV cores that were released from the endosomes after membrane fusion. The latter cores did not move along microtubules but rather showed undirected and limited displacement (Fig. 1c, ellipses), as we reported before .
Since GFP+DiD+ particles moved along microtubules, we proceeded to compare their movement parameters with those of endosomes in U2OS cells. To visualize the dynamics of these endosomes, we transfected U2OS cells with plasmid expressing the endosomal marker FYVE-GFP. Time-lapse sequences of the transfected cells (Additional file 3: Mov. S3) revealed two sub-populations of labeled puncta: small-motile and large puncta showing restricted motility (Additional file 4: Mov. S4), suggesting that different sub-classes of endosomes are found in U2OS cells. FYVE-GFP-labeled endosomes, like the GFP+DiD+ cores, presented maximal velocities in the range of 0.2–2 µm/s. These values fit those reported for transport of endosomes [39, 40] and other viral particles (discussed in ) along microtubules. This concordance of values further supports the notion that the movement of the GFP+DiD+ cores reflects their inclusion in endosomes. To directly test the localization of GFP+DiD+ particles to intracellular endocytic structures, we fed GFP+DiD+-infected U/R cells with fluorescently labeled transferrin, which is internalized by clathrin-mediated endocytosis and labels early and recycling endosomes. These cells were co-labeled with Hoechst 33342 dye (to visualize nuclei, shown in white) and imaged by spinning disk confocal live cell microscopy (Additional file 5: Fig. S1). Fluorescently-labeled particles showing signal in all three channels (blue- transferrin, red- viral membranes, and green- viral cores) were readily detected (Additional file 5: Fig. S1 and Additional file 6: Mov. S5). Moreover, the triple co-localization of signals persisted through multiple time points of the time lapse (Additional file 6: Mov. S5). Taken together, our data firmly demonstrate the endocytosis and endosomal localization of GFP+DiD+ particles.
At 24 h post infection, the near entirety of puncta was singly-labeled, either with GFP or DiD (Fig. 1d, Additional file 7: Fig. S2). Such scenario is in accord with post-fusion events, in which the GFP-labeled cores segregated from DiD-labeled cellular endocytic compartments. Moreover, green and red labeled puncta differed in size (average of 0.7 ± 0.04 and 0.4 ± 0.03 µm2 for red and green puncta, respectively) and motility (Additional file 7: Fig. S2; Additional file 8: Mov. S6). To quantify the difference in motility between the red and green puncta we visualized the “footprint” of each particle by adding its emitted signal overtime, i.e. time composite (Additional file 7: Fig. S2). We then calculated the difference in area of green and red signal between the initial frame and the time-composite over 2 min of a confocal time-lapse series (Additional file 8: Mov. S6). While the area occupied by the green signal increased 20 fold, in accord with motile particles; a much lesser increase (fourfold) was calculated for area of the red signal. Taken together, these data demonstrate that in interphase cells (ecotropic) MLV cores enter via endocytosis and are released from endosomes into the cytoplasm.
When quantitative analysis was applied for comparison of movement of intracellular, wt GFP cores in mitotic and interphase cells, we observed a reduction in the values of the maximal velocities of the labeled particles in the mitotic cells (Additional file 10: Fig. S4A; a left-shifted distribution of frequencies for mitotic cells). Mean square displacement (MSD) analysis of the movement of multiple viral cores in interphase cells showed heterogeneity in the slope and curve shape (MSD versus time graphs; Additional file 10: Fig. S4B). Typically, curves could be grouped into two subpopulations, presenting either a linear correlation between MSD and time, indicative of unperturbed diffusion (graphs labeled in blue colors); and a group showing an exponential-like pattern (labeled in red colors), suggestive of active transport. Notably, upon similar analysis applied to mitotic cells (Additional file 10: Fig. S4C), no curves of the latter category were observed, in line with the absence of polymerized microtubules. In these mitotic cells, in addition to freely diffusing particles (linear MSD/time ratio; graphs labeled in blue colors) we observed particles presenting anomalous curves (labeled in gray), for which we do not yet have an interpretation. Importantly, in mitotic cells we could also detect GFP+DiD− particles that overlapped dark areas inside the cells (Fig. 2a, asterisks), likely representing cores attached to mitotic chromosomes (see below). Taken together, these data reinforce the notion that the intracellular milieu of cells at different stages of the cell cycle influences the dynamics and motility of incoming viral cores.
Since ecotropic MLV requires the endosomal environment, which provides both low pH and cathepsins, for entry by fusion [24–29], we wanted to directly probe if wt GFP reaches internal membranous compartments in mitotic cells. To investigate this, we marked the lipid membranes of U/R/H2A-RFP cells (U/R cells that stably express the red fluorescent protein fused to histone H2A, which marks the chromosomes;  ) with DiD and washed away the unbound dye. Cells were incubated or not with nocodazole (24 h); treated and untreated cells were infected with wt GFP particles (for 1 h). In both nocodazole-treated and untreated cells prominent DiD staining on internal membranous compartments was observed (pseudocolored red; Fig. 2b, c). In single confocal mid-planes of mitotic cells, GFP signals (total of 150 dots, counted in eight cells) distributed into three categories: the first (55 % of total particles) consisted of peripheral (non-internalized) particles (Fig. 2b, full arrowheads); the second (30 %) overlapped with internal DiD-labeled membranes (Fig. 2b, empty arrowheads) and the third type (15 %) of GFP signal overlapped the chromosomal signal (pseudocolored blue, Fig. 2b, asterisks). The overlap between GFP and internal, DiD-labeled membranes implies for particles engulfed in endocytic compartments. This notion was further supported by the spatial restriction of the movement of the engulfed particles, which did not trespass the borders of the DiD-labeled endosomes (Additional file 11: Mov. S7). Such overlap between GFP and internal DiD-labeled membranes could be detected also in interphase cells (Fig. 2c, empty arrowheads). These results further suggest that the entry of ecotropic MLV to mitotic cells occurs by the endocytic pathway, similar to the entry into interphase cells. The overlap between GFP signal and the chromosomes suggests that MLV cores that entered mitotic cells could exit the endocytic compartments (see below).
Viral cores target mitotic chromosomes in the absence of radial microtubule network
Overall, these results suggest that in mitotic cells, in the absence of a microtubule network, MLV cores traffic from the plasma membrane to the chromosomes, where they stably dock.
Viral cores that target mitotic chromosomes in the absence of microtubule network support productive infection
Having observed reverse transcription in mitotic cells, we next quantitatively measured the percentage of infected cells, expressing GFP marker that is derived from a retroviral vector. For this, we infected nocodazole-arrested U/R cells with wt MLV that co-packaged a MLV self-inactivated (SIN) vector, harboring EGFP and puromycin-resistance genes (pQCXIP-GFP-C1; ). In preliminary experiments, cells that were replated following shakeoff failed to efficiently reenter the cell cycle, a pre-condition for efficient integration . Thus, we performed the experiment in attached cells, taking into account that our nocodazole-treatment (for 16 h) resulted in mitotic arrest of ~60 % of the treated cells [measured by Fluorescence-activated cell sorting (FACS), data not shown]. Arrested and non-arrested cultures were exposed to the virus for 6 h (in the presence or not of nocodazole, respectively), after which the supernatants were discarded; the cells were washed and incubated with complete medium for 2 days to allow the cells to exit mitosis. The percentage of GFP-positive cells was then determined by FACS analysis, as a measurement for the expression from the integrated vector. Of note the SIN vector cannot spread and thus such percentage reflects the initial portion of infected cells. This analysis revealed comparable percentages of GFP-positive cells for cultures that were either unsynchronized, or arrested at mitosis, at the time of infection (Fig. 4b). Since more than half of the cells in the arrested culture were in mitosis at time of infection, this implies that initial MLV infection in the absence of a polymerized microtubule network, results in integration and expression of the provirus. These integration and expression steps likely occurred upon exit from mitosis .
TRIM5α restriction is reduced in mitotic cells
Taken together our results show that MLV is capable of fulfilling all early steps of infection in mitotic cells where no radial microtubules network is present. Moreover, the mitotic cell presents a reduced barrier towards restriction-sensitive MLV strains, suggesting that viral restriction may be sensitive to cell-cycle dependent alterations.
Due to the proliferative nature of the hematopoietic cells, the natural milieu encountered by MLV is expected to consist of cells at different stages of the cell cycle, including mitotic cells. Indeed, the process by which MLV gains access to the chromosomes involves the mitotic breakdown of the NE ( and recently visualized by us in live cells ). Whereas MLV infection was extensively studied in unsynchronized cells, the question whether MLV infection can occur ab initio in mitotic cells has yet to be addressed.
Endocytic entry is considered as a necessary step for the productive infection of ectropic MLV, due to the requirements for low pH [24–26] and cleavage by cathepsins` for envelope-mediated fusion [27–29]. However, among the different alterations to the cellular context, the mitotic cell is characterized by alterations to the organization and dynamics of membrane compartments including changes to the endocytic machinery [19, 31, 32]. Thus, concerning early steps of infection, we asked two basic questions: (1) does ectropic MLV enter mitotic cells? (2) does MLV entry involve arrival to internal membranous compartments in cells arrested at mitosis? The presence of viral particles inside the plasma membrane perimeter observed in confocal mid-planes of mitotic cells; and the engulfment of these particles by membranous compartments of the infected cells (Fig. 2) allowed us to conclude that the mitotic cell is permissive for ecotropic MLV entry. Thus, also in mitotic cells MLV reaches the intracellular compartments that supply the molecular requirements for fusion.
Upon exit from these compartments, reverse transcription should occur. We directly tested if the mitotic cellular milieu supports this process. Indeed, generation of gDNA could be readily detected in infected cells, arrested at mitosis (Fig. 4). Thus, all cellular requirements for reverse transcription, such as sufficient concentration of dNTPs, are met by the mitotic cell.
In interphase cells, the movement of virus-containing endosomes along polymerized microtubules may serve as a mechanism to enhance the efficiency of approaching the NE. Indeed, such proximity between viral cores and the NE allows the coincidence of nuclear entry by the cores and the initial stages of NE breakdown . The usage of microtubules and related motor proteins for core trafficking and uncoating has been suggested also for HIV-1 [1–4]. Here we show that in mitotic cells, which are devoid of both intact NE and radial microtubule network, targeting of the mitotic chromosomes by the incoming viral cores still occurs, despite the lack of paths characteristic of active transport (Additional file 5: Fig. S4). Moreover, this process is relatively fast as cores that are docked to the chromosomes can be identified as early as 40 min postinfection (Figs. 2, 3). This implies that the microtubule network and the directed movement that it supports are not absolutely required for targeting the chromosomes. Moreover, the attachment to the chromosomes was followed by all subsequent steps of productive infection (measured upon reversal of the cell cycle arrest), since expression of GFP from MLV vector, which requires integration and transcription, was readily detected in cells where infection was initiated during mitosis.
The absence of a network of polymerized microtubules in mitotic cells, and the reported dependence on such network for optimal restriction of HIV infection by TRIM5α , raise the possibility that a similar scenario could occur in the context of N-tropic MLV infection of mitotic human cells. Thus, it is expected that in such cells, devoid of microtubule network, TRIM5α restriction should be specifically reduced towards the restricted MLV strain (N-tropic). Our results support this notion as GFP signals originating from N, but not B or NB, -tropic viruses were enhanced when infection was initiated in mitotic cells as compared to interphase cells. While changes to the cytoskeleton organization are a prominent feature of the altered cellular context of mitosis, additional changes in the milieu of mitotic cells may contribute to the reduced restriction.
Altogether, MLV can infect interphase or mitotic cells with comparable efficiencies. Yet, this occurs through compound alterations to different parameters of MLV infection, imposed by the specific stage of the cell cycle. Whereas entry in interphase cells is more efficient, compared to mitotic cells, so is the TRIM5α-mediated restriction. Analogously, the barrier of the NE on core access to chromosomes, which exists in interphase cells, is absent in mitotic cells. These compensations result in similar infection outcomes. One can speculate that the ability to overcome restrictions in different cell contexts may contribute to viral diversity.
NIH3T3, 293T, U20S, U/R, U/R/H2A-RFP and U/R/EMTB-mCherry cell lines were grown as described before [15, 37]. The U/R/EMTB-mCherry cell line was generated by co-transfecting U/R cells (U2OS human osteosarcoma cells that express the MLV receptor ) with a plasmid expressing two mCherry repeats fused to the N-terminus of the microtubule binding-domain of ensconsin (EMTB ); and a plasmid expressing the puromycin-resistance gene (PAC). A colony stably expressing the EMTB-mCherry fusion protein was selected with puromycin (1 µg/ml)-containing media. To label U/R cells with the lipophilic dye DiD (1,1′-dioctadecyl-3,3,3′,3′-tetramethylindodicarbocyanine perchlorate; Life Technologies, V-22887), cells (~50 % confluency; 60 mm plate) were incubated with 5 µM DiD for 20 min in Opti-MEM medium (Life Technologies); after which, the cells were trypsinized, washed and replated in complete medium [Dulbecco’s Modified Eagle’s Medium (DMEM; Gibco) supplemented with 10 % fetal calf serum] with or without nocodazole. Concentrations of nocodazole (Sigma M1404) or 2-methoxyestradiol (2ME2; Sigma M6383) were 50 ng/ml and 1.3 mg/ml, respectively for all experiments. To enrich mitotic cells to about 90 %, rounded cells were detached from nocodazole treated-cultures by vigorously slapping the dishes (the mitotic shakeoff method; ) and equal number of floating cells were re-plated and incubated with the indicated virus.
To label infected U/R cells with both Hoechst 33342 dye and fluorescently labeled transferrin, unsynchronized cells were infected with DiD-labeled wt GFP virions (see below). At 1 h postinfection, Hoechst 33342 (Invitrogen; 0.02 mg/ml) and fluorescently labeled transferrin (Alexa 546-conjugated transferrin, Molecular Probes; 50 µg/ml) were added to the culture medium and interphase cells were imaged by time-lapse microscopy for up to 1 h.
To generate cells stably expressing fluorescently tagged mCAT-1, we co-transfected the plasmids mCAT-1–mStrawberry (10 µg)  and PGK-puro (1 µg, expressing the puromycin-resistance gene) into U2OS cells, using the PolyJet reagent (SignaGen Laboratories) according to the manufacture’s protocol. A colony, stably expressing the mStrawberry-tagged mCAT-1, was selected with puromycin (1 µg/ml)-containing media. Cells, expanded from this colony, were arrested (or not) with 2ME2 for 48 h, fixed with 4 % paraformaldehyde, stained with DAPI and visualized by confocal microscopy. Specifically, entire cell volumes were acquired under identical illumination conditions for all cells (nine cells for each experimental condition). Plasma membrane and adjacent intracellular regions were demarked by masking with Slidebook program and employed for calculation of mean intensity of fluorescence signal. Significance was calculated by Student’s t test.
The generation of MLV virions labeled with GFP-p12 fusion molecules (wt GFP virions) was as described before . To label wt GFP virions with DiD, 293T cells that were transfected with plasmids expressing the components of wt GFP  were incubated 24 h posttransfection with 5 µM DiD for 4 h in Opti-MEM medium, after which the cells were washed and incubated with complete medium for additional 24 h. Virions-containing supernatants were filtered (0.45 µ), and frozen (−80 °C) in aliquots until use.
To examine the infectivity of the DiD-labeled wt GFP virions (GFP+DiD+), 293T cells that were transfected with plasmids expressing the components of wt GFP , in addition to a plasmid expressing the MLV-based vector pQCXIP-GFP-C1 , were divided 5 h posttransfection. One half was labeled with DiD as described above and the second half was left unlabeled. After additional 24 h, the culture supernatants were harvested and used to infect naïve U/R cells. 48 h postinfection, the numbers of GFP-positive cells and their mean fluorescence were quantified by FACS analyses.
wt Moloney MLV was harvested from cultures of chronically infected NIH3T3 cells. To encapsidate the pQCXIP-GFP-C1 vector  in wt Moloney MLV particles (NB-tropic), 293T cells (80 % confluency in a 60 mm plate) were co-transfected with pNCS plasmid (10 µg), expressing the wt Moloney MLV and the pQCXIP-GFP-C1 vector (5 µg). 48 h posttransfection the virion-containing culture supernatant was harvested, complemented with Hepes (50 mM; pH 7.4), filtered (0.45 µ) and kept frozen until use. To generate cognate particles with N- or B- tropism, a portion of Moloney MLV Gag-Pol sequence in pNCS was replaced with the related sequences derived from N or B -tropic MLV clones (pCIG3N or pCIG3B, generously provided by G. Towers, UCL), which contain the residues in capsid that define N and B tropism . The resulting N or B -tropic clones were able to spread in NIH (which restrict B-tropic viruses) or U/R (which restrict N-tropic viruses) cells, respectively, with the same kinetics of the NB -tropic Moloney MLV (data not shown), demonstrating the expected tropism. These clones were co-transfected with pQCXIP-GFP-C1 vector, as above. Normalization of MLV virions was achieved by exogenous RT assay .
Live-cell microscopy was performed essentially as described in . For analyses, confocal movies were first deconvolved with the No Neighbours deconvolution algorithm of Slidebook software (Intelligent Imaging Innovations). Where indicated, time-composite channels were produced by Slidebook. Following this, GFP and/or DiD fluorescence were identified through intensity-based segmentation; the signal area, number of objects or overlap between objects were calculated by Slidebook. Path tracking was carried out with the particle tracking algorithm of SlideBook. Deconvolved movies were filtered with the Laplacian 2D filter of the same software. Objects in the filtered images were identified through intensity-based segmentation. Paths consisting of a minimum of 10 consecutive steps were approved by visual inspection before analysis. Maximal velocity values were determined for two groups of 19 paths by SlideBook. This software was also used to generate path coordinates for representative tracks, which were then used to calculate the cognate mean square displacement (MSD) values.
Low molecular DNA, containing the MLV genome and mitochondrial DNA, was extracted from infected cells at the indicated time points by the Hirt extraction method . PCR amplification was applied using MLV specific primers (‘pNCS BsrGI FW’ 5′CCCAGGTTAAGATCAAGG3′ and ‘pNCS XhoI REV’ 5′CTTGGCCAAATTGGTGGG3′) and mitochondrial (cytochrome B-derived ; ‘CytB H15149′ 5′AAGCTTCCATCCAACATCTCAGCATGATGAAA3′ and ‘CytB L14841′ 5′ACTGCAGCCCCTCAGAATGATATTTGTCCTCA3′).
Quantification of viral restriction
U/R cells in 6-well plates (~50 % confluence) were treated, or not, for 16 h with nocodazole. Subsequently, cells were infected (in the presence, or not, of nocodaxzole), for 6 h (M.O.I = 0.3), after which the cells were trypsinized, washed and replated with complete medium (with no nocodazole). Two days later, the cells were analyzed by FACS and infection index was calculated by multiplying the percentage of GFP-positive cells and the normalized geometric mean of the GFP signal . Normalization took into account the increase in auto-fluorescence observed for all nocodazole-treated cells. For this, GFP signals in nocodazole-treated samples were corrected by division with the ratio of nocodazole-treated/untreated non-specific fluorescence values (~1.5).
EE carried out the experiments and drafted the manuscript. EE, ME and EB conceived and designed the study. All authors read and approved the final manuscript.
We thank Rachel Zamosatsiano for technical assistance, Eran Perlson (Tel Aviv University) for EMTB-mCherry construct, Greg Towers (University College London) for plasmids of N and B -tropic Gag proteins and Robert A. Davey (University of Texas) for mCAT-1–mStrawberry construct. This research was supported by the Israel Science Foundation (Grant No. 1824/13).
The authors declare that they have no competing interests.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
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