Rabies virus (RABV) is a highly neurotropic pathogen that typically leads to mortality of infected animals and humans. The precise etiology of rabies neuropathogenesis is unknown, though it is hypothesized to be due either to neuronal death or dysfunction. Analysis of human brains post-mortem reveals surprisingly little tissue damage and neuropathology considering the dramatic clinical symptomology, supporting the neuronal dysfunction model. However, whether or not neurons survive infection and clearance and, provided they do, whether they are functionally restored to their pre-infection phenotype has not been determined in vivo for RABV, or any neurotropic virus. This is due, in part, to the absence of a permanent “mark” on once-infected cells that allow their identification long after viral clearance. Our approach to study the survival and integrity of RABV-infected neurons was to infect Cre reporter mice with recombinant RABV expressing Cre-recombinase (RABV-Cre) to switch neurons constitutively expressing tdTomato (red) to expression of a Cre-inducible EGFP (green), permanently marking neurons that had been infected in vivo. We used fluorescence microscopy and quantitative real-time PCR to measure the survival of neurons after viral clearance; we found that the vast majority of RABV-infected neurons survive both infection and immunological clearance. We were able to isolate these previously infected neurons by flow cytometry and assay their gene expression profiles compared to uninfected cells. We observed transcriptional changes in these “cured” neurons, predictive of decreased neurite growth and dysregulated microtubule dynamics. This suggests that viral clearance, though allowing for survival of neurons, may not restore them to their pre-infection functionality. Our data provide a proof-of-principle foundation to re-evaluate the etiology of human central nervous system diseases of unknown etiology: viruses may trigger permanent neuronal damage that can persist or progress in the absence of sustained viral antigen.
Rabies is an ancient and fatal neurological disease of animals and humans, caused by infection of the central nervous system (CNS) with Rabies virus (RABV). It is estimated that nearly 55,000 human RABV fatalities occur each year, though this number is likely much higher due to unreported exposures or failure of diagnosis. No treatment has been identified to cure disease after onset of symptoms. Neurovirologists still do not know the cause of rabies' dramatic symptoms and fatality, though it is thought to be due to neuronal loss or dysfunction. Here, we use a novel approach to permanently and genetically tag infected cells so that they can be identified after the infection has been cleared. This allowed us to define neuronal survival time following infection, and to assess neuronal function through gene expression analysis. We found that RABV infection does not lead to loss of neurons, but rather induces a permanent change in gene expression that may be related to the ability of RABV to cause permanent CNS disease. Our study provides evidence that viral infection of the brain can initiate long-term changes that may have consequences for nervous system health, even after the virus has been cleared from the CNS.
Citation: Gomme EA, Wirblich C, Addya S, Rall GF, Schnell MJ (2012) Immune Clearance of Attenuated Rabies Virus Results in Neuronal Survival with Altered Gene Expression. PLoS Pathog 8(10): e1002971. https://doi.org/10.1371/journal.ppat.1002971
Editor: Stanley Perlman, University of Iowa, United States of America
Received: March 28, 2012; Accepted: August 30, 2012; Published: October 11, 2012
Copyright: © Gomme et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by grant R21NS074006 by the National Institute of Neurological Disorders and Stroke to MJS and GFR and P40 OD010996 to MJS. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Rabies is a fatal neurological disease of animals and humans for which there is no treatment once symptoms develop. The disease is caused by infection of the central nervous system (CNS) with the single-stranded RNA virus, Rabies virus (RABV). Infection results in dramatic neurological symptoms—aggression, hyperactivity, muscle weakness, paralysis, coma—invariably leading to fatality. The precise etiology of rabies pathogenesis is unknown and hypothesized to be either neuronal death or dysfunction. However, whether infected neurons can survive infection and the resultant immune response is unknown. Moreover, if these neurons survive, whether they are functionally restored to their pre-infection competence has not been determined in vivo for RABV, or for any neurotropic virus.
Analysis of human brains post-mortem reveals surprisingly little tissue damage and neuropathology, considering the dramatic clinical symptomology , . As seen for other viral infections both RABV replication and resultant anti-viral immune responses are believed to be non-cytolytic; the latter mediated by cytokines, including type I interferons, and neutralizing antibodies –. Acute infection induces global upregulation of proinflammatory and innate immunity genes, including IL-6, TNF-α, type I interferons, complement cascade genes, and toll-like receptors within the brain –. Though there is some evidence that infection induces morphologic changes in infected neurons , , there is a distinct lack of overt histopathological changes indicative of apoptosis or necrosis , . Attempts to recapitulate this ex vivo have been difficult; some viral strains induce neuronal apoptosis in tissue culture, while others do not –. This demonstrates the importance of studying neuronal cell fate in an animal model.
An alternative hypothesis is that neuronal dysfunction, rather than cell death, is responsible for the clinical features and fatal outcome in rabies. Neurological abnormalities are obvious, but studies in experimental rabies have revealed other phenomena, including disappearance of rapid eye movement (REM) sleep and initiation of facial twitching, called myoclonus, prior to development of classic symptoms. It was also found that brain electrical activity terminated about 30 minutes before cardiac arrest, indicating that cerebral death precedes organ failure , . This correlates with functional deficiencies observed during acute experimental RABV infection, including altered expression of proteins involved in synapse communication and ion homeostasis , as well as neuronal depolarization and decreased neurotransmitter binding –.
A challenge in studying the longevity of infected neurons is identifying and isolating them after resolution of the acute viral infection. In the absence of a permanent “mark” on once-infected cells, it is impossible to decisively answer the question as to whether infected cells survive and regain their pre-infection functionality. Instead, more general metrics of CNS health have been used, including histopathological assessments, absence of cell death (via assays with known limitations in vivo, such as TUNEL staining), and in vitro studies using neuroblastoma cells or primary neurons that may not faithfully recapitulate the biology of an infected neuron in vivo. Furthermore, control of viral replication by host immune responses in immunocompetent animal models may limit the infection to only a few cells, and apoptotic loss of these few cells may not be readily detected by most methods.
Here we present a novel approach to study neuronal cell fate after RABV infection. We infected Cre reporter mice with a sub-lethal dose of recombinant RABV expressing Cre-recombinase (RABV-Cre) to switch neurons constitutively expressing tdTomato (red) to expression of a Cre-inducible EGFP (green), permanently marking neurons that had been infected in vivo. This model allowed us to monitor neuronal survival after infection and to isolate neurons that resolved infection to characterize gene expression profiles relative to uninfected neurons. Our results support the notion that the majority of neurons survive infection, but remain impaired; this may account for the CNS disease caused by this neuropathogen.
Recovery and characterization of Cre-expressing RABV (RABV-Cre)
In order to identify and isolate cells (specifically, neurons) after resolution of a viral infection, we adopted a double-fluorescent Cre reporter mouse model . These Cre reporter mice constitutively and ubiquitously express membrane-targeted tandem dimer Tomato (tdTomato); upon exposure to Cre recombinase, the tdTomato gene is deleted, and membrane-targeted EGFP is induced (Figure 1D). We generated a recombinant rabies virus (RABV-Cre) expressing Cre-recombinase (Figure 1A) , , which, in combination with the Cre reporter mouse, provided a model to permanently change the color of an infected cell from red to green, even after the virus was cleared. Cre was modified by the addition of a 5′ nuclear localization signal to promote high efficiency, in vivo recombination between loxP sites, and cloned into the an empty recombinant RABV backbone previously published as “BNSP” . This recombinant virus is based on the SAD B19 RABV vaccine strain, which is moderately pathogenic after intracranial inoculation , but known to infect neurons efficiently . Of note, to study long-term effects of RABV infection on neurons, it was imperative to choose a viral strain that efficiently infected the brain but that resulted in full recovery of the host: our previous work indicated that doses of this strain could be delivered that resulted in extensive neuronal infection, a robust antiviral response, and no mortality .
A) Genome of rabies virus (RABV) and the recombinant RABV expressing Enterobacteria phage P1 Cre recombinase (RABV-Cre) with a 5′ nuclear localization signal (shown in orange). B) Cre expression was confirmed by western blot analysis. Neuroblastoma cells were infected with either RABV-Cre, RABV expressing HIV-1 Gag (RABV-Gag), or mock infected (uninfected). Proteins were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis and subjected to Western blotting with antibodies specific for Cre, RABV P or N, and actin. C) Viral growth kinetics were evaluated by multi-step growth curve assay in which BSR cells were infected at MOI 0.01 with either RABV or RABV-Cre, and viral titers determined from samples taken at the indicated time points post-infection. D) A schematic depicting the Cre-specific expression cassette in the Cre reporter mouse. In the absence of Cre, the chicken β-actin core promoter with a CMV enhancer (CAG) drives constitutive expression of membrane-targeted tandem dimer tomato (tdTomato) expression; EGFP is not expressed. After Cre-mediated excision of the tdTomato gene at the loxP sites, membrane-targeted enhanced green fluorescent protein (EGFP) is expressed. pA denotes polyadenylation sites. E) Cre functionality was evaluated in vitro by infecting primary fibroblasts isolated and cultured from Cre reporter mice for 96 hours with either RABV-Cre or RABV at MOI 20. EGFP and tdTomato labeling were detected by fluorescence microscopy (top) and flow cytometry (bottom) (using FITC and PE channels, respectively).
RABV-Cre was recovered by standard methods  and the fitness of the recombinant RABV, as well as the expression of the inserted Cre gene, was evaluated ex vivo. BSR fibroblasts were infected with RABV or RABV-Cre and analyzed by western blot for protein expression (Figure 1B) as well as one-step growth curves for viral replication (Figure 1C). These assays demonstrated that insertion of Cre between the RABV nucleoprotein (N) and phosphoprotein (P) genes had no effect on the rate of viral replication, or relative viral gene expression (Figure 1B and C). To analyze the functionality of the virus-encoded Cre, primary mouse fibroblasts harvested from Cre reporter mice were infected with RABV or RABV-Cre. Functional expression of Cre was indicated by EGFP expression in Cre reporter mouse fibroblasts after infection with RABV-Cre but not after infection with wildtype RABV (Figure 1D and E). Of note, these cells are double-labeled with EGFP and tdTomato; this delayed loss of tdTomato is likely due to a long protein half-life. Published data shows loss of tdTomato upwards of 9 days post-excision , though this may vary from tissue to tissue.
RABV infection of brain neurons in Cre reporter mouse are ‘permanently marked’ by constitutive EGFP expression.
Cre reporter mice were infected intranasally (IN) with 105 foci forming units (ffu) RABV-Cre (Figure 2A). This sub-lethal dose was specifically chosen to permit the study of neuronal survival and integrity at later time points post-infection. Infected mice became moribund by day 15 post-infection and developed classic signs of rabies—weight loss, fur ruffling, ataxia, hunched posture—though none displayed hind limb paralysis (Figure 2B). The lack of peripheral neuropathy, as seen before , is likely due to the route of administration, because IN-administered RABV directly invades the CNS without infecting the peripheral nervous system. 65% to 75% of the infected mice survived acute infection and regained body weight after day 15 (Figure 2B).
A) Timeline of mouse experiment. Cre reporter mice were infected intranasally (IN) with 105 ffu RABV-Cre and sacrificed at the specified times. B) Weights of infected mice were monitored as a measure of disease throughout the experiment and demonstrate productive infection in all mice within this experiment. C) Brains collected at different time points post-infection were analyzed for the presence of EGFP-expressing cells in the following anatomical regions: olfactory bulb (OB), cerebral cortex (CC), cerebrum (CR), hippocampus (HIP), cerebellum (CB) and midbrain/hindbrain (MB-HB).
Cre reporter mice were maintained up to 6 months post-infection with groups of 3–4 mice being sacrificed at the time points depicted in Figure 2A. At each time point, brains were collected from the mice for imaging and RNA analysis. We initially imaged brains collected from mice 15 days post-infection—a point when viral replication was still active ,  and clinical signs of RABV peaked (Figure 2B). Only brain tissue from infected mice showed regions of EGFP expression amid non-transformed tdTomato-expressing brain tissue (Figure 3 and 4). Because the fluorophores are membrane-targeted, we were able to detect single-cell morphology including individual dendrites using confocal microscopy (Figure 3). To further characterize the EGFP+ regions after RABV infection, we stained for RABV P antigen and cell-specific markers for neurons (NeuN) and astrocytes (GFAP) (Figure 4). In vivo, RABV is known to replicate almost exclusively in neurons  and rarely in glial cells . As shown in Figure 4C, we detected perinuclear RABV P amid clusters of infected neurons only within the EGFP+ regions.
Fifteen days post-infection, brains were collected, cryosectioned, and imaged without secondary staining on a standard fluorescent microscope (20× and 40× images) or confocal microscope (63× image). All images shown are from the olfactory bulb region.
Brains were collected from Cre reporter mice fifteen days post-infection, cryosectioned, and EGFP+ regions compared to cell-specific labeling, A) NeuN (blue, neuronal nuclei antibody, 20× fluorescence imaging), B) GFAP (blue, astrocyte antibody, 40× confocal imaging), or C) RABV P antigen (purple) and DAPI nuclear stain (blue, 63× confocal imaging). White arrows in (C) indicate regions positive for RABV P.
Neurons survive RABV infection and viral clearance in vivo.
Having validated that the EGFP+ regions correspond to RABV-infected neurons, we examined the distribution and duration of EGFP foci over the course of 6 months during which RABV infection would have been cleared. Though rabies can be cleared as early as 18 days post-infection , , we detected EGFP+ foci out to 6 months post-infection (Figure 5). Single EGFP+ cells begin to appear as early as day 7 post-infection, but stable numbers of multi-nucleated foci were present in all areas evaluated in the brain parenchyma from day 15 through 6 months post-infection (Figures 5 and 6). Of note, the sizes of these foci were morphologically similar across this timeline. Only the hippocampus becomes EGFP+ later than the other regions, between 15 days and 1.5 months post-infection, but then remains unchanged through the rest of the time course. Moreover, the hippocampus is the most brightly labeled anatomical region of the brain. In contrast, the least prominent labeling was found in the cerebellum, though these levels of labeling are clearly higher than naïve cerebellar sections. This agrees with other reports that RABV is distributed throughout various regions of the brain, including cerebral cortex, hippocampus, and cerebellum , . These neurons are either survivors of RABV infection, or newly-infected cells.
The spread of the RABV infection was detected by identifying regions of EGFP fluorescence in different neuroanatomical regions (see Figure 2C) over a 6 month time course. Images are representative of 3–4 mice analyzed at each time point.
Brains from infected mice were collected at the indicated time points and immunostained. The panels show cryosections stained for RABV P antigen (purple) and DAPI nuclear stain (blue; 63× confocal imaging). White arrows indicate regions positive for RABV P.
To elucidate whether EGFP+ foci observed at later time points are products of new infection or previously-infected neurons, we used quantitative real time PCR to compare levels of viral genome and messenger RNA to that of EGFP from the same brains used to image the tdTomato/EGFP in Figure 5. Similar to the immunofluorescence data, EGFP RNA peaks at day 15 post-infection and remains stably expressed through our last time point, 6 months post-infection (Figure 7). In contrast, active RABV infection, as measured by RABV N mRNA production, peaks at day 15 post-infection and decreases thereafter, with fewer than 100 copies of viral message detected by 3 months post-infection. This is supported by immunohistochemical detection of RABV P at these time points (Figure 6). While others have reported viral mRNA peaking at days 6–8 post-infection with near complete clearance by day 18 , our more sensitive quantification shows sustained viral persistence, particularly of the genome that is still present at approximately 1000 copies as late as 6 months post-infection (Figure 7). It has been suggested that viral genome persistence for negative-stranded RNA viruses is due to the stabilizing effects of the nucleoprotein which closely encapsidates the genome, and not necessarily to the production of new genomes. Because negative-stranded RNA viruses cannot replicate without the production of the RABV N, P, or L proteins, the lack of N mRNA clearly indicates the lack of active replication.
RNA was isolated from brains of mice at the indicated time points post-infection and assayed by real-time quantitative PCR for RABV genomic RNA (blue circles and line; left y-axis), RABV messenger RNA (black squares and line; left y-axis), and relative EGFP expression (green bars; right y-axis). Gene expression of all targets was normalized to the RPL13A (L13A) housekeeping gene. Data displayed was collected from 3 to 4 mice at each time point.
Microarray analysis of RABV-infected neurons isolated by FACS 3 months after infection indicates gene dysregulation
Neuronal survival following viral infection next prompted us to investigate the functional integrity of these “cured cells”. We used fluorescence activated cell sorting (FACS) to isolate the EGFP+ population (“infected”) and the tdTomato+ population (“uninfected”) from individual mice 3 months post-infection (Supplemental Figure S1), a time when viral transcription was undetectable (Figure 7). Of note, the endogenous fluorescence of these populations precluded the need for intracellular staining that compromises RNA integrity. Affymetrix Gene Microarray was used to measure transcriptional profiles of the infected and uninfected cells from two independent cell sorting events (n = 2 for each group). This analysis identified 1248 genes differentially expressed between the sorted groups (infected vs. uninfected, ≥1.5 fold change, p<0.05), 361 genes of which were down-regulated, 887 genes that were up-regulated. Gene expression levels ranged from 3.09-fold up-regulation to 2.72-fold down-regulation, and only 127 genes differed by more than 2-fold (Supplemental Table S1). Though the overall change in gene expression was modest, these transcriptional changes may be implicated in neuronal dysfunction. We saw no decrease in neuron-specific genes classically down-regulated in neurological disorders; in fact, there was up-regulation of neuronal receptors (glutamate receptor, GABA receptor), ion channels (potassium, sodium, and hydrogen), neurotransmitter transporter (Cacna1b), and synapse-specific genes (synaptotagmin I, synaptophysin) (Supplemental Table S2), strongly supporting our contention that these analyzed cells are of neuronal origin. However, it is not a given that the change in expression of “neuron-specific” genes is responsible for the dysfunction of the neuron. More likely it is the virus' interaction with ubiquitous cellular genes that induces functional changes within the neuron. For example, genes encoding proteins that play critical roles in ion homeostasis, exocytosis, or mitochondrial function have been shown to have a great effect on neuronal function – however these genes are commonly expressed in a large variety of cells. Ingenuity Pathway Analysis (IPA) was used to identify biological functions most significantly impacted; cell-to-cell signaling was the most significant molecular and cellular function impacted, whereas behavior and nervous system development/function were the two most significant physiological systems impacted (Figure 8). Analyzing the regulation of groups of related genes, IPA predicted decreased function (those with an absolute z-score value≥1.96) in the following areas: neurite growth/outgrowth, organization of cytoskeleton, organization of cytoplasm, and microtubule dynamics (genes involved in these functions are listed in Table 1).
Cell suspensions prepared from whole mouse brains 3 months post-infection were sorted on a MoFlo cell sorter for EGFP+ (previously infected) and EGFP- (uninfected) cell populations. The 1248 transcripts differentially expressed between infected and uninfected cells (≥1.5 fold change, p<0.05) were analyzed by Ingenuity Pathway Analysis (IPA) to identify biological functions most significantly affected by the infection (significance predicted by p-value). Shown are the top ten most significant biological systems affected by the gene dysregulation, with the horizontal bars representing the negative log of their p-value (greatest significance at the top). Below each bar is the top three sub-categories affected by gene dysregulation in the respective categories. Each category/sub-category has the number of genes involved (up or down-regulated).
Neurons are particularly vulnerable to the consequences of viral infection and/or the anti-viral immune response in the brain. Evidence suggests that neuropathology induced directly or indirectly by infection may lead to symptoms of disease. For example, caspase-dependent apoptosis has been implicated in pathogenesis of vesicular stomatitis virus (VSV) and WNV, and cytomegaloviruses induce lysis of the host cell –. For RABV, the basis of neuropathogenesis is unknown, and predicted to be due either to neuronal death or dysfunction.
A challenge in studying the longevity of infected neurons is identifying and isolating them after resolution of the acute viral infection. To study rabies, approaches used in the past have included histopathology, measurements of cell death (via TUNEL assay), and in vitro studies that may not represent the biology of an infected neuron in vivo. These assays have known limitations and may account for the inconsistent results in this research area, making it hard to draw a conclusion as to neuronal cell fate after viral infection. Here we examined the survival and functionality of neurons infected with RABV using a novel and innovative approach: the Cre reporter mouse model. Of note, our results are based on attenuated RABV which only models what may happen in a natural RABV infection. We appreciate the fact that pathogenic rabies virus is invariably lethal and few survive to the later timepoints evaluated in this study. However, by using a less virulent strain of virus, we were able to sufficiently infect brain neurons without killing the mice, and study the impact of the infection on these cells long after clearance of substantial inflammation and bystander effects, which may complicate data analysis. More pathogenic RABV variants could be used, though the window of time between infection and death is brief and catching these cells for analysis would be challenging. However, we speculate that in the rare event of an animal (or person) surviving a RABV infection, the changes within the previous infected neurons are similar to what have been observed for the attenuated RABV. Though we do not have direct evidence that infection with a pathogenic RABV will result in similar changes in gene expression as observed here for the attenuated RABV, there is indirect support for this hypothesis. This is based on the findings that the major difference between a pathogenic and attenuated RABV is the faster spread within the CNS of the pathogenic strain  which, in combination with the lack of immunogenicity of the pathogenic strain, normally results in death of the infected host. However, the lack of any pathology within the RABV-infected brain, which is especially true for an infection with pathogenic RABV strain, , – strongly argues for functional changes within the infected neurons, including pathogenic strains.
Our results show that experimental RABV does not induce cell loss as a result of direct or indirect cytopathic effects of the virus, nor a cytotoxic immune response. RABV G has been implicated in apoptotic signaling in vitro; for many years it was believed that the quantity of RABV G expressed correlated with both apoptosis and pathogenicity , . Recently this paradigm was challenged, and abundance alone was shown not to be the only determinant of apoptosis . Préhaud et al. demonstrated that pathogenic and attenuated strains recruit different intracellular proteins that mediate either cell survival or cell death, respectively . The in vivo relevance of their work remains to be determined; in vitro infection of pure cultures of neurons, at a high multiplicity of infection, in the absence of an intact immune response may not represent events in vivo. Our results indirectly support the claims that RABV immunity is rapid and mediated by non-cytolytic immune responses, likely antibody and cytokine secretion . The role of type I interferons, specifically, has been of great research interest. RABV-infected neurons can produce type I interferons in vitro , and interferon-α receptor knock out mice are unable to control the virus and ultimately succumb to infection . What impact these cytokines have on neuronal integrity is unclear. Though CD8+ T cells have been found in brain sections of human rabies victims , their deletion appears to have no significant effect on the survival of challenged mice .
Our data supports the hypothesis that RABV pathogenesis is not due to loss of neurons, but rather to neuronal dysfunction. Evolutionarily this makes sense, as preservation of the neuronal network by inhibition of apoptosis and limitation of inflammation is advantageous for RABV to complete its lifecycle. The Cre reporter model allowed us to isolate “cured” neurons from mice 3 months post-infection to study their transcriptional profiles compared to uninfected cells from the same mice. Comparing one cell population to another in the same mouse acted as an internal control, avoiding differences based on age, treatment, and normal biological variance. We show evidence that neurons exhibit permanent transcriptional differences from uninfected cells long after resolution of the viral infection. We used a bioinformatics tool, Ingenuity Pathway Analysis (IPA), to identify biological functions most significantly impacted by this dysregulated gene set. Our results showed a modest change in gene transcription (rarely over 3-fold difference between infected and uninfected) with most affected genes involved in cell-to-cell signaling and nervous system development/function. The most interesting aspect of the transcriptional data was the prediction of functional consequences potentially induced by the pattern of gene changes: decreased neurite growth, decreased organization of cytoskeleton, decreased organization of cytoplasm, and decreased microtubule dynamics. For example, we observed a down-regulation of many key microtubule/microtubule-associated genes by microarray. Our results, which were acquired through an unbiased assay, are in agreement with others; Li et al. found similar down-regulation of microtubule-related genes in acute pathogenic RABV infection, and this directly correlated to degeneration of neuronal processes . Furthermore, decreased neurite growth and dendritic/axonal swelling has been detected by microscopic examination of infected neurons in culture , , , , though it may be strain dependent. Together, these hypothesized gene expression changes may reflect an overall failure to reorganize the cytoskeleton for growth or repair of cellular processes. Future examination of live EGFP labeled cells purified from the brains of these Cre reporter mice may fully elucidate the functionality, or lack thereof, of once-infected neurons compared to never-infected neurons. Furthermore, alternative approaches, such as laser capture microdissection, may be useful in future efforts to monitor transcriptional changes in specific sub-populations of neurons.
We anticipate that an understanding of the deficiencies of RABV infected cells will provide useful insights into the development of novel treatment options for the acute disease based on restoring lost cellular function. The incubation period, or period between infection and development of symptoms, is extremely variable and can range from 1 week to over 1 year in duration. Post-exposure prophylaxis is highly effective during this period; however, once symptoms develop, survival is extremely rare. Our data provides hope that living neurons may be a possible target for intervention. If research can elucidate the precise effect of viral infection of brain neurons, it may be possible to develop novel treatments effective during these late stages of disease. This data also provides reason to be concerned with the use of recombinant rabies vectors for treatment of neurological disorders or infections.
This model may also be used as a tool to study the regenerative capacity of neurons. We looked at neuronal gene expression from one time point only, but analyzing the expression of select genes at several points over a period of time would provide information regarding the ability of these cells to regenerate. Furthermore, viral genome was still present at the 3 month timepoint; is functionality regained after complete genome clearance? Latent herpesvirus induces neuronal deficits, though this is likely due to transcription of latency-associated genes . We believe that the RABV genome is persisting due to the stabilizing effects of the viral nucleocapsid as described for other negative-stranded RNA viruses, including VSV , and RABV does not express latency-associated genes. We do not anticipate that the persistent genome will play a role in neuronal dysfunction, though this would need to be confirmed experimentally.
Lastly, this model may be used to study the link between viral infection and chronic neurodegenerative diseases. This link has been suggestive for other abortive or latent viral infections in which the host survives (e.g. herpesviruses, measles, Polio, Epstein-Barr). Multiple sclerosis, for example, is suspected by some of having a viral etiology. A virus-induced disturbance may be, in a subset of patients, the starting point for autoimmune demyelination. There is compelling evidence for involvement of Human herpesvirus 6 (HHV-6), as viral antigen has been found in sclerotic lesions, and virus-specific IgM antibodies increase in relapsing-remitting MS patients , though proving a causative link between viral infection and chronic dysfunction has been difficult. The Cre mouse model proposed here provides a powerful tool to study other neurotropic viruses and show causation between virus and chronic disease. Our data clearly demonstrates that neurotropic viral infection can cause persistent neurological deficits long after active infection has been cleared, and that once-infected neurons may not be restored to their pre-infection phenotype. The implications of these findings are substantial, as surviving neurons, which have a remarkable capacity to recover following damage , , may be targeted for novel treatment options in rabies and other neurological infections by restoring compromised cellular functions.
Materials and Methods
All animals were handled in strict accordance with good animal practice as defined by the relevant international (Association for Assessment and Accreditation of Laboratory Animal Care (AAALAC) (Accreditation Status TJU: Full)) and national (TJU Animal Welfare Assurance Number: A3085-01), and all animal work was approved by the Institutional Animal Care and Use Committee (IACUC) at Thomas Jefferson University TJU. Animal use protocols are written and approved in accordance with Public Health Service Policy on Humane Care and Use of Laboratory Animals, The Guide for the Care and Use of Laboratory Animals. TJU IACUC protocol number 414 I (Pathogenesis of rabies virus and vaccine vectors in mice) was utilized in this study. Cre reporter mice, strain B6.129(Cg)-Gt(ROSA)26Sortm4(ACTB-tdTomato,-EGFP)Luo/J, were purchased from the Jackson Laboratory, USA. Heterozygotes were bred and offspring were genotyped as recommended by Jackson Laboratories.
Mice were anesthetized with 4% isoflurane by inhalation and inoculated intranasally with 1×105 ffu virus diluted to 20 µL with phosphate-buffered saline (PBS)(10 µL per nostril). Mice were sacrificed at the indicated time points post-infection and brain tissue harvested for RNA and immunohistochemistry.
Construction, recovery, and characterization of Cre-expressing RABV
cBNSP is an infectious clone based on the RABV vaccine strain SAD B19, which contains two single restriction sites (BsiWI and NheI) for inserting foreign genes . Enterobacteria phage P1 Cre Recombinase (Genbank accession number X03453) was engineered to include a 5′ nuclear localization signal (ATG GCA CCC AAG AAG AAG AGG AAG) to promote high efficiency in vivo recombination between loxP sites, and is hereafter referred to simply as Cre (Cre cDNA was kindly provided by Dr. Jianke Zhang, Thomas Jefferson University, Philadelphia). The Cre gene was amplified using forward primer 5′-cac CGT ACG acc atg gca ccc aag aag aag-3′ (BsiWI site in caps, ATG start codon for the nuclear localization signal is underlined) and reverse primer 5′-cga GCT AGC cta atc gcc atc ttc cag cag g-3′ (NheI site in caps), and cloned into cBNSP using the unique BsiWI and NheI sites between RABV nucleoprotein (N) and phosphoprotein (P). The resulting cDNA was termed RABV-Cre. RABV-Cre was recovered as previously described .
Multi- and single-step growth curves were conducted on BSR cells as previously described . Cre functionality was evaluated in vitro by infecting primary fibroblasts cultured from Cre reporter mice. To isolate primary fibroblasts, leg muscle was dissected from euthanized adult Cre reporter mice and dissociated using a protocol adapted from Blau et al. . Briefly, muscle tissue was minced into 3- to 4-mm pieces in PBS, incubated in an enzyme mixture of collagenase D (0.75 units/mL, Roche Applied Science, 11088858001), Dispase II (1.2 units/mL, Roche Applied Science, 10295825001), and 2.5 mM CaCl2 for 45 min in a 37°C water bath, triturating with a 5 mL pipette 3 times throughout the incubation. Ten milliliters of PBS was added to the cell suspension and passed through a 70 µm filter, spun at 300×g for 5 min, resuspended in DMEM supplemented with 10% FBS and penicillin-streptomycin (DMEM10), and plated in a standard T75 tissue culture flask. To enrich for fibroblasts, cells were allowed to attach to the flask for 1 h at 37°C, at which time the unattached cells were aspirated and the adherent cells were passaged in DMEM10 for 5 to 7 d. Cre reporter primary fibroblasts plated at 80–90% confluency in 6-well plates were infected with 2.4×106 ffu recombinant virus at 37°C. After 96 h, the cells were assayed for color change from TdTomato to EGFP by fluorescent imaging and flow cytometry. For imaging, plated cells were fixed with 4% PFA (pH 7) for 20 min at 4°C and viewed under a fluorescence microscope. For flow cytometry, trypsinized cells were fixed in suspension with 4% PFA (pH7) for 20 min at 4°C, washed once in PBS supplemented with 2% BSA, and analyzed on a BD FACSCalibur (50,000 events collected).
NA cells plated at 80–90% confluency in 12-well plates were infected with 3×106 ffu recombinant virus at 37°C in serum-free media. After 1 h, inoculum was replaced with RPMI supplemented with 5% FBS and penicillin-streptomycin and incubation was continued at 34°C. After 48 h, the cells were washed in PBS, lysed on ice in RIPA buffer (25 mM Tris pH 7.5, 150 mM NaCl, 1% NP-40, 0.4% sodium deoxycholate, 1 mM EDTA) containing 1× protease inhibitor cocktail (Sigma), and centrifuged at 12,000×g for 10 min. The protein concentration in the supernatant was determined using a BCA kit (Pierce, 23227) and the supernatants were denatured with urea buffer (125 mM Tris–HCl pH 6.8, 8 M urea, 4% sodium dodecyl sulfate, 5% beta-mercaptoethanol, 0.02% bromophenol blue) at 56°C. Five micrograms of protein were resolved on an SDS-10% polyacrylamide gel and transferred to a nitrocellulose membrane in Towbin buffer (192 mM glycine, 25 mm Tris, 20% methanol). The membrane was then blocked in TBST (100 mM Tris-HCl pH7.9, 150 mM NaCl, 0.01% Tween20) containing 5% dried milk at 4°C for several hours. After blocking, the membrane was incubated overnight with rabbit anti-Cre polyclonal antibody (Novagen, 69050) at a dilution of 1∶10,000, anti-RABV serum from reconvalescent RABV-infected mice diluted 1∶6,000, and a mouse monoclonal antibody against Actin (Sigma, A5441), all diluted 1∶250,000 in TBST containing 5% BSA. After washing, the blot was incubated for 1 h in anti-rabbit-HRP conjugate and anti-mouse-HRP conjugate, both diluted 1∶50,000 in blocking buffer. Bands were developed with SuperSignal West Pico Chemiluminescent substrate (Pierce, 34080).
Immediately after dissection, the mouse brains were bisected laterally using a sterile scalpel. One half was immediately immersed in RNAlater (Qiagen, 1 mL/100 mg tissue) for the purpose of RNA isolation. The second half was placed in 4% PFA (pH 7.0) for immunohistochemical analysis.
Immediately after dissection, brains were fixed 24 h in 4% paraformaldehyde (pH 7.0) and cryoprotected by sequential saturations in 10%, 20%, and 30% sucrose/PBS (each for 24 h). Samples were embedded, frozen, and cut by the Kimmel Cancer Center's Pathology Core Facility. Brains were embedded in Tissue-Tek O.C.T. compound (Sakura), frozen and cut at −20°C on a Microm HM550 cryostat (Thermo Scientific) into 10 µm sections, and mounted onto charged slides (Thermo Scientific Superfrost Plus). Slides were stored at −20°C and either directly imaged or stained for cell- and virus-specific antigens and then imaged. In preparation for staining, sections were permeabilized in 0.2% TritonX-100/PBS for 1 h at room temperature (RT), washed in 0.05% TritonX-100/PBS (wash buffer), and blocked in wash buffer supplemented with 5% BSA. For neuronal staining, slides were stained with a 1∶100 dilution of mouse anti-NeuN (MAB377; Millipore), washed 3×, stained with 1∶300 dilution of Pacific Blue goat anti-mouse (P-10993; Invitrogen). For astrocyte staining, slides were stained with a 1∶250 dilution of rabbit anti-GFAP (NB300-141; Novus), washed 3×, stained with 1∶300 dilution of Pacific Blue goat anti-rabbit (P-10994; Invitrogen). For RABV P staining, slides were directly stained with a 1∶300 dilution of AlexaFluor647 mouse anti-RABV P antibody. This antibody was generated by conjugating AF647 (A20173; Invitrogen) to purified RABV P-specific IgG produced from hybridoma cells kindly provided by Dr. Danielle Blondel, Gif sur Yvette, France . Specifically, antibody-containing supernatant was purified using Nunc ProPur Midi G Kit, dialyzed in PBS, and conjugated. Images were acquired using a Leica DM5000B fluorescence microscope equipped with the DFC340FX camera or a Zeiss LSM 510 META Confocal microscope.
Brain tissues immersed in RNAlater were transferred to RLT Buffer (Qiagen) supplemented with beta-mercaptoethanol (10 µL BME/1 mL RLT) at a ratio of 100 µL RLT-BME per 10 mg tissue. Tissue was homogenized with Hard Tissue Omni Tip probes (Omni International). RNA was isolated using the RNAeasy Mini Kit (Qiagen) according to the manufacturer's protocol. A 15 min on-column DNaseI digest (Qiagen) was included for all samples during the purification. RNA concentration and purity were determined using the NanoDrop 2000c (Thermo Scientific).
Reverse transcription and real-time quantitative PCR
RNA was reverse transcribed into cDNA using the Omniscript Reverse Transcription Kit (Qiagen) according to the manufacturer's protocol. Each 20 µL reaction contained 2 µg of purified RNA, 10 units RNaseOut ribonuclease inhibitor (Invitrogen), and 0.5 µM primer. Reaction mixtures were incubated at 37°C for 1 h, followed by 5 min at 95°C to inactivate the enzyme. All primers/probes used throughout were designed using Sigma-Aldrich's OligoArchitect and purchased from Sigma-Genosys. The following reverse transcription primers were used, 5′ to 3′: RV-N genome (CAT GGA ACT GAC AAG AGA), messenger RNA (for subsequent QPCR of RV-N sense message; TTT TTT TTT TTT TTT TTT TTV; V = G, C, or A), EGFP (CGG ATC TTG AAG TTC ACC), RPL13A housekeeping gene (CTT TTC TGC CTG TTT CCG TA; part of MHK-1 primer set from RealTimePrimers.com). Quantitative analysis of all genes was conducted on the MX3005P QPCR Machine (Agilent Technologies). All genes (except RPL13A, described below) were quantified using the QuantiFast Probe PCR Kit containing ROX internal reference dye (Qiagen, 204256) according to the manufacturer's protocol. Each of these 20 µL reactions contained 2 µL of the reverse transcription reaction, 0.4 µM each primer, and 0.2 µM TaqMan probe. QPCR cycling began with one hot start cycle of 95°C for 15 min, followed by 45 amplification cycles of 95°C for 15 sec, and 60°C for 1 min (data acquired at end of each step). RPL13A was quantified using Brilliant II SYBR Green QPCR Master Mix (Agilent; 600828) according to the manufacturer's protocol. Each of these 20 µL reactions contained 2 µL of the reverse transcription reaction and 0.1 µM each primer. QPCR cycling began with one cycle of 95°C for 15 min, followed by 45 cycles of 95°C for 30 sec, 58°C for 1 min (data acquired at end of this step), and 72°C for 30 sec. Sequences of the QPCR forward primer, reverse primer, and TaqMan probe (respectively) are as follows, 5′ to 3′: RV-N anti-sense genome and RV-N sense message (CAT GGA ACT GAC AAG AGA, TGC TCA ACC TAT ACA GAC, [6-FAM]ATG CGT CCT TAG TCG GTC TTC TC[TAMRA]), EGFP (AGC TGG AGT ACA ACT ACA, CGG ATC TTG AAG TTC ACC, [6-FAM]ATG CCG TTC TTC TGC TTG TCG[TAMRA]), RPL13A housekeeping gene (ATG ACA AGA AAA AGC GGA TG, CTT TTC TGC CTG TTT CCG TA, [no probe]; primers from MHK-1 primer set from RealTimePrimers.com). Primer pairs for all genes were validated by measuring product linearity (R2>0.99) and amplification efficiency (E = 98–102%). SYBR Green reactions were further validated for specificity by running dissociation curves after quantification (using default program on MX3005P) and by running PCR products on 2.5% agarose gel. All samples were run in triplicate alongside negative controls (water and No RT). For absolute quantification of RV-N anti-sense genome and RV-N sense message, an eight point standard curve was generated from 10-fold serial dilutions of cDNA of known copy number (ranging 108 to 101 transcripts). Copy numbers were normalized to RPL13A housekeeping gene. For relative quantification of EGFP, the DDCt method  was used to measure fold-change of EGFP relative to RPL13A housekeeping gene.
Brain tissue dissociation and EGFP+ FACS purification
Whole brains with olfactory bulbs attached were dissected from adult (>8 wks) Cre reporter mice and dissociated using a well-described protocol adapted from Huettner and Baughman , . Brain tissue was minced into 3- to 4-mm pieces in Earle's Balanced Salt Solution (EBSS, HyClone, SH3002902). Papain enzyme (Worthington Biochemical, LS003126) was preactivated in EBSS/0.5 mM EDTA/1 mM L-cysteine by incubating 10 min at 37°C. Minced tissue was incubated in 20 units/mL preactivated papain and 125 units/mL DNase I (Worthington Biochemical, LS002006) for 85 min in a 37°C water bath, triturating gently with a 10 mL pipette twice throughout the incubation. The cell suspension was passed through a 70 µm filter, spun at 300×g for 5 min, and resuspended in 3 mL of dilute protease inhibitor solution (EBSS, 1 mg/mL ovomucoid inhibitor [Worthington Biochemical, LS003085], 1 mg/mL BSA, 125 units/mL DNase I). A discontinuous density gradient was made by layering the cell suspension on top of 5 mL concentrated protease inhibitor (EBSS, 10 mg/mL ovomucoid inhibitor, 10 mg/mL BSA) and centrifuging at 70×g for 8 min to separate cells (pellet) from debris (supernatant). Cells were washed once in PBS supplemented with 2% BSA, and FACS-purified based on EGFP and TdTomato fluorescence utilizing a Coulter MoFlo sorter. EGFP-positive and EGFP-negative populations were saved for RNA extraction.
RNA purification and cDNA amplification
RNA was isolated using the RNAeasy Mini Kit (Qiagen) according to the manufacturer's protocol. RNA was quantified on a NanoDrop 2000c (Thermo Scientific), followed by RNA quality assessment on an Agilent 2100 Bioanalyzer (Agilent, Palo Alto, CA, USA). Amplification and labeling was performed using the Ovation Pico WTA-system V2 RNA amplification system (NuGen Technologies, Inc.). Briefly, 50 ng of total RNA was reverse transcribed using a chimeric cDNA/mRNA primer, and a second complementary cDNA strand was synthesized. Purified cDNA was then amplified with ribo-SPIA enzyme and SPIA DNA/RNA primers (NuGEN Technologies, Inc.). Amplified DNA was purified with Qiagen MinElute reaction cleanup kit. The concentration of Purified ST-cDNA was measured using the Nanodrop. 2.5 µg ST-cDNAs were fragmented and chemically labeled with biotin to generate biotinylated ST-cDNA using FL-Ovation cDNA biotin module V2 (NuGen Technologies, Inc.).
Affymetrix gene chips, mouse gene 1.0 ST array (Affymetrix, Santa Clara, CA), were hybridized with fragmented and biotin-labeled target (2.5 µg) in 110 µl of hybridization cocktail. Target denaturation was performed at 99°C for 2 min and then 45°C for 5 min, followed by hybridization for 18 h. Arrays were then washed and stained using Genechip Fluidic Station 450, and hybridization signals were amplified using antibody amplification with goat IgG (Sigma-Aldrich) and anti-streptavidin biotinylated antibody (Vector Laboratories, Burlingame, CA, USA). Chips were scanned on an Affymetrix Gene Chip Scanner 3000, using Command Console Software. Background correction and normalization were done using Iterative Plier 16 with GeneSpring V11.5 software (Agilent, Palo Alto, CA, USA). 1.5-fold differentially expressed gene list was generated. The differentially expressed gene list was loaded into Ingenuity Pathway Analysis (IPA) 5.0 software (http://www.ingenuity.com) to perform biological network and functional analyses. The microarray data can be accessed at the GEO - repository access number GSE38975 (http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE38975)
Fluorescence-activated cell sorting (FACS) of brain cells isolated from infected or naive Cre reporter mice three months post-infection. EGFP+ cells were collected from the “infected” gate and used for gene expression analysis.
Microarray analysis of RABV-infected neurons 3 months after infection. Our analysis identified 1248 genes differentially expressed between the sorted groups (infected vs. uninfected, ≥1.5 fold change, p<0.05), 361 genes of which were down-regulated, 887 genes that were up-regulated. Gene expression levels ranged from 3.09-fold up-regulation to 2.72-fold down-regulation.
Microarray analysis of RABV-infected neurons 3 months after infection. The table shows “neuron-specific genes” up- or down-regulated in RABV infected Cre-mice.
The authors want to thank Dr. Maria Yolanda Covarrubias of the Bioimaging Facility and Matthew Farabaugh of the Flow Cytometry Facility, Kimmel Cancer Center, JMC, TJU.
Conceived and designed the experiments: MJS EAG GFR CW. Performed the experiments: EAG CW SA. Analyzed the data: EAG MJS GFR CW SA. Contributed reagents/materials/analysis tools: EAG MJS GFR CW SA. Wrote the paper: EAG MJS GFR.
- 1. Jackson AC, Randle E, Lawrance G, Rossiter JP (2008) Neuronal apoptosis does not play an important role in human rabies encephalitis. J Neurovirol 14: 368–375.
- 2. Suja MS, Mahadevan A, Madhusudana SN, Shankar SK (2011) Role of apoptosis in rabies viral encephalitis: a comparative study in mice, canine, and human brain with a review of literature. Patholog Res Int 2011: 374286.
- 3. Tishon A, Lewicki H, Rall G, Von Herrath M, Oldstone MB (1995) An essential role for type 1 interferon-gamma in terminating persistent viral infection. Virology 212: 244–250.
- 4. Hooper DC, Morimoto K, Bette M, Weihe E, Koprowski H, et al. (1998) Collaboration of antibody and inflammation in clearance of rabies virus from the central nervous system. J Virol 72: 3711–3719.
- 5. Parra B, Hinton DR, Marten NW, Bergmann CC, Lin MT, et al. (1999) IFN-gamma is required for viral clearance from central nervous system oligodendroglia. J Immunol 162: 1641–1647.
- 6. Burdeinick-Kerr R, Griffin DE (2005) Gamma interferon-dependent, noncytolytic clearance of sindbis virus infection from neurons in vitro. J Virol 79: 5374–5385.
- 7. Hooper DC, Phares TW, Fabis MJ, Roy A (2009) The production of antibody by invading B cells is required for the clearance of rabies virus from the central nervous system. PLoS Negl Trop Dis 3: e535.
- 8. Wang ZW, Sarmento L, Wang Y, Li XQ, Dhingra V, et al. (2005) Attenuated rabies virus activates, while pathogenic rabies virus evades, the host innate immune responses in the central nervous system. J Virol 79: 12554–12565.
- 9. Zhao P, Zhao L, Zhang T, Qi Y, Wang T, et al. (2011) Innate immune response gene expression profiles in central nervous system of mice infected with rabies virus. Comp Immunol Microbiol Infect Dis 34: 503–512.
- 10. Sugiura N, Uda A, Inoue S, Kojima D, Hamamoto N, et al. (2011) Gene Expression Analysis of Host Innate Immune Responses in the Central Nervous System following Lethal CVS-11 Infection in Mice. Jpn J Infect Dis 64: 463–472.
- 11. Scott CA, Rossiter JP, Andrew RD, Jackson AC (2008) Structural abnormalities in neurons are sufficient to explain the clinical disease and fatal outcome of experimental rabies in yellow fluorescent protein-expressing transgenic mice. J Virol 82: 513–521.
- 12. Jackson AC, Kammouni W, Zherebitskaya E, Fernyhough P (2010) Role of oxidative stress in rabies virus infection of adult mouse dorsal root ganglion neurons. J Virol 84: 4697–4705.
- 13. Sarmento L, Tseggai T, Dhingra V, Fu ZF (2006) Rabies virus-induced apoptosis involves caspase-dependent and caspase-independent pathways. Virus Res 121: 144–151.
- 14. Thoulouze MI, Lafage M, Montano-Hirose JA, Lafon M (1997) Rabies virus infects mouse and human lymphocytes and induces apoptosis. J Virol 71: 7372–7380.
- 15. Morimoto K, Hooper DC, Spitsin S, Koprowski H, Dietzschold B (1999) Pathogenicity of different rabies virus variants inversely correlates with apoptosis and rabies virus glycoprotein expression in infected primary neuron cultures. J Virol 73: 510–518.
- 16. Guigoni C, Coulon P (2002) Rabies virus is not cytolytic for rat spinal motoneurons in vitro. J Neurovirol 8: 306–317.
- 17. Prehaud C, Lay S, Dietzschold B, Lafon M (2003) Glycoprotein of nonpathogenic rabies viruses is a key determinant of human cell apoptosis. J Virol 77: 10537–10547.
- 18. Prehaud C, Wolff N, Terrien E, Lafage M, Megret F, et al. (2010) Attenuation of rabies virulence: takeover by the cytoplasmic domain of its envelope protein. Sci Signal 3: ra5.
- 19. Gourmelon P, Briet D, Court L, Tsiang H (1986) Electrophysiological and sleep alterations in experimental mouse rabies. Brain Res 398: 128–140.
- 20. Gourmelon P, Briet D, Clarencon D, Court L, Tsiang H (1991) Sleep alterations in experimental street rabies virus infection occur in the absence of major EEG abnormalities. Brain Res 554: 159–165.
- 21. Dhingra V, Li X, Liu Y, Fu ZF (2007) Proteomic profiling reveals that rabies virus infection results in differential expression of host proteins involved in ion homeostasis and synaptic physiology in the central nervous system. J Neurovirol 13: 107–117.
- 22. Tsiang H (1982) Neuronal function impairment in rabies-infected rat brain. J Gen Virol 61(Pt 2): 277–281.
- 23. Bouzamondo E, Ladogana A, Tsiang H (1993) Alteration of potassium-evoked 5-HT release from virus-infected rat cortical synaptosomes. Neuroreport 4: 555–558.
- 24. Ceccaldi PE, Fillion MP, Ermine A, Tsiang H, Fillion G (1993) Rabies virus selectively alters 5-HT1 receptor subtypes in rat brain. Eur J Pharmacol 245: 129–138.
- 25. Dumrongphol H, Srikiatkhachorn A, Hemachudha T, Kotchabhakdi N, Govitrapong P (1996) Alteration of muscarinic acetylcholine receptors in rabies viral-infected dog brains. J Neurol Sci 137: 1–6.
- 26. Iwata M, Komori S, Unno T, Minamoto N, Ohashi H (1999) Modification of membrane currents in mouse neuroblastoma cells following infection with rabies virus. Br J Pharmacol 126: 1691–1698.
- 27. Muzumdar MD, Tasic B, Miyamichi K, Li L, Luo L (2007) A global double-fluorescent Cre reporter mouse. Genesis 45: 593–605.
- 28. Schnell MJ, Mebatsion T, Conzelmann KK (1994) Infectious rabies viruses from cloned cDNA. EMBO J 13: 4195–4203.
- 29. Gomme EA, Faul EJ, Flomenberg P, McGettigan JP, Schnell MJ (2010) Characterization of a single-cycle rabies virus-based vaccine vector. J Virol 84: 2820–2831.
- 30. McGettigan JP, Pomerantz RJ, Siler CA, McKenna PM, Foley HD, et al. (2003) Second-generation rabies virus-based vaccine vectors expressing human immunodeficiency virus type 1 gag have greatly reduced pathogenicity but are highly immunogenic. J Virol 77: 237–244.
- 31. Wirblich C, Tan GS, Papaneri A, Godlewski PJ, Orenstein JM, et al. (2008) PPEY motif within the rabies virus (RV) matrix protein is essential for efficient virion release and RV pathogenicity. J Virol 82: 9730–9738.
- 32. Park CH, Kondo M, Inoue S, Noguchi A, Oyamada T, et al. (2006) The histopathogenesis of paralytic rabies in six-week-old C57BL/6J mice following inoculation of the CVS-11 strain into the right triceps surae muscle. J Vet Med Sci 68: 589–595.
- 33. Phares TW, Kean RB, Mikheeva T, Hooper DC (2006) Regional differences in blood-brain barrier permeability changes and inflammation in the apathogenic clearance of virus from the central nervous system. J Immunol 176: 7666–7675.
- 34. Preuss MA, Faber ML, Tan GS, Bette M, Dietzschold B, et al. (2009) Intravenous inoculation of a bat-associated rabies virus causes lethal encephalopathy in mice through invasion of the brain via neurosecretory hypothalamic fibers. PLoS Pathog 5: e1000485.
- 35. Ugolini G (1995) Specificity of rabies virus as a transneuronal tracer of motor networks: transfer from hypoglossal motoneurons to connected second-order and higher order central nervous system cell groups. J Comp Neurol 356: 457–480.
- 36. Rutherford M, Jackson AC (2004) Neuronal apoptosis in immunodeficient mice infected with the challenge virus standard strain of rabies virus by intracerebral inoculation. J Neurovirol 10: 409–413.
- 37. Sur JH, Allende R, Doster AR (2003) Vesicular stomatitis virus infection and neuropathogenesis in the murine model are associated with apoptosis. Vet Pathol 40: 512–520.
- 38. Samuel MA, Morrey JD, Diamond MS (2007) Caspase 3-dependent cell death of neurons contributes to the pathogenesis of West Nile virus encephalitis. J Virol 81: 2614–2623.
- 39. Tsutsui Y, Kosugi I, Kawasaki H (2005) Neuropathogenesis in cytomegalovirus infection: indication of the mechanisms using mouse models. Rev Med Virol 15: 327–345.
- 40. Sarmento L, Li XQ, Howerth E, Jackson AC, Fu ZF (2005) Glycoprotein-mediated induction of apoptosis limits the spread of attenuated rabies viruses in the central nervous system of mice. J Neurovirol 11: 571–581.
- 41. Dietzschold B, Li J, Faber M, Schnell M (2008) Concepts in the pathogenesis of rabies. Future Virol 3: 481–490.
- 42. Morimoto K, Foley HD, McGettigan JP, Schnell MJ, Dietzschold B (2000) Reinvestigation of the role of the rabies virus glycoprotein in viral pathogenesis using a reverse genetics approach. J Neurovirol 6: 373–381.
- 43. Pulmanausahakul R, Faber M, Morimoto K, Spitsin S, Weihe E, et al. (2001) Overexpression of cytochrome C by a recombinant rabies virus attenuates pathogenicity and enhances antiviral immunity. J Virol 75: 10800–10807.
- 44. Faber M, Pulmanausahakul R, Hodawadekar SS, Spitsin S, McGettigan JP, et al. (2002) Overexpression of the rabies virus glycoprotein results in enhancement of apoptosis and antiviral immune response. J Virol 76: 3374–3381.
- 45. Dietzschold B, Schnell M, Koprowski H (2005) Pathogenesis of rabies. Curr Top Microbiol Immunol 292: 45–56.
- 46. Yan X, Prosniak M, Curtis MT, Weiss ML, Faber M, et al. (2001) Silver-haired bat rabies virus variant does not induce apoptosis in the brain of experimentally infected mice. J Neurovirol 7: 518–527.
- 47. Wirblich C, Schnell MJ (2011) Rabies virus (RV) glycoprotein expression levels are not critical for pathogenicity of RV. J Virol 85: 697–704.
- 48. Chopy D, Detje CN, Lafage M, Kalinke U, Lafon M (2011) The type I interferon response bridles rabies virus infection and reduces pathogenicity. J Neurovirol 17: 353–367.
- 49. Prehaud C, Megret F, Lafage M, Lafon M (2005) Virus infection switches TLR-3-positive human neurons to become strong producers of beta interferon. J Virol 79: 12893–12904.
- 50. Fernandes ER, de Andrade HF Jr, Lancellotti CL, Quaresma JA, Demachki S, et al. (2011) In situ apoptosis of adaptive immune cells and the cellular escape of rabies virus in CNS from patients with human rabies transmitted by Desmodus rotundus. Virus Res 156: 121–126.
- 51. Li XQ, Sarmento L, Fu ZF (2005) Degeneration of neuronal processes after infection with pathogenic, but not attenuated, rabies viruses. J Virol 79: 10063–10068.
- 52. Dosa S, Castellanos K, Bacsa S, Gagyi E, Kovacs SK, et al. (2011) Chronic progressive deficits in neuron size, density and number in the trigeminal ganglia of mice latently infected with herpes simplex virus. Brain Pathol 21: 583–593.
- 53. Simon ID, van Rooijen N, Rose JK (2010) Vesicular stomatitis virus genomic RNA persists in vivo in the absence of viral replication. J Virol 84: 3280–3286.
- 54. Cermelli C, Jacobson S (2000) Viruses and multiple sclerosis. Viral Immunol 13: 255–267.
- 55. Brendza RP, Bacskai BJ, Cirrito JR, Simmons KA, Skoch JM, et al. (2005) Anti-Abeta antibody treatment promotes the rapid recovery of amyloid-associated neuritic dystrophy in PDAPP transgenic mice. J Clin Invest 115: 428–433.
- 56. Zhu B, Luo L, Moore GR, Paty DW, Cynader MS (2003) Dendritic and synaptic pathology in experimental autoimmune encephalomyelitis. Am J Pathol 162: 1639–1650.
- 57. Springer ML, Rando TA, Blau HM (2002) Gene delivery to muscle. Curr Protoc Hum Genet Chapter 13: Unit13 14.
- 58. Raux H, Iseni F, Lafay F, Blondel D (1997) Mapping of monoclonal antibody epitopes of the rabies virus P protein. J Gen Virol 78 (Pt 1): 119–124.
- 59. Bookout AL, Cummins CL, Mangelsdorf DJ, Pesola JM, Kramer MF (2006) High-throughput real-time quantitative reverse transcription PCR. Curr Protoc Mol Biol Chapter 15: Unit 15 18.
- 60. Huettner JE, Baughman RW (1986) Primary culture of identified neurons from the visual cortex of postnatal rats. J Neurosci 6: 3044–3060.
- 61. Lobo MK, Karsten SL, Gray M, Geschwind DH, Yang XW (2006) FACS-array profiling of striatal projection neuron subtypes in juvenile and adult mouse brains. Nat Neurosci 9: 443–452.