- Open Access
Cassava geminivirus agroclones for virus-induced gene silencing in cassava leaves and roots
Plant Methods volume 14, Article number: 73 (2018)
We report the construction of a Virus-Induced Gene Silencing (VIGS) vector and an agroinoculation protocol for gene silencing in cassava (Manihot esculenta Crantz) leaves and roots. The African cassava mosaic virus isolate from Nigeria (ACMV-[NOg]), which was initially cloned in a binary vector for agroinoculation assays, was modified for application as VIGS vector. The functionality of the VIGS vector was validated in Nicotiana benthamiana and subsequently applied in wild-type and transgenic cassava plants expressing the uidA gene under the control of the CaMV 35S promoter in order to facilitate the visualization of gene silencing in root tissues. VIGS vectors were targeted to the Mg2+-chelatase gene in wild type plants and both the coding and promoter sequences of the 35S::uidA transgene in transgenic plants to induce silencing. We established an efficient agro-inoculation method with the hyper-virulent Agrobacterium tumefaciens strain AGL1, which allows high virus infection rates. The method can be used as a low-cost and rapid high-throughput evaluation of gene function in cassava leaves, fibrous roots and storage roots.
VIGS is a powerful tool to trigger transient sequence-specific gene silencing in planta. Gene silencing in different organs of cassava plants, including leaves, fibrous and storage roots, is useful for the analysis of gene function.
We developed an African cassava mosaic virus—based VIGS vector as well as a rapid and efficient agro-inoculation protocol to inoculate cassava plants. The VIGS vector was validated by targeting endogenous genes from Nicotiana benthamiana and cassava as well as the uidA marker gene in transgenic cassava for visualization of gene silencing in cassava leaves and roots.
The African cassava mosaic virus—based VIGS vector allows efficient and cost-effective inoculation of cassava for high-throughput analysis of gene function in cassava leaves and roots.
Validation of gene function in plants can be challenging in non-model species for which T-DNA insertion lines are not available and/or genetic transformation is time-consuming and inefficient. Therefore, reverse genetics tools such as virus-induced gene silencing (VIGS) are particularly useful when facing these limitations . Initially, the VIGS technique was established to silence leaf-expressed genes [2, 3]. VIGS vectors were subsequently shown to effectively silence genes expressed in Nicotiana benthamiana, Arabidopsis and tomato roots  as well as potato tubers .
Cassava (Manihot esculenta Crantz) is one of the most important root crops worldwide, producing starchy roots used as staple food by more than 800 million people . Over the last decade, the use of cassava for industrial applications has also increased [7, 8]. Although reliable cassava genetic transformation protocols are now available, transformation of cassava remains a lengthy process and several cassava varieties are recalcitrant to genetic transformation [9,10,11,12]. Therefore, efficient reverse genetic tools appear as particularly suitable to investigate the function of cassava genes for example those identified in large-scale omics studies [13,14,15]. Those studies are now facilitated by the release of cassava reference genome sequences [16,17,18].
Cassava mosaic geminiviruses are bipartite DNA begomoviruses causing the cassava mosaic disease (CMD)  and infecting a wide range of cassava varieties grown in Asia, South America and Africa [20,21,22,23]. We previously established African cassava mosaic virus isolate ACMV-[NOg] DNA-A and DNA-B clones to agro-inoculate cassava plants and screen varieties for CMD resistance . Biolistic delivery of a modified Cameroon isolate ACMV-[CM] can trigger VIGS in cassava leaves . Recently, a VIGS vector based on the East African cassava mosaic virus isolate EACMV-[K201] was developed to screen for virus resistance by biolistic delivery . The high cost of commercial gene guns makes VIGS vectors relying on biolistic delivery methods not affordable to all labs . Other methods for the inoculation of geminiviruses to plants include DNA abrasion  and Agrobacterium [24, 29, 30]. DNA abrasion is not suitable for all type of host plants [27, 28] and reports of successful geminivirus inoculation in cassava by abrasion have so far been scarce. On the contrary, efficient agro-inoculation with cassava geminiviruses agroclones has been previously established in cassava [24, 31]. Therefore, development of agroclones for VIGS in cassava appears to be a suitable strategy to enable the cost-effective use of this reverse genetics tool in cassava.
Because geminiviruses are detectable in the roots of tomato, Arabidopsis and cotton plants [32,33,34,35,36], we also hypothesized that cassava geminiviruses could sustain VIGS in cassava roots, further expanding the use of VIGS as a reverse genetic tool.
Here we present the development of a VIGS agroclone and the establishment of a robust and efficient inoculation protocol that leads to VIGS in cassava leaves as well as in fibrous and storage roots.
VIGS vector construction, functionality check in N. benthamiana and cassava agro-inoculation
We constructed a VIGS vector based on the DNA-A ACMV-[NOg] agroclone  by partial replacement of the coat protein sequence with a target sequence [3, 25, 36]. A 459 bp fragment of the ACMV AV1 gene coding for the capsid protein was replaced by a 30 bp multiple cloning site (VIGS-MCS; Fig. 1 and Additional file 1: Fig. S1). The infectious agroclones assembled as tandem repeats in a binary vector were previously used for the evaluation of ACMV resistance in transgenic cassava as well as in wild-type cassava varieties [20, 24]). The infectivity of the VIGS-MCS agroclone along with the VIGS-Chl1 construct, targeting the Mg2+-chelatase gene, were first confirmed in Nicotiana benthamiana using the Agrobacterium tumefaciens strain LBA4404. These DNA-A-based agroclones co-inoculated with the agroclone DNA-B resulted in 100% infection rates in Nicotiana benthamiana. We concluded that the infectivity of VIGS-MCS and VIGS-Chl1 agroclones did not differ from the non-modified ACMV DNA-A agroclone in Nicotiana benthamiana (Additional file 1: Fig. S2 and Table S1 A, C and D). Inoculation of the agroclones was subsequently tested on wild-type cultivar 60,444 cassava plants propagated via stem cuttings and grown in the greenhouse. We adapted a previously established method  to agro-inoculate cassava (Fig. 2). Because agro-inoculation with the VIGS-MCS and VIGS-Chl1 agroclones using the LBA4404 strain did not result in symptomatic cassava (Additional file 1: Table S1 C and D), the agroclones were transferred to the hyper-virulent strain AGL1. Performing the agro-inoculation with the AGL1 strain, infection rates of 27% and 92% were recorded for the VIGS-MCS agroclone and the VIGS-Chl1 agroclone respectively (Additional file 1: Table S1 C and D).
Visualization of VIGS in cassava leaves and roots
In order to visualize gene silencing in both leaves and roots, we used a transgenic cassava line transformed with the pCambia1301 vector (GenBank: AF234297.1) containing a 35S::uidA gene construct. The 35S::uidA transgenic line expresses the uidA reporter gene encoding the β-glucuronidase enzyme (GUS) under the control of the CaMV 35S promoter. The 35S::uidA cassava plants were agro-inoculated with VIGS constructs carrying either a DNA fragment of the uidA coding sequence (VIGS-uidA) or DNA fragment of the 35S promoter (VIGS-35S). Both VIGS constructs resulted in high infection rates (Additional file 1: Table S1 E and F). We consistently observed higher GUS staining in young leaves as compared to old leaves in the control cassava plants (Fig. 3a and Additional file 1: Fig. S3A). Infection of 35S::uidA cassava leaves with the wild-type ACMV virus led to increased GUS staining of symptomatic leaves (Fig. 3b and Additional file 1: Fig. S3B). Visual observation of GUS silencing in leaves of plants infected with VIGS-uidA and VIGS-35S vectors suggested that the silencing of the uidA transgene was higher with the VIGS-35S vector (Fig. 3c, d and Additional file 1: Fig. S3C, D).
We previously found that the 35S::uidA reporter gene is strongly expressed in fibrous roots of transgenic pCambia1301 cassava lines . In order to assess the level of uidA silencing in the roots of 35S::uidA plants inoculated with the VIGS constructs, stem cuttings from the VIGS-uidA and VIGS-35S infected plants were propagated in vitro and adventitious roots emerging from these cuttings were tested for GUS activity. Infections with both VIGS-uidA and VIGS-35S resulted in uidA silencing in adventitious roots (Fig. 4 and Additional file 1: Fig. S4). The GUS-staining was consistently weaker in the roots of the VIGS-35S infected plants as compared to the roots of the VIGS-uidA infected plantlets (Fig. 4c, d and Additional file 1: Fig. S4C, D). The in vitro plantlets were subsequently transferred to the greenhouse and grown for 6 months to produce storage roots. Both VIGS-uidA and VIGS-35S vectors caused reduced GUS activity and staining in the fibrous and storage roots from VIGS-infected plants (Fig. 4 and Additional file 1: Fig. S5). As previously found for the in vitro adventitious roots (Fig. 4 and Additional file 1: Fig. S4), the VIGS-35S vector consistently caused stronger silencing of the uidA gene in both fibrous and storage roots as compared to VIGS-uidA vector.
VIGS of endogenous genes in wild-type cassava
Since the VIGS vectors could efficiently silence the uidA transgene in cassava plants, we also tested the VIGS vector to silence endogenous genes. We targeted the Chl1 gene (Manes.17G053100), which encodes the first enzyme of the chlorophyll biosynthesis pathway (Mg2+-chelatase subunit I), because the pale phenotype in tissues that have lost the function of the enzyme can be easily observed . Three to four weeks after agro-inoculation, both CMD symptoms and Chl1 silencing were visible in infected cassava plants (Fig. 5 and Additional file 1: Fig. S6). The Chl1 silencing pattern followed the viral movement through the stem, vascular tissue and leaves. The extent of silencing appears to be correlated with symptom severity. Silencing of the Chl1 gene was maintained during 10 sequential multiplications of the original inoculated plants and was visible in plants propagated in vitro and in the greenhouse (Additional file 1: Fig. S7A). The Chl1 silencing could also be transmitted from VIGS-inoculated 60,444 rootstocks to non-infected scions of the BRA222 cassava cultivar (Additional file 1: Fig. S7B). RT-qPCR analysis of VIGS-Chl1-infected 60,444 plants confirmed that Chl1 expression was significantly down-regulated in intermediate leaves displaying clear CMD symptoms with patches of silenced and non silenced tissue areas (Fig. 6a). Thermotherapy of in vitro plantlets was effective in eliminating the VIGS-Chl1 vector and restoring a fully green phenotype after a four-cycle treatment (Additional file 1: Fig. S7C). In addition, an endogenous root-expressed gene coding for a lysin motif (LysM) receptor kinase (Manes.12G071800) and present on a cassava genomic scaffold associated with the CMD2 locus , was targeted with a VIGS construct containing a 500 bp fragment homologous to exons from the 5′ and 3′ ends of the Manes.12G071800 gene (Additional file 1: Table S1 G). A moderate and significant silencing (ranging from 1.4 to 3.7 fold as compared to control VIGS-uidA inoculated plants) of Manes.12G071800 gene could be detected by RT-qPCR in fibrous roots, root tips and storage roots from symptomatic plants inoculated with the VIGS-71800 vector (Fig. 6b).
In the present work, we demonstrated that the expression of genes and transgenes can be effectively downregulated after infection with a modified ACMV agroclone in Nicotiana benthamiana and cassava leaves.
Using 35S::uidA cassava plants we observed that the uidA transgene can be silenced more effectively with a VIGS construct targeting the 35S promoter (VIGS-35S) than the coding sequence (VIGS-uidA). The efficacy of gene silencing by targeting a promoter has been previously reported for transgenic maize . It remains to be demonstrated that the stronger silencing of the uidA gene in cassava plants inoculated with the VIGS-35S construct as compared to VIGS-uidA construct is caused by 35S promoter methylation and concomitant reduction of its transcriptional activity in transgenic cassava. The more intense GUS staining in leaves, fibrous roots and storage roots of 35S::uidA transgenic cassava infected with the non-modified virus also suggests a basal transgene silencing in this transgenic line, that is suppressed by the presence of ACMV-[NOg] and the production of viral suppressor(s) of RNA silencing, possibly AC2 and/or AC4 viral proteins .
Our results showed that an ACMV-based VIGS vector is also able to trigger silencing in cassava fibrous and storage roots. While visual observation of silencing in the transgenic 35S::uidA cassava line suggested a relatively strong silencing in cassava fibrous and storage roots, expression analysis of endogenous cassava genes revealed a moderate gene silencing in root tissues for the selected gene candidate.
Once infectious clones of cassava brown streak viruses (CBSVs) become available, they could also be developed into VIGS vectors to silence root-expressed genes in cassava, given their replication rate in cassava roots [41, 42]. However, development of CBSV-based VIGS vectors might require the use of attenuated CBSV isolates to avoid the interference of CBSV root symptoms in gene function analysis and phenotype evaluation. It should also be noted that geminivirus-based VIGS technique remains constrained to cassava genotypes susceptible to cassava geminiviruses. Therefore development of other VIGS vectors such as ipomovirus-based vectors could also be instrumental to expand the use of the VIGS technique to genotypes resistant or tolerant to geminiviruses.
This VIGS protocol for cassava reported here allows cost-effective and high-throughput silencing of candidate genes by a simple agro-inoculation method in cassava. Given that most cassava genotypes are CMD susceptible, this reverse genetic tool can be widely used for gene validation studies. In addition, the VIGS observed in cassava fibrous and storage roots increases the versatility of this technique, which was originally developed and tested for leaf-expressed genes.
The cassava VIGS vector was designed by replacing 459 bp of the AV1 sequence (without affecting the AV2 gene) in the ACMV-[NOg] DNA A genome with a 30 bp multiple cloning site (Additional file 1: Fig. S1). The primers and plasmids used for the generation of the VIGS construct are listed in the Additional file 1: Tables S1 and S2. Sequence from the Chl1 first exon (Manes.17G053100, 454 bp) was kindly provided by Stephan Winter (DSMZ, Germany). The cassava genome assembly employed to design the DNA fragments for specific gene silencing was based on the cassava AM560 reference genome version 4.1 . DNA fragments with flanking Spe I and Kpn I restriction sites were first ligated in pJET1.2 (Life Technologies) and subsequently sequenced. After sequence confirmation, the fragments were mobilized into the VIGS vector digested with the Spe I and Kpn I restriction enzymes. The final constructs were transferred to Agrobacterium tumefaciens AGL1 competent cells using electroporation.
Plant material and transgenic lines
All the experiments were performed using the cassava cultivar 60,444, except for the grafting experiment in which the BRA222 genotype was used. The 35S:::uidA cassava transgenic plant was generated using the pCambia 1301 vector (GenBank: AF234297.1) and the genetic transformation protocol previously established in our laboratory [9, 12]. The transfer of greenhouse material to in vitro conditions and thermotherapy treatment of in vitro material for virus elimination was performed as described in the CIAT handbook (Mafla et al. . Briefly, in vitro cuttings were incubated at 37 °C for 12 days and emerging shoots were employed as new cuttings. The procedure was repeated three times.
VIGS assay in cassava and N. benthamiana
For VIGS inoculation experiments, 6 weeks-old cassava plants grown from stem cuttings and 3 weeks-old N. benthamiana plants grown from seeds in the greenhouse were used for agroinoculation.
Agrobacterium tumefaciens LBA4404 and AGL1 strains containing the different VIGS constructs were refreshed from glycerol stocks on YEBA plates (5 g/L beef extract, 1 g/L yeast extract, 5 g/L peptone, 5 g/L sucrose, 0.5 g/L MgCl2, 1.5% agar) containing 100 mg/L carbenicillin (C), 20 mg/L rifampicin (R) and 50 mg/L kanamycin (K), and grown for 48 h at 28 °C in the dark. Fifty-ml sterile tubes containing 5 mL of YEB + C100/R20/K50 were inoculated with the different clones separately and grown for 24–36 h at 28 °C and 150 rpm until they reached an OD600 nm > 1. Two mL of the starter cultures were added to 1 L Erlenmeyer flasks containing 100 mL of YEB + C100/R20/K50. Cultures were grown for 24–36 h at 28 °C and 150 rpm until they reached an OD600 nm = 1.5–2. Agrobacteria suspensions were centrifuged in 250 mL bottles, previously sterilized with 70% EtOH and rinsed with sterile deionized water. After centrifugation at 4000g for 20 min at room temperature, the bacterial pellets were carefully re-suspended in 300 mL of sterile deionized water at room temperature, and centrifuged again as indicated previously. The washed bacterial pellets were re-suspended carefully in 10–20 mL of LB and OD600 nm adjusted with LB to a final value of 4. A defined volume of suspension of Agrobacterium carrying the DNA-A vector (or VIGS vector) combined with the same volume of suspension of Agrobacterium carrying the DNA-B vector was prepared. After addition of acetosyringone to a final concentration of 200 μM, the bacterial suspensions were kept at room temperature for 3 h at 50 rpm. To agro-inoculate the plants, we adapted a protocol previously established in the laboratory to screen for ACMV resistance . A 1 mL insulin syringe (0.33 mm/29 G/12.7 mm) was used to inject agrobacteria suspension at least three times near the axillary buds without damaging the meristems and the same syringe is used to gently puncture the stem 5–7 times. Inoculated plantlets were kept overnight at 20–24 °C in the dark and then placed in the greenhouse (28 °C, 16-h day length, 22 klx, 50% humidity). Alternatively, when more than 10 plants for a particular construct were agro-inoculated, we employed a high-throughput option of this protocol: the upper leaves were removed and a 21G needle, previously soaked in agrobacteria suspension, was used to puncture the stem at least 3 times prior to dipping the 4–5 week-old plantlets into a 50 mL tube containing the agrobacteria suspension for 30 s. Plantlets were subsequently allowed to recover for 4 days in a high humidity chamber (28 °C, 16-h day length, 22 klx, >80% humidity) before being placed under greenhouse conditions (28 °C, 16-h day length, 22 klx, 50% humidity). All experiments included at least three biological replicates per treatment.
GUS staining and image processing
Plant tissue samples were first incubated in pre-cooled (− 20 °C) 90% acetone for 2 h at − 20 °C. The material was rinsed with freshly prepared GUS buffer (100 mM NaH2PO4 pH 7, 10 mM EDTA-Na2, 0.5 mM K4[Fe(CN)6], 0.5 mM K3[Fe(CN)6], 0.1% Triton-X100) , and then incubated for 20 min in GUS buffer at room temperature. The buffer was discarded and fresh GUS buffer containing 1 mM X-Gluc was added. The staining was performed for 24 h at 37 °C in the dark. Every step in the staining protocol included 20 min of vacuum infiltration at room temperature. For the staining of fibrous roots from in vitro plants, the agar media was carefully removed with tap water. For staining intermediate and storage roots from greenhouse plants, the X-Gluc concentration was increased to 2 mM. After the 24 h incubation, the staining solution was discarded and the samples were de-stained three times and stored in 70% EtOH. After 5 min of rehydration in deionized water, leaves and fibrous roots from in vitro plantlets were photographed on a light chamber with a Nikon D700 camera (VR AF-S Micro Nikkor 105 mm 1:2:8 G ED objective), and image brightness was adjusted using Adobe Photoshop software. Intermediate and storage roots were photographed with the same equipment under standard room illumination conditions and images were not adjusted for brightness.
RNA extraction and RT-qPCR
Three symptomatic intermediate leaves were pooled for each biological replicate and total RNA was extracted according to the protocol by Soni and Murray . Fibrous and storage roots from plants displaying leaf symptoms were collected for RNA extraction. Total RNA from fibrous roots was prepared using the Invitrap Spin Plant RNA Mini Kit (Stratec Molecular GmbH, Berlin, Germany) according to the manufacturer’s instructions and using the “RP lysis” solution option. Total RNA from storage roots was extracted using a protocol established for nucleic acid extraction from pineapple samples . All RNA samples were quality checked using the NanoDrop system (Thermo Scientific, Wilmington, USA). RNA samples were treated with DNase I and converted to cDNA using the RevertAid First Strand cDNA Synthesis Kit (Thermo Scientific, Wilmington, USA) according to the manufacturer’s instructions. qPCR was performed using the 7500 Fast Real-Time PCR System (Applied Biosystems) and 5–50 ng of cDNA, 1 μM of primers and Fast SYBR Green Master Mix (Applied Biosystems) in a final volume of 20 μL. Each cDNA sample was checked for DNA contamination by including in parallel a total RNA sample treated with DNAse I as blank for qPCR. The RT-qPCR analysis included at least two technical replicates per sample. Relative gene expression was calculated using the  method and the PP2A gene (Manes.09G039900) expression values for normalization .
Differences in gene expression levels measured by RT-qPCR, were analyzed using two-tailed T tests.
African Cassava Mosaic Virus
100 mg/L carbenicillin
cauliflower mosaic virus
cassava brown streak viruses
cassava mosaic disease
50 mg/L kanamycin
multiple cloning site
20 mg/L rifampicin
virus-induced gene silencing
Lacomme C. Strategies for altering plant traits using virus-induced gene silencing technologies. Methods Mol Biol. 2015;1287:25–41.
Ratcliff F, Martin-Hernandez AM, Baulcombe DC. Tobacco rattle virus as a vector for analysis of gene function by silencing. Plant J. 2001;25:237–45.
Turnage MA, Muangsan N, Peele CG, Robertson D. Geminivirus-based vector for gene silencing in Arabidopsis. Plant J. 2002;20:107–14.
Valentine T, Shaw J, Blok VC, Phillips MS, Oparka KJ, Lacomme C. Efficient virus-induced gene silencing in roots using a modified tobacco rattle virus vector. Plant Physiol. 2004;136:3999–4009.
Faivre-Rampant O, Gilroy EM, Hrubikova K, Hein I, Millam S, Loake GJ, Birch P, Taylor M, Lacomme C. Potato virus X-induced gene silencing in leaves and tubers of potato. Plant Physiol. 2004;134(4):1308–16.
FAO. Save and grow: cassava. A guide to sustainable production intensification. Rome: FAO; 2013. p. 23–53.
Balat M, Balat H. Recent trends in global production and utilization of bio-ethanol fuel. Appl Energy. 2009;86:2273–82.
Jansson C, Westerbergh A, Zhang J, Xinwen Hu SC. Cassava, a potential biofuel crop in (the) People’s Republic of China. Appl Energy. 2009;86:S95–9.
Bull SE, Owiti JA, Niklaus M, Beeching JR, Gruissem W, Vanderschuren H. Agrobacterium-mediated transformation of friable embryogenic calli and regeneration of transgenic cassava. Nat Protoc. 2009;4(12):1845–54.
Chetty CC, Rossin CB, Gruissem W, Vanderschuren H, Rey MEC. Empowering biotechnology in southern Africa: establishment of a robust transformation platform for the production of transgenic industry-preferred cassava. New Biotechnol. 2013;30(2):136–43.
Niklaus M, Gruissem W, Vanderschuren H. Efficient transformation and regeneration of transgenic cassava using the neomycin phosphotransferase gene as aminoglycoside resistance marker gene. GM Crops. 2011;2(3):193–200.
Zainuddin IM, Schlegel K, Gruissem W, Vanderschuren H. Robust transformation procedure for the production of transgenic farmer-preferred cassava landraces. Plant Methods. 2012;8(1):24.
Maruthi MN, Bouvaine S, Tufan HA, Mohammed IU, Hillocks RJ. transcriptional response of virus-infected cassava and identification of putative sources of resistance for cassava brown streak disease. PLoS ONE. 2014;9(5):e96642.
Vanderschuren H, Nyaboga E, Poon JS, Baerenfaller K, Grossmann J, Hirsch-Hoffmann M, Kirchgessner N, Nanni P, Gruissem W. Large-scale proteomics of the cassava storage root and identification of a target gene to reduce postharvest deterioration. Plant Cell. 2014;26(5):1913–24.
Zhang Y, Ding Z, Ma F, Chauhan RD, Allen DK, Brutnell TP, Wang W, Peng M, Li P. Transcriptional response to petiole heat girdling in cassava. Sci Rep. 2015;5:8413.
Bredeson JV, Lyons JB, Prochnik SE, Wu GA, Ha CM, Edsinger-Gonzales E, Grimwood J, Schmutz J, Rabbi IY, Egesi C, Nauluvula P, Lebot V, Ndunguru J, Mkamilo G, Bart RS, Setter TL, Gleadow RM, Kulakow P, Ferguson ME, Rounsley S, Rokhsar DS. Sequencing wild and cultivated cassava and related species reveals extensive interspecific hybridization and genetic diversity. Nat Biotechnol. 2016;34:562.
Prochnik S, Marri PR, Desany B, Rabinowicz PD, Kodira C, Mohiuddin M, Rodriguez F, Fauquet C, Tohme J, Harkins T, Rokhsar DS, Rounsley S. The cassava genome: current progress, future directions. Trop Plant Biol. 2012;5(1):88–94.
Wang W, Feng B, Xiao J, Xia Z, Zhou X, Li P, Zhang W, Wang Y, Møller BL, Zhang P, Luo MC, Xiao G, Liu J, Yang J, Chen S, Rabinowicz PD, Chen X, Zhang HB, Ceballos H, Lou Q, Zou M, Carvalho LJ, Zeng C, Xia J, Sun S, Fu Y, Wang H, Lu C, Ruan M, Zhou S, Wu Z, Liu H, Kannangara RM, Jørgensen K, Neale RL, Bonde M, Heinz N, Zhu W, Wang S, Zhang Y, Pan K, Wen M, Ma PA, Li Z, Hu M, Liao W, Hu W, Zhang S, Pei J, Guo A, Guo J, Zhang J, Zhang Z, Ye J, Ou W, Ma Y, Liu X, Tallon LJ, Galens K, Ott S, Huang J, Xue J, An F, Yao Q, Lu X, Fregene M, López-Lavalle LA, Wu J, You FM, Chen M, Hu S, Wu G, Zhong S, Ling P, Chen Y, Wang Q, Liu G, Liu B, Li K, Peng M. Cassava genome from a wild ancestor to cultivated varieties. Nat Commun. 2014;5:5110.
Rey C, Vanderschuren H. Cassava mosaic and brown streak diseases: current perspectives and beyond. Annu Rev Virol. 2017;4(1):429.
Bi H, Aileni M, Zhang P. Evaluation of cassava varieties for cassava mosaic disease resistance jointly by agro-inoculation screening and molecular markers. Afr J Plant Sci. 2010;4(9):330–8.
Legg JP, Lava Kumar P, Makeshkumar T, Tripathi L, Ferguson M, Kanju E, Ntawuruhunga P, Cuellar W. Cassava virus diseases: biology, epidemiology, and management. Adv Virus Res. 2015;91:85–142.
Mallowa SO, Isutsa DK, Kamau AW, Obonyo R, Legg JP. Current characteristics of cassava mosaic disease in post-epidemic areas increase the range of possible management options. Ann Appl Biol. 2006;149:137–44.
Thresh JM, Fargette D, Otim-Nape GW. Effects of African cassava mosaic geminivirus on the yield of cassava. Trop Sci. 1994;34:26–42.
Vanderschuren H, Alder A, Zhang P, Gruissem W. Dose-dependent RNAi-mediated geminivirus resistance in the tropical root crop cassava. Plant Mol Biol. 2009;70(3):265–72.
Fofana IB, Sangaré A, Collier R, Taylor C, Fauquet CM. A geminivirus-induced gene silencing system for gene function validation in cassava. Plant Mol Biol. 2004;56(4):613–24.
Beyene G, Chauhan RD, Ilyas M, Wagaba H, Fauquet CM, Miano D, Alicai T, Taylor N. A virus-derived stacked RNAi construct confers robust resistance to cassava brown streak disease. Front Plant Sci. 2016;7:2052.
Tuttle J, Haigler CH, Robertson D. Method: low-cost delivery of the cotton leaf crumple virus-induced gene silencing system. Plant Methods. 2012;8(1):27.
Ascencio-Ibanez JT, Settlage SB. DNA abrasion onto plants is an effective method for geminivirus infection and virus-induced gene silencing. J Virol Methods. 2007;142:198–203.
Elmer JS, Sunter G, Gardiner WE, Brand L, Browning CK, Bisaro DM, Rogers SG. Agrobacterium-mediated inoculation of plants with tomato golden mosaic virus DNAs. Plant Mol Biol. 1988;10:225–34.
Stenger DC, Revington GN, Stevenson MC, Bisaro DM. Replicational release of geminivirus genomes from tandemly repeated copies: evidence for rolling-circle replication of a plant viral DNA. Proc Natl Acad Sci USA. 1991;88(18):8029–33.
Mittal D, Borah BK, Dasgupta I. Agroinfection of cloned Sri Lankan cassava mosaic virus DNA to Arabidopsis thaliana, Nicotiana tabacum and cassava. Arch Virol. 2008;153:2149–55.
Lozano-Durán R, Rosas-Díaz T, Luna AP, Bejarano ER. Identification of host genes involved in geminivirus infection using a reverse genetics approach. PLoS ONE. 2011;6(7):e22383.
Navot N, Pichersky E, Zeidan M, Zamir D, Czosnek H. Tomato Yettow Leaf Curl Virus: a whitefly-transmitted geminivirus with a single genomic component. Virology. 1991;185:151–61.
Nagar S, Hanley-Bowdoin L, Robertson D. Host DNA replication is induced by geminivirus infection of differentiated plant cells. Plant Cell. 2002;14:2995–3007.
Rasheed MS, Selth LA, Koltunow AM, Randles JW, Rezaian MA. Single-stranded DNA of Tomato leaf curl virus accumulates in the cytoplasm of phloem cells. Virology. 2006;348(1):120–32.
Tuttle JR, Idris AM, Brown JK, Haigler CH, Robertson D. Geminivirus-mediated gene silencing from cotton leaf crumple virus is enhanced by low temperature in cotton. Plant Physiol. 2008;148:41–50.
Hiriart JB, Aro EM, Lehto K. Dynamics of the VIGS-mediated chimeric silencing of the Nicotiana benthamiana ChlH gene and of the tobacco mosaic virus vector. Mol Plant Microbe Interact. 2003;16(2):99–106.
Rabbi IY, Hamblin MT, Kumar PL, Gedil MA, Ikpan AS, Jannink JL, Kulakow PA. High-resolution mapping of resistance to cassava mosaic geminiviruses in cassava using genotyping-by-sequencing and its implications for breeding. Virus Res. 2014;186:87–96.
Cigan AM, Unger-Wallace E, Haug-Collet K. Transcriptional gene silencing as a tool for uncovering gene function in maize. Plant J. 2005;43(6):929–40.
Bisaro DM. Silencing suppression by geminivirus proteins. Virology. 2006;344(1):158–68.
Mohammed IU, Abarshi MM, Muli B, Hillocks RJ, Maruthi MN. The symptom and genetic diversity of cassava brown streak viruses infecting cassava in East Africa. Adv Virol. 2012;2012:795697.
Moreno I, Gruissem W, Vanderschuren H. Reference genes for reliable potyvirus quantitation in cassava and analysis of Cassava brown streak virus load in host varieties. J Virol Methods. 2011;177:49–54.
Mafla GM, Roa JC, Aranzales E, Debouck DG. Manual de procedimientos para la conservación in vitro del germoplasma del género Manihot. Palmira; 2010: Programa Recursos Genéticos. Centro Internacional de Agricultura Tropical (CIAT). http://isa.ciat.cgiar.org/urg/. Accessed 1 June 2013.
McCabe DE, Swain WF, Martinell BJ, Christou P. Stable transformation of soybean (Glycine Max) by particle acceleration. Nat Biotechnol. 1988;6(8):923–6.
Soni R, Murray JA. Isolation of intact DNA and RNA from plant tissues. Anal Biochem. 1994;218(2):474–6.
Cazzonelli CI, Cavallaro AS, Botella JR. Cloning and characterisation of ripening-induced ethylene biosynthetic genes from non-climacteric pineapple (Ananas comosus) fruits. Aust J Plant Physiol. 1998;25:513–8.
Pfaffl MW. A new mathematical model for relative quantification in real-time RT-PCR. Nucl Acids Res. 2001;29(9):e45.
HV, JK and EML designed the experiments; EML constructed the VIGS vector and tested it in N. benthamiana; HV, RAB and EML optimized the protocol A of agroinoculation; HV, AA, NM and IZ optimized the protocol B of agroinoculation; EJM produced and characterized the uidA cassava line; EML performed the experiments with the uidA transgenic plants and the Chl1 silencing experiments with wild type cassava; JK, AA, NM, IZ and RAB tested the VIGS vector for the silencing of endogenous cassava genes; JK performed the VIGS experiments for the Manes.12G071800 gene, and expression levels were quantified by JK and EML. HV, WG, JK and EML analyzed the data; EML and HV wrote the manuscript with contributions from all authors, and WG edited the manuscript. All authors read and approved the final manuscript.
We thank Irene Zurkirchen for care of the plants in the greenhouse, and Doris Russenberger, Daniela Rothe, Kim Schlegel and Serena Rigotti for their assistance in the lab. We thank Chrissie Rey (University of the Witwatersrand) for providing the AGL1 strain and Dr. Stephan Winter for the plasmid containing MeChl1 gene fragment.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
No human subjects involved in this study.
This work was supported by the Swiss-Brazilian joint project BJRP 011202, the Plant Fellows Programme (Zurich-Basel Plant Science Center) from the Seven Framework Programme (FP7) of Marie Curie actions and ETH Zurich.
Use of plant material
Genetically modified cassava plants and cassava infected with recombinant CMD virus were generated and used in accordance with regulation of ETH Zurich.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Lentz, E.M., Kuon, JE., Alder, A. et al. Cassava geminivirus agroclones for virus-induced gene silencing in cassava leaves and roots. Plant Methods 14, 73 (2018). https://doi.org/10.1186/s13007-018-0340-5
- Agrobacterium tumefaciens
- Gene silencing