Get Our e-AlertsSubmit Manuscript
BioDesign Research / 2020 / Article

Review Article | Open Access

Volume 2020 |Article ID 8189219 |

Mitchell G. Thompson, William M. Moore, Niklas F. C. Hummel, Allison N. Pearson, Collin R. Barnum, Henrik V. Scheller, Patrick M. Shih, "Agrobacterium tumefaciens: A Bacterium Primed for Synthetic Biology", BioDesign Research, vol. 2020, Article ID 8189219, 16 pages, 2020.

Agrobacterium tumefaciens: A Bacterium Primed for Synthetic Biology

Received15 Mar 2020
Accepted26 Apr 2020
Published26 May 2020


Agrobacterium tumefaciens is an important tool in plant biotechnology due to its natural ability to transfer DNA into the genomes of host plants. Genetic manipulations of A. tumefaciens have yielded considerable advances in increasing transformational efficiency in a number of plant species and cultivars. Moreover, there is overwhelming evidence that modulating the expression of various mediators of A. tumefaciens virulence can lead to more successful plant transformation; thus, the application of synthetic biology to enable targeted engineering of the bacterium may enable new opportunities for advancing plant biotechnology. In this review, we highlight engineering targets in both A. tumefaciens and plant hosts that could be exploited more effectively through precision genetic control to generate high-quality transformation events in a wider range of host plants. We then further discuss the current state of A. tumefaciens and plant engineering with regard to plant transformation and describe how future work may incorporate a rigorous synthetic biology approach to tailor strains of A. tumefaciens used in plant transformation.

1. Introduction

Agrobacterium tumefaciens is a soil-dwelling plant pathogen that has been well studied due to its unique natural ability to transform many species of plants and other eukaryotes. Naturally, A. tumefaciens pursues a pathogenic lifestyle by transforming plants with an ssDNA that induces the plant to form a tumor (termed a gall) via the synthesis of phytohormones. Additionally, the bacterium coerces the plant to synthesize compounds known as opines from plant metabolites whose use as a nutrient source is restricted to the pathogen [1]. The DNA that is transferred to the host (termed T-DNA) is encoded on a large virulence plasmid (pTi), which also encodes most of the genes necessary to carry out pathogenic functions [2]. These virulence (or vir) genes encode the machinery required to process T-DNA and translocate it efficiently into the plant cell nucleus, where its tumorigenic genes can be integrated into the chromosome or transiently expressed [3].

Very soon after the molecular details of A. tumefaciens pathogenesis were elucidated, its value as a biotechnological tool was realized. Researchers were able to introduce transgenes into plants by replacing the oncogenic loci with other genetic elements [4]. Since that initial leap, A. tumefaciens has become the single most important tool in agricultural biotechnology. A great amount of optimization has been required to increase the efficiency by which A. tumefaciens introduces DNA into the host and expand the host range [5]. Many external factors dramatically influence Agrobacterium-mediated transformation (AMT), including the age of the plant, tissue type, length of agroinfiltration, day-night cycling, and method of agroinfiltration (Table 1). However, modulating the pathogenicity of the bacterium itself has been proven extremely useful in broadening the utility of A. tumefaciens as a tool for both transient expression and stable genetic integration.

VariableKey points of optimization from studyCitation

Day-night cyclesBest Arabidopsis transient expression was shown in plants grown in short day conditions, kept in 85-90% relative humidity for 24 h after infiltration, using Agrobacterium strain LAB4404, and addition of 0.01% Triton X-100 to infiltration media[140]
Plant tissue pretreatmentHighest transformation efficiency of Sorghum bicolor L. by heat treating immature embryos at 43°C for 3 min then cooling to 25°C prior to infection[141]
Cultivar optimizationFound optimal infiltration of Glycine max (soy) to occur in cultivars Jack Purple or Tianlong 1 with Agrobacterium suspension of containing 154.2 mg/L dithiothreitol and cocultured for 5 days[142]
Plant ageFound optimal infiltrations of Brassica oleracea var. botrytis (cauliflower) to occur in 7-day-old seedlings, 50 μM acetosyringone, 3-day cocultivation at 22°C, using agro strain GV2260[143]
Antioxidant additionFound the addition of antioxidants (lipoic acid or glycine betaine) increased transformation efficiency in Citrus aurantifolia Swingle (Mexican lime)[144]
Duration of agroinfiltrationPerformed transient expression in the adaxial epidermis and mesophyll of onion scales. Found the agroinfiltration durations and OD600 to be the largest factors (best: 43.87% transformation efficiency with conditions of 72 h and OD600 of 0.10). Also found all components of their infiltration media to be necessary (1 component missing reduced efficiency by 30-41%)[145]
Method of agroinfiltrationFound use of 6 min sonication and 6 min vacuum infiltration (750 mmHg) provided highest efficiency (39.4%) in banana cv. Rasthali. This seems to be a common method for increasing transformation efficiency in rarely transformed plants (e.g., de Oliveira et al., 2008; Bakshi et al., 2011; Liu et al., 2005)[146]

Nearly twenty years ago, Gelvin reviewed the biological basis of A. tumefaciens pathogenesis through the lens of genetic engineering [6]. They highlighted virulence factors and host proteins that could be modulated or engineered to affect the rates of AMT or broaden the host range of A. tumefaciens. Since that time, cheap, accurate DNA sequencing and tools to precisely edit genomes, such as CRISPR/Cas9, have spurred major shifts in the technology used to study biological systems. The field of synthetic biology, which seeks to rationally design and engineer biological systems to generate predictable, useful outcomes, has also rapidly matured. While perhaps most prominently utilized in the field of metabolic engineering, synthetic biology has also been invoked to rewire other complex biological phenomena such as nitrogen fixation [7], respiration through changes in membrane viscosity [8], and altering the plant cell wall [9]. This engineering is predicated on the existence of well-characterized DNA elements that can precisely control the expression of genetic circuits; however, we still lack the DNA parts needed to enable complex and fine-tuned engineering efforts in Agrobacterium.

In this review, we focus on recent advances in the understanding of Agrobacterium-host interactions that may serve as targets for synthetic biology approaches to increase the potency of A. tumefaciens as a tool for precisely engineering a broad range of plants. Furthermore, we highlight technological advances in the delivery of T-DNA to host cells, as well as the current repertoire of genetic tools available to control gene expression in A. tumefaciens. Finally, we discuss which areas the field may focus on to improve the control of Agrobacterium-based genetic circuits in the future.

2. Engineerable Targets of A. tumefaciens

Agrobacterium pathogenesis of plant tissues progresses in a stepwise manner, requiring attachment to the plant cell surface, small molecule perception for virulence induction, T-DNA transfer into the host cell, nuclear import of the proposed T-complex (the assemblage of a T-DNA covalently attached to a VirD2 molecule and putative associations with other vir proteins), and stable integration into the host genome. Each step represents a potential bottleneck. Here, we will briefly cover the basic biological steps of A. tumefaciens pathogenesis that may lend themselves to useful engineering.

2.1. Induction of vir Genes

In natural settings, A. tumefaciens pathogenesis begins when the bacterium migrates towards the site of wounded plants, attracted to a myriad of phenolics and sugars [10, 11]. This chemotaxis machinery has been reviewed in depth elsewhere [12, 13], and although flagella mutants do show reduced virulence [14], motility towards the plant is generally thought to be irrelevant during laboratory transformation protocols, where plant material is directly infiltrated with bacterial culture. However, many of the signals that are proposed to draw A. tumefaciens to the plant also induce the vir genes required to initiate pathogenic DNA transfer into the host plant.

The vir genes are regulated by the master regulator two-component system (TCS) VirA (the sensor kinase) and VirG (the response regulator), which is able to integrate multiple environmental signals. The VirA sensor is thought to be directly activated by plant-derived phenolic compounds, such as acetosyringone (AS) [15] but can indirectly sense plant-derived monosaccharides via the aid of the chromosomally encoded periplasmic sugar-binding protein ChvE [16] and pH through the chromosomally encoded ChvG/I TCS [17]. These environmental factors contribute to the induction of the vir genes located on the pTi plasmid and also to an increase in the copy number of pTi itself, ensuring efficient synthesis of T-DNA. The molecular details of these pathways have been extensively reviewed elsewhere [12, 13, 18].

Much research has focused on optimizing vir gene induction by VirG, often with the addition of exogenous AS or other media components that are sensed directly or indirectly by VirA. A recent work in rice showed that for large (50 kb) T-DNA insertions, cultures of A. tumefaciens could require as much as 24 hours of AS induction before robust T-DNA formation could be observed [19]. In another recent study, transient expression of T-DNA was optimized in Arabidopsis seedlings in a method termed AGROBEST [20]. A key finding of the study was that buffered infection media with pH of 5.5 increased transient β-glucuronidase (GUS) activity 20-fold. A further work in Brazilian wheat and the algae Dunaliella has optimized levels of glucose, AS, and pH for more efficient transformation [21, 22]. These studies are just a few examples of how titrating the signal inputs that activate VirG can shape the outcome of transformation. Beyond the VirA/G TCS, a more recent work has also implicated the role of small noncoding RNAs (ncRNAs) in the regulation of A. tumefaciens virulence and has been recently reviewed [23]. One example of the role of ncRNAs play in A. tumefaciens virulence is a work demonstrating that the chromosomally encoded ncRNA AbcR1 negatively regulates ChvE, amongst other nutrient transporters that may affect vir gene induction [24, 25]. As work on these RNAs matures, more insight will be gained into how these systems may be engineered to optimize AMT.

Almost universally, AMT relies on induction of the vir genes by the native regulatory machinery. This reliance on natural regulation leaves the system susceptible to host interference with VirG activation and may disallow for specific titration of key vir genes. It has been demonstrated that when the constitutively active VirG mutant virGN54D was overexpressed on a compatible plasmid, transformation efficiency increases in a variety of plants and even broadening the host range to include the legume Melilotus alba and the flowering plant Heteromorpha arborescens [26, 27]. This work suggests that high-level constitutive activation of the vir genes is a formidable strategy for Agrobacterium-mediated gene transfer. Completely decoupling native regulation from vir gene expression could reduce the likelihood of plant repression of gene expression and allow researchers to precisely tune vir gene levels to specific experimental needs [28, 29].

2.2. Attachment to Plant Surfaces

The attachment of A. tumefaciens to both abiotic and biotic surfaces has also been reviewed extensively elsewhere [30, 31]. In a natural environment, it is commonly believed that A. tumefaciens must first establish a physical interaction with a host plant in order to then initiate the transfer of T-DNA. Attachment to surfaces is thought to occur in a stepwise fashion: first a potentially transient reversible attachment is established, followed by irreversible attachment to a surface. Flagellar motility facilitates initial surface contact, where reversible attachment is potentially mediated by a variety of pili (Ctp and conjugative) or protein adhesins [30]. Subsequent irreversible attachment is mediated by exported polymers, primarily cellulose and unipolar polysaccharide (UPP) [31]. However, in common laboratory models, these attachment structures are largely unnecessary for virulence [30], likely due to the large amount of bacteria that are directly added to already wounded tissues in laboratory conditions. It has also been noted that none of these attachment structures are coded for on the virulence plasmid and the att genes that are on pAtC58 which are not essential for virulence [30]. Despite these observations, it is still unknown whether attachment to the plant surfaces may play an important role in expanding the host range of A. tumefaciens. A recent work demonstrated that addition of exogenous cellulose to barley callus cultures not only increased bacterial adherence to callus cells but also increased GUS staining by 50% compared to conventional conditions [32]. Given such observations, it is valuable to have control over known attachment structures and continue to search for novel mediators of Agrobacterium-plant interactions.

In A. tumefaciens, the biosynthesis of both cellulose and UPP are posttranslationally regulated by the global secondary messenger cyclic diguanylate (c-di-GMP), with higher intracellular levels of c-di-GMP generally resulting in greater polysaccharide production [33, 34]. The levels of c-di-GMP are most often controlled by two competing classes of enzymatic activities: c-di-GMP forming diguanylate cyclases (DGCs) and c-di-GMP hydrolyzing phosphodiesterases (PDEs) [35]. A. tumefaciens has numerous enzymes that have DGC or PDE activity, in some cases in the same protein [36]. A recent work has shown that the activity of the bifunctional DGC/PDE enzyme DcpA was also curiously dependent on the pteridine reductase PruA [36]. The authors showed that when bound to a novel pteridine-derived cofactor, the pterin-binding family protein PruR enhances the PDE activity of DcpA. Disruption of pterin biosynthesis resulted in A. tumefaciens that formed large clumps in liquid culture, likely due to an increased synthesis of UPP. This work suggests that engineers could control the “stickiness” of A. tumefaciens by titrating the relative levels of pterin biosynthesis as well as expression of DcpA.

An active area of research that remains mostly unexplored is the interaction between A. tumefaciens and the plant cell wall. To date, there are no proven direct interactions between specific cell wall moieties and specific attachment appendages in A. tumefaciens. However, it has recently been shown that multiple glycoside hydrolases play a role in A. tumefaciens virulence of tomato and Bryophyllum daigremontianum [37]. By screening deletion mutants of all 48 predicted glycoside hydrolases of A. tumefaciens, Mathews and colleagues showed that mutants in enzymes predicted to degrade polygalacturonic acid, xylan, and arabinogalactans were all less virulent than wild-type A. tumefaciens. Furthermore, mutants in multiple enzymes predicted to possess β-glycosidase activity and an arabinofuranosidase that may cleave arabinose from the ends of polysaccharide strands were also shown to be less virulent. As mutation to any of the identified hydrolases nearly completely abolished tumor formation in both host plants, these results suggest that cell wall degradation or polysaccharide catabolism may play key steps in establishing pathogenicity. The logical next step may be to explore additional cell wall degradative enzymes to test whether they can further increase the efficiency of T-DNA transfer.

2.3. T-DNA Generation and Transfer

Upon induction by the VirA/G TCS, A. tumefaciens begins the process of creating ssDNA T-DNA strands destined for export to host cells via a type IV secretion system (T4SS) encoded by the virB cluster of genes and virD4. The A. tumefaciens T4SS has served as a model for other bacterial T4SSs, and both its structure and function have been reviewed extensively [38]. However, the T4SS itself has rarely been the target of efforts to increase the efficiency of T-DNA transfer. Other steps in T-DNA generation have been extensively modified to augment transformation efficiency. T-DNA strand formation largely relies on the formation of a DNA nicking complex consisting of the proteins VirD1, VirD2, VirC1, and VirC2 [39]. VirD2 initially acts as an endonuclease that nicks the cis-acting left and right borders (termed LB and RB, respectively) to generate the T-DNA [3]. Subsequently, VirD2 is covalently bonded to the 5-end to form a nascent T-strand, which is critical for stability, export, and future localization [3]. VirC1 binds to a cis-acting site proximal to the T-DNA border termed overdrive [40] and in association with VirC2 increases the production of T-strands [39]. An exceptional work done by Atmakuri et al. demonstrated that VirC1 initiates the assembly of the relaxosome and dramatically stimulates the production of T-DNA strands in conjunction with VirC2 [39]. T-DNA strand generation is also influenced by the copy number of the virulence plasmid, which is increased by VirA/VirG when stimulated by plant wound signals [41]. In later sections, we will discuss in detail how binary vectors have been designed to optimally produce T-DNA strands.

Beyond the canonical vir genes, it has recently come to light that the membrane composition of A. tumefaciens can play an important role in shaping the pathogenicity of the bacterium. When potato is infected with A. tumefaciens that lack ornithine lipids, tumors form much more rapidly [42]. To date, the specific physiological function of ornithine lipids in bacteria has not been precisely defined, though it is believed to be associated with resistance to abiotic stresses. It has yet to be understood whether the lack of ornithine lipids may increase A. tumefaciens resistance to plant immunity or signaling, or rather increase the ability for A. tumefaciens to transfer T-DNA [42]. Another work has shown that the levels of lysyl-phosphatidylglycerol (L-PG) in the membrane can dramatically alter A. tumefaciens virulence [43]. Researchers showed that mutation of the L-PG hydrolase AcvB increased the levels of L-PG in the membranes ~10-fold, which dramatically reduced T-DNA transfer in a transient A. thaliana GUS-assay. The precise mechanism by which the level of L-PG affects virulence is still unknown. It is possible that changes in membrane composition reduce the ability of the VirA/G TCS to activate vir gene expression, though it is just possible that these changes make it difficult for the T-pilus to properly assemble. As more light is shed on the role of how membrane composition affects virulence, rational engineering of lipid compositions could become another means of controlling Agrobacterium-plant interactions.

2.4. T-DNA Trafficking in the Host

The assembly of the T-complex and subsequent trafficking to the nucleus has been reviewed extensively elsewhere [44, 45]. It has been suggested that once the T-DNA-VirD2 complex enters the host cell, it is rapidly coated by VirE2, which serves partly to protect the ssDNA from nuclease-mediated degradation [45]. Both VirD2 and VirE2 contain predicted nuclear localization sequences (NLSs) and interact with host factors that guide the T-complex to the chromatin [45]. VirD2 is known to interact directly with the nuclear localization machinery component importin α [45]. Initially, it was believed that VirE2 requires additional factors from the plant host, termed VirE2 Interacting Proteins (VIPs), to act as intermediaries with importins [45]. However, this view has been challenged by a work that used yeast two-hybrid (Y2H) assays to show that VirE2 can interact with multiple importin α proteins of A. thaliana. This same research also showed that A. thaliana mutants in IMPα-4 are resistant to infection by A. tumefaciens, suggesting that IMPα-4 may facilitate VirE2 nuclear translocation [46]. Further research demonstrated that VIP1, which had been believed to assist VirE2 nuclear translocation, was dispensable for A. thaliana transformation by multiple A. tumefaciens strains [47]. The putative roles VIPs may play in A. tumefaciens virulence are discussed in detail in later sections. The ambiguity of how the T-DNA complex is imported into the nucleus extends to the host-specificity factor VirE3, which was thought to be able to mimic VIP1 function by facilitating importin interaction, thus allowing for infection in plants with low or absent VIP1 expression [48]. However, a recent work has shown that VirE3 localizes to the plasma membrane of N. benthamiana where it colocalizes with VirE2 and is required to protect the T-DNA, calling in to question its function as a VIP1 mimic [49]. Given that the current data conflict on the mechanisms of T-DNA trafficking, more work likely must be done before these processes can be rationally engineered to optimize AMT.

Once the T-complex has entered the nucleus, it has been hypothesized that the VirE2 coating is degraded for efficient transient expression or chromosomal integration to occur. VirF is believed to be another host-specificity factor that plays an important role in the degradation of the VirE2 coating [50]. VirF acts as an F-box protein within the nucleus and aids in the ubiquitination and degradation of both VIP1 and VirE2, though its specific role in pathogenesis may be debatable given our current understanding of T-complex nuclear translocation [50]. VirF itself is also proteolytically degraded, which can be mitigated by binding to an additional virulence effector, VirD5 [51]. VirF is required for infection in some plants, but not others—presumably due to other host factors filling the role of VirF [52]. Furthermore, in maize, its expression can actually inhibit the transfer of T-DNA, highlighting its variable role in AMT [52]. VirD5 has also been shown to be toxic to host cells, as it can cause chromosome missegregation in yeast by stimulating the activity of Aurora family kinase Ipl1, which leads to detachment between the kinetochore and mitotic spindles [53]. The variable effects of both VirF and VirD5 both highlight the importance of the ability to precisely regulate individual vir gene expression in future A. tumefaciens engineering efforts.

2.5. Host Evasion and Resistance

Like many plant pathogens, A. tumefaciens has evolved multiple mechanisms to evade and subvert the immune responses of plant hosts. This manipulation of the host response has also been reviewed extensively [3, 45, 54]. Wounded plants often produce toxic phenolic compounds, which in addition to stimulating the expression of the vir genes can also be toxic to A. tumefaciens [55]. An early work demonstrated that some pTi plasmids harbor VirH homologs that code for cytochrome p450 monooxygenases, which can be induced in the presence of phenolics and are capable of catabolizing toxic concentrations of ferulate [55]. In response to many bacterial pathogens, plants undergo a hypersensitive response (HR) that causes tissue necrosis to halt the spread of infection, producing reactive oxygen species such as H2O2 in the process [56]. Though A. tumefaciens does not induce HR in its native hosts, the ability of catalase mutants to form tumors in the nonnative host Kalanchoe was compromised [56]. These results indicate that engineering strains of A. tumefaciens that can perceive and respond to plant defenses may be critical as researchers try to expand its host range.

Beyond dealing with physical and chemical defenses imposed by the host, A. tumefaciens has the ability to actively modulate the host response by reprogramming host transcription. Host specificity factor VirE3 was shown to bind to the A. thaliana transcription factor (TF) pBrp and assist in its translocation to the nucleus, where it stimulates the expression of the F-box protein VBF [57]. Previously, VBF had been shown to perform the same function as VirF, enhancing the ability of A. tumefaciens to transform plants [50]. VirF has also been shown to modulate host transcription in A. thaliana by targeting the TF VFP4 for degradation via the proteasome [58]. Mutants in VFP4 showed reduced expression of multiple genes associated with bacterial defense, suggesting A. tumefaciens may actively repress the plant defenses. As our understanding of how A. tumefaciens modulates the plant-host response improves, it is foreseeable that specific proteins could be engineered into the bacterium to suppress plant bacterial defenses. These proteins need not necessarily be derived from any Agrobacterium species, but rather could draw upon the numerous bacterial effectors that are known to inhibit plant immunity [59].

3. Engineering Targets of Host Plants

During its pathogenesis, A. tumefaciens encounters a variety of plant host factors that can limit or aid plant transformation efficiency. Plant regeneration post T-DNA integration is yet another significant hurdle for many agronomically important plant species and genotypes. Here, we discuss known host factors that modulate AMT, as well as recent engineering strategies that increase plant regeneration efficiency.

3.1. Virulence Induction and Attachment

As discussed previously, small molecules derived from wounded host tissue act as potent inducers of A. tumefaciens virulence. Beyond the canonical inducer molecules, low environmental calcium content has been shown to influence bacterial polar attachment to root hairs [30]. Low-calcium content in A. tumefaciens suspension culture upregulates UPP production and polar attachment [30], while calli propagated on low calcium media also increased transformation efficiency [60]. Importantly, calcium also modulates plant cell wall architecture by crosslinking homogalacturonan pectic polysaccharides in the so-called “egg box conformation” and increases the rigidity of the cell wall [61]. As the cell wall is a barrier to pathogen attack and evidence from both A. tumefaciens and the plant host indicates that cell wall loosening is important for transformation, much effort has gone into identifying the genetic basis for plant resistance to A. tumefaciens.

Forward genetic screening for A. thaliana mutants resistant to Agrobacterium transformation (rat) identified a number of cell wall synthesis genes including a mannan synthase (rat4), β-expansin (ratT18), and arabinogalactan protein (AGP) or extensin-type glycoproteins (rat1 and rat3) [6, 62]. These enzymes may be important for cell wall loosening and also may release sugars that synergistically induce vir genes together with plant-derived phenolic compounds. Interestingly, the lysine-rich arabinogalactan protein 17 (AGP17/rat1) is required for polar attachment of A. tumefaciens to plant tissue and AMT [63]. The related alpha-Proteobacterium Rhizobium leguminosarum is able to bind gum arabic (a pure AGP fraction from Acacia senegal) and purified AGP from pea roots in vitro and form polarized arrays but is unable to form polar attachments with hemicelluloses or pectins [64]. Furthermore, chemical disruption of AGPs prevented the polar attachment R. leguminosarum in vitro [64]. Many AGPs including AGP17/rat1 contain glycosylphosphatidylinositol (GPI) lipid anchors that tether the glycoprotein to the outer leaflet of the plasma membrane. Conceivably, binding of periplasmic GPI-anchored proteins brings the bacterium into close proximity with the plant plasma membrane for pili formation and conjugation. Some evidence has shown that AGPs may also participate in endocytosis-driven mechanisms in pollen tube self-incompatibility [65] and microelement accumulation [66], which could potentially be relevant for endocytic trafficking of A. tumefaciens effectors. Though both A. tumefaciens and R. leguminosarum form polar attachment structures in response to AGP cell surface epitopes, the underlying mechanisms and biology are not well understood. As our knowledge of plant mediators of bacterial attachment expands, new engineering strategies may emerge. Beyond the natural attachment appendages encoded within A. tumefaciens, it may be feasible to engineer systems from other bacteria with better characterized plant interactions.

3.2. T-DNA Transfer and Nuclear Import

Currently, very little is known about plant host proteins involved in assisting T-DNA and effector protein delivery into the plant cell. However, Y2H assays using VirB2 as bait identified a group of reticulin-like B proteins (RTNLB) and a RAB GTPase as reciprocally interacting proteins associated with the T-pilus type IV secretion system [67]. A. thaliana rtnlb3 loss of function mutants had decreased levels of transient T-DNA expression [68], while lines overexpressing either RTNLB3 or RTNLB8 were hypersusceptible to both A. tumefaciens and Pseudomonas syringae DC3000 [68]. A recent work has also shown that RTNLB4 may participate in the VirB2 and ELF18 peptide-induced defense against A. tumefaciens [69]. RTNLB proteins likely have other roles in plants but may be commonly exploited by pathogenic bacteria for pathogenesis.

As previously discussed, nuclear import of T-DNA is largely mediated by VirE2 and VirD2, which contain nuclear localization signals, but have been shown to interact with a number of host factors. The most contested of theseis VIP1. In plants, VIP1 is a transcriptional activator of stress response with reported roles in mechanical wounding, salt stress, hypoosmotic stress, Botrytis infection, sulfur deficiency, and purportedly agrobacterium pathogenesis [7075]. VIP1 normally resides in the cytoplasm and localizes to the nucleus in response to stress to regulate transcription [45, 70, 74, 76]. VIP1 interacts with VirE2 in vitro and forms complexes in vivo in the plant cytoplasm [47, 75, 77]. It was reported that MAPK3 phosphorylation of VIP1 at Ser79 may enhance T-DNA nuclear import via interactions with VirE2 [74]. However, vip1 mutant plants are not impaired in AMT efficiency and subsequent rigorous studies have seriously challenged the VirE2 nuclear import capabilities of VIP1 and the Ser79 phosphorylation site [47]. More recently, VIP1 nuclear localization during mechanical stress was shown to be regulated by dephosphorylation at Ser35 and Ser115 by Protein Phosphatase 2A (PP2A) [73]. Alanine substitution at these sites triggered constitutive nuclear localization of VIP1 [73]. From this perspective, it would be interesting to test whether alanine-substituted VIP1 could increase AMT. However, further research into if VIP1 is necessary before it can be incorporated into rational engineering strategies applied to AMT.

Other factors influencing nuclear import include phosphorylation of VirD2. Dephosphorylation of VirD2 by PP2C has been shown to impair T-DNA nuclear import [78]. Therefore, engineering strategies that either reduce host PP2C expression [79] or include a phosphatase resistant VirD2 phospho-mimic may further increase nuclear import efficiency.

3.3. T-DNA Integration

After nuclear import, the T-complex is proposed to be disassembled by SCF complex E3 ubiquitin ligase-mediated proteolysis to expose the T-DNA strand for integration into the host genome. To date, many different host factors that affect T-DNA integration and transgene expression have been identified but can generally be grouped into three related categories including (1) DNA repair, (2) nonhomologous end joining, and (3) chromatin remodeling.

Many mutants that are sensitive to DNA damage or defective in nonhomologous end joining have increased transformation efficiency [8083]. Presumably, attenuated double stranded DNA break repair increases the probability of T-DNA integration. Further evidence suggests that either limiting nonhomologous recombination (NHR) or promoting homologous recombination (HRec) increases T-DNA integration. Multiple works have shown that Ku70, Ku80, Lig6, and XRCC4 are mediators of NHR that inversely affect DNA integration [84, 85]. VirE2 interacts with XRCC4 in Y2H assays and may have a function in titrating XRCC4 levels to favor T-DNA integration [82, 84]. Chromatin remodeling protein RAD54 is known to be important for HRec in both yeast and mammalian cells [86]. Expression of RAD54 in plants increased HRec T-DNA integration into a specific locus by 27-fold, and it was determined that chromatin remodeling in plants was the most limiting factor for HRec integration [87].

Alterations in chromatin structure influence DNA accessibility and the frequency of T-DNA integration into the host genome. Arabidopsis histone HTA-1 is a core H2A histone protein identified in a forward genetic mutant screen for plants resistant to Agrobacterium transformation (rat5) [88, 89]. Mutations in hta-1/rat5 inhibit AMT while HTA-1 overexpression increases transformation efficiency in both Arabidopsis and rice [8991]. Similarly, plants deficient in chromatin assembly factor (CAF-1) have higher levels of T-DNA integration, presumably due to increased accessibility of unbound DNA to invading T-DNA [81]. Lastly, the transcriptional activator VIP2 is also important for stable T-DNA integration and has been shown to influence chromatin structure by regulating histone expression [92]. However, overexpression of VIP2 did not increase T-DNA integration like HTA-1 [89, 90, 92]. Therefore, a future work that actively programs specific routes of DNA repair or chromatin remodeling can dramatically increase the efficiency and specificity of T-DNA integration.

3.4. Plant Defense and Stress Response

Transcriptomic and functional studies have shown that A. tumefaciens pathogenesis induces plant defense and cellular stress responses with concomitant downregulation of genes associated with plant growth [9395]. Localized plant defense responses are activated through the perception of pathogen-associated molecular patterns (PAMPs) like flagellin, chitin, and EF-Tu, by specific receptor-like kinases (RLK) at the cell surface. EF-Tu is the major Agrobacterium PAMP recognized by plants resulting in PAMP-Triggered Immunity (PTI). EF-Tu is recognized by the EF-Tu receptor (EFR) and activates MAPK signaling cascades resulting in a robust defense response through the production of reactive oxygen species [96]. A. thaliana efr mutants are hypersusceptible to Agrobacterium infection, and transient T-DNA expression is greatly increased [96]. However, it is unknown whether stable T-DNA integration is also affected in efr mutants. Lastly, while A. tumefaciens elicit a formidable localized PTI response, hypersensitive response characteristic of effector triggered immunity (ETI) has not been reported.

Post infection, the expression of A. tumefaciens T-DNAs elicits a potent RNA silencing response by the plant host resulting in the accumulation of small interfering RNAs (siRNA) [97]. Production of different cis and trans acting 21-24 nt siRNAs by Dicer-like RNA endonucleases (DCLs) activates the RNA interference silencing complex (RISC) to mediate target mRNA degradation and DNA methylation [98]. T-DNA has been shown to be rapidly methylated during transient expression in infiltrated tobacco leaves [99]. Furthermore, transformation efficiency and T-DNA integration of 17 soybean genotypes were correlated with transgene methylation [100]. Correspondingly, chemical methylation inhibitors increased both T-DNA integration and transgene expression [100]. It is therefore not surprising that A. thaliana deficient in RNA interference are hypersusceptible to A. tumefaciens with increased transformation efficiency [97]. Successful natural pathogenesis of A. tumefaciens relies on a state of silencing suppression for the expression of oncogenes necessary for the progression of the disease. Similarly, the utility of A. tumefaciens as a plant engineering tool also relies on the efficient and stable expression of integrated genetic constructs. In practice, coexpression of viral silencing suppressor proteins such as P19 and P38 has commonly been used to quell siRNA response [101, 102]. Construct design incorporating 5 and 3 UTR sequences and introns has also been shown to reduce DNA methylation and transgene silencing [99].

Lastly, plant cellular stress also plays a role in the governing susceptibility to A. tumefaciens. Arabidopsis loss of function mutants in the mitochondrial porin protein Voltage-Dependent Ion Channel 1 (VDAC1) is resistant to A. tumefaciens infection at early steps prior to T-DNA transfer [103]. Plants overexpressing VDAC1 were hypersusceptible to infection with increased transient T-DNA expression but not stable integration [103]. The authors speculate that VDAC1 may regulate cellular and metabolic stress homeostasis to prevent organelle ROS production and associated apoptosis. Clearly circumventing plant defense is critical for efficient AMT. Future engineering efforts in this area will increase AMT efficiency, host range, and transgene stability.

4. AMT Engineering to Date

Since the initial creation of the binary vector system, tremendous progress has been made to generate plasmids that are both easy to manipulate, and yield highly efficient AMT in a variety of plants. Though binary and ternary vector development has somewhat dominated AMT engineering, there have been preliminary efforts to characterize genetic parts, as well as rationally engineer the A. tumefaciens genome to be a better chassis for T-DNA transfer. Beyond A. tumefaciens, there has recently been extraordinary work done to dramatically increase the efficiency of plant regeneration. Together these advances hint at a promising future for AMT in more plants and with greater precision.

4.1. Binary and Ternary Vector Engineering

Synthetic biology in A. tumefaciens began with the outsourcing of the T-DNA portion of the Ti-plasmid into a smaller vector, while maintaining the vir genes on a separate helper plasmid. This “binary vector” design made it possible to easily modify the genes transferred as part of the T-DNA region, and AMT has since become a standard tool in the transformation and molecular study of a wide variety of plant and fungal species. A multitude of binary vector systems have been developed and extensively reviewed [104106]; however, the methodology is still not flawless. Problems with AMT include low transformation frequency, genome integration of multiple T-DNA copies, and genome integration of binary vector backbone, with the latter two often coinciding. [107]. Multiple T-DNA integrations can lead to silencing of the gene of interest [108], and transgenic plant lines harboring bacterial selection markers from backbone integration are a matter of public concern because horizontal gene transfer from transgenic plants to bacteria has been shown in recombination-favoring laboratory settings [109].

To address these issues, efforts have focused on minimizing binary vector size and utilizing standardized cloning techniques to speed up binary vector design, such as Golden Gate cloning, Gibson assembly, and the Gateway technology [110, 111]. The high copy binary vectors pBBR1 and pVS1 show increased transformation frequency after screening in different A. tumefaciens strains [100, 112]. Still, while plasmids with low copy Origin of Replication (ORI), like pRi, have a lower vector copy number and reduced transformation frequency, the frequency of single-copy integrations is significantly higher than the previously mentioned ORIs (Table 2) [113]. Anand et al. combined the strategies of size minimization and ORI change and induced and constitutively expressed vir genes in their dissection of the super binary vector pSB1. In their study, pSB1 was split into a pure T-DNA vector—with a backbone consisting of only replication machinery and antibiotic resistance—and pairs of pVIR accessory vectors that harbored different parts of the vir operons from the hypervirulent pTiBo524 binary vector and a constitutive VirG mutant. This ternary vector system was tested in different A. tumefaciens strains in combination with the expression of the BABY BOOM and WUSCHEL genes, leading to a transformation frequency of 83-103% and single copy frequencies of up to 34% in the PH2RT maize inbred line [114]. In a follow-up study, the system was applied in high efficiency transformation of sorghum variety Tx430 with a transformation frequency of 29.4% and single copy events (SC) at 54% [115].

ApproachAgro strain/helper plasmidEngineered plasmidOrganismTransformation frequency (%)Single-copy frequency (%)Backbone free (%)Source

Backbone-coded lethal genes adjacent to LBABI/pMP90RKpMON83916Glycine max2.383.967.6[117]
Low copy oriR derivativesABI/pMP90RKoriRi5.6/pMON83935Glycine max1.033.886[113]
ABI/pMP90RKoriRi4.2/pMON83937Brassica napus L.11.452.597
ABI/pMP90RKoriRi4.2/pMON97352Zea mays L.9.560.695
Strain & plasmid copy number optimizationAGL0/pTiBo542PHP51901Zea mays L.75.831.655.1[112]
LBA4404/pAL4404PHP51901Zea mays L.63.231.773.4
T-DNA launched from chromosomeGV3101/pMP30pTF101.1Arabidopsis thaliana2.117897[116]
GV3101/pMP30pTF101.1Zea mays L.0.96492
Ternary vector systemLBA4404 THY-/pAL4404pPHP71539Zea mays L.31.129.929.9[114]
LBA4404 THY-/pAL4404pSB1Zea mays L.13.736.636.6
Ternary vector systemLBA4404 THY-/pAL4404pPHP71539/pPHP78152Sorghum bicolor29.454100[115]
LBA4404 THY-/pAL4404pPHP71539/pPHP78233Sorghum bicolor24.865100
Coexpression of octopine and succinamopine vir genesEHA105/pTiEHA105pDAB112807/pDAB111437Zea mays13.497.590.1[118]

In the study, only single-copy events without backbone integration were monitored, thereby leading to 100% backbone-free events.

Two elegant solutions for higher SC and backbone-free transformants were explored: (1) launching the T-DNA from the bacterial chromosome (2.1% transformation frequency, 78% SC, and 97% backbone free) and (2) including a lethal gene cassette on the binary vector backbone next to the left border sequence (2.3% transformation frequency, 83.9% SC, and 67.6% backbone free) [116, 117]. These approaches did not outperform the transformation frequency of high plasmid copy number approaches, but depending on the aim of the study, low transformation frequency with high SC and backbone free frequency can outperform high transformation frequency, as high transformation frequency often does not correlate with SC events (Table 2). A study that mitigates this problem is the approach of Sardesai et al. [118]. In their work, octopine and succinamopine vir genes were coexpressed in a ternary vector system with the T-DNA flanked by three left border repeats, enhancing nicking efficiency and boosting the SC event rate to 97.5% with 90.1% backbone-free transformants and a transformation frequency of 13.4%. This work showcased the significant impact of the left border nicking on both SC without backbone integration.

A thoughtful binary or ternary vector design can significantly enhance desired T-DNA integration modification and reduce the time lost from failed experiments in slow turnover plant stable line experiments. Importantly, the precise control of vir gene expression could be essential to the understanding of the impact of different vir gene titers on host T-DNA titers, the transformation frequency, SC, and backbone free transformants.

4.2. Agrobacterium Synthetic Biology and Chassis Engineering

In comparison to the sophisticated synthetic biology toolboxes available in model bacteria, there has been little rigorous characterization of genetic parts in A. tumefaciens despite years of study and the development of many variants of binary vectors. At the time of publication, there have been few attempts to characterize the relative strengths of constitutive promoters in A. tumefaciens in a standardized manner; additionally, few examples exist of well-characterized inducible systems. An early work demonstrated that both araC- and lacI-based induction systems do work in A. tumefaciens [119], though the level of characterization was limited. A tetR system has also been used in A. tumefaciens to control the expression of cre-recombinase [120]. A later work by Khan et al. showed that Plac can generate ~20x induction over background as measured by the Miller assay and is titratable by IPTG in A. tumefaciens C58 [121]. A more comprehensive analysis of IPTG and cumic acid inducible systems in A. tumefaciens was done by examining the ability of engineered inducible promoters to complement a virE2 deletion when infecting tobacco plants [122]. Measuring the activity of promoters via Miller assay as well as efficiency of agroinfiltration, the authors found that in AT Plac was inducible but Ptac was constitutive. However, a PT5/lacOlacO promoter was shown to be 15x stronger than Plac by Miller assay and was 50x inducible above background. Interestingly, the authors showed that a lacI-regulated T7 system was nonfunctional in AT, though a previous group had shown functionality [123]. A cumic acid regulated PT5 promoter showed 50x the expression strength of Plac and showed 20x induction over background. However, the cumic acid regulated PT5 also showed 10x higher basal expression relative to the PT5/lacOlacO promoter. A cumic acid-inducible Ptac promoter showed comparable expression strength, but only half of the basal activity. While these works are an excellent starting point, there still remains great work to do in the development of reliable genetic control in A. tumefaciens.

In addition to the relative dearth of characterized genetic parts for A. tumefaciens, there has also been relatively little rational engineering of its genome to increase its ability to transform plants. Plants that produce ethylene had been known to be more resistant to A. tumefaciens infection, which was later shown to be caused by ethylene-mediated downregulation of the vir genes [124]. The same group then introduced 1-aminocyclopropane-1-carboxylate (ACC) deaminase—which cleaves the precursor of plant ethylene—into A. tumefaciens, increasing gene transfer into the ethylene producing melon Cucumis melo L. var. cantalupensis cv. Vedrantais [124]. Subsequently, Nonaka et al. suggested that γ-aminobutyric (GABA) may also inhibit T-DNA transfer, showing that introduction of the GABA transaminase gabT into A. tumefaciens moderately increased gene transfer into two tomato cultivars and the bioenergy crop Erianthus arundinaceus [125]. In both tomato and Erianthus ravennae, introduction of both ACC deaminase and gabT into A. tumefaciens resulted in increased T-DNA relative to when either of these genes was expressed individually [28]. Cysteine auxotrophic strains of A. tumefaciens—derived from Tn5 insertion mutants—have not only shown the ability to prevent plant suppression of vir gene expression but also resulted in an 85-fold increase in transient GUS expression in Nicotiana glutinosa tissue cultures [126]. A patent for using thymidine auxotrophic A. tumefaciens has also been filed, for the purposes of both biocontainment and more efficient genetic transformation [127]. A work that further explores the metabolic and physiological functions of A. tumefaciens and how these are needed to thrive in the plant-host environment will continue to provide targets for rational engineering of the bacterium.

4.3. Disruption of Host Response and Induction of Host Regeneration

Two major hurdles to recovering successfully transformed plants are (1) the selection of positive transformants and (2) plant regeneration of transformed cells. The selection of transformed plant tissues is typically done by antibiotic or herbicide resistance but can also be done through the expression of a marker gene. In either case, selection depends on transgene expression, which can be strongly influenced by the induction of the siRNA pathway and epigenetic silencing of integrated transgenes [97, 128, 129]. Suppression of the siRNA response, either through coexpression of viral silencing suppressors [130] or through targeted down regulation of DCLs or RNA-dependent RNA polymerases, greatly increases the efficiency of transgene expressing plant tissue [97].

Despite the multitude of barriers to A. tumefaciens infection and transgene expression, plant cell regeneration is perhaps the most formidable obstacle limiting plant transformation [131]. In many cases, agronomically important genotypes are recalcitrant to plant tissue culture and callus regeneration. For this reason, specific plant genotypes with either increased plant regeneration properties or somatic embryo formation are used [131]. Often, these genotypes are agronomically suboptimal and integrated transgenes of interest must be crossed into elite cultivars followed by successive backcrosses to limit the genome drag of undesirable traits. Recently, breakthrough technology using transcription factors controlling cell proliferation and meristematic identity has been successfully used to increase the regeneration and transformation efficiency of recalcitrant plant species and genotypes [132, 133]. Adding to this work, Maher and colleagues have recently shown that combinatorial expression of WUSCHEL, MERISTEMLESS, and BABYBOOM was able to initiate efficient meristem induction de novo, resulting in the outgrowth of miniature plantlets [134]. This is a major advance, as it circumvents the time-consuming and labor intensive process of tissue culture and somatic embryo development.

5. Future Directions

Through many technical innovations, A. tumefaciens can now be used to engineer the genomes of many plants well beyond its natural host range. While these developments are substantial, there has been a lack of precision genetic control in nearly all currently published binary or ternary systems. A critical first step remains in developing a robust A. tumefaciens synthetic biology toolkit of well-characterized constitutive and inducible promoters, terminators, and origins of replication (Figure 1(a)). There are now many examples of excellent toolkits being constructed for nonmodel bacteria such as Pseudomonas putida [135], Vibrio natriegens [136], Streptomyces venezuelae [137], and Cyanobacteria [138]. Once a toolkit is in place, the virulence plasmid would be able to be entirely synthetically refactored (Figure 1(b)). This would allow researchers to titrate the expression of specific virulence factors to engineer desired transformation outcomes (i.e., high transient T-DNA expression or increased host range). Furthermore, such precise genetic control would allow researchers to elegantly interrogate basic questions of A. tumefaciens virulence [139].

Similar synthetic biology principles can also be applied to interrogate plant host responses that influence plant transformation and regeneration. Combinatorial knockdown and overexpression of host genes may help tailor plant transformation to particular plant species or genotype, while also providing tools to probe the underlying host biology of A. tumefaciens pathogenesis (Figure 1(c)). Moving forward, exerting simultaneous, precise control over both host and pathogen systems may usher in a new era of agricultural biotechnology.

Data Availability

All data is freely available upon request.

Conflicts of Interest

The authors declare that there is no conflict of interest regarding the publication of this article.

Authors’ Contributions

Mitchell G. Thompson and William M. Moore contributed equally to this work.


This work conducted by the Joint BioEnergy Institute was supported by the US Department of Energy, Office of Science, Office of Biological and Environmental Research under contract no. DE-AC02-05CH11231 between Lawrence Berkeley National Laboratory and the US Department of Energy.


  1. T. Meyer, C. Thiour-Mauprivez, F. Wisniewski-Dyé et al., “Ecological conditions and molecular determinants involved in Agrobacterium lifestyle in tumors,” Frontiers in Plant Science, vol. 10, p. 978, 2019. View at: Publisher Site | Google Scholar
  2. B. Lacroix and V. Citovsky, “Pathways of DNA transfer to plants from Agrobacterium tumefaciensand related bacterial species,” Annual Review of Phytopathology, vol. 57, no. 1, pp. 231–251, 2019. View at: Publisher Site | Google Scholar
  3. E. W. Nester, “Agrobacterium: nature’s genetic engineer,” Frontiers in Plant Science, vol. 5, p. 730, 2014. View at: Google Scholar
  4. A. Hoekema, P. R. Hirsch, P. J. J. Hooykaas, and R. A. Schilperoort, “A binary plant vector strategy based on separation of vir- and T-region of the Agrobacterium tumefaciens Ti-plasmid,” Nature, vol. 303, no. 5913, pp. 179-180, 1983. View at: Publisher Site | Google Scholar
  5. M. Guo, J. Ye, D. Gao, N. Xu, and J. Yang, “Agrobacterium-mediated horizontal gene transfer: mechanism, biotechnological application, potential risk and forestalling strategy,” Biotechnology Advances, vol. 37, no. 1, pp. 259–270, 2019. View at: Publisher Site | Google Scholar
  6. S. B. Gelvin, “Agrobacterium-mediated plant transformation: the biology behind the “gene-jockeying” tool,” Microbiology and Molecular Biology Reviews, vol. 67, no. 1, pp. 16–37, 2003. View at: Publisher Site | Google Scholar
  7. K. Temme, D. Zhao, and C. A. Voigt, “Refactoring the nitrogen fixation gene cluster from Klebsiella oxytoca,” Proceedings of the National Academy of Sciences, vol. 109, no. 18, pp. 7085–7090, 2012. View at: Publisher Site | Google Scholar
  8. I. Budin, T. de Rond, Y. Chen, L. J. G. Chan, C. J. Petzold, and J. D. Keasling, “Viscous control of cellular respiration by membrane lipid composition,” Science, vol. 362, no. 6419, pp. 1186–1189, 2018. View at: Publisher Site | Google Scholar
  9. A. Eudes, N. Zhao, N. Sathitsuksanoh et al., “Expression of S-adenosylmethionine hydrolase in tissues synthesizing secondary cell walls alters specific methylated cell wall fractions and improves biomass digestibility,” Frontiers in Bioengineering and Biotechnology, vol. 4, p. 58, 2016. View at: Publisher Site | Google Scholar
  10. A. M. Ashby, M. D. Watson, G. J. Loake, and C. H. Shaw, “Ti plasmid-specified chemotaxis of Agrobacterium tumefaciens C58C1 toward vir-inducing phenolic compounds and soluble factors from monocotyledonous and dicotyledonous plants,” Journal of Bacteriology, vol. 170, no. 9, pp. 4181–4187, 1988. View at: Publisher Site | Google Scholar
  11. D. Parke, L. N. Ornston, and E. W. Nester, “Chemotaxis to plant phenolic inducers of virulence genes is constitutively expressed in the absence of the Ti plasmid in Agrobacterium tumefaciens,” Journal of Bacteriology, vol. 169, no. 11, pp. 5336–5338, 1987. View at: Publisher Site | Google Scholar
  12. A. Brencic and S. C. Winans, “Detection of and response to signals involved in host-microbe interactions by plant-associated bacteria,” Microbiology and Molecular Biology Reviews, vol. 69, no. 1, pp. 155–194, 2005. View at: Publisher Site | Google Scholar
  13. M. Guo, Z. Huang, and J. Yang, “Is there any crosstalk between the chemotaxis and virulence induction signaling in Agrobacterium tumefaciens?” Biotechnology Advances, vol. 35, no. 4, pp. 505–511, 2017. View at: Publisher Site | Google Scholar
  14. O. Chesnokova, J. B. Coutinho, I. H. Khan, M. S. Mikhail, and C. I. Kado, “Characterization of flagella genes of Agrobacterium tumefaciens, and the effect of a bald strain on virulence,” Molecular Microbiology, vol. 23, no. 3, pp. 579–590, 1997. View at: Publisher Site | Google Scholar
  15. D. M. Raineri, M. I. Boulton, J. W. Davies, and E. W. Nester, “VirA, the plant-signal receptor, is responsible for the Ti plasmid-specific transfer of DNA to maize by Agrobacterium,” Proceedings of the National Academy of Sciences, vol. 90, no. 8, pp. 3549–3553, 1993. View at: Publisher Site | Google Scholar
  16. X. Hu, J. Zhao, W. F. DeGrado, and A. N. Binns, “Agrobacterium tumefaciens recognizes its host environment using ChvE to bind diverse plant sugars as virulence signals,” Proceedings of the National Academy of Sciences, vol. 110, no. 2, pp. 678–683, 2013. View at: Publisher Site | Google Scholar
  17. L. Li, Y. Jia, Q. Hou, T. C. Charles, E. W. Nester, and S. Q. Pan, “A global pH sensor: Agrobacterium sensor protein ChvG regulates acid-inducible genes on its two chromosomes and Ti plasmid,” Proceedings of the National Academy of Sciences, vol. 99, no. 19, pp. 12369–12374, 2002. View at: Publisher Site | Google Scholar
  18. Y.-H. Lin, R. Gao, A. N. Binns, and D. G. Lynn, “Capturing the VirA/VirG TCS of Agrobacterium tumefaciens,” in Advances in Experimental Medicine and Biology, vol. 631, pp. 161–177, Springer, 2008. View at: Google Scholar
  19. J. Xi, M. Patel, S. Dong, Q. Que, and R. Qu, “Acetosyringone treatment duration affects large T-DNA molecule transfer to rice callus,” BMC Biotechnology, vol. 18, no. 1, p. 48, 2018. View at: Publisher Site | Google Scholar
  20. H. Y. Wu, K. H. Liu, Y. C. Wang et al., “AGROBEST: an efficient Agrobacterium-mediated transient expression method for versatile gene function analyses in Arabidopsis seedlings,” Plant Methods, vol. 10, no. 1, p. 19, 2014. View at: Publisher Site | Google Scholar
  21. E. Manfroi, E. Yamazaki-Lau, M. F. Grando, and E. A. Roesler, “Acetosyringone, pH and temperature effects on transient genetic transformation of immature embryos of Brazilian wheat genotypes by Agrobacterium tumefaciens,” Genetics and Molecular Biology, vol. 38, no. 4, pp. 470–476, 2015. View at: Publisher Site | Google Scholar
  22. R. Srinivasan and K. M. Gothandam, “Synergistic action of D-glucose and acetosyringone on Agrobacterium strains for efficient Dunaliella transformation,” PLoS One, vol. 11, no. 6, article e0158322, 2016. View at: Publisher Site | Google Scholar
  23. K. Lee and K. Wang, “Small noncoding RNAs in Agrobacterium tumefaciens,” Current Topics in Microbiology and Immunology, vol. 418, pp. 195–213, 2018. View at: Publisher Site | Google Scholar
  24. I. Wilms, P. Moller, A. M. Stock, R. Gurski, E. M. Lai, and F. Narberhaus, “Hfq influences multiple transport systems and virulence in the plant pathogen Agrobacterium tumefaciens,” Journal of Bacteriology, vol. 194, no. 19, pp. 5209–5217, 2012. View at: Publisher Site | Google Scholar
  25. A. Overlöper, A. Kraus, R. Gurski et al., “Two separate modules of the conserved regulatory RNA AbcR1 address multiple target mRNAs in and outside of the translation initiation region,” RNA Biology, vol. 11, no. 5, pp. 624–640, 2014. View at: Publisher Site | Google Scholar
  26. L. van der Fits, E. A. Deakin, J. H. C. Hoge, and J. Memelink, “The ternary transformation system: constitutive virG on a compatible plasmid dramatically increases Agrobacterium-mediated plant transformation,” Plant Molecular Biology, vol. 43, no. 4, pp. 495–502, 2000. View at: Publisher Site | Google Scholar
  27. G. Hansen, A. Das, and M. D. Chilton, “Constitutive expression of the virulence genes improves the efficiency of plant transformation by Agrobacterium,” Proceedings of the National Academy of Sciences, vol. 91, no. 16, pp. 7603–7607, 1994. View at: Publisher Site | Google Scholar
  28. S. Nonaka, T. Someya, Y. Kadota, K. Nakamura, and H. Ezura, “Super-Agrobacterium ver. 4: improving the transformation frequencies and genetic engineering possibilities for crop plants. Front,” Plant Science, vol. 10, p. 1204, 2019. View at: Google Scholar
  29. S. Nonaka, K. I. Yuhashi, K. Takada, M. Sugaware, K. Minamisawa, and H. Ezura, “Ethylene production in plants during transformation suppresses vir gene expression in Agrobacterium tumefaciens,” New Phytologist, vol. 178, no. 3, pp. 647–656, 2008. View at: Publisher Site | Google Scholar
  30. A. G. Matthysse, “Attachment of Agrobacterium to plant surfaces,” Frontiers in Plant Science, vol. 5, p. 252, 2014. View at: Google Scholar
  31. M. A. Thompson, M. C. Onyeziri, and C. Fuqua, “Function and regulation of Agrobacterium tumefaciens cell surface structures that promote attachment,” Current Topics in Microbiology and Immunology, vol. 418, pp. 143–184, 2018. View at: Publisher Site | Google Scholar
  32. F. Gürel, C. Uçarlı, F. Tufan, and D. M. Kalaskar, “Enhancing T-DNA transfer efficiency in Barley (Hordeum vulgare L.) cells using extracellular cellulose and lectin,” Applied Biochemistry and Biotechnology, vol. 176, no. 4, pp. 1203–1216, 2015. View at: Publisher Site | Google Scholar
  33. J. Xu, J. Kim, B. J. Koestler, J. H. Choi, C. M. Waters, and C. Fuqua, “Genetic analysis of Agrobacterium tumefaciens unipolar polysaccharide production reveals complex integrated control of the motile-to-sessile switch,” Molecular Microbiology, vol. 89, no. 5, pp. 929–948, 2013. View at: Publisher Site | Google Scholar
  34. D. Amikam and M. Benziman, “Cyclic diguanylic acid and cellulose synthesis in Agrobacterium tumefaciens,” Journal of Bacteriology, vol. 171, no. 12, pp. 6649–6655, 1989. View at: Publisher Site | Google Scholar
  35. U. Römling, M. Y. Galperin, and M. Gomelsky, “Cyclic di-GMP: the first 25 years of a universal bacterial second messenger,” Microbiology and Molecular Biology Reviews, vol. 77, pp. 1–52, 2013. View at: Publisher Site | Google Scholar
  36. N. Feirer, J. Xu, K. D. Allen et al., “A Pterin-dependent signaling pathway regulates a dual-function diguanylate cyclase-phosphodiesterase controlling surface attachment in Agrobacterium tumefaciens,” mBio, vol. 6, no. 4, article e00156, 2015. View at: Publisher Site | Google Scholar
  37. S. L. Mathews, H. Hannah, H. Samagaio, C. Martin, E. Rodriguez-Rassi, and A. G. Matthysse, “Glycoside hydrolase genes are required for virulence ofAgrobacterium tumefaciensonBryophyllum daigremontianaand tomato,” Applied and Environmental Microbiology, vol. 85, no. 15, 2019. View at: Publisher Site | Google Scholar
  38. Y. G. Li and P. J. Christie, “The Agrobacterium virb/vird4 T4SS: mechanism and architecture defined through in vivo mutagenesis and chimeric systems,” Current Topics in Microbiology and Immunology, vol. 418, pp. 233–260, 2018. View at: Publisher Site | Google Scholar
  39. K. Atmakuri, E. Cascales, O. T. Burton, L. M. Banta, and P. J. Christie, “Agrobacterium ParA/MinD-like VirC1 spatially coordinates early conjugative DNA transfer reactions,” The EMBO Journal, vol. 26, no. 10, pp. 2540–2551, 2007. View at: Publisher Site | Google Scholar
  40. N. Toro, A. Datta, O. A. Carmi, C. Young, R. K. Prusti, and E. W. Nester, “The Agrobacterium tumefaciens virC1 gene product binds to overdrive, a T-DNA transfer enhancer,” Journal of Bacteriology, vol. 171, no. 12, pp. 6845–6849, 1989. View at: Publisher Site | Google Scholar
  41. K. M. Pappas and S. C. Winans, “A LuxR-type regulator from Agrobacterium tumefaciens elevates Ti plasmid copy number by activating transcription of plasmid replication genes,” Molecular Microbiology, vol. 48, no. 4, pp. 1059–1073, 2003. View at: Publisher Site | Google Scholar
  42. M. Á. Vences-Guzmán, Z. Guan, J. R. Bermúdez-Barrientos, O. Geiger, and C. Sohlenkamp, “Agrobacteria lacking ornithine lipids induce more rapid tumour formation,” Environmental Microbiology, vol. 15, no. 3, pp. 895–906, 2013. View at: Publisher Site | Google Scholar
  43. M. K. Groenewold, S. Hebecker, C. Fritz et al., “Virulence of Agrobacterium tumefaciens requires lipid homeostasis mediated by the lysyl-phosphatidylglycerol hydrolase AcvB,” Molecular Microbiology, vol. 111, no. 1, pp. 269–286, 2019. View at: Publisher Site | Google Scholar
  44. S. Bourras, T. Rouxel, and M. Meyer, “Agrobacterium tumefaciens gene transfer: how a plant pathogen hacks the nuclei of plant and nonplant organisms,” Phytopathology, vol. 105, no. 10, pp. 1288–1301, 2015. View at: Publisher Site | Google Scholar
  45. B. Lacroix and V. Citovsky, “The roles of bacterial and host plant factors in Agrobacterium-mediated genetic transformation,” The International Journal of Developmental Biology, vol. 57, no. 6-7-8, pp. 467–481, 2013. View at: Publisher Site | Google Scholar
  46. S. Bhattacharjee, L. Y. Lee, H. Oltmanns et al., “IMPa-4, an Arabidopsis importin alpha isoform, is preferentially involved in Agrobacterium-mediated plant transformation,” The Plant Cell, vol. 20, no. 10, pp. 2661–2680, 2008. View at: Publisher Site | Google Scholar
  47. Y. Shi, L.-Y. Lee, and S. B. Gelvin, “Is VIP1 important for Agrobacterium-mediated transformation?” The Plant Journal, vol. 79, no. 5, pp. 848–860, 2014. View at: Publisher Site | Google Scholar
  48. B. Lacroix, M. Vaidya, T. Tzfira, and V. Citovsky, “The VirE3 protein of Agrobacterium mimics a host cell function required for plant genetic transformation,” The EMBO Journal, vol. 24, pp. 428–437, 2004. View at: Publisher Site | Google Scholar
  49. X. Li, H. Tu, and S. Q. Pan, “Agrobacterium delivers anchorage protein VirE3 for companion VirE2 to aggregate at host entry sites for T-DNA protection,” Cell Reports, vol. 25, no. 2, pp. 302–311.e6, 2018. View at: Publisher Site | Google Scholar
  50. A. Zaltsman, A. Krichevsky, A. Loyter, and V. Citovsky, “Agrobacterium induces expression of a host F-box protein required for tumorigenicity,” Cell Host & Microbe, vol. 7, no. 3, pp. 197–209, 2010. View at: Publisher Site | Google Scholar
  51. Y. Wang, S. Zhang, F. Huang et al., “VirD5 is required for efficient Agrobacterium infection and interacts with Arabidopsis VIP2,” New Phytologist, vol. 217, no. 2, pp. 726–738, 2018. View at: Publisher Site | Google Scholar
  52. E. Jarchow, N. H. Grimsley, and B. Hohn, “virF, the host-range-determining virulence gene of Agrobacterium tumefaciens, affects T-DNA transfer to Zea mays,” Proceedings of the National Academy of Sciences, vol. 88, no. 23, pp. 10426–10430, 1991. View at: Publisher Site | Google Scholar
  53. X. Zhang and P. J. J. Hooykaas, “The Agrobacterium VirD5 protein hyperactivates the mitotic Aurora kinase in host cells,” New Phytologist, vol. 222, no. 3, pp. 1551–1560, 2019. View at: Publisher Site | Google Scholar
  54. A. Pitzschke, “Agrobacterium infection and plant defense—transformation success hangs by a thread,” Frontiers in Plant Science, vol. 4, p. 519, 2013. View at: Publisher Site | Google Scholar
  55. V. S. Kalogeraki, J. Zhu, A. Eberhard, E. L. Madsen, and S. C. Winans, “The phenolic vir gene inducer ferulic acid is O-demethylated by the VirH2 protein of an Agrobacterium tumefaciens Ti plasmid,” Molecular Microbiology, vol. 34, no. 3, pp. 512–522, 1999. View at: Publisher Site | Google Scholar
  56. X. Q. Xu and S. Q. Pan, “An Agrobacterium catalase is a virulence factor involved in tumorigenesis,” Molecular Microbiology, vol. 35, no. 2, pp. 407–414, 2000. View at: Publisher Site | Google Scholar
  57. X. Niu, M. Zhou, C. V. Henkel, G. P. H. van Heusden, and P. J. J. Hooykaas, “The Agrobacterium tumefaciens virulence protein VirE3 is a transcriptional activator of the F-box gene VBF,” The Plant Journal, vol. 84, no. 5, pp. 914–924, 2015. View at: Publisher Site | Google Scholar
  58. E. García-Cano, H. Hak, S. Magori, S. G. Lazarowitz, and V. Citovsky, “The Agrobacterium F-Box protein effector VirF destabilizes the Arabidopsis GLABROUS1 enhancer/binding protein-like transcription factor VFP4, a transcriptional activator of defense response genes,” Molecular Plant-Microbe Interactions, vol. 31, no. 5, pp. 576–586, 2018. View at: Publisher Site | Google Scholar
  59. J. H. Lee, H. Kim, W. B. Chae, and M.-H. Oh, “Pattern recognition receptors and their interactions with bacterial type III effectors in plants,” Genes & Genomics, vol. 41, no. 5, pp. 499–506, 2019. View at: Publisher Site | Google Scholar
  60. P. Montoro, N. Teinseree, W. Rattana, P. Kongsawadworakul, and N. Michaux-Ferriere, “Effect of exogenous calcium on Agrobacterium tumefaciens-mediated gene transfer in Hevea brasiliensis (rubber tree) friable calli,” Plant Cell Reports, vol. 19, no. 9, pp. 851–855, 2000. View at: Publisher Site | Google Scholar
  61. A. Peaucelle, S. Braybrook, and H. Höfte, “Cell wall mechanics and growth control in plants: the role of pectins revisited,” Frontiers in Plant Science, vol. 3, p. 121, 2012. View at: Publisher Site | Google Scholar
  62. Y. Zhu, J. Nam, J. M. Humara et al., “Identification of Arabidopsis rat mutants,” Plant Physiology, vol. 132, no. 2, pp. 494–505, 2003. View at: Publisher Site | Google Scholar
  63. Y. M. Gaspar, J. Nam, C. J. Schultz et al., “Characterization of the Arabidopsis lysine-rich arabinogalactan-protein AtAGP17 mutant (rat1) that results in a decreased efficiency of Agrobacterium transformation,” Plant Physiology, vol. 135, no. 4, pp. 2162–2171, 2004. View at: Publisher Site | Google Scholar
  64. F. Xie, A. Williams, A. Edwards, and J. A. Downie, “A plant arabinogalactan-like glycoprotein promotes a novel type of polar surface attachment by Rhizobium leguminosarum,” Molecular Plant-Microbe Interactions, vol. 25, no. 2, pp. 250–258, 2012. View at: Publisher Site | Google Scholar
  65. J. L. Lind, I. Bönig, A. E. Clarke, and M. A. Anderson, “A style-specific 120-kDa glycoprotein enters pollen tubes of Nicotiana alata in vivo,” Sexual Plant Reproduction, vol. 9, no. 2, pp. 75–86, 1996. View at: Publisher Site | Google Scholar
  66. L. Wang, M. Cheng, Q. Yang et al., “Arabinogalactan protein–rare earth element complexes activate plant endocytosis,” Proceedings of the National Academy of Sciences, vol. 116, no. 28, pp. 14349–14357, 2019. View at: Publisher Site | Google Scholar
  67. H.-H. Hwang and S. B. Gelvin, “Plant proteins that interact with VirB2, the Agrobacterium tumefaciens pilin protein, mediate plant transformation,” The Plant Cell, vol. 16, no. 11, pp. 3148–3167, 2004. View at: Publisher Site | Google Scholar
  68. F.-C. Huang, B. J. Fu, Y. T. Liu et al., “Arabidopsis RETICULON-LIKE3 (RTNLB3) and RTNLB8 participate in Agrobacterium-mediated plant transformation,” International Journal of Molecular Sciences, vol. 19, no. 2, p. 638, 2018. View at: Publisher Site | Google Scholar
  69. F.-C. Huang and H.-H. Hwang, “Arabidopsis RETICULON-LIKE4 (RTNLB4) protein participates in Agrobacterium infection and VirB2 peptide-induced plant defense response,” International Journal of Molecular Sciences, vol. 21, no. 5, p. 1722, 2020. View at: Publisher Site | Google Scholar
  70. D. Tsugama, S. Liu, and T. Takano, “A bZIP protein, VIP1, is a regulator of osmosensory signaling in Arabidopsis,” Plant Physiology, vol. 159, no. 1, pp. 144–155, 2012. View at: Publisher Site | Google Scholar
  71. R. Lapham, L. Y. Lee, D. Tsugama, S. Lee, T. Mengiste, and S. B. Gelvin, “VIP1 and its homologs are not required for Agrobacterium-mediated transformation, but play a role in Botrytis and salt stress responses,” Frontiers in Plant Science, vol. 9, p. 749, 2018. View at: Publisher Site | Google Scholar
  72. Y. Wu, Q. Zhao, L. Gao et al., “Isolation and characterization of low-sulphur-tolerant mutants of Arabidopsis,” Journal of Experimental Botany, vol. 61, no. 12, pp. 3407–3422, 2010. View at: Publisher Site | Google Scholar
  73. D. Tsugama, H. S. Yoon, K. Fujino, S. Liu, and T. Takano, “Protein phosphatase 2A regulates the nuclear accumulation of the Arabidopsis bZIP protein VIP1 under hypo-osmotic stress,” Journal of Experimental Botany, vol. 70, no. 21, pp. 6101–6112, 2019. View at: Publisher Site | Google Scholar
  74. A. Djamei, A. Pitzschke, H. Nakagami, I. Rajh, and H. Hirt, “Trojan horse strategy in Agrobacterium transformation: abusing MAPK defense signaling,” Science, vol. 318, no. 5849, pp. 453–456, 2007. View at: Publisher Site | Google Scholar
  75. T. Tzfira and V. Citovsky, “Partners-in-infection: host proteins involved in the transformation of plant cells by Agrobacterium,” Trends in Cell Biology, vol. 12, no. 3, pp. 121–129, 2002. View at: Publisher Site | Google Scholar
  76. A. Pitzschke, A. Schikora, and H. Hirt, “MAPK cascade signalling networks in plant defence,” Current Opinion in Plant Biology, vol. 12, no. 4, pp. 421–426, 2009. View at: Publisher Site | Google Scholar
  77. L. Wang, B. Lacroix, J. Guo, and V. Citovsky, “The Agrobacterium VirE2 effector interacts with multiple members of the Arabidopsis VIP1 protein family,” Molecular Plant Pathology, vol. 19, no. 5, pp. 1172–1183, 2018. View at: Publisher Site | Google Scholar
  78. Y. Tao, P. K. Rao, S. Bhattacharjee, and S. B. Gelvin, “Expression of plant protein phosphatase 2C interferes with nuclear import of the Agrobacterium T-complex protein VirD2,” Proceedings of the National Academy of Sciences, vol. 101, no. 14, pp. 5164–5169, 2004. View at: Publisher Site | Google Scholar
  79. S. B. Gelvin, “Agrobacterium and plant genes involved INT-DNA transfer and integration,” Annual Review of Plant Physiology and Plant Molecular Biology, vol. 51, no. 1, pp. 223–256, 2000. View at: Publisher Site | Google Scholar
  80. R. V. Sonti, M. Chiurazzi, D. Wong et al., “Arabidopsis mutants deficient in T-DNA integration,” Proceedings of the National Academy of Sciences, vol. 92, no. 25, pp. 11786–11790, 1995. View at: Publisher Site | Google Scholar
  81. M. Endo, Y. Ishikawa, K. Osakabe et al., “Increased frequency of homologous recombination and T-DNA integration in Arabidopsis CAF-1 mutants,” The EMBO Journal, vol. 25, no. 23, pp. 5579–5590, 2006. View at: Publisher Site | Google Scholar
  82. S.-Y. Park, Z. Vaghchhipawala, B. Vasudevan et al., “Agrobacterium T-DNA integration into the plant genome can occur without the activity of key non-homologous end-joining proteins,” The Plant Journal, vol. 81, no. 6, pp. 934–946, 2015. View at: Publisher Site | Google Scholar
  83. N. Kleinboelting, G. Huep, I. Appelhagen, P. Viehoever, Y. Li, and B. Weisshaar, “The structural features of thousands of T-DNA insertion sites are consistent with a double-strand break repair-based insertion mechanism,” Molecular Plant, vol. 8, no. 11, pp. 1651–1664, 2015. View at: Publisher Site | Google Scholar
  84. Z. E. Vaghchhipawala, B. Vasudevan, S. Lee, M. R. Morsy, and K. S. Mysore, “Agrobacterium may delay plant nonhomologous end-joining DNA repair via XRCC4 to favor T-DNA integration,” The Plant Cell, vol. 24, no. 10, pp. 4110–4123, 2012. View at: Publisher Site | Google Scholar
  85. M. van Kregten, S. de Pater, R. Romeijn, R. van Schendel, P. J. J. Hooykaas, and M. Tijsterman, “T-DNA integration in plants results from polymerase-θ-mediated DNA repair,” Nature Plants, vol. 2, no. 11, article 16164, 2016. View at: Publisher Site | Google Scholar
  86. S. J. Ceballos and W.-D. Heyer, “Functions of the Snf2/Swi2 family Rad54 motor protein in homologous recombination,” Biochimica et Biophysica Acta (BBA) - Gene Regulatory Mechanisms, vol. 1809, no. 9, pp. 509–523, 2011. View at: Publisher Site | Google Scholar
  87. H. Shaked, C. Melamed-Bessudo, and A. A. Levy, “High-frequency gene targeting in Arabidopsis plants expressing the yeast RAD54 gene,” Proceedings of the National Academy of Sciences, vol. 102, no. 34, pp. 12265–12269, 2005. View at: Publisher Site | Google Scholar
  88. H. Yi, K. S. Mysore, and S. B. Gelvin, “Expression of the Arabidopsis histone H2A-1 gene correlates with susceptibility to Agrobacterium transformation,” The Plant Journal, vol. 32, no. 3, pp. 285–298, 2002. View at: Publisher Site | Google Scholar
  89. K. S. Mysore, J. Nam, and S. B. Gelvin, “An Arabidopsis histone H2A mutant is deficient in Agrobacterium T-DNA integration,” Proceedings of the National Academy of Sciences, vol. 97, no. 2, pp. 948–953, 2000. View at: Publisher Site | Google Scholar
  90. Y. E. Zheng, X. W. He, Y. H. Ying, J. F. Lu, S. B. Gelvin, and H. X. Shou, “Expression of the Arabidopsis thaliana histone gene AtHTA1 enhances rice transformation efficiency,” Molecular Plant, vol. 2, no. 4, pp. 832–837, 2009. View at: Publisher Site | Google Scholar
  91. G. N. Tenea, J. Spantzel, L. Y. Lee et al., “Overexpression of several Arabidopsis histone genes increases Agrobacterium-mediated transformation and transgene expression in plants,” The Plant Cell, vol. 21, no. 10, pp. 3350–3367, 2009. View at: Publisher Site | Google Scholar
  92. A. Anand, A. Krichevsky, S. Schornack et al., “Arabidopsis VIRE2 interacting protein2 is required for Agrobacterium T-DNA integration in plants,” The Plant Cell, vol. 19, no. 5, pp. 1695–1708, 2007. View at: Publisher Site | Google Scholar
  93. K. Duan, C. J. Willig, J. R. De Tar, W. G. Spollen, and Z. J. Zhang, “Transcriptomic analysis of Arabidopsis seedlings in response to an Agrobacterium-mediated transformation process,” Molecular Plant-Microbe Interactions, vol. 31, no. 4, pp. 445–459, 2018. View at: Publisher Site | Google Scholar
  94. Y. Liu, Z. Zhang, J. Fu, G. Wang, J. Wang, and Y. Liu, “Transcriptome analysis of maize immature embryos reveals the roles of cysteine in improving Agrobacterium infection efficiency,” Frontiers in Plant Science, vol. 8, p. 1778, 2017. View at: Publisher Site | Google Scholar
  95. C. J. Willig, K. Duan, and Z. J. Zhang, “Transcriptome profiling of plant genes in response to Agrobacterium tumefaciens-mediated transformation,” in Current Topics in Microbiology and Immunology, vol. 418, pp. 319–348, Springer, 2018. View at: Google Scholar
  96. C. Zipfel, G. Kunze, D. Chinchilla et al., “Perception of the bacterial PAMP EF-Tu by the receptor EFR restricts Agrobacterium-mediated transformation,” Cell, vol. 125, no. 4, pp. 749–760, 2006. View at: Publisher Site | Google Scholar
  97. P. Dunoyer, C. Himber, and O. Voinnet, “Induction, suppression and requirement of RNA silencing pathways in virulent Agrobacterium tumefaciens infections,” Nature Genetics, vol. 38, no. 2, pp. 258–263, 2006. View at: Publisher Site | Google Scholar
  98. Z. Xie, E. Allen, A. Wilken, and J. C. Carrington, “DICER-LIKE 4 functions in trans-acting small interfering RNA biogenesis and vegetative phase change in Arabidopsis thaliana,” Proceedings of the National Academy of Sciences, vol. 102, no. 36, pp. 12984–12989, 2005. View at: Publisher Site | Google Scholar
  99. J. G. Philips, K. J. Dudley, P. M. Waterhouse, and R. P. Hellens, “The rapid methylation of T-DNAs upon Agrobacterium inoculation in plant leaves,” Frontiers in Plant Science, vol. 10, p. 312, 2019. View at: Publisher Site | Google Scholar
  100. Q. Zhao, Y. du, H. Wang et al., “5-Azacytidine promotes shoot regeneration during Agrobacterium-mediated soybean transformation,” Plant Physiology and Biochemistry, vol. 141, pp. 40–50, 2019. View at: Publisher Site | Google Scholar
  101. T. Iki, M.-A. Tschopp, and O. Voinnet, “Biochemical and genetic functional dissection of the P38 viral suppressor of RNA silencing,” RNA, vol. 23, no. 5, pp. 639–654, 2017. View at: Publisher Site | Google Scholar
  102. L. Lakatos, G. Szittya, D. Silhavy, and J. Burgyán, “Molecular mechanism of RNA silencing suppression mediated by p19 protein of tombusviruses,” The EMBO Journal, vol. 23, no. 4, pp. 876–884, 2004. View at: Publisher Site | Google Scholar
  103. T. Kwon, “Mitochondrial porin isoform AtVDAC1 regulates the competence of Arabidopsis thaliana to Agrobacterium-mediated genetic transformation,” Molecules and Cells, vol. 39, no. 9, pp. 705–713, 2016. View at: Publisher Site | Google Scholar
  104. L.-Y. Lee and S. B. Gelvin, “T-DNA binary vectors and systems,” Plant Physiology, vol. 146, no. 2, pp. 325–332, 2008. View at: Publisher Site | Google Scholar
  105. R. Hellens, P. Mullineaux, and H. Klee, “Technical focus:a guide to Agrobacterium binary Ti vectors,” Trends in Plant Science, vol. 5, no. 10, pp. 446–451, 2000. View at: Publisher Site | Google Scholar
  106. J. E. Gordon and P. J. Christie, “The Agrobacterium ti plasmids,” Microbiology Spectrum, vol. 2, no. 6, 2014. View at: Publisher Site | Google Scholar
  107. S. De Buck, C. De Wilde, M. Van Montagu, and A. Depicker, “T-DNA vector backbone sequences are frequently integrated into the genome of transgenic plants obtained by Agrobacterium-mediated transformation,” Molecular Breeding, vol. 6, no. 5, pp. 459–468, 2000. View at: Publisher Site | Google Scholar
  108. D. Schubert, B. Lechtenberg, A. Forsbach, M. Gils, S. Bahadur, and R. Schmidt, “Silencing in Arabidopsis T-DNA transformants: the predominant role of a gene-specific RNA sensing mechanism versus position effects,” The Plant Cell, vol. 16, no. 10, pp. 2561–2572, 2004. View at: Publisher Site | Google Scholar
  109. A. Pontiroli, A. Rizzi, P. Simonet, D. Daffonchio, T. M. Vogel, and J. M. Monier, “Visual evidence of horizontal gene transfer between plants and bacteria in the phytosphere of transplastomic tobacco,” Applied and Environmental Microbiology, vol. 75, no. 10, pp. 3314–3322, 2009. View at: Publisher Site | Google Scholar
  110. F. Pasin, L. C. Bedoya, J. M. Bernabé-Orts et al., “Multiple T-DNA delivery to plants using novel mini binary vectors with compatible replication origins,” ACS Synthetic Biology, vol. 6, no. 10, pp. 1962–1968, 2017. View at: Publisher Site | Google Scholar
  111. M. A. Smedley and W. A. Harwood, “Gateway®-compatible plant transformation vectors,” in Methods in Molecular Biology, vol. 1223, pp. 3–16, Springer, 2015. View at: Google Scholar
  112. L. Zhi, S. TeRonde, S. Meyer et al., “Effect of Agrobacterium strain and plasmid copy number on transformation frequency, event quality and usable event quality in an elite maize cultivar,” Plant Cell Reports, vol. 34, no. 5, pp. 745–754, 2015. View at: Publisher Site | Google Scholar
  113. X. Ye, E. J. Williams, J. Shen et al., “Enhanced production of single copy backbone-free transgenic plants in multiple crop species using binary vectors with a pRi replication origin in Agrobacterium tumefaciens,” Transgenic Research, vol. 20, no. 4, pp. 773–786, 2011. View at: Publisher Site | Google Scholar
  114. A. Anand, S. H. Bass, E. Wu et al., “An improved ternary vector system for Agrobacterium-mediated rapid maize transformation,” Plant Molecular Biology, vol. 97, no. 1-2, pp. 187–200, 2018. View at: Publisher Site | Google Scholar
  115. A. Anand, P. Che, E. Wu, and T. J. Jones, “Novel ternary vectors for efficient sorghum transformation,” in Methods in Molecular Biology, vol. 1931, pp. 185–196, Humana Press, 2019. View at: Google Scholar
  116. H. Oltmanns, B. Frame, L. Y. Lee et al., “Generation of backbone-free, low transgene copy plants by launching T-DNA from the Agrobacterium chromosome,” Plant Physiology, vol. 152, no. 3, pp. 1158–1166, 2010. View at: Publisher Site | Google Scholar
  117. X. Ye, E. J. Williams, J. Shen et al., “Plant development inhibitory genes in binary vector backbone improve quality event efficiency in soybean transformation,” Transgenic Research, vol. 17, no. 5, pp. 827–838, 2008. View at: Publisher Site | Google Scholar
  118. N. Sardesai, S. Foulk, W. Chen, H. Wu, E. Etchison, and M. Gupta, “Coexpression of octopine and succinamopine Agrobacterium virulence genes to generate high quality transgenic events in maize by reducing vector backbone integration,” Transgenic Research, vol. 27, no. 6, pp. 539–550, 2018. View at: Publisher Site | Google Scholar
  119. J. R. Newman and C. Fuqua, “Broad-host-range expression vectors that carry the L-arabinose-inducible Escherichia coli araBAD promoter and the araC regulator,” Gene, vol. 227, no. 2, pp. 197–203, 1999. View at: Publisher Site | Google Scholar
  120. Z. Liu, Y. Xie, X. Zhang et al., “Efficient construction of large genomic deletion in Agrobacterium tumefaciens by combination of Cre/loxP system and triple recombineering,” Current Microbiology, vol. 72, no. 4, pp. 465–472, 2016. View at: Publisher Site | Google Scholar
  121. S. R. Khan, J. Gaines, R. M. Roop II, and S. K. Farrand, “Broad-host-range expression vectors with tightly regulated promoters and their use to examine the influence of TraR and TraM expression on Ti plasmid quorum sensing,” Applied and Environmental Microbiology, vol. 74, no. 16, pp. 5053–5062, 2008. View at: Publisher Site | Google Scholar
  122. E. Denkovskienė, Š. Paškevičius, S. Werner, Y. Gleba, and A. Ražanskienė, “Inducible expression of Agrobacterium virulence gene VirE2 for stringent regulation of T-DNA transfer in plant transient expression systems,” Molecular Plant-Microbe Interactions, vol. 28, no. 11, pp. 1247–1255, 2015. View at: Publisher Site | Google Scholar
  123. Y. Kang, M. S. Son, and T. T. Hoang, “One step engineering of T7-expression strains for protein production: increasing the host-range of the T7-expression system,” Protein Expression and Purification, vol. 55, no. 2, pp. 325–333, 2007. View at: Publisher Site | Google Scholar
  124. S. Nonaka, M. Sugawara, K. Minamisawa, K.-I. Yuhashi, and H. Ezura, “1-Aminocyclopropane-1-carboxylate deaminase enhances Agrobacterium tumefaciens-mediated gene transfer into plant cells,” Applied and Environmental Microbiology, vol. 74, no. 8, pp. 2526–2528, 2008. View at: Publisher Site | Google Scholar
  125. S. Nonaka, T. Someya, S. Zhou, M. Takayama, K. Nakamura, and H. Ezura, “An Agrobacterium tumefaciens Strain with Gamma-Aminobutyric Acid Transaminase Activity Shows an Enhanced Genetic Transformation Ability in Plants,” Scientific Reports, vol. 7, no. 1, article 42649, 2017. View at: Publisher Site | Google Scholar
  126. J. I. Collens, D. R. Lee, A. M. Seeman, and W. R. Curtis, “Development of auxotrophic Agrobacterium tumefaciens for gene transfer in plant tissue culture,” Biotechnology Progress, vol. 20, no. 3, pp. 890–896, 2004. View at: Publisher Site | Google Scholar
  127. J. P. Ranch, M. Liebergesell, C. W. Garnaat, and G. A. Huffman, “Auxotrophic Agrobacterium for plant transformation and methods thereof,” 2012, US Patent 8-334429. View at: Google Scholar
  128. S. Rajeevkumar, P. Anunanthini, and R. Sathishkumar, “Epigenetic silencing in transgenic plants,” Frontiers in Plant Science, vol. 6, p. 693, 2015. View at: Publisher Site | Google Scholar
  129. M. A. Escobar, E. L. Civerolo, V. S. Polito, K. A. Pinney, and A. M. Dandekar, “Characterization of oncogene-silenced transgenic plants: implications for Agrobacterium biology and post-transcriptional gene silencing,” Molecular Plant Pathology, vol. 4, no. 1, pp. 57–65, 2003. View at: Publisher Site | Google Scholar
  130. A. C. Mallory, B. J. Reinhart, D. Bartel, V. B. Vance, and L. H. Bowman, “A viral suppressor of RNA silencing differentially regulates the accumulation of short interfering RNAs and micro-RNAs in tobacco,” Proceedings of the National Academy of Sciences\, vol. 99, no. 23, pp. 15228–15233, 2002. View at: Publisher Site | Google Scholar
  131. M. Ikeuchi, Y. Ogawa, A. Iwase, and K. Sugimoto, “Plant regeneration: cellular origins and molecular mechanisms,” Development, vol. 143, no. 9, pp. 1442–1451, 2016. View at: Publisher Site | Google Scholar
  132. K. Lowe, E. Wu, N. Wang et al., “Morphogenic RegulatorsBaby boomandWuschelImprove monocot transformation,” The Plant Cell, vol. 28, no. 9, pp. 1998–2015, 2016. View at: Publisher Site | Google Scholar
  133. T. Jones, K. Lowe, G. Hoerster et al., “Maize transformation using the morphogenic genes baby boom and wuschel2,” in Methods in Molecular Biology, pp. 81–93, Humana Press, 2019. View at: Publisher Site | Google Scholar
  134. M. F. Maher, R. A. Nasti, M. Vollbrecht, C. G. Starker, M. D. Clark, and D. F. Voytas, “Plant gene editing through de novo induction of meristems,” Nature Biotechnology, vol. 38, no. 1, pp. 84–89, 2020. View at: Publisher Site | Google Scholar
  135. T. B. Cook, J. M. Rand, W. Nurani, D. K. Courtney, S. A. Liu, and B. F. Pfleger, “Genetic tools for reliable gene expression and recombineering in Pseudomonas putida,” Journal of Industrial Microbiology & Biotechnology, vol. 45, no. 7, pp. 517–527, 2018. View at: Publisher Site | Google Scholar
  136. T. Tschirhart, V. Shukla, E. E. Kelly et al., “Synthetic biology tools for the fast-growing marine BacteriumVibrio natriegens,” ACS Synthetic Biology, vol. 8, no. 9, pp. 2069–2079, 2019. View at: Publisher Site | Google Scholar
  137. R. M. Phelan, D. Sachs, S. J. Petkiewicz et al., “Development of next generation synthetic biology tools for use in Streptomyces venezuelae,” ACS Synthetic Biology, vol. 6, no. 1, pp. 159–166, 2017. View at: Publisher Site | Google Scholar
  138. A. Behle, P. Saake, A. T. Germann, D. Dienst, and I. M. Axmann, “Comparative dose–response analysis of inducible promoters in Cyanobacteria,” ACS Synthetic Biology, vol. 9, no. 4, pp. 843–855, 2020. View at: Publisher Site | Google Scholar
  139. I. Budin and J. D. Keasling, “Synthetic biology for fundamental biochemical discovery,” Biochemistry, vol. 58, no. 11, pp. 1464–1469, 2019. View at: Publisher Site | Google Scholar
  140. M. J. Kim, K. Baek, and C.-M. Park, “Optimization of conditions for transient Agrobacterium-mediated gene expression assays in Arabidopsis,” Plant Cell Reports, vol. 28, no. 8, pp. 1159–1167, 2009. View at: Publisher Site | Google Scholar
  141. S. Gurel, E. Gurel, R. Kaur et al., “Efficient, reproducible Agrobacterium-mediated transformation of sorghum using heat treatment of immature embryos,” Plant Cell Reports, vol. 28, no. 3, pp. 429–444, 2009. View at: Publisher Site | Google Scholar
  142. S. Li, Y. Cong, Y. Liu et al., “Optimization of Agrobacterium-mediated transformation in soybean,” Frontiers in Plant Science, vol. 8, p. 246, 2017. View at: Publisher Site | Google Scholar
  143. R. Chakrabarty, N. Viswakarma, S. R. Bhat, P. B. Kirti, B. D. Singh, and V. L. Chopra, “Agrobacterium-mediated transformation of cauliflower: optimization of protocol and development of Bt-transgenic cauliflower,” Journal of Biosciences, vol. 27, no. 5, pp. 495–502, 2002. View at: Publisher Site | Google Scholar
  144. M. Dutt, M. Vasconcellos, and J. W. Grosser, “Effects of antioxidants on Agrobacterium-mediated transformation and accelerated production of transgenic plants of Mexican lime (Citrus aurantifolia Swingle),” Plant Cell, Tissue and Organ Culture (PCTOC), vol. 107, no. 1, pp. 79–89, 2011. View at: Publisher Site | Google Scholar
  145. K. Xu, X. Huang, M. Wu et al., “A rapid, highly efficient and economical method of Agrobacterium-mediated in planta transient transformation in living onion epidermis,” PLoS One, vol. 9, no. 1, article e83556, 2014. View at: Publisher Site | Google Scholar
  146. K. Subramanyam, K. Subramanyam, K. V. Sailaja, M. Srinivasulu, and K. Lakshmidevi, “Highly efficient Agrobacterium-mediated transformation of banana cv. Rasthali (AAB) via sonication and vacuum infiltration,” Plant Cell Reports, vol. 30, no. 3, pp. 425–436, 2011. View at: Publisher Site | Google Scholar

Copyright © 2020 Mitchell G. Thompson et al. Exclusive Licensee Nanjing Agricultural University. Distributed under a Creative Commons Attribution License (CC BY 4.0).

 PDF Download Citation Citation
Altmetric Score