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The Infection Route of Tomato Zonate Spot Virus in the Digestive System of Its Insect Vector Frankliniella occidentalis

Tomato zonate spot virus (TZSV) is a phytopathogen of the genus Orthotospovirus (Bunyaviridae) that is widespread in many areas of Southwest China. TZSV is mainly transmitted by Frankliniella occidentalis, but its exact infection route remains unclear. To explore this issue, we detected the nucleocapsid protein of TZSV in the digestive systems of first-instar F. occidentalis nymphs fed with TZSV-infected pepper leaves. TZSV infection in the F. occidentalis digestive system begins within 4 h post-first access to diseased plants: The foregut is likely the primary site of infection, and primary salivary glands (PSGs) are the destination. There are three potential routes for TZSV transmission from the alimentary canal to the PSGs: (1) virus dissemination from the midgut to hemocoel followed by movement to the PSGs; (2) accumulation in midgut epithelial cells and arrival at PSGs via tubular salivary glands and efferent ducts; and (3) arrival at epitheliomuscular cells of the forepart of the midgut and movement along the ligament to the PSGs. We tested the transmission efficiency of F. occidentalis in second-instar nymphs and female and male adults. TZSV was transmitted in a persistent-propagative mode by both nymphs and adults, with adults appearing to show slightly higher transmission efficiency than nymphs. We confirmed the presence of all three routes for TZSV transmission in F. occidentalis and determined that like other Orthotospoviruses, TZSV is transmitted in a persistent-propagative manner. These results should facilitate the control of TZSV-related diseases and further our understanding of the transmission biology of Orthotospoviruses in general.


INTRODUCTION
Tomato zonate spot virus (TZSV) is a recently identified species in the genus Orthotospovirus of the Bunyaviridae family belonging to the watermelon silver mottle virus (WSMoV) serogroup. TZSV was first isolated from infected tomato samples in Yunnan Province (Dong et al., 2008) and is now widespread in many regions of Southwest China. To date, 25 plant species from June 2022 | Volume 13 | Article 911751 Chen et al. TZSV Infection Route in Thrips 7 families have been reported as hosts of TZSV, including such economically important crops as tomato (Solanum lycopersicum), potato (Solanum tuberosum), and pepper (Capsicum annuum) and several ornamental plants, including crinum (Crinum asiaticum) and iris (Iris tectorum; Dong et al., 2008Dong et al., , 2010Li et al., 2014;Zheng et al., 2014;Huang et al., 2015;Liu et al., 2015;Wu et al., 2015). Thus, TZSV poses a threat to the local agricultural economy in Southwest China. Plant infection with TZSV is often associated with consistent symptoms, such as concentric zoned rings pots and necrotic lesions on fruits, leaves, and stems (Dong et al., 2008;Zhao and Wang, 2012).
Orthotospoviruses rely on different species of thrips for horizontal transmission among plant hosts. These viruses are ingested into the digestive canals of thrips vectors and enter the primary salivary glands (PSGs) before being transmitted to plant hosts . According to studies of the tomato spotted wilt virus (TSWV)-Frankliniella occidentalis model system, TSWV must overcome several barriers, such as the midgut infection barrier (Nagata et al., 1999) and midgut escape barrier (Ullman, 1992) before it is successfully transmitted. The infection of PSGs always occurs after the infection of alimentary canals (Kritzman et al., 2002), and viral particles have been observed in the hemocoel of viruliferous F. occidentalis (Ullman, 1992). The ligaments connect the anterior midgut with the PSGs. The tubular salivary glands (TSGs) connecting the middle part of the midgut with the PSGs also enable viral entry into the PSGs (Nagata et al., 1999;de Assis Filho et al., 2002;Montero-Astúa et al., 2016).
TZSV can be transmitted by four species of thrips: F. occidentalis, F. schultzei, Thrips palmi and T. tabaci (Dong et al., 2008;Zhao and Wang, 2012;Zheng et al., 2014;Chen et al., 2021). F. occidentalis, the dominant thrips species in several areas of China, is also the main vector of TZSV (Zheng et al., 2014;Yin et al., 2018;He et al., 2020). Much is known about the behaviors and related infection mechanisms of TZSV in thrips vectors (Zheng et al., 2014(Zheng et al., , 2019Chen et al., 2021), whereas the infection route of TZSV in thrips vectors remains poorly understood.
Based on the transmission of other Orthotospoviruses, we propose three potential routes of TZSV infection of PSGs: (1) the virus passes through the outer membrane of the epitheliomuscular cells and remains in the hemolymph until its arrival at the PSGs (Ullman, 1992); (2) the virus reaches the anterior region of the epitheliomuscular cells of midgut 1 (Mg1) and then moves to the salivary cells of the PSGs via the ligaments that connect Mg1 to the PSGs (Nagata et al., 1999;Montero-Astúa et al., 2016); and (3) the TSGs connecting Mg2 to the PSGs may play an intermediary role in viral delivery (Montero-Astúa et al., 2016).
In this study, we used confocal laser scanning microscopy (CLSM) and transmission electron microscopy (TEM) to study the infection route of TZSV in its insect vector F. occidentalis. The results increase our understanding of the transmission mechanism of Orthotospoviruses, provide a fundamental basis for further studies of the interaction between TZSV and its thrips vectors, and may facilitate the control of the associated diseases.

Virus, Plant, Antibodies, and Insects
Samples of tomato (S. lycopersicum) infected with TZSV were provided by the Institute of Biotechnology and Germplasm Resources, Yunnan Academy of Agricultural Sciences, Kunming 650,205, China. The virus was mechanically inoculated onto pepper (C. annuum, Zunla-1) leaves. Healthy pepper plants were obtained locally and grown in a greenhouse maintained at 25°C under natural light conditions and used for virus transmission by thrips. A polyclonal antibody against the nucleocapsid protein of TZSV (TZSV-N) was prepared in rabbit as previously described (Jia et al., 2012a). The actin dye phalloidin-rhodamine was purchased from Invitrogen. IgGs isolated from the polyclonal antibodies were conjugated to fluorescein isothiocyanate (FITC; Invitrogen) according to the manufacturer's instructions.
F. occidentalis thrips were originally donated by the Institute of Plant Protection, Hunan Academy of Agricultural Sciences, China. The insects were reared on broad beans (Vicia faba) in a climate chamber (25°C; 65 ± 5% relative humidity and a light: dark regime of 14 h: 10 h) as described previously (Lin et al., 2021). Adult thrips used for reproduction were collected every 24 h in a clean container to allow them to spawn on freshly soaked beans.

Dissection of the Digestive System
A drop of phosphate-buffered saline (PBS) solution (0.01 M, pH7.4) was placed on the surface of a slide. Thrips were chilled on ice for 20 s and transferred to the drop of PBS, and the digestive system was dissected under an optical microscope. A dissecting needle was pressed onto the hind part of each thrips to hold it tightly, another dissecting needle was used to carefully remove the head, and the digestive system was extruded through the abdomen.

Immunofluorescence Assays
To visualize the viral infection cycle in F. occidentalis, firstinstar F. occidentalis nymphs (12 h old) were fed for an acquisition access period of 12 h on TZSV-infected pepper leaves and transferred to freshly soaked beans. At different times (1, 4, 24, 48, 72, 144, or 216 h) post-first access to diseased plants (padp), 40 thrips digestive organs were dissected, fixed, and immunolabeled before observation. F. occidentalis fed with healthy pepper leaves was used as a negative control. The digestive organs were dissected carefully in PBS solution (0.01 M, pH7.4) under an optical microscope. The PBS was removed, and the samples were fixed with 4% paraformaldehyde (PFA) for 2 h and subsequently permeabilized with 16% PFA (Alfa Aesar, United States) for 1 h at room temperature. After removing of the Triton solution and subsequent washing steps, the tissues were incubated with anti-rabbit antibodies against the nucleocapsid protein of TZSV (TZSV-N) conjugated to fluorescein isothiocyanate (FITC) and the actin dye phalloidin-rhodamine (Invitrogen) in PBS supplemented with 3% bovine serum albumin (BSA) Frontiers in Microbiology | www.frontiersin.org for 2 h at 37°C. The samples were washed three times with PBS and placed on a clean slide. Anti-fade mounting medium (20 μl) with DAPI (Vectashield) was added to the guts and salivary glands, which were then covered with a coverslip. The slides were kept at 4°C and protected from light before being processed for immunofluorescence microscopy (Leica SP8, Germany).

Hemolymph Collection
To examine the ability of TZSV to overcome the membrane barriers of the midgut to complete its infection route, the following method was used to extract the hemolymph from TZSV-infected F. occidentalis (Liu et al., 2006;Jia et al., 2012b). First-instar thrips were fed on TZSV-infected pepper leaves for 12 h for viral acquisition and transferred to freshly soaked beans. At 48 h padp, 30 thrips were selected and chilled on ice for 2 min. A drop of PBS solution was placed onto the surface of a Polysine slide (Epredia, United States). All six legs were removed from each thrips, and the wounded body was soaked rapidly in PBS, which helped the hemolymph flow from the wounds into the PBS. The collected hemolymph was then fixed with 4% PFA for 20 min, permeabilized with 2% Triton X-100 for 30 min, incubated with anti-TZSV-N antibodies and DAPI, and observed under the CLSM to monitor the presence of TZSV-N. In addition, some of the isolated hemolymph samples were used for RNA extraction and PCR analysis to confirm the presence of TZSV.

TEM Analysis
The guts and salivary glands of TZSV-infected F. occidentalis were dissected and fixed with 1% glutaraldehyde and 4% PFA in PBS overnight at 4°C. The fixed samples were washed three times with PBS on ice and dehydrated through an ethanol gradient (30, 50, 50, 70, 90, 95, 100, and 100%) at −20°C. The dehydrated tissues were permeated with a graded series (30, 50, and 100%) of LR Gold Resin (Bioscience) at −20°C and embedded in 0.13% benzil in LR Gold Resin. All samples were polymerized under ultraviolet light at −20°C for 3 days. The samples were sectioned on an ultramicrotome (Leica UC5, Germany) with a diamond knife and incubated with rabbit antiserum against TZSV-N and immunogold-labeled anti-goat antibodies against rabbit IgG that had been conjugated with 6-nm gold particles (Jackson). The sections were stained with 2% uranyl acetate, followed by 3% lead citrate for 10 min each time and observed under an electron microscope (HitachiH-7,700, Japan).
Immunogold labeling negative staining with TZSV-N-specific rabbit polyclonal antibody was used to identify viral particles in the sap of TZSV-infected pepper leaves as a positive control as previously described (Zhang et al., 2016). The samples were observed under an electron microscope (HitachiH-7,700, Japan).

Transmission Efficiency Assay
First-instar nymphs (12 h old) were fed on TZSV-infected pepper leaves for a 12-h viral acquisition period and then transferred to a transparent container, and reared on freshly soaked beans. The top of the container was covered with two layers of Parafilm. At approximately 48 h padp, 20 second-instar nymphs were chosen and placed individually into 50-mL tubes containing a healthy pepper plant (four leaf stage). The plants were inoculated for 48 h with potentially viruliferous thrips. In addition, at ~192 h padp, the rest of first-instar nymphs (which were given a 12-h TZSV acquisition period) had grown into adults. Subsequently, female and male potentially viruliferous thrips were collected individually to test the TZSV transmission efficiency as described previously. After the inoculation access period, the thrips were removed, and the inoculated test plants were maintained at 25°C under natural light conditions for 240 h prior to the RT-PCR assay. Total RNA was extracted from pepper plants or thrips as described previously (Chen et al., 2016), and the viruliferous rate and transmission rate were measured by RT-PCR with TZSV-N-encoding gene primers (F: 5′-AAAGATTCAAGAACTATT GGCT-3′; R: 5′-TCTCAGTGAACTCCACGCTA-3′). Transmission rate (%) = (number of TZSV-infected pepper plants/number of TZSV-infected thrips) × 100. The data were analyzed by one-way analysis of variance (ANOVA) using IBM SPSS statistics 20. The experiment was performed in triplicate.

Morphology of the Digestive System of Frankliniella occidentalis
To better understand the infection route of TZSV within its dominant insect vectors, we dissected the digestive organs of F. occidentalis infected (or not) with TZSV and examined them by CLSM and TEM (Figures 1-3). The digestive system of F. occidentalis contains a pair of oval PSGs; two long, slim TSGs; four Malpighian tubules (MTs); and a main digestive tract consisting of a conical foregut, tubular midgut, and short hindgut. The midgut is further divided into three parts: midgut 1 (Mg1; anterior), midgut 2 (Mg2; central), and midgut 3 (Mg3; posterior; Figures 1A,B). The PSGs are composed of several binuclear and mononuclear cells and contain a large central cistern lumen. The pair of PSGs is connected to the anterior portion of the midgut by a pair of tenuous ligaments. The efferent ducts located at the tips of TSGs are also linked with the apical regions of the PSGs (Figure 1A).

The TZSV Infection Route in Digestive Organs
We investigated the dynamics of TZSV infection in the digestive system of F. occidentalis (Table 1). More than 500 first-instar nymphs of thrips were fed with virus-infected pepper leaves for 12 h and transferred to freshly soaked beans. At 1, 4, 24, 48, 72, 144, and 216 h after viral acquisition, 40 digestive organs were dissected from the thrips and processed for immunofluorescence microscopy. We observed TZSV fluorescent signals in virus-infected digestive organs, whereas we detected no FITC signals in the digestive organs of F. occidentalis fed with healthy pepper leaves (Figure 1A). At 1 h padp, the weak green signal of TZSV-N was present only in some of the midgut lumen, which could be considered a prelude to further infection ( Figure 1B). Signals began to be detectable the epithelial cells at 4 h padp, and the infection rate increased from 0% at 1 h padp to 62.50% at 4 h padp. TZSV was detected in 60.00% of the dissected foreguts, and the signals appeared as several bright green spots localized to the epithelium ( Figure 1C). Moreover, the infection rates of TSGs (42.50%), PSGs (37.50%), and Mg1 (30.00%) indicated that TZSV particles rapidly infected the PSGs ( Table 1). Using immunogold labeling with TZSV-N-specific rabbit polyclonal antibody, we observed dense TZSV-N proteins localized to the surfaces of virion particles ( Figure 2D). Electron micrographs of the foregut and anterior midgut of TZSV-infected F. occidentalis showed that viral particles clustered into small groups in vesicles that remained in the foregut (Figure 2a1). Furthermore, the membrane of one vesicle was fused with the junction between the foregut and midgut (Figure 2a2).
To determine the TZSV infection rates in the digestive tissues, we detected the presence of TZSV-N-FITC fluorescence.
Data from 24 h padp showed a high infection rate in the foregut (80.00%), TSGs (65.00%), and PSGs (42.50%) compared to the data from 4 h padp, and the total infection rate increased to 80.00%. More viral particles clustered in the epithelium and the adjoining epitheliomuscular cells (Figures 1D, 2B). However, the infection rates of Mg2, Mg3, the hindgut, and MTs were less than 30% at both 4 and 24 h padp. At 48 and 72 h padp, the TZSV-N signals were dispersed among different digestive tissues. The total infection rates at 48 and 72 h padp were 85.00 and 82.50%, respectively, and the infection rate of each part of the digestive system exceeded 30.00%. Electron micrographs of F. occidentalis at 72 h padp showed that TZSV-N labeled with 6-nm gold particles was located in the mass of viroplasm structures in the senescent secretory cells of the PSGs (Figure 2C), indicating that the PSGs were a site of viral replication. At 144 and 216 h padp, the total infection rate was maintained at approximately 85.00% (Table 1).

Potential Route of TZSV Infection of PSGs
There are three potential routes of infection of thrips PSGs by Orthotospoviruses (Ullman, 1992;Nagata et al., 1999;Kritzman et al., 2002;de Assis Filho et al., 2002;Montero-Astúa et al., 2016). First, we determined the presence of TZSV in the hemocoel by performing immunofluorescence assays. TZSV-N (green signal) was detected in the hemolymph cells of TZSV-infected F. occidentalis ( Figure 1F) after 72 h padp, but no signal was detected in the hemolymph of the TZSV-uninfected F. occidentalis controls ( Figure 1E). RT-PCR also demonstrated TZSV infection in the hemolymph of TZSV-infected F. occidentalis, indicating that TZSV could pass through the midgut barrier into the hemocoel.  We reanalyzed all images from the immunofluorescence assay and counted the percentage of infection in the midgut, foregut, ligaments, and TSGs in all samples that contained infected PSGs. In total, we counted 130 TZSV-infected samples containing TZSV-positive PSGs ( Table 2). In these samples, the TZSV-N signal was mainly localized to the foregut, midgut, and TSGs, and the percentage of virus infection was 84.62, 87.69, and 80.77%, respectively. Efferent ducts that connect TSGs and PSGs are important conduits of viral movement from the midgut to PSGs (Montero-Astúa et al., 2016). Of the efferent ducts examined, 73.85% contained TZSV. Green TZSV-N signals were simultaneously detected in the TSGs, PSGs, and efferent ducts ( Figure 3A). The ligaments connecting Mg1 and PSGs were also found to be a secondary route for viral movement. By contrast, the percentage of TZSV in the ligaments was much lower: We observed green signal representing TZSV-N localization in only 12 of 130 pairs of ligaments. The related morphological characteristics are shown in Figure 3B. Therefore, transmission via ligaments might be a less important route of TZSV movement to PSGs ( Table 2).

Transmission Efficiency of TZSV by Frankliniella occidentalis
To test whether F. occidentalis transmits TZSV persistently, like other Orthotospoviruses, and to compare the transmission efficiency of different metamorphosis stages, we collected first-instar nymphs and fed them with TZSV-infected pepper leaves for 48 h for viral acquisition. We then transferred the nymphs to freshly soaked beans as a food source and reared them for 2 or 8 days. At these time points, we transferred the second-instar nymphs and adult females and males individually to 50-mL Eppendorf (EP) tubes containing a healthy pepper plant (four leaf stage) and performed a virus transmission assay (Table 3). At these two metamorphosis stages, F. occidentalis was able to transmit TZSV into healthy pepper plants in a persistent transmission mode. The transmission rates by female adults (46.67 ± 4.41) and male adults (51.67 ± 6.67) appeared to be slightly higher than that by nymphs (41.67 ± 3.33), but these differences were not statistically significant (p > 0.05).

DISCUSSION
Like most plant viruses, Orthotospoviruses require specific insect vectors for their effective long-distance transmission . Thrips are the primary vectors for Orthotospoviruses, and they also serve as important hosts that provide sites for viral replication Gupta et al., 2018;Rotenberg and Whitfield, 2018). Understanding the interactions between thrips and Orthotospoviruses is a key to controlling the diseases caused by these viruses, which have been the focus of much research (Zhao and Rosa, 2020;Chen et al., 2021;Mou et al., 2021).
To better understand the transmission route of TZSV through the digestive system of its dominant insect vector F. occidentalis, we performed a series of transmission experiments. The transmission electron micrographs from immunolabeling experiments showed that TZSV particles mainly formed small clusters that were enclosed within vesicles in the digestive system. Many vesicles were observed adjacent to the basal lamina between the foregut and midgut epithelial cells (Figure 2A). The viral particles could move intercellularly in an exocytosis-like manner (Figure 2a2). Viral particles could first enter the epithelial cells of the foregut or midgut and then be transmitted very rapidly into the adjacent epithelial or epitheliomuscular cells (Table 1). This suggests that TZSV can propagate well and circulate in its vector F. occidentalis. TZSV particles also showed a similar cellular distribution pattern in the cytoplasm as in the plant host of F. occidentalis: They were usually present as single particles or small groups of particles that clustered within the cytoplasm or at the ER membrane (Zhang et al., 2016).
The three routes for TZSV movement from the alimentary canal to the PSGs are depicted in Figure 4: (1) dissemination from the epitheliomuscular cells to the hemocoel, followed by movement to the PSGs; (2) accumulation in the epithelial cells of Mg1 and Mg2 and transfer into the apical regions of PSGs through the TSGs and efferent ducts; and (3) arrival at the epitheliomuscular cells of the forepart of Mg1, followed by movement along the "rope"-like ligaments to the secretory cells of the PSGs. Due to the difficulty in collecting hemolymph, we could not obtain data for the infection rate of hemolymph alone. However, transmission via the ligaments might be less important than the other two transmission mechanisms ( Table 2). Given the higher infection rates of TSGs and efferent ducts, we hypothesize that the primary mechanism of TZSV transmission from the alimentary canal to the PSGs occurs via the TSGs. Previous studies suggested a fourth hypothetical mode of Orthotospoviruses movement from the midgut to the PSGs that depends on the ontogeny of the thrips (Moritz et al., 2004). Based on images of the positions of the internal organs of F. occidentalis at different developmental stages, the movement of Orthotospoviruses was proposed to occur during metamorphosis, when direct contact exists between the digestive organs. This might explain the observation that adult thrips can transmit some Orthotospoviruses only when they are infected at the nymph stage (Whitfield et al., 2005). Four transmission modes have been categorized in virusvector interactions: non-persistent, semi-persistent, persistentcirculative, and persistent-propagative (Ng and Falk, 2006).
Orthotospoviruses are transmitted by their thrips vectors in a persistent-propagative manner (Whitfield et al., 2005). In this transmission mode, viruses enter the alimentary canals of their vectors; infect several insect tissues, where they replicate; and then arrive at the PSGs as their final destination . Previous studies of Orthotospoviruses have demonstrated that TSWV is transmitted in a persistent-propagative manner by F. occidentalis (Wijkamp et al., 1996;Margaria et al., 2014), T. palmi is a vector species of capsicum chlorosis virus (Chiaki et al., 2020), and WSMoV can be transmitted in a semi-persistent manner by T. palmi nymphs but is primarily transmitted in a persistent-propagative manner by adult T. palmi after the viruses have been acquired at the first-instar nymph stage (Mou et al., 2021). In this study, we tested the transmission efficiency of different developmental stages of F. occidentalis and determined that, like to other Orthotospoviruses, TZSV is transmitted in a persistent-propagative manner. This was confirmed by electron  micrography of the viroplasm in the PSGs ( Figure 2C). However, whether TZSV can be transmitted in a semi-persistent manner remains to be further studied.
To conclusion, our results demonstrated three routes for TZSV transmission in F. occidentalis and confirm that, like other Orthotospoviruses, TZSV is transmitted in a persistent-propagative manner. These results provide a better understanding of the transmission mode of Orthotospoviruses, provide a fundamental basis for further research into the interaction between TZSV and its thrips vector and may aid attempts to control the related diseases.

DATA AVAILABILITY STATEMENT
The raw data supporting the conclusions of this article will be made available by the authors, without undue reservation.

AUTHOR CONTRIBUTIONS
YoC and HW contributed to conception and design of the study. YL, LW, HL, TL, SL, and XZ conducted the experiments. YL, YiC, and HT performed the statistical analysis. YoC and YL wrote the manuscript. All authors contributed to the article and approved the submitted version.