|Home | About | Journals | Submit | Contact Us | Français|
Conceived and designed the experiments: SSC SM RWB KJK. Performed the experiments: SSC CAS BM YA. Analyzed the data: SSC SM RWB KJK. Contributed reagents/materials/analysis tools: SSC CAS BM RWB. Wrote the paper: SSC RWB SM KJK.
Molting, or the replacement of the old exoskeleton with a new cuticle, is a complex developmental process that all insects must undergo to allow unhindered growth and development. Prior to each molt, the developing new cuticle must resist the actions of potent chitinolytic enzymes that degrade the overlying old cuticle. We recently disproved the classical dogma that a physical barrier prevents chitinases from accessing the new cuticle and showed that the chitin-binding protein Knickkopf (Knk) protects the new cuticle from degradation. Here we demonstrate that, in Tribolium castaneum, the protein Retroactive (TcRtv) is an essential mediator of this protective effect of Knk. TcRtv localizes within epidermal cells and specifically confers protection to the new cuticle against chitinases by facilitating the trafficking of TcKnk into the procuticle. Down-regulation of TcRtv resulted in entrapment of TcKnk within the epidermal cells and caused molting defects and lethality in all stages of insect growth, consistent with the loss of TcKnk function. Given the ubiquity of Rtv and Knk orthologs in arthropods, we propose that this mechanism of new cuticle protection is conserved throughout the phylum.
The outer shell of an insect serves both as protective skin and rigid exoskeleton that must be periodically replaced with a new, larger one during development. During this molting process, the inner layers of the old exoskeleton are digested and recycled, while the outer layers are discarded. Secretion of the new skin necessarily commences before the partial recycling and shedding of the old shell. This creates a problem for the insect, namely how to protect the new skin from digestive enzymes intended for the old shell that closely enwraps it. Previously we showed that such protection is afforded by the Knickkopf (Knk) protein, which is secreted from the epidermis and infiltrates the new skin, rendering it resistant to enzymatic degradation. In this work, we show that another protein, called Retroactive (Rtv), ensures the proper trafficking of Knk into the newly secreted skin. Rtv remains inside the epidermal cells, while directing the transport of Knk to the cell surface and ensuring its export into the new skin. Digestive enzymes are then secreted and target the old exoskeleton while leaving the new one intact. This dependence of Knk on Rtv function is probably true for all insects and other arthropods.
A critical feature of the insect molting process is the simultaneous synthesis and degradation of chitin at different sites associated with the cuticle , . Chitinolytic enzymes (molting fluid chitinases and N-acetylglucosaminidases) dissolve parts of the old chitinous exoskeleton into oligomeric and monomeric N-acetylglucosamine (GlcNAc) units, which are subsequently recycled into the collective pool of biosynthetically derived activated precursors of GlcNAc monomers (UDP-GlcNAc) used for the synthesis of new cuticular chitin , . The enzyme that catalyzes the addition of these monomers onto the growing chitin oligosaccharide is the membrane-bound chitin synthase , , . Upon synthesis and secretion into the extracellular (subcuticular) space by epidermal cells, nascent chitin aggregates into microfibrils and accumulates within the assembly zone (the layer immediately above the apical surface of the epidermal cells) to eventually organize into new cuticular laminae , .
At the ultrastructural level, the new cuticle extends from its inner boundary on the apical side of the epidermal cell membrane to its outer “envelope” layer that appears to partition it from the overlying old procuticle . However the envelope layer functions only as a structural boundary at the early stages of molting, and does not function as a barrier against molting fluid chitinases . Indeed, the molting fluid chitinase of T. castaneum (TcCht-5) was observed throughout the new procuticle co-localized with chitin. The mysterious stability of the new cuticle in intimate contact with enzymatically active chitinases was shown to be due to its physical association with the cuticle assembly protein, Knickkopf (TcKnk; homologue of D. melanogaster knickkopf, DmKnk) .
Like DmKnk, the protein Retroactive from Drosophila melanogaster (DmRtv) was also previously demonstrated to affect cuticle differentiation and tracheal tube morphogenesis , , . DmRtv was predicted to form a membrane-anchored, three-finger loop structure that interacts with chitin via two aromatic residues situated in each loop . Although a direct role for this protein in cuticular chitin filament organization in embryonic tracheal tubules of D. melanogaster was envisaged, the mechanism of this ordering process is unclear. In the current study we show that a direct effect of the T. castaneum Rtv homologue (TcRtv) on cuticular chitin organization is unlikely, given its predominant intracellular distribution within epidermal cells. Instead, its activity is shown to be crucial for the proper trafficking of TcKnk to the procuticle where the latter protein associates with and protects chitin. Hence, TcRtv promotes cuticle synthesis and organization by facilitating TcKnk's localization in the integument.
TBLASTN and BLASTP searches of the T. castaneum genome using the DmRtv protein sequence as query identified only a single gene coding for an orthologous protein. T. castaneum retroactive (TcRtv) (JX470185) maps on LG4, position 24.3 cM. TcRtv is composed of three exons and encodes a 150- amino acid residue long protein with a predicted C-terminal GPI anchor and an ω-asparagine at position 124 (Figure S1A and S1B) (GPIPred). A predicted cleavable signal peptide at its N-terminus suggests that this protein enters the ER secretory pathway prior to GPI-anchoring and is transported to the cell surface via intracellular secretory vesicles. Expression analysis revealed the presence of TcRtv transcripts throughout development including embryonic, larval, pupal and adult stages (Figure 1A). Lower levels of TcRtv expression were detected at the embryonic and young larval stages relative to later stages of development. Tissue-specific expression of TcRtv revealed that TcRtv transcripts could only be detected in the hindgut and carcass but not in midgut tissues indicating that this gene is expressed in tissues of ectodermal origin (Figure 1B). TcRtv transcripts were also detected in pharate adult elytra and hindwings (Figure 1B).
When other fully sequenced arthropod genomes were queried with DmRtv or TcRtv sequences, only a single homolog was identified in all the insect species. The presence of an ortholog of TcRtv gene in all sequenced insect genomes suggests an essential function for this protein in insect survival and development (Figure 1C). Interestingly, a single Rtv ortholog is also present even in non-insect arthropod species including the water flea, Daphnia pulex, and the deer tick, Ixodes scapularis, suggesting that Rtv may have a conserved biological function in all species that produce a chitinous exoskeleton. On the other hand, we could not identify Rtv homologs in the genome of the nematode, Caenorhabditis elegans, which does synthesize chitin in its eggshells and the pharyngeal lumenal walls. Thus Rtv may have appeared early during arthropod evolution.
Given the ubiquitous presence of TcRtv transcripts during insect growth, we hypothesized a critical role for this protein in post-embryonic development. To test this hypothesis, we depleted TcRtv transcripts via RNA interference (RNAi) by administration of TcRtv-specific dsRNA (dsRtv) during multiple developmental stages of T. castaneum. RNAi of TcRtv led to molting arrest at larval-larval, larval-pupal or pupal-adult stages, depending upon the developmental stage at the time of injection, with significant reductions in transcript levels at each stage tested (Figure 1D and 1E). Apolysis and partial slippage of the old larval cuticle proceeded at the subsequent molt after injection of TcRtv dsRNA into penultimate-instar larvae, but the larvae failed to complete the larval-larval molt and remained entrapped within their old larval cuticle. Similarly, insects injected with TcRtv dsRNA at later stages were arrested at the larval-pupal or pupal-adult molts and failed to shed their old cuticle. These phenotypes were reminiscent of those that we have reported previously following RNAi for TcChs-A . Control insects injected with the same dose of dsRNA for the eye pigmentation gene, TcVer (T. castaneum Vermilion), developed normally except for the loss of eye color. These results demonstrate that Rtv is essential for molting in T. castaneum.
Because of the terminal phenotypic resemblance of insects treated with dsRNAs against TcRtv or TcChs-A , we suspected a reduction of procuticular chitin content resulting in loss of mechanical strength of the new cuticle may account for the failure to complete ecdysis. To test this hypothesis, insects at the pharate pupal stage were treated with TcRtv-specific dsRNA and their chitin contents were probed qualitatively and quantitatively just prior to the adult molt (pharate adult). Confocal microscopic analysis of the pharate adult elytra stained with a chitin-binding domain (CBD) probe (rhodamine-conjugated CBD) showed a near complete loss of chitin in the new cuticle of TcRtv-depleted insects when compared to control insects (Figure 2A). A similar reduction in new cuticular chitin was also detected in the pharate adult insect body wall after RNAi for TcRtv compared to TcVer-depleted insects (Figure 3B, column 1- row 2). Independently, quantitative analysis of total body chitin content by a modified Morgan-Elson assay confirmed chitin depletion in these insects during both larval-pupal and pupal-adult molts (Figure 2B). The reduction of chitin content following RNAi of TcRtv was comparable to that observed in TcChs-A-depleted insects, and varied depending on the stage of insect development from ~2- to 10-fold relative to control insects (Figure 2B). Collectively, these data reveal that TcRtv affects molting by modulating the level of chitin, predominantly in the newly forming cuticle.
The total amount of chitin in an insect is likely to change dynamically during periods of growth as a result of repeated cycles of cuticle deposition and turnover. The dynamics are more complex during molting when there is an overlap of the period of chitin synthesis in the new cuticle with that of chitin degradation in the old cuticle. As a result, several possible mechanisms by which TcRtv may regulate chitin levels in the procuticle can be envisioned. The loss of chitin following RNAi for TcRtv suggests that this protein might be an activator of chitin synthesis or an inhibitor of chitin degradation. In the first scenario, TcRtv might affect chitin synthesis via its effect on TcChs-A at the transcriptional, post-transcriptional, translational or post-translational levels. However, our observation that steady-state levels and cellular distribution of TcChs-A protein were similar in control and TcRtv-depleted insects (Figure S2) argues against a direct effect of TcRtv on TcChs-A expression and localization. An alternative hypothesis that would explain the observed reduction in chitin in the newly forming procuticle following TcRtv RNAi is that TcRtv protects newly synthesized chitin from molting fluid chitinases. Indeed, we have shown recently that chitin is co-localized with chitinases, which are not excluded from the newly forming procuticle as had been assumed in the past. We have further shown that the chitin-binding protein, TcKnk, is needed to protect the nascent chitin in the procuticle from chitinase-mediated degradation . To test the hypothesis that TcRtv also protects chitin, we down-regulated the expression of the major molting fluid chitinase (TcCht-5) at the pharate adult stage either alone or in combination with TcRtv and subjected these samples to quantitative chitin content analysis. Remarkably, the analysis revealed that insects subjected to RNAi for TcRtv alone exhibited significant chitin reduction, but co-depletion of both TcRtv and TcCht-5 transcripts resulted in nearly a complete rescue of cuticular chitin content relative to control levels (Figure 3A). These results also rule out a requirement for TcRtv for the synthesis and transport of chitin to the procuticle by Chs-A and suggest that Rtv-mediated stabilization of chitin involves a step after the synthesis of chitin.
This conclusion was further supported by confocal microscopy, which showed a near complete loss of chitin in the procuticle following depletion of TcRtv transcripts compared to the dsRNA TcVer-treated insects. But RNAi for both TcCht-5 and TcRtv, rhodamine-CBD staining indicated that the level of chitin within the new cuticle of body wall was restored to the same level as dsTcVer controls (Figure 3B, compare row 3 with row 1).
To gain a better understanding of the nature of the restored chitin in the procuticle following depletion of transcripts for both TcCht-5 and TcRtv, we performed Transmission Electron Microscopic (TEM) analysis of the elytra, body wall, tracheae and denticles of insects treated with the indicated combination of dsRNAs. Ultrathin sections of elytral and body wall cuticle from control insects were characterized by a well-organized laminar architecture. Along with the drastic reduction in procuticular chitin, the laminar architecture was completely disrupted following RNAi for TcRtv. Although simultaneous down-regulation of TcRtv and TcCht-5 transcripts resulted in the restoration of chitin within the procuticle, the laminar organization was not reestablished (Figure 4). Interestingly, this phenotype was indistinguishable from the phenotype that we have recently observed in elytra of pharate adults depleted of transcripts for both TcKnk and TcCht-5.
Additional analyses also revealed structural deformities of denticles protruding at the lateral body wall that is consistent with loss of laminar architecture in denticular procuticle following down-regulation of TcRtv in these insects (Figure 4). Similarly the taenidial cuticle that lines the tracheal lumen and stabilizes the tracheal tube in these insects also appeared to exhibit structural defects possibly due to the disorganized procuticle (Figure 4) and electron-dense inclusions they harbored. Simultaneous down-regulation of TcRtv and TcCht-5 transcripts, which restores chitin back to normal levels, did not rescue these phenotypes in either the denticles or taenidia, indicating the importance of TcRtv in maintaining the morphology of both taenidia and denticles (Figure 4).
Since the phenotypes of RNAi for TcRtv and TcKnk are indistinguishable, we considered the possibility that these two proteins may be involved in the same linear pathway. Immunohistochemistry carried out on sections of control insects (dsTcVer-treated) and those treated with dsRNAs specific for TcRtv, using a polyclonal antibody against Knk indicated that depletion of TcRtv transcripts alone resulted in the mislocalization of TcKnk from its normal distribution predominantly in the procuticle to an exclusive presence within the epidermal cells, perhaps with some TcKnk in the plasma membrane (Figure 5, compare row 3 with row 1).
However it is likely that the altered localization of TcKnk may have been brought about indirectly by a reduction of chitin which acts as a signal for TcKnk's release into the procuticle and not by a direct effect of TcRtv on TcKnk trafficking. To distinguish between these two possibilities, TcKnk localization was examined in insects depleted of both TcRtv and TcCht-5 transcripts by co-injection of both dsRNAs. This enabled us to disable TcRtv function without concomitant depletion of procuticular chitin, and thus observe the direct effect of TcRtv on localization of TcKnk independently of any possible contributing effects of procuticular chitin itself. Although chitin levels remained at near normal levels in the procuticle after such treatment, TcKnk was mislocalized, remaining entirely inside the cell rather than being secreted into the procuticle (Figure 5, compare row 4 with row 1). The distribution of TcKnk in these double-knockout insects was indistinguishable from that observed in those treated with dsRNA for TcRtv alone. These observations support the hypothesis that TcRtv facilitates the trafficking of TcKnk into the procuticle.
The assembly of chitin into the laminated procuticle of insects is a complex process that involves the coordinated action of multiple proteins involved in the synthesis and modification of chitin as well as other chitin-binding and chitin-organizing proteins. While the functions of chitin synthases, deacetylases and chitinases have been studied in some detail , , , , the role of non-enzymatic chitin-binding and organizing proteins are less well understood , . Mutational analysis in D. melanogaster has implicated two genes, Knk and Rtv, in the organization of tracheal tube chitin and of the embryonic cuticular matrix , . More recently, we have shown that the TcKnk protein is localized primarily in the procuticle, possibly bound to chitin . Furthermore, we have shown that procuticular TcKnk is crucial to the protection of chitin from the action of chitinases, which are not excluded from chitin in the newly forming procuticle as previously believed. In addition, TcKnk is needed for the organization of procuticular chitin into an ordered laminar array. However, the role of the protein TcRtv has not been studied extensively even though the phenotypes of Rtv and Knk mutants of D. melanogaster are virtually indistinguishable , .
Both TcKnk and TcRtv are predicted to encode proteins with GPI anchors by bioinformatic prediction tools (big-PI Predictor, PredGPI and GPI-SOM). However, experimental evidence for the GPI anchor is available only in the case of Knk. TcKnk and DmKnk are released from the plasma membrane of cells expressing this protein by treatment with phosphatidylinositol-specific phospholipase C (PI-PLC), an enzyme known to cleave the GPI anchor of membrane-bound proteins , . TcRtv expressed in insect cell lines infected with a recombinant virus containing the Rtv coding sequences is not released by PI-PLC treatment (Figure S3). We suspect that TcRtv does not have a true GPI anchor and may merely have a membrane-spanning segment at the C-terminus, suggesting that this protein remains embedded in the ER or attached within vesicles and plasma membranes. Therefore, we propose that TcRtv may not have a direct role in protecting chitin from chitinases and that the loss of procuticular chitin observed after RNAi of TcRtv expression must be via an indirect effect. The finding that there are no significant differences in the amount or localization of TcChs-A in control and dsRNA TcRtv-treated insects also suggests that TcRtv does not have a direct effect on TcChs-A expression or localization. Finally, the full recovery of chitin levels in the procuticle in the absence of TcRtv upon down-regulation of chitinases rules out any role for TcRtv in the synthesis and transport of chitin to the procuticle.
Then how does TcRtv affect cuticle integrity? We have demonstrated that the absence of chitin in the procuticle alone does not account for the mislocalization of the TcKnk protein after RNAi-mediated transcript depletion of TcRtv, because simultaneous RNAi of TcRtv and chitinase genes, while restoring procuticular chitin, fails to rescue the intracellular mislocalization of TcKnk. Rather, it appears that the targeting of TcKnk protein to the procuticle requires the presence of TcRtv. Whether this is due to a direct protein-protein interaction between TcRtv and TcKnk or through a more complex targeting pathway remains to be established.
A search of the SCOP database revealed that the insect Retroactive proteins share broad structural similarity with the snake toxin-like superfamily of proteins with the three-finger domain (TFD) or Ly-6/uPAR domain implicated in protein-protein interactions (Figure S4) , . The Ly-6 protein family is composed of several membrane-bound receptors, GPI-anchored proteins, and soluble ligands. These proteins are characterized by the presence of an approximately 100-residue long extracellular motif called the three-finger domain (TFD) . In the prototypical structure described for proteins of this family, the sea snake venom neurotoxin or erabutoxin b, 10 cysteines form a series of disulfide bridges that stabilize the protein core and allow three finger-like loops to protrude , . These finger-like extensions with variable sequences are believed to enable interaction of these proteins with a broad range of substrates or ligands, each with a high degree of specificity. Insect Rtv proteins contain 10 cysteines that are predicted to adopt the TFD fold (Figure S4) , suggesting that they may be members of the snake toxin-like superfamily of proteins.
Our work has uncovered a novel mechanism involved in cuticular chitin maintenance, wherein presence of TcRtv inside the cells triggers the accretion of TcKnk to the growing chitinous matrix of the procuticle whereupon the latter protein facilitates chitin organization and confers protection from chitinolytic enzymes during the process of molting . The mechanism described herein is probably conserved in all chitinous invertebrates.
The GA-1 strain of T. castaneum was used for all experiments. Insects were reared at 30°C in wheat flour containing 5% brewer's yeast under standard conditions as described previously .
An extensive, genome-wide search for homologs of DmRtv in the T. castaneum genome database was performed using NCBI programs TBLASTN and BLASTP and using the amino acid sequence of DmRTV as query.
A DNA fragment containing the complete coding sequence of TcRtv (453 bp) was amplified by reverse transcriptase-PCR (RT-PCR) using the gene-specific primers (forward primer 5′- ATGGGTCTGTTTAGATCAATTT-3′ and the reverse primer 5′- TTACAAAAATCGTAAAATCAGTCT-3′) using cDNA prepared from the RNA extracted from different stages of beetle development as template. Additional 5′ and 3′ UTR sequences were obtained by 5′- and 3′- RACE. The amplified fragment was cloned into the pGEMT vector. Sequencing of the cDNA clone was carried out at the DNA sequencing facility at Kansas State University.
Rtv-like proteins were identified by TBLASTN searches of the fully sequenced genomes of T. castaneum, Anopheles gambiae, Aedes aegypti, Culex quinquefasciatus, Bombyx mori, Acyrthosiphon pisum, Nasonia vitripennis and Ixodes scapularis using the amino acid sequence of DmRtv as query. Multiple sequence alignments of TcRtv and the related Rtv-like proteins from other insects and arthropods were carried out using the ClustalW software prior to phylogenetic analysis. A consensus phylogenetic tree was constructed using MEGA 4.0 neighbor joining method .
The isolation of RNA and preparation of cDNA from different stages of T. castaneum development were carried out as described previously . These cDNA templates and the pair of TcRtv-specific primers, forward primer 5′-ATGGGTCTGTTTAGATCAATTT-3′ and reverse primer 5′- TTACAAAAATCGTAAAATCAGTCT -3′, were used for RT-PCR to determine the TcRtv expression profile. The T. castaneum ribosomal protein-6 (TcRpS6) gene was used as an internal control for equal loading of cDNA templates .
Two different regions of the TcRtv gene were selected for making dsRNAs. Pairs of forward and reverse primers for the chosen regions (Table S1) were used to amplify the dsRNA sequences by using the cloned TcRtv cDNA as template. The Ampliscribe T7-Flash Transcription Kit (Epicentre Technologies) was used to synthesize dsRNA as described previously . dsRNA for the tryptophan oxygenase, dsVermilion (dsVer) gene, which is required for eye pigmentation, was used as a control. dsRNAs for TcRtv or TcVer were injected into animals in the young larval, last instar larval, or pharate pupal stages of T. castaneum development (200 ng per insect, n=30). Five insects were collected at the young larval, pharate pupal and pharate adult stages of development 3–5 d after dsRNA treatment. Total RNA was extracted from the collected insects for measuring transcript levels by RT-PCR using gene-specific primer-pairs.
The full-length TcRtv cDNA clone was used as template to amplify the complete coding region of the TcRtv gene. A primer pair containing appropriate restriction enzyme sites [forward primer 5′-TATCCCGGGATGGGTCTGTTTAGATC-3′ (Sma I) and a reverse primer 5′-CAGACTGATTTTACGATTTTTGTAATCTAGATAT-3′ (Xba I)] was used to facilitate directional cloning of the TcRtv open reading frame (ORF) DNA in the pVL1393 baculovirus expression vector (BD Pharmingen). PCR-amplified, full length TcRtv DNA and the pVL1393 vector DNA were digested with the same pair of restriction enzymes and ligated as described previously . Hi-5 cells (Trichoplusia ni cell line) were used to express the TcRtv protein as described earlier .
TcRtv dsRNA-treated pharate adult insects were collected and fixed as described previously . Cryosections of 20 µm thickness were made and stained for specific proteins using chicken antiserum to T. castaneum Rtv (1100), rabbit antiserum (1100) to D. melanogaster Knk and rabbit antiserum to T. castaneum Chs-A (150) as primary antibodies. Alexa 488 goat-anti-chicken IgG (11000) or Alexa 488 goat-anti-rabbit IgG (11000) were used as secondary antibodies for the fluorescence detection of TcRtv, TcKnk and TcChs-A proteins. Rhodamine conjugated chitin-binding probe (1100) and DAPI (115) were used for staining of chitin and nuclei, respectively. Confocal microscopy was performed with an LSM META 510 laser scanning confocal microscope using laser lines of 405 nm, 488 nm and 543 nm for excitation. Images were taken using an oil objective (40×/1.3 NA) with 8× zoom and processed in Adobe Photoshop 7.0.
Hi-5 cells were infected with a recombinant baculovirus containing the TcRtv and TcKnk open reading frame and incubated at 30°C for 3 d for expression of proteins. Three days post-infection, Hi-5 cells expressing respective proteins were treated with PI-PLC as described previously .
Following dsRNA treatment, pharate pupae and pharate adults of T. castaneum were collected for chitin content analysis by a modified Morgan-Elson method as described previously . TcVer dsRNA and TcChs-A dsRNA-treated insects were used as negative and positive controls for the experiment, respectively.
Pharate pupae were injected with dsRNA and pharate adult samples were collected on pupal day 5, fixed and embedded in EMBED 812/Araldite resin as described previously . Resin embedded samples were then thin-sectioned (silver to gold section) and imaged on a CM-100 TEM.
cDNA sequence for T. castaneum Retroactive (TcRtv) is deposited at NCBI with accession number JX470185.
(A) Schematic diagram of the exon–intron organization of TcRtv gene. The exon–intron organization of TcRtv gene was determined by sequence comparison between genomic sequence and the full-length cDNA sequence containing 5′- and 3′-UTR regions. This gene is composed of three exons. * and closed triangle indicates start and stop codons, respectively. (B) TcRtv encodes a 15 kDa protein with an N-terminal signal peptide (red; SignalP prediction) and a C-terminal hydrophobic region (Yellow; PredGPI prediction). Ten conserved cysteine and aromatic residues are shown in blue and pink color, respectively. The ω-asparagine residue where the cleavage is predicted to occur for GPI anchoring is underlined (PredGPI).
Localization of TcChs-A in insects treated with dsRNA for TcVer (control, dsTcVer) and TcRtv (dsTcRtv). T. castaneum pharate adult lateral body wall sections (20 µm) were stained with TcChs-A antibody. No visible differences in the cellular distribution of TcChs-A protein localization were detected in absence of TcRtv. Chitin (red); TcChs-A (green); DAPI (blue); C, cuticle; E, epithelial cell. Scale bar=5 µm.
TcRtv is not released to the medium by PI-PLC treatment. Recombinant TcRtv and TcKnk proteins were expressed in Hi-5 cells infected with recombinant baculoviruses containing the ORF of TcRtv or TcKnk. After 72 h of infection, the medium was removed and fresh medium was added along with 100 µl of phosphatidylinositol-specific phospholipase-C (PI-PLC) from Bacillus cereus (7.89 units/mg) for 4 h and the proteins in the medium and cell pellet were subjected to western blot analysis using an anti-Knk or anti-Rtv antiserum. Lanes: 1, Size marker; 2, Medium from TcRtv/TcKnk-expressing Hi-5 cells after 72 h of infection; 3, Cell pellet from TcRtv/TcKnk-expressing Hi-5 cells 72 h after infection. For lanes 4–7, old medium was removed and replaced with fresh medium with or without added PI-PLC. 4, Medium from TcRtv/TcKnk-expressing Hi5 cells after mock-treatment for 4 h without PI-PLC; 5, TcRtv/TcKnk-expressing Hi-5 cell pellet without PI-PLC treatment; 6, Medium from TcRtv/TcKnk-expressing Hi-5 cells 4 h after PI-PLC treatment; 7, Cell pellet from TcRtv/TcKnk-expressing Hi-5 cells after 4 h of PI-PLC treatment. TcRtv was found in the cell pellet fraction (lane 3 versus lane 2) and it was not released to the medium after 4 h of PI-PLC treatment (lane 6 versus lane 4). TcKnk was used as a control for PI-PLC treatment and it was released to the medium after 4 h of PI-PLC treatment (compare lane 6 versus lane 4).
Insect Rtv proteins have the conserved three-finger domain (TFD). Alignment of Rtv proteins from different insect species shows 10 conserved cysteines (solid red boxes) and aromatic residues (blue), which are predicted to bind with chitin.
Primers used for dsRNA synthesis.
We thank Dr. Hans Merzendorfer for critical reading of this manuscript. We thank Joel Sanneman and Dr. Philine Wangemann for the use of the COBRE Confocal Microfluorometry and Microscopy Core Facility. We thank Dr. Bernard Moussian for the use of the TEM Core Facility at Max Plank Institute at Tübingen that is supported by Dr. Matthias Floetenmeyer. Mention of trade names or commercial products in this publication is solely for the purpose of providing specific information and does not imply recommendation or endorsement by the U.S. Department of Agriculture. USDA is an equal opportunity provider and employer.
This work was supported by National Science Foundation grant IOS-1022227. This is contribution 13-036-J from the Kansas Agricultural Experiment Station. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.