key: cord-0783402-k8u7i5ki
authors: Ren, Meishen; Mei, Hong; Zhou, Jiaojiao; Zhou, Ming; Han, Heyou; Zhao, Ling
title: Early diagnosis of rabies virus infection by RPA-CRISPR techniques in a rat model
date: 2021-02-05
journal: Arch Virol
DOI: 10.1007/s00705-021-04970-x
sha: b6290b0018e0125cb6a61cedf5d65998813bea85
doc_id: 783402
cord_uid: k8u7i5ki

Rabies, which is caused by rabies virus (RABV), poses an ever-present threat to public health in most countries of the world. Once clinical signs appear, the mortality of rabies approaches 100%. To date, no effective method for early rabies diagnosis has been developed. In this study, an RPA-CRISPR nucleic-acid-based assay was developed for early rabies diagnosis by detecting viral RNA shedding in the cerebrospinal fluid (CSF) of rats. This method can detect a single copy of RABV genomic RNA in 1 μL of liquid. RABV genomic RNA released from viral particles in the CSF could be detected via RPA-CRISPR as early as 3 days postinfection in a rat model. This study provides an RPA-CRISPR technique for early detection of RABV with potential application in the clinical diagnosis of human rabies.

Rabies is an old infectious disease with clinical signs of lethal encephalitis that poses a threat to public health worldwide [1] . More than 59,000 people reportedly die from rabies every year [2] . The disease is caused by rabies virus (RABV), a neurotropic virus belonging to the genus Lyssavirus in the family Rhabdoviridae that has a negative-sense single-stranded RNA genome that encodes five structural proteins.

In cases of rabies, the time between infection and the onset of signs is variable. Since its early clinical signs are often nonspecific, RABV infection may go undetected until the virus reaches the central nervous system (CNS) [3] . After being introduced by a bite from a rabid animal, RABV may maintain a low level of replication in muscle cells [4, 5] before moving to the peripheral nervous system (PNS) and interacting with cell receptors, including the nicotinic acetylcholine receptor (nAChR), the neuronal cell adhesion molecule (NCAM), and the low-affinity nerve growth factor receptor (p75NTR) [6] [7] [8] [9] [10] . After invading the PNS by retrograde axonal transport, RABV replicates in the motor neurons of the spinal cord, finally entering the CNS [11] . Once the virus has entered the brain, there is no effective treatment, and mortality is 100%, except for a few individual cases described in the literature [12] [13] [14] [15] .

Direct fluorescent antibody (DFA) and direct rapid immunohistochemistry (dRIT) tests are the primary diagnostic assays for RABV antigen identification in the CNS [16, 17] . RT-PCR and qPCR are also widely used, and their sensitivity and specificity for RABV are similar to those of DFA or dRIT [18] [19] [20] . These assays are reliable for detecting RABV in samples from hosts with mild-to-severe neurological signs [21] [22] [23] . However, they may not be sensitive enough to detect RABV in samples with low viral loads, particularly in the early stage of RABV infection.

Recently, recombinase polymerase amplification (RPA) and CRISPR-LwCas13a collateral cleavage were combined to develop a highly sensitive nucleic acid detection method [24] . This combination assay was found to be capable of detecting Zika virus (ZIKV) at concentrations as low as 2 aM without compromising specificity [24] . This detection method has also been termed as "specific high-sensitivity enzymatic reporter unlocking" (SHERLOCK). HUD-SON (heating unextracted diagnostic samples to obliterate nucleases), a kind of sample treatment method, can be paired with RPA-CRISPR for viral detection directly from bodily fluids. Employing RPA-CRISPR in combination with HUD-SON has allowed the direct detection of ZIKV from clinical samples of serum, urine, and saliva at concentrations as low as 3.2 aM (2 copies/μL) [24] . To overcome the limitation of sensitivity, in the present study, an RPA-CRISPR detection method was applied for the early diagnosis of RABV infection. We applied the RPA-CRISPR technique to detect RABV before it reaches the brain in a rat model. Our study indicates that RPA-CRISPR is a reliable tool for the early diagnosis of RABV infection. This method has potential application for the early diagnosis of RABV infection in mammals, especially humans, and will provide a basis for timely clinical treatment for rabies.

CVS-B2c is an attenuated RABV strain that was derived from the mouse-adapted rabies strain CVS-24 by serial passaging in BHK-21 cells. RABV SAD-B19 is a widely used vaccine strain. DRV-Mexico is a wild-type RABV strain isolated from a rabid dog in Mexico. SHBRV is a bat-associated RABV strain isolated from a human patient. DRV-AH08 is a wild-type RABV strain isolated from a rabid dog from Anhui Province, China. DRV-HuNPN01 is a wildtype RABV strain isolated from a rabid pig from Hunan Province, China. References for the above RABV strains are listed in Table 1 . Canine distemper virus (CDV) and canine parvovirus (CPV) were obtained from the animal hospital of Huazhong Agricultural University, Wuhan, China. Vesicular stomatitis virus (VSV) and Sendai virus (SeV) were obtained from Dr. Mingzhou Chen, Wuhan University, China. Japanese encephalitis virus (JEV) was obtained from Dr. Shengbo Cao, Huazhong Agricultural University, China.

Mouse neuroblastoma (NA) cells were cultured in Dulbecco's modified Eagle's medium (DMEM) (Gibco, Grand Island, NY) containing 12% fetal bovine serum (FBS) (Gibco). BSR cells, derived from BHK-21 cells, were maintained in DMEM containing 10% FBS. Human embryonic kidney 293T cells (HEK-293T) were cultured in DMEM containing 10% FBS.

An RABV-P-protein-specific monoclonal antibody was prepared in our laboratory as described previously [25] . Plasmid pC013-Twinstrep-SUMO-huLwCas13a (a LwCas13a bacterial expression vector) was obtained from Addgene (Addgene plasmid # 90097; http://n2t.net/addge ne:90097 ; RRID: Addgene_90097) [24] . RABV CVS-B2c genomic backbone plasmid and helper plasmids were prepared in our laboratory as described previously [26] .

Six-week-old female specific-pathogen-free (SPF) Sprague-Dawley (SD) rats were purchased from the Hubei Center for Disease Control, Wuhan, China. All animal experiments were performed in accordance with the Ministry of Science and Technology of China protocol for the care and use of laboratory animals and approved by the Scientific Ethics Committee of Huazhong Agricultural University (permit number HZAURA-2018-012).

E. coli BL21 (DE3) competent cells were transformed with the plasmid pC013-Twinstrep-SUMO-huLwCas13a and grown in LB medium (10 g of tryptone, 5 g of yeast extract, and 10 g of NaCl per liter; Sigma) at 37 °C until reaching an OD 600 of 0.6. Protein expression was then induced with 500 µM IPTG (Invitrogen), and the cells were incubated for an additional 16 h at 18 °C. Cells were collected by centrifugation, resuspended in lysis buffer (20 mM Tris-HCl, 500 mM NaCl, pH 8.0) containing protease inhibitors (cOmplete™ Protease Inhibitor Cocktail, Roche) and then lysed using a nano homogenizer (ATS Engineering Inc.) at a pressure of 600 bar. After the lysate was centrifuged for 50 min at 13,000 × g, the supernatant was collected and filtered using a 0.22-μm filter (Millipore). The filtrate was purified using an NGC Quest 100 protein purification system (Bio-Rad) fitted with a HisTrap FF Column (GE Healthcare Life Sciences). The purified protein was digested by SUMO protease (Invitrogen) overnight at 4 °C and then further purified using a Superdex® 200 gel filtration column (GE Healthcare Life Sciences). After the fractions of interest were identified by SDS-PAGE, the fractionation buffer was replaced with storage buffer (600 mM NaCl, 50 mM Tris-HCl, 5% glycerol, pH 7.5), and the fractions were stored at − 80 °C until use. 

The RPA forward primer contained a T7 transcription region and the target region 

For direct detection of RABV viral genomic RNA (vRNA) released from viral particles in cerebrospinal fluid (CSF) samples, the HUDSON method was used to lyse viral particles and inactivate ribonucleases [27] . Tris (2-carboxyethyl) phosphine hydrochloride (Sigma) and EDTA (Sigma) were added to a single CSF solution containing RABV particles to a final concentration of 100 mM and 1 mM, respectively. Inactivation for 20 min at 50 °C was followed by lysis for 5 min at 95 °C in a thermocycler. The sample solution was used directly as template for RPA-CRISPR.

The qPCR protocol was developed according to some wellestablished qPCR methods and a recommended assay in the OIE Terrestrial Manual [18, 28, 29] . vRNA was extracted using TRIzol Reagent (Invitrogen) and was reverse transcribed into cDNA using an FSQ-201 ReverTra Ace kit (TOYOBO). RABV vRNA levels were quantified using the forward primer 5'-AGC ATA CAG GCT TGA CTC CG-3' and the reverse primer 5'-ACA TCC AAG AGG CTC AAA ATGT-3', which anneal to the noncoding regions of the RABV genome. The forward primer 5'-AGA GCA GAT TTT CGA GAC AGC-3' and the reverse primer 5'-GGT TCC GGC CAA AAA TCT GAA-3' were used to quantify the transcribed ssRNA; each 10-μL reaction consisted of 5 μL of 2× SYBR Green (Bio-Rad), 1 μL of forward primer (0.75 μM), 1 μL of reverse primer (0.75 μM), 1 µL of cDNA template, and 2 µL of ddH 2 O. All reactions were performed on a CFX96 Real-Time System (Bio-Rad) using the following conditions: 95 °C for 5 min, followed by 40 cycles of 95 °C for 15 s and 60 °C for 30 s.

Viral titers were determined by DFA. Briefly, tenfold serial dilutions of viral supernatant were inoculated onto BSR cells in 96-well plates in quadruplicate and then incubated for 48 h at 37 °C. Cells were fixed with 80% acetone and then incubated with an FITC-conjugated P-protein-specific mouse monoclonal antibody (1:500) for 1 h at 37 °C. Antigen-positive cells were visualized using an IX51 Olympus fluorescence microscope. Virus titers were calculated and presented as numbers of focus-forming units per milliliter (FFU/ml) as described previously [12] .

Thirty-three six-week-old female rats were randomly divided into 11 groups with three rats per group. Five groups of rats were inoculated intramuscularly (i.m.) with 100 times the 50% lethal dose (LD 50 ) of RABV-CVS in 100 μL of DMEM. Another five groups were i.m. inoculated with 100× LD 50 of RABV-DRV in 100 μL of DMEM. One group of rats was i.m. injected with 100 μL of saline as a mock-infection control. From 3 to 7 days post infection (dpi), one group of RABV-infected rats was taken every other day to collect CSF (50 μL per rat) for early diagnosis by RPA-CRISPR test.

GraphPad Prism 8 (GraphPad Software, Inc., CA) was used for data analysis. An unpaired two-tailed Student's t-test was used to test for significant differences. Kaplan-Meier survival curves were used to determine the statistical significance of the survivor ratio in the LD 50 assays. Statistically significant differences are denoted as *, P < 0.05; **, P < 0.01; ***, P < 0.001; and ****, P < 0.0001.

RPA-CRISPR consists of recombinase polymerase amplification (RPA) followed by T7 transcription and collateral cleavage by CRISPR-LwCas13a (Fig. 1A) . The optimal amounts of crRNA and CRISPR-LwCas13a, determined by titration, were 480 ng of crRNA mixture (Fig. 1B) and 1400 ng of CRISPR-LwCas13a protein per tube (Fig. 1C) .

The limits of detection for RPA-CRISPR and qPCR were determined using serial dilutions of RABV genomic RNA (vRNA) and ssRNA. ssRNA was transcribed from a 1353-bp dsDNA fragment within the coding sequence of the RABV N protein. RPA-CRISPR was sensitive to 1 copy/μL for both vRNA and ssRNA ( Fig. 2A and B) , and qPCR was sensitive to 100 copies/μL for vRNA (Fig. 2C ) and 10 copies/μL for ssRNA (Fig. 2D) .

For RPA-CRISPR detection, the HUDSON method was used to release viral RNA from viral particles in CSF samples [27] . Both RABV vRNA and viral particles were serially diluted tenfold using CSF collected from SD rats as dilution buffer and subjected to RPA-CRISPR. The results revealed that the level of sensitivity of RPA-CRISPR to vRNA and viral particles was 10 0.5 copies/μL and 10 0.5 FFU/μL, respectively ( Fig. 3A and B) .

To evaluate the specificity of RPA-CRISPR, six RABV strains (CVS-B2c, SAD-B19, SHBRV, DRV-Mexico, DRV-AH08, and DRV-HuNPN01), five other RNA viruses (CDV, CPV, SeV, JEV, VSV), and two mock-infected cell types (293T and NA) were used as templates for RPA-CRISPR detection. The crRNA mixture was composed so as to ensure that all RABV strains could be detected, with complementary sequences of the RABV strains included in the crRNA mixture with no mismatch in the target regions of standard RABV strains or wild-type strains ( Table 1 ). The results showed that RPA-CRISPR accurately detected the RABV strains with no cross-reactivity (Fig. 3C ).

Early diagnosis of rabies is a prerequisite for timely treatment but remains a large challenge for researchers. Thus, we tested the ability of RPA-CRISPR to achieve early detection in a rat model. A schematic of the strategy is shown in Fig. 4A . CSF samples from RABV-infected or mock-infected rats were collected on the indicated days post infection and subjected to RPA-CRISPR. The results showed that RABV-CVS and RABV-DRV strains were detected as early as 3 dpi by RPA-CRISPR ( Fig. 4B and C) . However, by the qPCR method, the earliest that RABV was detected in CSF was 5 dpi ( Table 2 ). The rats used for RPA-CRISPR were housed until clinical signs of rabies infection were evident, at which point they were euthanized, and their brains were collected for RABV vRNA detection by qPCR (Table 3 ).

There remain numerous limitations to the early diagnosis of rabies. Before invading the brain, RABV replicates slowly, making it difficult to detect by traditional methods. Due to its high sensitivity, RPA-CRISPR has been increasingly used for detecting nucleic acids of viruses, parasites, and cancer cells [24, [30] [31] [32] [33] [34] [35] . Most recently, RPA-CRISPR was applied to the diagnosis of infection with the betacoronavirus severe acute respiratory syndrome coronavirus 2 (SARS-CoV-2) [36] [37] [38] . Some extended applications have been described, such as field-deployable diagnostics, single-nucleotide polymorphism (SNP) detection, miRNA quantification, and species identification in ecological studies [24, 27, 39, 40] . In this study, an RPA-CRISPR method was developed for the early diagnosis of RABV infection in a rat model.

Because of its high specificity and reliability, the direct fluorescent antibody test is the gold standard assay for rabies diagnosis [17] . The sensitivity of the DFA test depends on the freshness of the specimen and the degree of autolysis. In many cases, the sensitivity of the DFA test is lower than that of PCR and qPCR [41] . Conventional PCR and qPCR used for measuring viral RNA have detection limits ranging from 10 2 copies/μL to 10 1 copies/μL [18, 29] . In contrast, the RPA-CRISPR method developed in this study is very sensitive and can detect viral RNA at concentrations as low as a single copy per microliter.

As we reported previously, mild clinical signs such as weight loss began to appear at 6 or 7 dpi [25] in RABVinfected mice. By that time, the virus had already invaded the brain. Early diagnosis may allow for the timely initiation of appropriate treatment and increase the chance of recovery. For early diagnosis, RPA-CRISPR or other methods targeting either viral RNA or viral antigens could be used. However, the viral load in the early stage of infection is ng, 1050 ng, 1400 ng, 1750 ng, 2100 ng, 2450 ng) were used for optimizing the RPA-CRISPR reaction system. PBS was used as a control in the NTC groups. The bar graph shows the mean ± stardard deviation (SD) (n = 3). *, P < 0.05; **, P < 0.01; ***, P < 0.001 extremely low. Furthermore, false-negative detection results may be obtained due to the limitation of sensitivity. The RPA-CRISPR system is suitable for testing of low-viral-load samples due to its high sensitivity. According to our results, RPA-CRISPR could detect viral RNA in CSF samples as early as 3 dpi (Fig. 4B) , demonstrating that RPA-CRISPR is a potential tool for early diagnosis of RABV infection.

Despite its superior sensitivity, RPA-CRISPR has some limitations. The RPA amplification component depends on the availability of optimal primers. However, no primer design tool is available to predict the amplification performance in the RPA reaction. Therefore, stringent primer screening should be performed before sample analysis by RPA-CRISPR.

In summary, we report that RPA-CRISPR can accurately detect RABV in the CSF of infected rats during the early stage of infection. RPA-CRISPR has great potential for application in the early diagnosis of RABV infection in mammals, especially humans. Tenfold gradient dilutions of RABV vRNA and ssRNA were used for qPCR sensitivity validation. PBS was used as a control in the NTC groups. The bar graph shows the mean ± SD (n = 3). *, P < 0.05; **, P < 0.01; ***, P < 0.001; ****, P < 0.0001; ns, no significant difference Another five groups of rats were i.m. inoculated with 100 LD 50 of wild-type RABV strain DRV-Mexico (C). The mock infection group was i.m. inoculated with the same volume of DMEM. From 3 to 7 dpi, one group of infected rats was taken every other day to collect CSF (50 μL per rat). At each of the indicated days postinfection, CSF from a group of rats was subjected to RPA-CRISPR analysis. PBS was used as control in the NTC group. The bar graph shows the mean ± standard error (SE) (n = 3). 

The spread and evolution of rabies virus: conquering new frontiers

Rabies as a transneuronal tracer of circuits in the central nervous system

Involvement of the rabies virus phosphoprotein gene in neuroinvasiveness

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Subversion of the immune response by rabies virus

The cell biology of rabies virus: using stealth to reach the brain

The neural cell adhesion molecule is a receptor for rabies virus

Rabies virus receptors

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Immunological aspects of rabies: a literature review

Overexpression of interleukin-7 extends the humoral immune response induced by rabies vaccination

Current status of rabies and prospects for elimination

Cases of human convalescence from rabies and lifetime diagnostics of lyssavirus encephalitis

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Rabies diagnosis for developing countries

Application and comparative evaluation of fluorescent antibody, immunohistochemistry and reverse transcription polymerase chain reaction tests for the detection of rabies virus antigen or nucleic acid in brain samples of animals suspected of rabies in India

Development and validation of sensitive real-time RT-PCR assay for broad detection of rabies virus

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Evaluation of rt-PCR assay for routine laboratory diagnosis of rabies in post mortem brain samples from different species of animals

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Critical role of K1685 and K1829 in the large protein of rabies virus in viral pathogenicity and immune evasion

Field-deployable viral diagnostics using CRISPR-Cas13

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Real-time RT-PCR for the detection of Lyssavirus species

CRISPR-Cas13 precision transcriptome engineering in cancer

Rapid and fully microfluidic ebola virus detection with CRISPR-Cas13a

Visual detection of porcine reproductive and respiratory syndrome virus using CRISPR-Cas13a

Chaijarasphong T (2020) CRISPR-Cas fluorescent cleavage assay coupled with recombinase polymerase amplification for sensitive and specific detection of Enterocytozoon hepatopenaei

High-throughput and all-solution phase African Swine Fever Virus (ASFV) detection using CRISPR-Cas12a and fluorescence based point-of-care system

Dynamic aqueous multiphase reaction system for one-pot CRISPR-Cas12a-based ultrasensitive and quantitative molecular diagnosis

CRISPR-Cas12-based detection of SARS-CoV-2

SARS-CoV-2 detection with CRISPR diagnostics

Clinical validation of a Cas13-based assay for the detection of SARS-CoV-2 RNA

High-fidelity and rapid quantification of miRNA combining crRNA programmability and CRISPR/Cas13a trans-cleavage activity

Rapid and accurate species identification for ecological studies and monitoring using CRISPR-based SHERLOCK

Effects of carcase decomposition on rabies virus infectivity and detection

Rabies virus glycoprotein is an important determinant for the induction of innate immune responses and the pathogenic mechanisms

Molecular cloning and complete nucleotide sequence of the attenuated rabies virus SAD B19

Complete genome sequence of a street rabies virus from Mexico

Identification of viral genomic elements responsible for rabies virus neuroinvasiveness

Complete genome sequence of a street rabies virus isolated from a rabid dog in China

An outbreak of pig rabies in Hunan province

Genealogical analyses of rabies virus strains from Brazil based on N gene alleles

Defining objective clusters for rabies virus sequences using affinity propagation clustering

Molecular inferences suggest multiple host shifts of rabies viruses from bats to mesocarnivores in Arizona during

Host phylogeny constrains cross-species emergence and establishment of rabies virus in bats

The authors declare no potential conflicts of interest with respect to the research, authorship, and/or publication of this article.Ethical approval All animal experiments were performed in accordance with the Ministry of Science and Technology of China protocol for the care and use of laboratory animals and approved by the Scientific Ethics Committee of Huazhong Agricultural University (permit number HZAURA-2018-012).