Background
Severe fever with thrombocytopenia syndrome (SFTS) is an infectious tick-borne disease caused by the SFTS Virus (SFTSV), which emerged in China in 2009 [
1]. Cases present with various clinical signs and symptoms, including fever, thrombocytopenia, leukocytopenia, and gastrointestinal symptoms [
2,
3]. Since the first cases report, SFTS has been reported in most East Asian countries, including Korea and Japan [
4,
5], with increasing frequency [
6‐
8]. In Korea, SFTS was classified as a national legal infectious disease in 2020, and has since been closely monitored [
9]. As such, the rapid and efficient diagnosis of SFTSV has become a national concern along with the development of vaccines and therapeutics.
Initially, SFTSV was classified within the genus Phlebovirus of the family Phenuiviridae, but it was later reclassified into the genus Bandavirus and renamed the
Dabie bandavirus based on the 2020 ICTV (International Committee on Taxonomy of Viruses) taxonomy release [
10,
11]. Regardless, the name SFTSV, derived from the symptoms, is still commonly used among scientists. Similar to viruses in the Phenuiviridae family, the SFTSV is a negative-strand RNA virus that possesses three single-stranded RNA segments: large (L), medium (M), and small (S) [
12,
13]. The L segment encodes an RNA-dependent RNA polymerase (RdRp); the M segment encodes a glycoprotein (Gn,Gc); and the S segment encodes two proteins, a nucleocapsid protein (N) and a non-structural protein (NS).
The N protein is important for virus replication and transcription because it protects the viral RNA through encapsidation [
14‐
17]. The N protein binds with the viral RNA and forms ring-like oligomers that facilitate packing and stabilization of the viral RNA. Furthermore, the N protein plays a critical role in virion assembly by forming a ribonucleoprotein (RNP) with the L protein (RNA polymerase) [
14]. The N protein is the most abundant and highly conserved protein in most viruses [
18‐
20]. Therefore, this protein is often targeted in viral detection assays [
21‐
23]. Various N-protein-based SFTSV detection methods have been developed [
24‐
26]; however, the known methods provide limited information about their antibodies and binding epitopes.
In this study, we postulated that immune response to the SFTSV N protein is limited due to the small size of the SFTSV-N-protein oligomer in native conditions. Therefore, we produced SFTSV-N-protein-specific antibodies to assess the immune response to SFTSV N protein, the antibody binding affinity, and the epitopes involved. We conducted an antibody pair test using the generated antibodies to find the best pairs for SFTSV detection. The results provided important information for future development of more effective methods to diagnose SFTS caused by SFTSV, such as a commercial rapid antigen detection test kit.
Materials and methods
Expression and purification of recombinant full-length and truncated SFTSV N protein
The recombinant SFTSV N protein was cloned into a pET21(a) vector with N-terminal His-tag and expressed in the Rosetta™ 2 (DE3; BL21 derivative) cell line. The transformed cells were induced with IPTG (Isopropyl-ß-D-thio-galactopyranoside) and lysed by sonication in binding buffer (100 mM Tris–HCl, 200 mM NaCl, 10 mM Imidazole, pH 8.0). The total soluble protein was purified using Ni–NTA agarose (Qiagen, Valencia, CA) according to the manufacturer’s recommendations.
Truncated SFTSV N proteins were designed to remove the predicted α–helix from the N-terminus (Additional file
1: Fig. S1) [
27‐
29]. Five N proteins truncated at the N-terminus, dN1(13–256 AA), dN2(33–245 AA), dN3(47–245 AA), dN4(65–245 AA), and dN5(75–245 AA), were cloned into pET21(a) with an N- or C- terminal His-tag for purification and expressed in BL21 or Rosetta cells. The purification procedure was performed as described above. The truncated dN1, dN4, and dN5 proteins were highly soluble, but dN2 and dN3 required solubilization in 0.8 M urea.
SDS-PAGE and native-PAGE
Purified protein samples were separated on 12% polyacrylamide gels and stained using Coomassie brilliant blue R-250 (Sigma-Aldrich, USA). For the native-PAGE, 4–15% polyacrylamide gels and running buffer without SDS were used, and gel runs were performed in ice water.
Western blot analyses
Protein samples were separated by SDS-PAGE and transferred to PVDF (polyvinylidene difluoride) membranes (Invitrogen, USA) for western blotting. An anti-His-tag antibody (Santa Cruz, USA) and the SFTSV-N- protein-specific monoclonal antibodies were used to confirm the immune response to the injected recombinant SFTSV N protein antigen. These primary antibodies were used at 5,000-fold dilution with 3% (w/v) skim milk in PBS. The horseradish-peroxidase (HRP)-conjugated anti-mouse IgG secondary antibody was diluted 10,000-fold with 3% skim milk in PBS. The signals were detected using ECL (Enhanced Chemiluminescence) (GE Healthcare, USA).
Monoclonal antibody production
After mixing the full-length SFTSV N protein (1 mg/mL) with an equal volume of incomplete adjuvant (Sigma, USA), 150 µL of the mixture was injected into each footpad of BALB/c mouse three times at three-week intervals. After immunization, the lymph nodes were collected to obtain B cells that then were fused with Sp2/O myeloma cells to produce hybridoma cells [
30]. The hybridoma cells were incubated for two weeks in a 96-well plate. Cell culture medium containing the antibodies was transferred into a new 96-well plate coated with 1 µg/mL of SFTSV N protein to test their immune responses using an indirect ELISA method. The cells confirmed to produce SFTSV N protein-specific antibodies were processed by serial dilution, transferred to a new 96-well plate, and incubated for one week. The ELISA test was performed again to confirm antibody production by the hybridoma cells. The verified cells were then cultured up to a 250 mL volume through sequential scale-up and were concentrated as appropriate. About 0.5 mL of the antibody-producing hybridoma cells (1 × 10
6) were injected into a BALB/c mouse intraperitoneally, and monoclonal antibodies were harvested and purified from ascites fluid.
Dot blot analysis
Dot blot analysis were conducted to confirm that SFTSV monoclonal antibodies were specific for the native conformation and epitopes of SFTSV N protein. Expressed and purified full-length and truncated SFTSV N protein samples were loaded onto a nitrocellulose membrane. After blocking, each anti-SFTSV primary antibody was applied at a 5000-fold dilution with 3% (w/v) skim milk in PBS. The secondary antibody and detection process were the same as for the western blot procedure.
Indirect ELISA
Recombinant full-length SFTSV N protein (3 µg/mL) was added to 96-well ELISA plates overnight at 4 °C. The plates were washed with PBS-T (0.05%, v/v) and blocked with 3% (w/v) skim milk in PBS for 2 h. After washing out the blocking solution, each SFTSV monoclonal antibody in PBS was added according to a concentration gradient. Anti-His6 antibody and anti-2B8 antibody (Biojane Co., Ltd., South Korea) were used as the positive and negative controls, respectively, for experimental validation. After a 1 h incubation, the plates were washed with PBS-T, HRP-conjugated goat anti-mouse IgG diluted 1:10,000 in PBS was added, and the plates were incubated for 1 h. After washing, TMB (3,3′,5,5′-tetramethylbenzidine) substrate was added for reaction with HRP until it was stopped by addition of sulfuric acid. The optical density of the plate was read at 450 nm using a microplate reader (Thermofisher, USA).
Antibody pair test for diagnosis
A paired-antibody test was performed using the lateral flow immunoassay (LFIA) method. Half-strip testing was carried out in advance using all antibody combinations [
31]. Half-strip testing was performed without a sample and conjugate pad. The test line was coated with each SFTSV antibody as a capture antibody (2 mg/mL), and the control line was coated with goat anti-mouse IgG (2 mg/mL). The assay was performed using 5 µL of each SFTSV antibody conjugated with gold as a detection antibody and mixed with 45 µL of SFTSV N protein (100 ng/mL) or 45 µL of 0.1 M PBS as a negative control (1% Tween-20, pH 7.4). Each strip was dipped in the mixed solution for absorption. After 12 min, the visibility of the red lines on the strips was compared among samples, and their immune responses were analyzed to select good pairs. Selected antibody pairs were made into complete test kits. The full strip had a sample pad and a conjugate pad that held the gold-conjugated SFTSV antibody. The test and control lines of the strip were the same as those of the half strip test. For each pair, three identical kits were prepared and 100 µL of 0.1 M PBS, 1 ng/mL of SFTSV N protein, and 0.1 ng/mL of SFTSV N protein were applied, respectively. After waiting for 12 min, the visibility of the lines on the kits was analyzed.
Sequence alignment and secondary structure depiction
The N protein sequences of three
Bandavirus species were collected from GeneBank; SFTSV (
Dabie bandavirus) (GenBank: KC505125.1),
Guertu bandavirus (GenBank: QBQ64952.1), and
Heartland bandavirus (GenBank: AFP33391.1). ESPript (espript.ibcp.fr) software was used for sequence alignment and secondary structure depiction. Secondary structure information files for the SFTSV pentamer (4J4U) or hexamer (4J4R) were input from PDB for reference (Additional file
1: Fig. S1) [
27‐
29].
Denaturation test
Since truncated dN2 and dN3 required solubilization in 0.8 M urea solution, we assessed whether or not their native structures were maintained. Full-length and truncated dN2 and dN3 SFTSV N proteins were subjected to four denaturation factors; urea (0.8 M, 2 M, 4 M, or 6 M), SDS, β-mercaptoethanol, or heat.
Discussion
In this study, recombinant SFTSV N protein was expressed in
E. coli. Mice were immunized with this protein to produce monoclonal antibodies specific for the SFTSV N protein. Two sequential antibodies and seven conformational antibodies were generated. These antibodies showed immune responses to the native SFTSV N protein in dot-blot analyses, and their binding affinities were confirmed through indirect ELISA. In addition, the binding positions of the generated antibodies within the SFTSV N protein were identified. The binding-domain mapping with truncated SFTSV N proteins indicated that the epitopes bound by eight of the nine tested antibodies were localized to narrow α-helix 1 and 2 regions corresponding to the SFTSV N-arm [
17,
27,
34]. The N-arm of the SFTSV N protein stretches between adjacent molecules within N protein oligomers. Our study confirmed that the N-arm of antigen, which is relatively exposed on the surface, triggered immune responses in host cells. On the other hand, α-helix 5 is located adjacent to the neighboring N protein molecules in a ring-shaped, making this helix is less exposed than α-helix 1 and 2 [
27‐
29]. However, through the binding of antibody #10(B2H12), it is confirmed that the epitope is at least exposed.
The nine antibodies were classified into three groups according to binding positions. Unexpectedly, the binding sites of six antibodies in Group 2 were localized to a narrow area comprising only the 20 amino acids between positions 13 through 33. Since it is thought that most epitopes that generate immune responses are about 15–30 amino acids in length [
35], more detailed epitope mapping is required to determine whether the epitopes bound by these six antibodies overlap; however, detailed mapping was beyond the scope of the current study. For our study, we hypothesized that two antibodies that bind different epitopes would be required to develop an effective SFTSV-antigen-detection tool for diagnostic use. Therefore, we conducted pairwise testing of the nine antibodies using the full-length SFTSV N protein as the target to find the optimal capture-detection antibody combination/s for SFTSV detection. The unexpected result was that positive detection signals were (also) evident for antibody pairs recognizing the same binding epitope position. This finding may be explained by the oligomerization of SFTSV N proteins. The SFTSV N protein is a homo-oligomeric protein (a pentamer or hexamer) that forms a ring-like structure. Therefore, five or six identical epitopes may be present on the oligomer complex molecule [
36‐
38], and captured oligomer complexes of SFTSV N protein by surface-immobilized antibody may leave exposed the remaining epitopes on the other subunits of SFTSV N proteins. Oligomerization of the SFTSV N proteins used in this study was confirmed in the native-PAGE assay (Fig.
1C).
Consequently, the results indicated that the best candidates for the capture-detection pair are antibodies #3, #4, and #5, and that the #3(B4E2)-#4(C2G1) and #4(C2G1)-#5(B4D9) combinations were suitable for use in diagnostic tools. Among the three candidates, antibodies #3(B4E2) and #5(B4D9) were sequential, suggesting that sequential antibodies may be advantageous for a diagnosis system because they detect both native and denatured antigens. Among the two best antibody pairs identified, those of the #3(B4E2)-#4(C2G1) pair recognize different epitopes, while the antibodies of the #4(C2G1)-#5(B4D9) pair recognize the same epitope; however, we do not know whether these two antibodies recognize the exact same epitope. If the exact same epitope is bound by the two antibodies, the results of the pair test can be explained by binding to different N subunits. Considered together, the results indicate that the best pair of antibodies for development of SFTSV diagnostic tools is likely the [#3(B4E2)-#4(C2G1)] pair.
Conclusions
Given the steady increase in SFTSV infections, development of a rapid and efficient diagnostic tools is of national and global interest. An approach to understanding the SFTSV N protein and its specific antibodies is crucial for optimized diagnosis. We produced SFTSV-N-protein-specific monoclonal antibodies and characterized their biochemical and immunological functions with respect to the SFTSV N protein. Based on the epitope mapping results, we confirmed that most of the anti-SFTSV antibodies generated in immunized mice recognized highly exposed regions of the N protein. In addition, we were able to identify the #3(B4E2)-#4(C2G1) antibody pair as the best for SFTSV detection. The results from this study will serve as crucial insights into detection mutations in the SFTSV N protein and furthermore, these insights will be instrumental for the development of effective commercial diagnostic tools for SFTSV.
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