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Many host factors have been identified to be involved in viral infection. However, although furoviruses cause important diseases of cereals worldwide, no host factors have yet been identified that interact with furoviral genes or participate in the viral infection cycle. In this study, both TaHSP70 and NbHSP70 were up-regulated in Chinese wheat mosaic furovirus (CWMV)-infected plants. Their overexpression and inhibition were correlated with the accumulation of viral genomic RNAs, suggesting that the HSP70 genes could be necessary for CWMV infection. The subcellular distributions of TaHSP70 and NbHSP70 were significantly affected by CWMV infection or by infiltration of RNA1 alone. Further assays showed that the viral replicase encoded by CWMV RNA1 interacts with both TaHSP70 and NbHSP70 in vivo and vitro and that its region aa167–333 was responsible for the interaction. Subcellular assays showed that the viral replicase could recruit both TaHSP70 and NbHSP70 from the cytoplasm or nucleus to the granular aggregations or inclusion-like structures on the intracellular membrane system, suggesting that both HSP70s may be recruited into the viral replication complex (VRC) to promote furoviral replication. This is the first host factor identified to be involved in furoviral infection, which extends the list and functional scope of HSP70 chaperones.
RNA viruses are ubiquitous biotic stresses on both unicellular and multicellular organisms and include many important pathogens of humans, domestic and farm animals and of crops. Their successful infection and symptom development depends on complex molecular interactions between viral and host factors. In recent years, many host factors have been identified that interact with viral genes and are involved in viral infection cycles and symptom expression. Among these, heat shock proteins (HSPs), highly conserved and ubiquitous cytoprotective proteins, often play crucial roles in important processes,. including replication, virion assembly, and intracellular movement1. Based on molecular mass and sequence homology, HSPs can be classified into five major categories: HSPp100/ClpB, HSP90, 70kDa heat shock protein (HSP70/DnaK), chaperonin (HSP60/GroEL), and small heat shock protein (sHSP).
HSP70s are central to the cellular chaperone network, and have long been recognized as among the most abundant conserved molecular chaperones in all living organisms2,3, assisting nascent protein folding in normal physiological conditions as well as under biotic and abiotic stress. In Arabidopsis, at least 14 members of the HSP70 family have been found to be unequally distributed among its five chromosomes and to have enhanced expression at particular developmental stages or to be induced by stresses4,5. Genetic evidence has illustrated the essential functions of HSP70s in embryogenesis6, root and shoot development, hormone signalling pathways7 and immune and abiotic stress responses8,9. In wheat, a major staple crop plant, quantitative PCR and proteomic analysis showed that its HSP70 genes are expressed throughout the early grain development stages10,11,12; and are up-regulated by the addition of CaCl213, by heat stress10,14 and by infection with the stripe rust fungus15. suggesting that wheat HSP70s play important roles although their detailed functions remain largely unknown.
Chinese wheat mosaic virus (CWMV) is a member of the genus Furovirus, family Virgaviridae16. Like all known furoviruses, CWMV causes a damaging disease of cereal plants and has rigid rod-shaped particles with a bipartite single-strand positive RNA (ssRNA) genome17. RNA1 (7,147nt) encodes three proteins: (1) a 153KDa replicase protein (p153); (2) a 212KDa protein (p212) produced by occasional read-through of the UGA termination codon of p153 to incorporate an RdRP domain; (3) a cell-to-cell movement protein (MP). RNA2 (3,564nt) is predicted to encode four proteins: the major coat protein (CP: 19kDa), two minor CP-related proteins (N-CP: 23kDa; CP-RT: 84kDa) produced by translation initiation at a non-canonical CUG start codon or occasional read-through of the UGA termination codon, respectively, and a cysteine-rich RNA silencing suppressor (CRP: 19kDa)17,18. Recently, infective full-length cDNA clones of CWMV have been developed19 but so far no host factors have been identified that interact with the furoviral genes and participate in the infection cycle of CWMV, or of other furoviruses. In this study, the expression of a host HSP70 gene was found to be regulated by CWMV infection and required for replication of CWMV. Its functions during viral infection were further dissected in host plants.
Western blot analysis of systemically infected leaves collected from N. benthamiana plants 7 days post-infiltration (dpi) with infectious CWMV cDNA clones and from infected Triticum aestivum with typical mosaic symptoms showed that they had significantly more HSP70 than the corresponding healthy plants (Fig. 1A).
To investigate the roles of HSP70 in CWMV infection, its expression was reduced in N. benthamiana (Supplemental Figure S1A) by quercetin, a flavonoid chemical inhibitor specific for HSP70 expression in both single cells and whole organisms20. Interestingly, the accumulation of CWMV RNA in N. benthamiana was severely reduced when infected leaves were treated with 100 or 150μM quercetin and no CWMV RNA was detected 4 days after treatment with 200μM (Fig. 1B,C). These experiments suggested that HSP70s might be required for CWMV infection.
The initial experiments could not distinguish which member(s) of the HSP70 family were affected by CWMV infection. We therefore searched the NCBI transcriptional database of wheat and found 27 expressed sequence tags (ESTs). These ESTs were assembled into four contigs of HSP70-like genes, which were almost identical to those in previous reports, including AF00599310,14, AF07496921, GQ28038215, and KJ02755122. We then designed primer pairs for quantitative RT-PCR (qRT-PCR) and characterized the expression profile of these genes in Triticum aestivum with or without CWMV infection. The genes corresponding to AF074969, GQ280382, and KJ027551 increased 2 to 5-fold (Fig. 2A) while the gene of AF005993 increased by more than 25-fold in infected wheat plants, indicating that these HSP70 genes could be regulated to varying degrees by CWMV infection. We selected the most sensitive gene (accession number: AF005993, designated TaHSP70 in this study for convenience) for further investigation.
N. benthamiana is an excellent experimental host of CWMV18 and an efficient and reliable agro-infiltration method has been developed for viral reverse genetic assays on it19. To further characterize the relationship between HSP70s and CWMV infection, we then examined the expression of an ortholog of TaHSP70 from N. benthamiana (Genbank accession number: KX912913) which was designated NbHSP70 for convenience in this study and had 93.1% aa identity (98.3% similarity) to TaHSP70 (See Supplementary Figure S2). A quantitative assay showed that the transcriptional expression of NbHSP70 was up-regulated by more than 30-fold at 7 dpi in CWMV-infected N. benthamiana (Fig. 2B).
To investigate the function of HSP70, a binary vector (35S:TaHSP70) was constructed and introduced into N. benthamiana epidermal cells for transient overexpression of TaHSP70 (see Supplementary Figure S1B). To analyze the effect of its overexpression on CWMV infection, the binary vector was co-infiltrated with CWMV infectious clones. As controls, plants were mock-inoculated with ddH2O or co-infiltrated with an empty binary vector with CMV 35S promoter (35S:00) and CWMV infectious clones. Total RNAs were extracted from the inoculated or mock-inoculated leaves at 4dpi and used for Northern blot assays. CWMV genomic RNA (gRNA) accumulated much more highly in the plants expressing TaHSP70 than in control plants (Fig. 3). Similar overexpression of NbHSP70 in N. benthamiana also enhanced the accumulation of CWMV genomic RNAs (data not shown).
To further assess the potential function of HSP70 in CWMV infection, tobacco rattle virus (TRV)-induced gene silencing (VIGS) was used to investigate the effect of NbHSP70 silencing on CWMV infection in N. benthamiana. TRV vectors harboring a partial fragment of the NbHSP70 gene (TRV:NbHSP70) were constructed and agro-infiltrated into plants while the empty TRV vector (TRV:00) was used as control. The specific reduction of NbHSP70 transcripts was validated by qRT-PCR assays in plants infiltrated with TRV:HSP70 at 7dpi and the distinct crinkles and abnormal veins were observed on the upper leaves of plants infiltrated with TRV:HSP70 at 10dpi (Fig. 4A,B). Death of some young leaves and shoot apical meristems occurred at 14dpi. The newly developed leaves were inoculated at 10dpi with CWMV infectious clones by Agrobacterium infiltration and monitored for virus accumulation. Total RNA was extracted from the systemic leaves 4 days after CWMV inoculation (i.e. at 14dpi). Northern blotting assays showed that the accumulation of CWMV RNAs was significantly reduced in the TRV:NbHSP70-infiltrated plants when compared with TRV:00 plants (Fig. 4C).
CWMV has two genomic RNAs but only RNA1 encodes proteins required for viral replication23. To validate the effect of NbHSP70 on CWMV replication, full-length RNA1 clones were agro-inoculated onto the newly developed leaves of N. benthamiana in which the silencing phenotype had been fully established by prior inoculation with the TRV:NbHSP70 construct. N. benthamiana plants agri-inoculated with the empty TRV vector and the CWMV RNA1 clone were used as controls. Total RNA was extracted from the inoculated leaves at 4dpi and used for Northern blotting assays with a RNA1-specific probe. Accumulation of RNA1 was reduced in NbHSP70-silenced plants (Fig. 4D, lane 5) when compared with that of non-silenced plants (Fig. 4D, lane 4). However, the accumulation of CWMV RNA1 was increased sharply in NbHSP70-silenced plants co-infiltrated with CWMV RNA1 and 35S:NbHSP70 (Fig. 4D, lane 3) or 35S:TaHSP70 constructs (data not shown), to a greater extent even than in plants inoculated only with the CWMV RNA1 clone (Fig. 4D, lane 6). Thus, silencing of NbHSP70 appeared to inhibit the accumulation of RNA1 but addition of NbHSP70 or TaHSP70 to the silenced plants enhanced RNA accumulation. Since there were similar adverse and advantageous effects of NbHSP70 on RNA1 alone and on the fully infective clones of CWMV, it appears that the function(s) of NbHSP70 and TaHSP70 could be closely related to the proteins encoded on CWMV RNA1.
To examine the sub-cellular localization of NbHSP70 and TaHSP70 proteins, constructs expressing NbHSP70 or TaHSP70 fused with eGFP at their C terminus (NbHSP70:GFP and TaHSP70:GFP) were constructed and introduced into N. benthamiana epidermal cells by Agrobacterium infiltration. At 3dpi, GFP fluorescence was detected by confocal microscopy and found to be mainly in localized parts of the cytoplasm and nucleus of cells expressing NbHSP70:GFP or TaHSP70:GFP (Fig. 5B,C). In the control, the non-fused GFP was distributed generally in the cytoplasm and nucleus (Fig. 5A), consistent with previous reports24. However, in CWMV-infected cells, fluorescence of both GFP-fused proteins was limited to numerous granules of various sizes in the cytoplasm and no fluorescence was observed in the nucleus (Fig. 5), suggesting that the distribution pattern of both NbHSP70:GFP and TaHSP70:GFP was severely affected by CWMV infection.
Furthermore, when NbHSP70:GFP or TaHSP70:GFP were agro-infiltrated together with the CWMV RNA1 clone into N. benthamiana epidermal cells, a large number of irregular fluorescent granules were also observed in the cytoplasm (Fig. 5). By contrast, in cells of CWMV-infected plants either expressing the non-fused GFP or co-expressing NbHSP70:GFP or TaHSP70-GFP with the CWMV RNA2 clone, the fluorescence patterns were similar to those of the cells expressing non-fused GFP, NbHSP70:GFP, or TaHSP70-GFP alone (data not shown). These results suggest that CWMV infection modifies the subcellular distribution pattern of TaHSP70 and NbHSP70 and that the proteins encoded by CWMV RNA1 are responsible for this subcellular modification.
To examine the interactions of NbHSP70 and TaHSP70 with the proteins encoded on CWMV RNA1, a series of yeast two-hybrid (YTH) assays were performed. On the basis of their predicted functional domains17, the replicase proteins were divided into three fragments, namely Rep1–670 (encoding aa 1–670, containing a domain for methyltransferase activity), Rep670–1430 (encoding aa 670–1430, containing a domain for helicase activity), and Rep1430–1840 (encoding aa 1430–1840, containing a domain for RNA-dependent RNA polymerase activity) (Fig. 6A). These three fragments and the full-length encoding region of the MP were then separately cloned into to the GAL4 activation domain (AD) vector pGADT7 as prey proteins AD-Rep1–670, AD-Rep670–1430, AD-Rep1430–1840, and AD-MP while both full-length coding regions of NbHSP70 and TaHSP70 were respectively cloned into the GAL4 DNA binding domain (BD) vector pGBKT7 as bait proteins BD-NbHSP70 and -TaHSP70. Expression of these fusion genes was under the control of galactose-inducible promoters. Combinations of plasmids expressing bait and prey proteins were then co-transformed into S. cerevisiae using the plasmid combinations BD-Lam/AD-T, AD/BD-NbHSP70 or AD/BD-TaHSP70 as negative controls and BD-53/AD-T as a positive control. The transformants expressing AD-Rep1–670/BD-NbHSP70 and AD-Rep1–670/BD-TaHSP70 grew well on the selective medium and turned as blue as the positive control (Fig. 6B,C). In contrast, no growth was observed in the transformants with any combination using prey plasmids AD-Rep670–1430, AD-Rep1430–1840 or AD-MP with bait plasmids BD-NbHSP70 or BD-TaHSP70, or in the negative controls (Fig. 6B,C). These results consistently indicated a strong interaction between the NbHSP70 or TaHSP70 proteins and the N-terminal region (aa 1–670) of the CWMV replicase. To determine the key domain for interaction, the terminal region (aa 1–670) of CWMV replicase was further divided into two smaller fragments, Rep1–333 and Rep333–670 for similar yeast two hybrid assays which showed that the crucial domain for interaction with HSP70 was within the N-terminal region (residues aa 1–333) of the replicase. This region was then divided again into two smaller fragments, Rep1–167 and Rep167–333, and the region aa 167–333 identified as crucial for its interaction with NbHSP70 or TaHSP70 (Fig. 6).
To verify the YTH results, we then used bimolecular fluorescence complementation (BiFC) assays to test the in vivo interactions between the N-terminus (residues 1–333) of CWMV replicase and NbHSP70 or TaHSP70 in living plant cells. The coding sequence of Rep1–333 was cloned into the vector pCV-nYFP-C and that of NbHSP70 or TaHSP70 into pCV-cYFP-C to generate plasmids pCV-nYFP-Rep1–333, pCV-cYFP-NbHSP70 and pCV-cYFP-TaHSP70, respectively. Two pairs of combinations, pCV-nYFP-Rep1–333/pCV-cYFP-NbHSP70 and pCV-nYFP-Rep1–333/pCV-cYFP-TaHSP70, were generated, while the pairs of pCV-nYFP-Rep1–333/pCV-cYFP, pCV-nYFP/pCV-cYFP-TaHSP70 and pCV-nYFP/pCV-cYFP-NbHSP70 were used as the negative controls. These combinations were used to agro-infiltrate N. benthamiana leaves. Three days after agroinfiltration, the inoculated leaves were examined for YFP fluorescence using laser confocal scanning microscopy. As shown in Fig. 7A, strong reconstitution of YFP fluorescence was detected in leaf epidermal cells co-infiltrated with pCV-nYFP-Rep1–333/pCV-cYFP-NbHSP70 and pCV-nYFP-Rep1–333/pCV-cYFP-TaHSP70, whereas no fluorescence was observed in the negative controls.
To test for the direct interaction of NbHSP70 or TaHSP70 and the N-terminus of the replicase in vitro, an enzyme linked immunosorbent assay (ELISA)-based binding assay was then performed. For this purpose, Rep1–670 was bacterially expressed as a GST-tagged fusion GST-Rep1–670 (Figure S3) and NbHSP70 or TaHSP70 was expressed as a 6×histidine-tagged fusion His-NbHSP70 and His-TaHSP70, respectively (Figure S3). ELISA plate wells were coated with purified GST-Rep1–670. The coated wells were then incubated with increasing concentrations of purified 6×His-tagged NbHSP70 or TaHSP70. Complex retention was detected using an anti-His antiserum. Saturation binding curves were established for NbHSP70 (Fig. 7B) and TaHSP70d (Fig. 7C). No signal was detected when His-NbHSP70 or His-TaHSP70 was replaced with the His protein. These results confirmed that the replicase directly interacted with both NbHSP70 and TaHSP70 and the mechanisms of their interaction were similar.
We next examined the subcellular distribution of the CWMV replicase when expressed alone or together with NbHSP70 or TaHSP70. The replicase (aa 1–1350, without the read through domain) was fused to the C terminus of green fluorescent protein (Rep1–1350-GFP) or of red fluorescent protein (Rep1–1350-mCherry) and introduced into N. benthamiana epidermal cells by Agrobacterium infiltration. When the fluorescence was observed by confocal microscopy, Rep1–1350-GFP (Fig. 8A) or Rep1–1350-mCherry (Fig. 8A) were distributed in the cytoplasm forming numerous granular aggregations or inclusion-like structures, which were different from the subcellular distribution of NbHSP70 and TaHSP70 when expressed alone (Fig. 5 Mock). When Rep1–1350-mCherry was co-expressed with NbHSP70:GFP or TaHSP70:GFP, Rep:mCherry appeared to be co-localized with NbHSP70:GFP or TaHSP70:GFP in most of the granular aggregations or inclusion-like structures within the co-transfected cells (Fig. 8B), a pattern similar to the subcellular distribution of NbHSP70 or TaHSP70 in the cells inoculated with RNA1 or RNA1/RNA2 of CWMV (Fig. 5 RNA1 and RNA1/RNA2) and shown in BiFC assays (Fig. 7A) but different from the subcellular distribution of NbHSP70 and TaHSP70 when expressed alone (Fig. 5 Mock) or co-expressed with mCherry in cells (Fig. 8), suggesting that the interaction is responsible for the differences in subcellular localization of NbHSP70 and TaHSP70. We also noted that the granular aggregations or inclusion-like structures formed in co-transinfected cells were similar in size and appearance to those of cells expressing Rep:mCherry alone. Based on these results, we formed a hypothesis that the viral replicase might recruit NbHSP70 or TaHSP70 into the granular aggregations or inclusion-like structures.
In all plant RNA viruses, the viral replicases are major components of the viral inclusions, which are thought to be related to the intracellular membrane system and to serve as a factory for viral replication or assembly25. To validate the hypothesis, we expressed TaHSP70 and the viral replicase or its truncated mutants alone or co-expressed a mixture of them and then performed subcellular fractionation assays as described previously. As shown in Fig. 9A, TaHSP70 was always detectable in both nuclear and cytoplasmic fractions when expressed alone; interestingly, Rep1–1430 and its truncated mutants, Rep1–670 and Rep670–1430, were detectable in membrane fractions but not in nuclear or cytoplasmic fractions when expressed alone, suggesting that the viral replicase is a membrane protein. However, TaHSP70 was detectable in the membrane fraction but not in nuclear or cytoplasmic fractions when co-expressed with Rep1–1430 and its truncated mutant Rep1–670. When co-expressed with Rep670–1430, TaHSP70 was detectable in all fractions (Fig. 9B). In another series of subcellular fractionation assays, NbHSP70 appeared to have a similar behavior to that of TaHSP70 (Data not shown). Taken together, these results supported the hypothesis that the viral replicase recruits NbHSP70 or TaHSP70 to the membrane fraction by specific and direct interaction and suggests that the interaction may be involved in the formation of functional inclusion-like structures.
HSPs are essential for cell viability, the cell cycle, apoptosis and the innate immunity pathway by preventing protein misfolding and aggregation, promoting protein complex assembly and disassembly, facilitating protein trafficking and activating the regulation of proteins in signal transduction pathways2,3,30. A HSP70 from wheat germ lysate has the ability to interact functionally with chaperone proteins of the animal kingdom to cooperate in protein folding26, suggesting that the HSP70 family has a highly-conserved function. Here TaHSP70 and NbHSP70 were shown to be expressed at relatively low levels under normal conditions, suggesting that this type of HSP70 could have functions in growth and development. The TRV-based silencing of NbHSP70 resulted in distinct crinkles and abnormal veins on leaves of N. benthamiana plants at 10dpi (Fig. 3A,B) and even the death of young leaves and shoot apical meristem at 14dpi, which were effects similar to those seen in N. benthamiana plants with PVX-based silencing of NbHSP70c-1 (accession number: AB105430; partial sequence: 1203nt; 383 aa), a cytoplasmic member of the HSP70 family27,28. Sequence analysis showed that these two HSP70s had 86.6% nucleotide and 79.6% amino acid identity and their similar silencing phenotypes suggested that they might be required for normal growth and development of N. benthamiana and that they could have redundant functions. NbHSP70c-1 has been shown to be involved in plant defense signaling pathways and its silencing reduces the expression of defense genes, thus compromising plant resistance to bacterial or fungal disease27. Silencing of NbHSP70c-1 impaired viral multiplication and movement of tobacco mosaic virus (TMV), reflecting the distinct roles of plant HSP70s in viral, as opposed to bacterial or fungal infection28. In this study, both VIGS silencing and treatment with quercetin, a specific inhibitor of HSP7020, significantly decreased the accumulation of CWMV genomic RNAs. In these and overexpression assays, we also noted that the expression level of the HSP70s appeared to be positively correlated with the accumulation of CWMV genomic RNA in N. benthamiana. This supports the idea that the HSP70s are functionally redundant during viral infection although there may be some differences in function since, for example, NbHSP70c-1 was thought to be a cytoplasmic protein whereas in our experiments NbHSP70 and TaHSP70 were present in both the cytoplasm and nucleus.
Infection and replication of all viruses greatly depends on host proteins, And HSP70s are one of the best studied of such host factors1,29,30. Members of the HSP70 family can participate in various steps of the viral infection cycles, including viral RNA replication, viral protein folding, virion assembly, and viral movement, perhaps depending on the different virus-host systems1,31,32. In geminiviruses, HSP70s can interact with the coat protein (CP)33 or movement protein (MP)34; in potexviruses, HSP70 has also been implicated in an interaction with CP35. However, we found no interaction between NbHSP70 or TaHSP70 and the MP or CP of CWMV, suggesting that these HSP70s may not be directly involved in CWMV movement or other specific functions of the MP and CP. Previous studies have shown that HSP70s interact with different viral replicases and are involved in replication and transcription of some eukaryotic RNA viruses36,37,38,39,40,41. During potyviral infection, HSP70 interacts with the viral replicase and regulates gene expression in co-operation with CPIP31,38,42. In our experimental system, TaHSP70 or NbHSP70 was required for accumulation of CWMV genomic RNAs. This is consistent with previous studies showing the importance of HSP70s for efficient viral infection38,43,44 and which may indicate that HSP70s regulate replication or transcription. To our knowledge, this is the first host factor identified to play a crucial role in furoviral infection.
In host cells, viruses often induce host membrane rearrangements to form novel cytoplasmic vesicular compartments where viral RNA, replicases, or replicase-associated proteins interact with host factors and assemble the viral replicase complexes (VRC) for their own efficient replication45. VRC studies have provided important information about viral pathogenicity, virus-host interactions and the mechanisms regulating viral genome replication45,46. In tombusviruses, HSP70 promotes the subcellular transport of replicase proteins to intracellular membranes and is required for the in vitro activity or assembly of the viral replicase complex (VRC)40,47. HSP70s have also been found to be necessary for the proper conformational arrangement of the replicase and its assembly at sites of viral replication48,49,50,51. In this study, the viral replicase, a major component of VRC, could form granular aggregations or viral inclusion-like structures in membranes when expressed alone, suggesting that it may be the skeleton or organizer for VRC formation. NbHSP70 and TaHSP70 appeared to be translocated into the intracellular membrane when co-expressed with the CWMV replicase. In addition, NbHSP70 or TaHSP70 also formed granules or viral inclusion-like structures in CWMV-infected cells. All of these results suggests that the host factor is a component of the VRC and that it is recruited by the replicase during CWMV infection. The regulated and re-localized molecular chaperones may regulate the conformation or replication activity rather than formation of VRC.
CWMV-infected wheat plants with typical mosaic symptoms were collected from a disease nursery in Yantai city, Shangdong province, China. Nicotiana benthamiana plants at the six-leaf stage were mechanically inoculated with mixtures of in vitro transcripts from RNA1 and RNA2, as described previously19. Systemic infection was confirmed by RT-PCR 14 days after inoculation. All N. benthamiana plants were grown in a cabinet at 17°C, with 16h light/8h dark and 70% r.h. Leaves were collected from the infected plants, frozen and stored at −80°C until use. Total RNAs were extracted from plants using the Trizol Reagent (Invitrogen) and stored at −80°C.
About 0.1g leaf tissue frozen in liquid nitrogen was ground to a fine powder and thawed in plant protein extraction buffer (Sigma) containing Protease Inhibitor Cocktail Tablets (Roche; 1 Tablet/50ml). The mixture was centrifuged at 18,000g for 10min at 4°C. 20μg of each protein sample was boiled in SDS-PAGE buffer at 100°C for 10min and centrifuged at 18,000g for 5min. The supernatant was separated in 15% SDS-PAGE, followed by Western blot analysis using rabbit polyclonal antibody against purified CWMV particles or other commercial antibodies as the primary antibodies (1:5000) and anti-rabbit goat IgG conjugated with alkaline phosphatase as the secondary antibody (1:10000) following the method described previously19.
Tobacco Rattle Virus (TRV)-based vectors, pYL196 (RNA1) and pTRV (RNA2), were kindly provided by Dr Yule Liu, Tsinghua University, Beijing, China52. The partial sequence of NbHSP70 was amplified by RT-PCR with the primer pair Nb70F/Nb70R (Table S1) from a leaf cDNA library of N. benthamiana plants, ligated into pTRV vector digested with XbaI and KpnI restriction enzymes, producing vector TRV:NbHSP70 for silencing the expression of endogenous NbHSP70 in N. benthamiana plants. The empty vector, TRV:00, was used for the control treatment. Agro-infiltration for VIGS was performed as previous described53. The upper leaves were inoculated with CWMV at 7–10dpi when silencing was fully established.
Northern blot analysis was performed essentially as previously described19. Total RNAs were extracted from leaf tissues using TRIzol reagent (Invitrogen) and treated with DNase (TAKARA). 3μg of total RNAs were separated on a denaturing 2% formaldehyde agarose gel and transferred to Hybond-N+ membranes (Amersham Bioscience) using 20×SSC. The RNAs were cross-linked to the membrane matrix by UV for 45s. Northern blotting for assays of CWMV genomic RNAs were carried out using DIG High Prime DNA Labeling and Detection Starter Kit II (Roche). DNA oligonucleotides complementary to the 3′-terminus of the CWMV genome or specifically complementary to CWMV RNA1 were labeled with digoxigenin (DIG) at their 3′ ends using the DIG Oligonucleotide Tailing Kit (Roche) and then purified using a G25 Sephadex column (GE). Membranes were prehybridized for 2h and hybridized overnight at 42°C using the DIG Luminescent Detection Starter Kit for Nucleic Acids (Roche). The hybridization signals were visualized by the Amersham Imager 600 (GE). All these procedures followed the manufacturers’ instructions.
The yeast GAL4 binding domain vector pGBKT7 and GAL4 activation domain vector pGADT7 (Clontech, Palo Alto, CA) were used for yeast two hybrid (YTH) assays. To construct plasmids for YTH analysis, the coding sequence of TaHSP70 (GenBank accession no. AF005993) and NbHSP70 (GenBank accession no. KX912913) were amplified separately by PCR from Triticum aestivum and N. benthamiana cDNA libraries using primer pairs BD-Ta70N/BD-Ta70C and BD-Nb70N/ BD-Nb70C (Table S1). The amplified fragments were digested with NdeI/BamHI and cloned into similarly digested yeast GAL4 binding domain pGBKT7 vectors creating the recombinant bait plasmids BD-TaHSP70 and BD-NbHSP7d, respectively. In further YTH assays, a series of truncated mutants of the CWMV replicase (aa 1–670, 670–1430, 1430–1840, 1–333, 333–670, 1–167, and 167–333) were amplified separately from CWMV cDNA using the primer pairs shown in Table S1. These amplified fragments were digested with XmaI /BamHI and then inserted into pGADT7 vector digested with XmaI/BamHI creating the recombinant prey plasmids, AD-Rep1–670, -Rep670–1430, -Rep1430–1858, -Rep1–333, -Rep333–670, -Rep1–167, and -Rep167–333, respectively.
Yeast transformation was conducted in accordance with the recommended procedures (Matchmaker Gold Yeast Two-Hybrid System; Yeastmaker Yeast Transformation System 2, Clontech). Briefly, bait and prey plasmids were co-transformed into S. cerevisiae strain Y2HGold. The co-transformants were first plated on SD/-Ade/-His/-Leu/-Trp medium, and yeast colonies that grew on the auxotrophic medium were then tested for α-galactosidase activity on SD/-Ade/-His/-Leu/-Trp/X-α-Gal/ AbA medium. BD-53 and AD-T were also co-transformed as a positive control, while BD-Lam and AD-T were co-transformed as a negative control. Three independent experiments were performed to confirm the results.
To construct the vector coding for the histidine-tagged full-length NbHSP70 and TaHSP70 fusion proteins, NbHSP70 and TaHSP70 were amplified by PCR from cDNA libraries prepared from leaves of N. benthamiana or Triticum aestivum using primers pET-Nb70N/pET-Nb70C and pET-Ta70N/pET-Ta70C (Table S1), respectively. The amplified fragments were digested with BamHI/NotI and cloned into digested pET28a vector (Novagen). For construction of the vector coding for the C-terminus GST fusion of Rep1–670 fusion protein, CWMV Rep1–670 sequences were amplified from a CWMV cDNA library using the primer pair p6P1Rep1–670 N / p6P1Rep1–670 C (Table S1). The amplified fragments were digested with BamHI/EcoRI and cloned into digested pGEX-6P1 vector (GE Healthcare).
For purification of GST-tagged Rep1–670, or the GST tag itself, a 20ml overnight culture of E. coli BL21 cells containing the recombinant plasmid pGEX-Rep1–670 or pGEX6P1 vector alone was used to inoculate 100ml of LB media containing 75μg/ml of carbenicillin. Cells were grown at 37°C to an OD600 of 0.4. Protein expression was induced with 0.1mM of IPTG for 3h for Rep1–670-GST and GST. Bacterial cells were re-suspended in 20ml of phosphate buffered saline solution (PBS; 4.3mM Na2HPO4, 1.47mM KH2PO4, 137mM NaCl, 2.7mM KCl, pH 7.3) supplemented with 1mM DTT, 40mg of lysozyme, and 1× complete EDTA-free protease inhibitor. The cells were disrupted by sonication and supplemented with 1% Triton-X-100. Lysate was centrifuged at 30,000×g for 30min at 4°C. The supernatant was filtered through a 0.45μm Millex HV PVDF filter (Millipore) and used for affinity purification of either Rep1–670-GST or GST on glutathione sepharose 4B (GE Healthcare) according to the manufacturer’s protocol. For purification of histidine-tagged TaHSP70 and NbHSP70, a 5ml overnight culture of E. coli BL21(DE3) cells containing the recombinant plasmid pET28(a)-TaHSP70 or pET28(a)-NbHSP70 was used to inoculate 100ml of LB media containing 50μg/ml of kanamycin. Cells were grown at 37°C to an OD600 of 0.4 to 0.6. Protein expression was induced with 1mM of IPTG for 2h at 37°C. Bacterial cells were re-suspended in 5ml of buffer A (50mM sodium phosphate buffer pH 8.0, 300mM NaCl, 5mM β-mercaptoethanol, 0.1% Tween-20, 10% glycerol, 1× complete EDTA-free protease inhibitor). The cells were disrupted by sonication and the resulting lysate centrifuged at 30,000×g for 30min at 4°C. The supernatant was used for immobilized metal affinity purification on Talon resin (BD Biosciences). Resin was washed with buffer A supplemented with 10mM imidazole and proteins eluted with buffer B (20mM Tris-HCl pH 7.5, 300mM NaCl, 250mM imidazole, 2.5mM DTT). Concentration of all recombinant proteins produced was measured using a Bradford assay (Bio-Rad) using bovine serum albumin as standard. Protein purity and molecular weight were assessed by Coomassie staining and immunoblot analysis using monoclonal anti-histidine, monoclonal anti-GST.
Replicase protein (100μl of protein at 50ng /μl in PBS buffer) was adsorbed to wells of a polystyrene plate (Costar) by incubation at 4°C for 2h and wells were blocked with 5% milk PBS solution for 2h at room temperature. TaHSP70-His or NbHSP70-His proteins were diluted in PBS with 1% milk and 0.1% Tween-20 and incubated for 2h at 4°C in the coated wells. Detection of retained protein was achieved with a mouse monoclonal anti-His-tag antibody (Abcam, England) and horseradish peroxidase-coupled goat anti-mouse immunoglobulin (Abcam, England). Between each incubation, wells were washed three times with PBS supplemented with 0.05% Tween-20. Enzymatic reactions were performed in 100μl of OPD citrate buffer (50mM citric acid, 100mM sodium phosphate dibasic, pH 5.0, 0.5mg/ml o-phenylenediamine dihydrochloride, and 0.1% H2O2) and stopped with a solution of 3M H2SO4. Absorbance was measured at 492nm. The S.E.M. was calculated for three biological replicates from a minimum of three technical replicates.
For subcellular localization analyses, a series of recombinant plasmids including Rep1–1350-GFP, Rep1–1350-mCherry, NbHSP70-GFP and TaHSP70-GFP were constructed by the Gateway technology according to the manufacturer’s instructions (Invitrogen). The first PCR used the primer pairs Rep1–1350-GFPN/Rep1–1350-GFPC, Rep1–1350–mCherryN/Rep1–1350–mCherryC, Nb70-GFPN/Nb70-GFPC and Ta70-GFPN/Ta70-GFPC (Table S1). The second PCR was performed with the primers attB1 and attB2 and the amplified product of the first PCR as the template. The amplified product was then introduced into pDONR207 by the BP reaction and the entry clones pENTR-Rep1–1350-GFP, pENTR-Rep1–1350-mCherry, pENTR-NbHSP70-GFP and pENTR-TaHSP70-GFP were constructed. Finally, the LR clonase reaction was used to transfer Rep1–1350, NbHSP70 and TaHSP70 fragments from the entry clones to the destination vector and recombinant plasmids including pMDC43-Rep1–1350, pGWB5C-Rep1–1350, pGWB5C-NbHSP70 and pGWB5C-TaHSP70 were constructed. These recombinanats were used to transform competent E.coli strain DH5α using heat shock and selected on a medium containing 50μg/ml kanamycin and 50μg/ml hygromycin.
The BiFC vectors pCV-nYFP-C and pCV-cYFP-C (for split YFP N- terminal/C-terminal fragment expression) were previously constructed in our laboratory. For BiFC assays, the coding sequence of the N-terminal fragment (residues 1–670) of CWMV replicase was amplified using primer pair BRepF/BRepR (Table S1) and cloned into pCV-nYFP-C as a fusion with the N-terminal fragment of YFP via the BamHI/SacI sites, forming pCV-nYFP-Rep1–670. The full-length coding sequences of TaHSP70 and NbHSP70 were amplified by PCR using primer pairs BTa70F/BTa70R and BNb70F/BNb70R (Table S1), respectively. PCR products were cloned into the BamHI/SacI or BamHI/NotI sites of pCV-cYFP-C as a fusion with the C-terminal fragment of YFP, resulting in pCV-cYFP-TaHSP70 and pCV-cYFP-NbHSP70.
The recombinant binary constructs were introduced into Agrobacterium tumefaciens strain C58C1 by electroporation (Bio-Rad Gene Pulser, 0.2cm cuvettes, 25 microF, >2.5kV). Agroinfiltration was done as described24. Briefly, cultures of C58C1 harbouring a relevant binary plasmid were grown in YEP medium containing rifampicin (50μg/ml) and kanamycin (100μg/ml) at 28°C for 16h. For the BiFC assay, C58C1 strains containing the BiFC plasmids with pCV-nYFP-Rep1–670/pCV-cYFP-TaHSP70 and pCV-nYFP-Rep1–670/pCV-cYFP-NbHSP70 were re-suspended and adjusted to an OD600 of 1.0:1.0 with infiltration medium (10mM MES, pH 5.6, 10mM MgCl2, 200mM acetosyringone) before leaf infiltration, while the combinations pCV-nYFP-Rep1–670/pCV-cYFP, pCV-nYFP/pCV-cYFP-TaHSP70 and pCV-nYFP/pCV-cYFP-NbHSP70 were used as the negative controls. For sub-cellular localization, Agrobacterium cultures containing pGWB5C-Rep1–1350, pGWB5C-Rep1–1350, pGWB5C-NbHSP70 and pGWB5C-TaHSP70 were re-suspended and diluted to an OD600 of 0.6 before leaf infiltration. The cell suspensions were incubated at room temperature for 2 to 4h and then used to infiltrate 5- to 6-week-old N. benthamiana leaves. Expression of fluorescent proteins was examined at 48h post agroinfiltration54.
Plant nuclear and cytoplasmic fractionation was performed using the Plant nuclei and cytoplasmic protein extraction kit (BestBio, Shanghai) according to the manufacturer’s protocol. Membrane fractionation assays were performed as previously described55. Briefly, plant material was ground to fine powder under liquid nitrogen. 2×volumes of homogenization buffer (Sorbitol 0.5M, EDTA 10mM, PVP 40 0.5%, Protease inhibitor cocktail) were added and debris was removed by centrifugation at 8000g for 15min at 4°C. After centrifugation at 100 000g for 30min at 4°C, the supernatant corresponds to the soluble (S100) and the pellet to the particulate (P100) fraction. For the re-solubilization test, the P100 fraction was re-suspended in 5×volume of the same buffer supplemented with detergent, incubated for 30min on ice and centrifuged at 100 000g for 30min at 4°C. The supernatant corresponds to the S100 and the pellet to the P100. The S100 fraction was precipitated before analysis. The proteins were pelleted at 5000g for 5min at 4°C, washed with 80% acetone and finally re-suspended in 300μl of resuspension solution (3% SDS; 62.5mM TrisHCl pH 6.8; 10% glycerol). The samples were incubated at 65°C for 10min, centrifuged at 13 000g for 5min and the supernatant was kept for quantification and analysis. Ten micrograms were diluted in 1:5 SDS loading buffer and subjected to SDS-PAGE and immunoblotting.
Fluorescence analysis was performed using a Leica TCS SP5 confocal laser scanning microscope (Leica Microsystems, Heidelberg, Germany). GFP was excited at 488nm and the emitted light captured between 500–550nm, YFP was excited at 514nm and the emitted light captured between 530–600nm, and mCherry was excited at 561nm and emission light captured between 570–630nm. For analysis of co-localization assays, multi-tracking was used to prevent emission cross-talk between the channels. Images were captured digitally and handled using the Leica TCS software. Post-acquisition image processing was done with Adobe Photoshop version 7.0 software (Adobe Systems Inc., San Jose, CA, USA).
How to cite this article: Yang, J. et al. A furoviral replicase recruits host HSP70 to membranes for viral RNA replication. Sci. Rep. 7, 45590; doi: 10.1038/srep45590 (2017).
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This work was funded by Natural Science Foundation of China (31501604, 31601603), Project of New Varieties of Genetically Modified Wheat of China (2016ZX08002001), the Special Fund for Agro-scientific Research in the Public Interest of China (201303021), China Agriculture Research System (CARS-3-1) from the Ministry of Agriculture of China, and State Key Laboratory Breeding Base for Zhejiang Sustainable Pest and Disease Control (No. 2010DS700124-KF1512 and -KF1607)”. We thank Professor M. J. Adams, Stevenage, UK for help in correcting the English of the manuscript.
The authors declare no competing financial interests.
Author Contributions H.Z. and J.C. were responsible for study conception, design, and coordination; J.Y., F.Z., N.C., N.W., X.C., and J.L. carried out the experiments for vector construction, yeast two hybridization, Northern Blotting, ELISA-based binding assays, subcellular fractionation, and fluorescence assays; M.X., T.Z., F.Z., and J.Y. performed the virus inoculation, agro-infiltration, sample collection, and RNA isolation for gene expression and blotting assays. H.Z., J.Y., and J.C. were responsible for data collection and analysis and drafted the manuscript. All authors read and approved the final manuscript.