Auxin Response Factor 2 (ARF2), ARF3, and ARF4 Mediate Both Lateral Root and Nitrogen Fixing Nodule Development in Medicago truncatula

Auxin Response Factors (ARFs) constitute a large family of transcription factors that mediate auxin-regulated developmental programs in plants. ARF2, ARF3, and ARF4 are post-transcriptionally regulated by the microRNA390 (miR390)/trans-acting small interference RNA 3 (TAS3) module through the action of TAS3-derived trans-acting small interfering RNAs (ta-siRNA). We have previously reported that constitutive activation of the miR390/TAS3 pathway promotes elongation of lateral roots but impairs nodule organogenesis and infection by rhizobia during the nitrogen-fixing symbiosis established between Medicago truncatula and its partner Sinorhizobium meliloti. However, the involvement of the targets of the miR390/TAS3 pathway, i.e., MtARF2, MtARF3, MtARF4a, and MtARF4b, in root development and establishment of the nitrogen-fixing symbiosis remained unexplored. Here, promoter:reporter fusions showed that expression of both MtARF3 and MtARF4a was associated with lateral root development; however, only the MtARF4a promoter was active in developing nodules. In addition, up-regulation of MtARF2, MtARF3, and MtARF4a/b in response to rhizobia depends on Nod Factor perception. We provide evidence that simultaneous knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b or mutation in MtARF4a impaired nodule formation, and reduced initiation and progression of infection events. Silencing of MtARF2, MtARF3, MtARF4a, and MtARF4b altered mRNA levels of the early nodulation gene nodulation signaling pathway 2 (MtNSP2). In addition, roots with reduced levels of MtARF2, MtARF3, MtARF4a, and MtARF4b, as well as arf4a mutant plants exhibited altered root architecture, causing a reduction in primary and lateral root length, but increasing lateral root density. Taken together, our results suggest that these ARF members are common key players of the morphogenetic programs that control root development and the formation of nitrogen-fixing nodules.

Introduction

Auxins play essential roles in diverse aspects of plant growth and development, including cell elongation, cell polarity, vascular tissue differentiation, embryo patterning, apical dominance, and leaf shape (Salehin et al., 2015). Auxins also control root system architecture by inhibiting primary root growth and promoting the emergence and growth of lateral roots (Overvoorde et al., 2010). In plants belonging to the nitrogen-fixing clade, which includes the orders Fabales, Fagales, Rosales, and Cucurbitales (Doyle, 2011), these phytohormones play major roles regulating the root nodule symbiosis (Kohlen et al., 2018). Lateral roots serve for soil anchoring as well as water and nutrient acquisition, whereas nodules are the result of a symbiotic relationship with nitrogen-fixing bacteria that allow these plants to overcome nitrogen deficiencies in the soil. It has been proposed that the program of nodule organogenesis, which is activated by bacteria-derived signals known as Nodulation (Nod) factors, has co-opted the endogenous developmental program of root and lateral root development during evolution (Bishopp and Bennett, 2019; Soyano et al., 2021). Up-regulation of meristematic markers such as WUSCHEL-RELATED HOMEOBOX 5 and PLETHORA has been observed during nodule formation (Osipova et al., 2012; Franssen et al., 2015). Notably, two recent reports conducted in Lotus japonicus and Medicago truncatula provided substantial evidence that the program of lateral root formation has been recruited to contribute to nodule formation in legumes (Schiessl et al., 2019; Soyano et al., 2019). Moreover, although both organs differ in the environmental stimuli and function, their developmental programs converged in the generation and interpretation of auxin maximum (Herrbach et al., 2014; Xiao et al., 2014; Schiessl et al., 2019). In addition, it was recently shown that Nuclear Factor YA (NF-YA) genes are important regulators of auxin signaling during nodule development via the direct control of SHORT INTERNODES/STYLISH (STY) transcription factor genes and their downstream targets, YUCCA1 and YUCCA11, involved in auxin biosynthesis (Shrestha et al., 2020). This implies that auxin biosynthesis, signaling, and responses must be integrated with the nodulation program, which is initiated by the LysM domain receptor kinases MtNFP (Nod Factor Perception, Amor et al., 2003) and MtLYK3 (Smit et al., 2007) in M. truncatula and followed by the activation of a number of transcription factors such as the ERF transcription factor MtERN1 (Ethylene response factor Required for Nodulation 1) (Middleton et al., 2007) and the three subunits of the NF-Y heterotrimeric complex (Combier et al., 2006; Laporte et al., 2014; Baudin et al., 2015). Auxins also interact with the ethylene signaling pathway during root nodule symbiosis, since the ethylene-insensitive sikle (skl) mutant, which forms numerous infection threads (ITs) and nodules under symbiotic conditions (Penmetsa and Cook, 1997), also exhibited altered auxin transport during nodulation (Prayitno et al., 2006).

Auxin signaling and responses are mediated by multiple members of the Auxin Response Factor (ARF) family of transcription factors and the Aux/IAA proteins. ARF proteins, which have been classified as transcriptional activators or repressors based on sequence analysis and transient expression assays, mediate transcriptional regulation by binding the Auxin response elements (AuxRE) in the promoters of auxin-responsive genes (Ulmasov et al., 1999; Tiwari et al., 2003). At low auxin concentrations, ARF activators form heterodimers with Aux/IAA proteins, which repress auxin-responsive genes by recruiting the TOPLESS repressor. At high auxin concentration, Aux/IAA proteins are ubiquitinated by the SCF E3 ubiquitin ligase complex and targeted to degradation via the 26S proteasome, releasing ARF repression and promoting ARF-mediated transcriptional activation of auxin-responsive genes (Guilfoyle and Hagen, 2007).

Depending on the species, plant genomes contain a variable number of ARF members, e.g., 23 ARF members in Arabidopsis, 39 members in Populus trichocarpa, 25 members in Oryza sativa, 22 members in Zea mays (Finet et al., 2013), 24 members in M. truncatula, and 51 members in Glycine max (Shen et al., 2015). A comprehensive phylogenetic analysis of the ARF family in all major living division of land plants—including eudicots, monocots, gymnosperms, and bryophytes—indicated that ARF genes split into three main clades during evolution: clade A, clade B, and clade C (Finet et al., 2013). In Arabidopsis, ARF activators were clustered mainly in clade A (including AtARF5, AtARF6, AtARF7, and AtARF8), whereas most ARF repressors were divided into both clades B (including AtARF1, AtARF2, AtARF3, AtARF4, and AtARF9) and C (including AtARF10, AtARF16, and AtARF17) (Finet et al., 2013). Several members of the ARF family have been implicated in distinct steps of the formation of lateral roots. In Arabidopsis, single mutants in AtARF7 or AtARF19 showed a mild reduction in lateral root number, whereas double arf7/arf19 mutants exhibited a marked reduction in the development of lateral root primordia, suggesting that these two members of the ARF family might display a certain degree of redundancy in lateral root initiation (Okushima et al., 2005; Wilmoth et al., 2005). AtARF5 was also implicated in the development of lateral roots. Loss-of-function arf5 mutants displayed a substantial reduction in the number of emerged lateral roots but exhibited clustering of lateral root primordia, leading to the suggestion that lateral root formation is subjected to a bimodular auxin response control: a first module composed by AtARF7/AtARF19 controls lateral root initiation and a second module involving AtARF5 is required for proper organogenesis of lateral roots (De Smet et al., 2010). Genetic evidence revealed that other ARF members could function as negative regulators of lateral root development. For example, Arabidopsis arf10/arf16 double mutants produced an increased number of lateral roots (Wang et al., 2005). Interestingly, ARF10, ARF16, and ARF17 have also been involved in the development of nitrogen-fixing nodules and the infection by rhizobia in legumes. Overexpression of the microRNA160, which targets ARF10, ARF16, and ARF17 transcripts, leads to a reduction in the number of nodules in G. max and M. truncatula roots (Bustos-Sanmamed et al., 2013; Turner et al., 2013; Nizampatnam et al., 2015). In addition, three M. truncatula arf16a-Tnt1 insertional mutants exhibited a reduced number of infection events upon inoculation with its symbiotic partner Sinorhizobium meliloti (Breakspear et al., 2014).

ARF2, ARF3, and ARF4 are post-transcriptionally regulated by the action of the trans-acting small interference RNAs (tasiRNAs)—referred to as tasiARFs—derived from the evolutionarily conserved pathway involving the microRNA390 (miR390) and the trans-acting small interference RNA 3 (TAS3) transcript (Xia et al., 2017). These members of the ARF family were also implicated in lateral root development in mono- and dicotyledonous species. In Arabidopsis, arf2, arf3, and arf4 single mutant plants or plants expressing an artificial microRNA that simultaneously knock down AtARF2, AtARF3, and AtARF4 exhibited longer lateral roots and lower lateral root density (Marin et al., 2010; Yoon et al., 2010). Congruently, plants that overproduce tasiARFs—by either activation tagging or overexpression of the TAS3 gene—also produced longer lateral roots. In P. trichocarpa, overexpression of a tasiARF-resistant form of PtARF4 suppressed lateral root elongation and reduced lateral root density, whereas knockdown of PtARF4 enhances both lateral root growth and density under normal and salt stress conditions (He et al., 2018). Conversely, Lu et al. (2018) showed that overexpression of TAS3 in O. sativa, which efficiently reduced OsARF3 mRNA levels, increased the number of lateral roots. These studies indicated that, albeit species-specific differences, the miR390/TAS3 pathway and its targets ARF2, ARF3, and ARF4 play essential roles in the development of lateral roots.

In a previous work, we have shown that the miR390/TAS3 pathway also mediates the development of nitrogen-fixing nodules (Hobecker et al., 2017). Activation of this pathway by overexpression of miR390b in M. truncatula roots led to enhanced lateral root growth, but impaired nodule organogenesis and reduced infection by the nitrogen-fixing bacteria S. meliloti. Conversely, inactivation of the miR390/TAS3 pathway by either expression of a target mimic of miR390 or mutation in the gene encoding ARGONAUTE7—the argonaute protein that binds miR390—increased the density of infection events and the number of nodules and altered their spatial distribution (Hobecker et al., 2017). Thus, the miR390/TAS3 module functions as a positive modulator of lateral root development and a negative modulator of nodulation in M. truncatula. However, whether this pathway operates through their target transcripts MtARF2, MtARF3, MtARF4a, and MtARF4b and the implications of these transcription factors in the development of lateral root organs have not been investigated in legumes. Here, we used M. truncatula roots with simultaneous knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b, as well as an arf4a Tnt1 insertional mutant, to show that these members of the ARF family contribute to modulation of root architecture and the development of nitrogen-fixing nodules.

Materials and Methods

Biological Material

Wild-type (WT) M. truncatula Jemalong A17 seeds were obtained from INRA Montpellier, France¹. M. truncatula arf4a Tnt-1 insertional mutant seeds were obtained from the Noble Research Institute LLC. nfp, nf-ya1, ern1, and skl mutants were previously described (Amor et al., 2003; Middleton et al., 2007; Laporte et al., 2014; and Penmetsa and Cook, 1997, respectively). S. meliloti strain 1021 (Meade and Signer, 1977) or the same strain expressing RFP (Tian et al., 2012) were used for root inoculation as in Hobecker et al. (2017). Agrobacterium rhizogenes strain Arqua1 was used for hairy root transformations (Quandt et al., 1993).

Constructs for Plant Transformation

The pMtARF3:GUS-GFP construct was generated by amplifying the 1,958-bp region upstream of the translational initiation codon of MtARF3 using the pMtARF3 F and pMtARF3 R primers listed in Supplementary Table 1. The resulting DNA fragment was cloned into the pENTR/D-TOPO vector (Thermo Scientific) and then recombined into the Gateway-compatible binary vector pKGWFS7,0 (Karimi et al., 2002) using LR Clonase according to the manufacturer’s instructions (Thermo Scientific). The pMtARF4:GUS-GFP construct was previously generated by Hobecker et al. (2017). The ARF2/3/4a/4b RNAi construct was generated by PCR amplification of an MtARF3 fragment that contains the binding sites for tasiARFs. PCR was conducted using cDNA from M. truncatula roots as template, the MtARF2/3/4 RNAi F and MtARF2/3/4 RNAi R primers (Supplementary Table 1) and pfu DNA polymerase (Promega). The GUS RNAi construct was generated by amplification of a β-glucuronidase (GUS) fragment using the pKGWFS7,0 vector (Karimi et al., 2002) as template and GUS RNAi F and GUS RNAi R primers listed in Supplementary Table 1. The GUS RNAi and ARF2/3/4a/4b RNAi amplified fragments were cloned into the pENTR/D-TOPO (Thermo Scientific) vector and then recombined into the destination vector pK7GWIWG2D (II) (Karimi et al., 2007) to produce GUS RNAi and ARF2/3/4a/4b RNAi constructs, respectively, following manufacturer’s instructions (Thermo Fisher). The pK7GWIWG2D (II) destination vector contains the rolD:gfp gene for the detection and selection of transgenic hairy roots; therefore, only roots with detectable GFP fluorescence (more than 80% of the roots) were taken into account for expression and phenotypic analyses. All constructs were verified by sequencing. Binary vectors were introduced into A. rhizogenes Arqua1 (Quandt et al., 1993) by electroporation.

Growth of Medicago truncatula, Hairy Root Transformation, Inoculation With Rhizobia and NF Treatment

Seeds were surface sterilized and germinated on 10% (w/v) agar plates at 25°C in the dark for 24 h. Transgenic roots were generated by A. rhizogenes-mediated transformation essentially as previously described (Boisson-Dernier et al., 2001) and transferred to Petri dishes containing agar Fahraeus media (Fahraeus, 1957) supplemented with 8 mM KNO₃ and 12.5 μg/ml of kanamycin for 7 days. Seedlings were grown at 25°C in a 16/8-h day/night cycle with radiation of 200 μmol m^–2 s^–1 using mixed lighting containing four OSRAM cool daylight L36W/765 tubes per one OSRAM FLUORA L36W/77 tube. For root architecture analysis, composite plants, consisting of a non-transgenic shoot and transgenic hairy roots, were transferred to slanted boxes containing Fahraeus media supplemented with 8 mM KNO₃ and grown under the conditions described above for 15 days. For inoculation with rhizobia, plants that developed hairy roots were transferred to slanted boxes containing Fahraeus media free of nitrogen covered with sterile filter paper. Germinated seedlings of WT and the arf4a mutant were transferred to Petri dishes containing agar Fahraeus media free of nitrogen for rhizobia inoculation or to the same media supplemented with 8 mM KNO₃ and grown for 7 or 15 days for root and shoot developmental phenotypic analysis. For rhizobia inoculation, 7 days after transplantation to slanted boxes, seedlings were inoculated with 10 ml of a 1:1,000 dilution of S. meliloti 1021 (Meade and Signer, 1977) or the same strain expressing RFP culture grown in liquid TY media until OD₆₀₀ reached 0.8 or with 10 ml of water as a control (mock treatment). The excess of liquid was removed 1 h after inoculation, and seedlings were incubated vertically under the growth conditions described above. For Nod Factor treatment, WT, nfp, nf-ya1, ern1, and skl mutants were grown on slanted boxes containing Fahraeus media free of nitrogen for 7 days and then treated with 10 ml of a suspension of 10^–8 M of NFs purified from S. meliloti or with 10 ml of water as a mock-treatment.

Tissue Expression Analysis Using Promoter:Reporter Fusions

Composite plants transformed with the pMtARF3:GFP-GUS or pMtARF4a:GFP-GUS were transferred to square petri dishes (12 cm × 12 cm) containing slanted agar-Fahraeus medium. GFP fluorescence of roots was visualized with an inverted microscope (Olympus IX51) using UV light with appropriate filters for GFP. For detection of GFP and RFP fluorescence in S. meliloti inoculated roots and in nodules, confocal microscopy was performed at 5 and 9 dpi with an S. meliloti strain expressing RFP (Tian et al., 2012) using an inverted SP5 confocal microscope (Leica Microsystems). GFP and RFP were excited using 488- and 543-nm lasers, and emissions were collected from 498 to 552 nm and from 578 to 626 nm, respectively. Images were processed with the LAS Image Analysis software (Leica Microsystems).

Phenotypic Analyses

For analysis of root architecture, germinated WT and arf4a mutant seedings, as well as composite GUS RNAi and ARF2/3/4a/4b RNAi plants generated by A. rhizogenes-mediated transformation, were transferred to slanted boxes containing agar-Fahraeus medium supplemented with 8 mM KNO₃. The number of lateral roots per centimeter of primary root and the length of primary and lateral roots were determined at 7 and 15 days after germination (dag) for WT and arf4a mutant plants. The length of aerial part and the number of true leaves of WT and arf4a mutants were also determined at 7 and 15 dag. For GUS RNAi and ARF2/3/4a/4b RNAi composite plants, each root that emerged directly from the sectioned site of the non-transgenic root inoculated with A. rhizogenes was considered an independent transgenic primary root in the hairy root system. Only first-order lateral roots that emerged from each independent transgenic primary root were considered to estimate lateral root length and density. The number of lateral roots per centimeter of transgenic primary root and the length of transgenic primary and lateral roots were determined at 15 days after transplantation. For the determination of shoot dry weight, the aerial part of composite plants was dried at 80°C for 24 h and weighed using an analytical balance. Three independent biological replicates were performed. For nodulation analysis, WT, arf4a mutants, or composite plants transformed with the GUS RNAi or ARF2/3/4a/4b RNAi construct were transferred to slanted boxes containing nitrogen-free Fahraeus medium and inoculated with S. meliloti 1021 7 days after transplantation. The number of nodules was recorded at different time points after inoculation with S. meliloti as previously described (Hobecker et al., 2017). Nodules were classified as pink (nitrogen-fixing mature nodules) or white (immature nodules) according to Traubenik et al. (2020). Only roots containing nodules were considered for the quantification and classification of pink and white nodules. Shoot dry weight and shoot length were determined at 21 dpi with S. meliloti. Three independent biological replicates were performed. For analysis of infection events, GUS and ARF2/3/4a/4b RNAi plants of 14 days after transformation or WT and arf4a plants of 14 dag were transferred to petri dishes containing agar-Fahraeus medium free of nitrogen. Seven days after transplantation, roots were inoculated with the S. meliloti strain expressing RFP (Tian et al., 2012) and grown as described above. Infection events were visualized, quantified, and classified at 7 dpi in an Olympus IX51 inverted microscope. Infection events were classified as microcolonies, ITs that end in the root hair, ITs that reached the base of the epidermal root hair, or ITs that reached and ramified in the cortical cells. Three independent biological replicates were performed. In all cases, statistical significance of the differences for each parameter was determined by unpaired two-tailed Student’s t tests for each construct or for the WT vs. the arf4a mutant line.

RNA Extraction, RT-PCR, and RT-qPCR

Total RNA extraction was performed with Trizol according to the manufacturer’s instructions (Thermo Fisher). RNA concentration was determined by measuring OD₂₆₀ using a Nanodrop ND-1000 (Nanodrop Technologies) and RNA integrity was evaluated by electrophoresis 1.2% (w/v) agarose gels stained with ethidium bromide. Total RNA was treated with DNase I according to the manufacturer’s instructions (Promega) and subjected to first-strand cDNA synthesis using M-MLV reverse transcriptase (Promega). Expression analysis was performed by RT-qPCR using the iQ SBR Green Supermix kit (BioRad) and the CFX96 qPCR system (BioRad) as previously described (Blanco et al., 2009). For each pair of primers, the presence of a unique product of the expected size was verified on 1.2% (w/v) agarose gels stained with ethidium bromide. In all cases, negative controls without template or without RT were included. Expression values were normalized to MtHIS3L, which has been validated by GNORM software (Vandesompele et al., 2002), as reported previously by Ariel et al. (2010) and Reynoso et al. (2013). Primers used for RT-qPCR are listed in Supplementary Table 1. For detection of MtARF4a mRNAs by semiquantitative RT-PCR on WT and the arf4a mutant roots, a pair of primers specific for MtARF4a (MtARF4a F and MtARF4a R) were used, which are listed in Supplementary Table 1.

Sequence Alignment and Phylogenetic Analysis

All members of the Arabidopsis ARF family were retrieved from the TAIR database². M. truncatula ARF members were retrieved from the recently released version of the M. truncatula genome MtrunA17r5.0-ANR³ (Pecrix et al., 2018). Amino acid and nucleotide alignments were generated with the Clustal Omega algorithm available at EMBL-EBI⁴ and decorated with BOXSHADE⁵. The phylogenetic tree was generated with MEGA X (Kumar et al., 2018) using the Neighbor-Joining method (Saitou and Nei, 1987). The percentage of replicate trees in which the associated taxa clustered together in the bootstrap test (10,000 replicates) was computed as described by Felsenstein (1985). The evolutionary distances were computed using the p-distance method (Nei and Kumar, 2000).

Accession Numbers

Sequence data from this article can be found at the M. truncatula genome Mt4.0v1 or MtrunA17r5.0-ANR databases under the following accession numbers, respectively: MtARF2 (Medtr8g100050 or MtrunA17_Chr8g0385791), MtARF3 (Medtr2g014770 or MtrunA17_Chr2g0282961), MtARF4a (Medtr4g060460 or MtrunA17_Chr4g0029671), MtARF4b (Medtr2g093740 or MtrunA17_Chr2g0326281), MtARF16a (Medtr1g094960 or MtrunA17_Chr1g0199681), MtARF19a (Medtr2g018690 or MtrunA17_Chr2g0301251), MtNSP1 (Medtr8g020840 or MtrunA17_Chr8g0344101), MtNSP2 (Medtr3g072710 or MtrunA17_Chr3g0114841), MtNIN (Medtr5g099060 or MtrunA17_Chr5g0448621), MtERN1 (Medtr7g085810 or MtrunA17_Chr7g0253424), MtNF-YA1 (MtrunA17_Chr1g0148951), MtENOD40 (MtrunA17_Chr8g0368441), MtNFP (MtrunA17_Chr5g0403371), and MtSKL (MtrunA17_Chr5g0427621).

Results

MtARF3 and MtARF4a Are Expressed During Lateral Root Development, but Only ARF4a Is Transcribed During the Root Nodule Symbiosis

Considering that expression of the MIR390 promoter was associated with the development of lateral roots and nodules, we aimed to characterize the spatial and temporal expression pattern of the targets of the miR390/TAS3 pathway during the development of both types of lateral organs. Previous phylogenetic analysis of the ARF family using ESTs or the Mt3.5 version of the M. truncatula genome identified single genes as putative orthologs of Arabidopsis AtARF2 and AtARF3, referred to as MtARF2 and MtARF3, respectively, and two genes evolutionarily closer to Arabidopsis AtARF4, designated as MtARF4a and MtARF4b (Zhou et al., 2013; Shen et al., 2015). Proteins encoded by MtARF4a and MtARF4b exhibited 75% of identity to each other (Supplementary Figure 1). Here, we generated a phylogenetic tree that includes all members of the Arabidopsis ARF family, and MtARF2, MtARF3, MtARF4a, and MtARF4b. In addition, the tree includes M. truncatula ARF members that have been involved in root development and nodulation in this legume, i.e., MtARF10, MtARF16, and MtARF17 (Bustos-Sanmamed et al., 2013; Breakspear et al., 2014), as well as best M. truncatula homologs of ARF members implicated in these processes in other plant species, such as AtARF5, AtARF7, and AtARF19 in lateral root development (Okushima et al., 2005; Wilmoth et al., 2005; De Smet et al., 2010) and GmARF6 and GmARF8 in nodulation (Wang et al., 2015). The amino acid sequences of M. truncatula ARF members were retrieved from the recently released version of the M. truncatula genome MtrunA17r5.0-ANR (Pecrix et al., 2018). This phylogenetic analysis verified that MtARF2, MtARF3, MtARF4a, and MtARF4b clustered in the same clades as their Arabidopsis counterparts (Supplementary Figure 2). Inspection of public RNA-sequencing data reported by Schiessl et al. (2019) indicated that MtARF4a increased at 5 days after spot-inoculation with droplets of a S. meliloti suspension, whereas MtARF4b decreased at all time points after inoculation (Supplementary Figure 3). On the other hand, MtARF3 transcript levels significantly increased in fully emerged lateral roots (72 h after induction of lateral root formation) but decreased at 7 days after spot-inoculation with rhizobia, whereas ARF2 levels did not increase neither during lateral root development nor after spot-inoculation with rhizobia (Supplementary Figure 3). To better characterize the spatial expression pattern of ARF genes during lateral root and nodule formation promoter:GUS-GFP transcriptional fusions were generated for MtARF3 and MtARF4a (pMtARF3:GFP-GUS and pMtARF4:GFP-GUS, respectively). Despite several attempts using different combinations of primers based on either the M. truncatula genome v4.0 or v5.0, we were unable to amplify a promoter region of ARF2. Introduction of pMtARF3:GFP-GUS and pMtARF4a:GFP-GUS constructs into M. truncatula hairy roots revealed that both promoters were active in the vascular tissue of the primary roots, as well as in the vasculature and the meristematic region of lateral roots. pMtARF3 and pMtARF4a expression was also detected in lateral root primordia prior to emergence and in emerged lateral roots (Figure 1). To evaluate the expression of pARF3 and pARF4 during symbiosis, hairy roots harboring pMtARF3:GFP-GUS or pMtARF4a:GFP-GUS were inoculated with a S. meliloti strain that expresses the red fluorescent protein (RFP) (Tian et al., 2012). This strain allows visualizing the root hairs that contain an IT, i.e., the tubular structure that allows the bacteria to cross the epidermis and reach the dividing cells of the nodule primordia, as well as infected cells of the nodule. Upon rhizobia inoculation, GFP fluorescence was not detected in the infected root hair or in the adjacent epidermal cells at 5 dpi, or in the infected or non-infected cells of developing nodules of 9 dpi when roots were transformed with the pMtARF3:GFP-GUS construct (Figure 2). On the other hand, expression of GFP driven by pMtARF4a promoter was found in the root hair containing elongating ITs and in the epidermal cells surrounding the infected root hair at 5 dpi, as well as in the non-infected cells that surround infected cells of nodules of 9 dpi (Figure 2), in agreement with previous results (Hobecker et al., 2017). Thus, the promoter reporter analysis presented here revealed that the activity of both pMtARF3 and pMtARF4a is associated with lateral root development. However, only pMtARF4a seems to be responsive to rhizobial infection and active in developing nodules, consistently with the mRNA expression pattern described in spot-inoculation experiments (Schiessl et al., 2019).

FIGURE 1

Figure 1. Promoter:reporter fusion expression analysis of MtARF3 and MtARF4a in primary and lateral roots. Expression of the GFP reporter gene in roots transformed with the pMtARF3:GUS-GFP (upper panels) or the pMtARF4a:GUS-GFP (bottom panels) construct was detected in the vasculature of the primary root (PR) and lateral root (LR), in lateral root primordia (LRP) prior to emergence and in emerged lateral roots (ELR). Bars = 50 μm.

FIGURE 2

Figure 2. Promoter:reporter fusion expression analysis of MtARF3 and MtARF4a at different stages of the symbiotic interaction with S. meliloti. GFP fluorescence was analyzed in roots transformed with the pMtARF3:GUS-GFP (upper panels) or the pMtARF4a:GUS-GFP (bottom panels) construct at 5 days post-inoculation (dpi) and in developing nodules at 9 dpi with a strain of S. meliloti that expressed the red fluorescent protein (RFP). Dashed lines mark the epidermal cells of roots and nodules. Dotted lines separate different nodule zones. ZI, meristematic zone; ZII, infection zone; ZIII, fixation zone; IT, infection thread. Bars = 50 μm.

Up-Regulation of MtARF2, MtARF3, and MtARF4a/b mRNAs Depends on the Nod Factor Signaling Pathway

Previously, we have shown that mRNA levels of MtARF2, MtARF4a/b, and, to a lesser extent, MtARF3 increased in M. truncatula roots upon inoculation with S. meliloti (Reynoso et al., 2013; Hobecker et al., 2017). Here, we investigated whether the Nod Factors (NFs) and their signaling pathway were responsible for up-regulation of this set of ARFs during symbiosis. Roots of WT plants were treated with purified NFs from S. meliloti for 48 h. Reverse transcription quantitative PCR (RT-qPCR) analysis revealed that these ARFs were extensively up-regulated by NFs; MtARF2 and MtARF4a/b mRNA levels increased by more than 25-fold in NF-treated roots as compared to mock-inoculated WT roots, whereas the increase was 12-fold for MtARF3 transcripts (Figure 3). Interestingly, mRNA levels of none of these ARFs were significantly up-regulated upon NF treatment in the nfp mutant, a loss-of-function mutant in the MtNFP gene involved in NF reception (Amor et al., 2003), albeit levels of MtARF2 and MtARF3 were slightly higher in this mutant than in WT under mock inoculation conditions. In addition, up-regulation of MtARF2 and MtARF3 or MtARF4a/b in response to NFs was partially or completely impaired, respectively, in mutants of the transcription factor MtNF-YA1. Up-regulation of MtARF2 and MtARF3 mRNA levels was not impaired in ern-1 and skl mutants (Figures 3A,B). Moreover, MtARF2 mRNA levels increased to a higher extent in skl mutants as compared to WT plants, which might be consistent with the enhanced auxin transport observed in skl (Prayitno et al., 2006). On the other hand, up-regulation of MtARF4a/b in response to NFs was partially impaired in ern1 and unaffected in skl mutants (Figure 3C). Altogether, these results suggest that induction of these ARFs, notably of MtARF4a/b, depends on NF perception and requires the function of the MtNF-YA1 transcription factor.

FIGURE 3

Figure 3. MtARF2, MtARF3, and MtARF4a/b are up-regulated by Nod Factors and depends on MtNFP and MtNF-YA1 genes. Transcript levels of MtARF2 (A), MtARF3 (B), and MtARF4a/b (C) were analyzed in root tissue of WT and nfp, nf-ya1, ern1, and skl mutant plants treated with 10^–8 M purified Nod Factors (NFs, blue bars) or water (mock, white bars) for 48 h. Expression levels were determined by RT-qPCR and normalized to the levels of the MtHIS3L transcript. Values are expressed relative to the WT mock-treated sample, which was set at 1. Different letters above the bars indicate statistically significant differences between samples in an unpaired two-tailed Student’s t test with a p value ≤ 0.05.

Knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b and Mutation of MtARF4a Reduce Nodulation and Infection by Rhizobia

To elucidate whether these three ARF members play a role in the control of nodule formation and/or rhizobial infection in M. truncatula, we applied an RNA interference (RNAi) strategy to simultaneously knock down MtARF2, MtARF3, MtARF4a, and MtARF4b. The fragment used for RNAi was designed in an mRNA region highly conserved across MtARF2, MtARF3, MtARF4a, and MtARF4b that includes the tasiARFs target sites (Supplementary Figure 4). Introduction of the ARF2/3/4a/4b RNAi construct in M. truncatula hairy roots reduced by 80, 70, and more than 90% MtARF2, MtARF3, and MtARF4a/b mRNA levels, respectively, relative to the levels of GUS RNAi roots used as the control (Figure 4A). However, this RNAi construct did not decrease levels of MtARF16a or MtARF19a (Supplementary Figure 5), evidencing the specificity of the RNAi approach. Reductions of MtARF2, MtARF3, MtARF4a, and MtARF4b transcript levels significantly impacted nodulation, reducing the number of nodulated plants, as well as the number of nodules formed over the time in hairy roots (Table 1 and Figure 4B). These differences were observed as early as 7 dpi, with a 70% reduction in the number of nodules formed in ARF2/3/4a/4b RNAi as compared with GUS RNAi plants, but continued over the time course of the experiment, with nearly a 50% reduction in the number of nodules at 21 dpi. However, the percentage of nodules that acquired the characteristic pink color caused by expression of leghemoglobin upon the onset of nitrogen fixation was not affected by knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b (Figure 4C). These results suggest that silencing of these ARFs negatively affects nodule formation, but once formed, these nodules develop the nitrogen fixation zone characteristic of indeterminate nodules. To evaluate whether infection by rhizobia was affected by knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b, the number of infection events and their progression were evaluated in hairy roots inoculated with the RFP-expressing S. meliloti strain. Knockdown of MtARF2, MtARF3, and MtARF4a/b caused a significant reduction in the total density of infection events, i.e., the number of infection events per centimeter of root (Figure 4D). A more notable effect was observed in the progression of the infection events, with 58% of the infection events remaining at the microcolony stage and only 10% of the ITs reaching the dividing cortical cells in ARF2/3/4a/4b RNAi roots, whereas over 50% of the infection events reached the base of the epidermal cells or reached the cortex in GUS RNAi roots (Figure 4E). Thus, these results indicate that simultaneous silencing of MtARF2, MtARF3, MtARF4a, and MtARF4b interferes not only with the initiation of infection events but also with their progression to the dividing cortical cell beneath the infection site. In addition, ARF2/3/4a/4b RNAi composite plants grown in the absence of nitrogen exhibited reduced shoot length and shoot dry weight as compared to GUS RNAi at 21 dpi with S. meliloti (Figures 4F,G, respectively), presumably because of poor nodulation and impaired infection that compromises nitrogen fixation.

FIGURE 4

Figure 4. Simultaneous knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b impaired nodule formation and infection by rhizobia. (A) Expression levels of MtARF2, MtARF3, and MtARF4a/b transcripts in GUS RNAi and ARF2/3/4a/4b RNAi roots. Expression values were determined by RT-qPCR, normalized to MtHIS3L, and expressed relative to the GUS RNAi sample, which was set at 1. Each bar represents the mean ± SE of three biological replicates (whole root tissue from at least three composite plants were collected in each biological replicate) with three technical replicates each. Asterisks indicate statistically significant differences between GUS and ARF2/3/4a/4b RNAi roots in an unpaired two-tailed Student’s t test (^∗p ≤ 0.05, ^∗∗p ≤ 0.01). (B) Time-course nodule formation in GUS and ARF2/3/4a/4b RNAi roots upon inoculation with S. meliloti. Error bars represent mean ± SE of three independent biological replicates, each with at least 50 roots. Four asterisks indicate statistically significant differences between GUS and ARF2/3/4a/4b RNAi roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001. (C) Percentage of pink and white nodules developed in GUS RNAi and ARF2/3/4a/4b RNAi roots at 21 dpi. Bars represent the mean ± SE of three independent biological replicates. More than 68 nodules from more than 15 independent plants per construct were quantified in each biological replicate. (D) Density of infection events in GUS and ARF2/3/4a/4b RNAi roots at 7dpi with a S. meliloti strain expressing the RFP protein. Each bar represents the mean ± SE of three biological replicates, each with more than 25 transgenic roots. The asterisks indicate statistically significant differences between GUS and ARF2/3/4a/4b RNAi roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.01. (E) Progression of infection events in GUS and ARF2/3/4a/4b RNAi roots. Infection events were classified as microcolonies, infection threads (ITs) that end in the root hair, in the epidermal cell layer, or reach the cortex at 7 dpi. Each category is presented as the percentage of total infection events. Data are representative of three independent biological replicates, each with more than 25 transgenic roots. The asterisk indicates that the percentage of microcolonies and ITs that end in cortex was significant different between GUS and ARF2/3/4a/4b RNAi roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.05. (F,G) Shoot length (F) and shoot dry weight (G) measured in GUS and ARF2/3/4a/4b RNAi composite plants grown on free-nitrogen slanted agar-Fahraeus at 21 dpi with S. meliloti_. Error bars represent the mean ± SE of three biological replicates, each performed with more than 10 composite plants. Asterisks denote a statistically significant difference between GUS and ARF2/3/4a/4b RNAi composite plants in an unpaired two-tailed Student’s t test (^∗p ≤ 0.05, ^****p ≤ 0.0001).

TABLE 1

Table 1. Number and percentage of plants with nodules.

Since the MtARF4a promoter was active during bacterial infection and nodule formation and up-regulation of ARF4a/b was completely impaired in nfp and nf-ya1 mutants, we analyzed the symbiotic phenotype caused by a mutation in the MtARF4a gene. A mutant carrying the Tnt1 insertion within the first exon of the MtARF4a gene (arf4a) was obtained by screening the collection available at Noble Research Institute LLC (Tadege et al., 2008; Cheng et al., 2014). Semiquantitative RT-PCR analysis revealed that levels of MtARF4a mRNAs were undetectable in arf4a mutants, whereas WT plants accumulated noticeable levels of MtARF4a transcripts (Figure 5A). Upon inoculation with rhizobia, the arf4a mutant developed a significantly lower number of nodules as compared with WT plants (Figure 5B). In agreement with what was observed in ARF2/3/4a/4b RNAi roots, roots of arf4a mutants exhibited a significant reduction in the density of the infection events (Figure 5C) as well as in their progression. In the arf4a mutants, 45% of the infection events remained at the microcolony stage and only 20% reached the root cortex, whereas in WT roots, nearly 55% of the infection events reached the cortical cells (Figure 5D). Reduced nodule formation and bacterial infection also impacted the development of the aerial part of the arf4a plants grown in the absence of nitrogen, which exhibited reduced shoot length and dry weight as compared with WT plants under symbiotic conditions (Figures 5E,F).

FIGURE 5

Figure 5. A Tnt1 insertional mutant in MtARFa gene (arf4a) exhibited reduced nodulation and infection by rhizobia. (A) Schematic representation of MtARF4a gene model and the insertion of the Tnt1 transposon (upper panel). The gene model is composed of 12 exons (gray blocks) and 11 introns (lines). The position of the Tnt1 insertion within the first exon in the NF17411 mutant line is indicated in base pairs (bp) with a black arrow. Black arrowheads indicate the position of MtARF4a F and MtARF4a R primers specific for ARF4a (listed in Supplementary Table 1) used for RT-PCR analysis. Expression levels of MtARF4a and MtHIS3L were determined by semiquantitative RT-PCR using 35 and 25 cycles, respectively, on WT and NF17411 (arf4a) roots at 48 hpi with S. meliloti (Sm) or water (mock) (lower panel). (B) Time-course nodule formation in roots of WT and arf4a plants upon inoculation with S. meliloti. Error bars represent the mean ± SE of three biological replicates, each performed with at least ten plants. Four asterisks indicate statistically significant differences between WT and arf4a mutant roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001. (C) Density of infection events developed at 7 dpi in WT and arf4a mutant roots. Error bars represent the mean ± SE of three biological replicates each performed with at least 10 plants. Four asterisks indicate statistically significant differences between WT and arf4a mutant roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001. (D) Progression of infection events in WT and arf4a mutant roots. Infection events were classified as microcolonies or ITs that end in the root hair, in the epidermal cell layer, or reach the cortex at 7 dpi. Each category is presented as the percentage of total infection events. Results are representative of three biological replicates, each with more than 10 plants. The asterisk indicates that the percentage of microcolonies and ITs that end in cortex was significantly different in an unpaired two-tailed Student’s t test between WT and arf4a roots with p ≤ 0.05. (E,F) Shoot length (E) and shoot dry weight (F) measured in WT and arf4a mutant plants grown on free-nitrogen slanted agar-Fahraeus at 21 dpi with S. meliloti_. Error bars represent the mean ± SE of three biological replicates, each performed with more than 10 plants. Four asterisks denote a statistically significant difference between WT and arf4a plants in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001.

Knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b Impairs Expression of Nodulation Signaling Pathway 2

Since silencing of MtARF2, MtARF3, MtARF4a, and MtARF4b or mutations in MtARF4a affected nodule formation and bacterial infection, we tested whether the expression of key genes of the nodulation signaling pathway is affected in plants with reduced levels of MtARF2, MtARF3, and MtARF4a/b transcripts (Figure 6). Transcript levels of the A and C subunits of the heterotrimeric transcription factor NF-Y accumulated to significantly higher levels in response to S. meliloti (>60- and >100-fold induction for MtNF-YA1 and MtNF-YC1, respectively) with no significant differences between ARF2/3/4a/4b RNAi and GUS RNAi roots. A similar scenario was found for transcripts of MtERN1, which accumulated more than 10-fold upon inoculation with S. meliloti as compared to mock in both ARF2/3/4a/4b RNAi and GUS RNAi roots. However, mRNA levels of the GRAS transcription factor nodulation signaling pathway 2 (MtNSP2) accumulated to a significantly lower extent in ARF2/3/4a/4b RNAi roots than in GUS RNAi roots after inoculation with S. meliloti, indicating that MtARF2, MtARF3, MtARF4a, and/or MtARF4b transcription factors might be required for full activation of MtNSP2, in agreement with that previously reported by Hobecker et al. (2017).

FIGURE 6

Figure 6. Simultaneous knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b interfered with up-regulation of NSP2 by rhizobia inoculation. Transcript levels of early nodulation markers MtNF-YA1, MtNF-YC1, MtERN1, and MtNSP2 in GUS and ARF2/3/4a/4b RNAi roots at 48 h post-inoculation (hpi) with S. meliloti (Sm, blue bars) or water (mock, white bars) were determined by RT-qPCR, normalized to MtHIS3L, and expressed relative to the GUS RNAi mock sample. Different letters indicate statistically significant differences in an unpaired two-tailed Student’s t test with a p value ≤ 0.05.

Knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b and Mutations in MtARF4a Alter Root Architecture

Recent studies have evidenced that genes required for lateral root development were co-opted for the nodulation program in legume plants, including those involved in auxin biosynthesis, signaling, and responses (Schiessl et al., 2019; Soyano et al., 2019). Thus, we investigated whether MtARF2, MtARF3, and MtARF4a/b members play a role in the control of root development in M. truncatula by analyzing the architecture of roots with reduced levels of MtARF2, MtARF3, and MtARF4a/b transcripts. Root architecture of ARF2/3/4a/4b RNAi roots was severely affected when plants were grown for 15 days under nitrogen availability. ARF2/3/4a/4b RNAi caused a significant reduction in the length of primary and lateral root but enhanced by more than twofold the lateral root density—i.e., the number of lateral roots per primary root centimeter—as compared with control GUS RNAi roots (Figures 7A–D). In addition, the dry weight of the shoot was reduced in these plants, most likely because of the limited growth of primary and lateral roots (Figure 7E). In accordance, arf4a mutants also exhibited a pronounced and significant reduction in primary and lateral root length as well as a significant increase in lateral root density as compared with WT plants at 7 and 15 dag when grown in the presence of nitrogen (Figures 8A–C and Supplementary Figures 6A–C, respectively). This indicates that MtARF4a might act as a modulator that promotes the elongation of primary and lateral roots but limits the formation of new lateral root in M. truncatula. On the other hand, arf4a mutant plants exhibited a pleiotropic phenotype in the aerial part (Figure 8D), with a significant reduction in shoot length (Figure 8E and Supplementary Figure 6D) and the number of true leaves (Figure 8F and Supplementary Figure 6E). Moreover, in plants of 15 dag, the shape and organ separation of the trifoliate leaves was also affected in arf4a mutants, with leaflets closer to each other as compared with WT plants (Supplementary Figure 6F). These results indicate that mutation in MtARF4a not only altered the root architecture, but also the shoot development in M. truncatula. Altered compound leaf patterning was previously observed in M. truncatula ago7 mutants, which exhibited reduced levels of MtARF2, MtARF3, and MtARF4a/b (Zhou et al., 2013), as well as in plants that overexpresses MtARF3 (Peng et al., 2017). Based on the results presented here, MtARF4a might have a direct role in shoot development, or alternatively, the shoot developmental defects observed in arf4a mutant plants might be the consequence of the altered growth of primary and lateral roots.

FIGURE 7

Figure 7. Knockdown of MtARF2, MtARF3, MtARF4a, and MtARF4b altered root architecture. (A–C) Length of independent primary transgenic roots (A) and lateral root (B) and density of lateral roots (C) were measured in GUS and ARF2/3/4a/b RNAi roots at 15 days after transplantation to square petri dishes slanted agar-Fahraeus medium supplemented with 8 mM KNO₃. Error bars represent mean ± SE of three independent biological replicates with more than 20 roots in each experiment. Four asterisks indicate statistically significant differences between GUS RNAi and ARF2/3/4a/4b RNAi roots in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001. (D) Image of GUS and ARF2/3/4a/4b RNAi composite plants illustrating the shorter primary and lateral roots observed in ARF2/3/4a/4b RNAi roots. Each root that emerged directly from the sectioned site of the non-transgenic roots inoculated with A. rhizogenes was considered independent transgenic primary root (PR), whereas first-order roots that emerged from each independent transgenic primary root were considered lateral roots (LRs) in the hairy root system. Scale bar: 1 cm. (E) Shoot dry weight measured in GUS and ARF2/3/4a/4b RNAi composite plants at 15 days after transplantation to square petri dishes slanted agar-Fahraeus medium supplemented with 8 mM KNO₃. Error bars represent mean ± SE of three independent biological replicates with more than 10 composite plants in each experiment. Four asterisks indicate statistically significant differences between GUS and ARF2/3/4a/4b RNAi composite plants in an unpaired two-tailed Student’s t test with a p value ≤ 0.0001.

FIGURE 8

Figure 8. The arf4a mutant exhibited altered root and shoot development. (A–C) Primary root length (A), lateral root length (B), and lateral root density (C) were measured in WT and arf4a mutant plants at 7 days after germination (dag). Plants were grown on slanted agar-Fahraeus medium supplemented with 8 mM KNO_3. Error bars represent mean ± SE of three biological replicates, each with at least 10 plants. Asterisks denote statistically significant differences between WT and arf4a plants in an unpaired two-tailed Student’s t test (^∗∗p ≤ 0.01, ^∗∗∗p ≤ 0.001, and ^****p ≤ 0.0001). (D) Image of WT and arf4a mutant plants at 7 dag illustrating the shorter primary and lateral roots observed in arf4a mutant roots. Scale bar: 1 cm. (E,F) Shoot length (E) and number of true leaves (F) measured in WT and arf4a mutant at 7 dag. Plants were grown on slanted agar-Fahraeus medium supplemented with 8 mM KNO₃. Error bars represent mean ± SE of three biological replicates, each with at least 10 plants. Three asterisks denote a statistically significant difference between WT and arf4a plants in an unpaired two-tailed Student’s t with a p value ≤ 0.001.

Discussion

ARF-Mediated Control of Nodule Organogenesis and Root Architecture

Auxin biosynthesis, signaling, and response are crucial for the developmental programs that control root architecture and the formation of symbiotic nodules (Overvoorde et al., 2010; Lin et al., 2020). Different lines of evidence revealed that there are extensive overlaps in the signaling components and developmental processes that lead to the formation of both types of organs, including those activated by auxin; however, there are also remarkable differences (reviewed by Kohlen et al., 2018). Different ARF members modulate root architecture in legume and non-legume species, some of which promote root development, while others exert inhibitory effects in root development. Here, we found that M. truncatula roots with reduced levels of MtARF2, MtARF3, MtARF4a, and MtARF4b or an arf4a single mutant exhibited shorter primary and lateral roots but enhanced lateral root density (Figures 7, 8), suggesting that these ARFs might function in promoting primary and lateral root growth and inhibiting the inception of lateral roots. We have previously shown that reduction of MtARF2, MtARF3, MtARF4a, and MtARF4b levels produced by overexpression of miR390 promotes elongation of lateral roots without affecting primary root length or lateral root density (Hobecker et al., 2017). This suggests either that miR390 mediates lateral root growth by acting through a pathway that is independent of MtARF2, MtARF3, MtARF4a, and MtARF4b or that the drastic reduction in the three ARF transcript levels caused by RNAi (70–90% depending on the ARF mRNA) or null levels of MtARF4a results in a distinct and more severe root phenotype than activation of the miR390/TAS3 pathway by overexpression of miR390, which reduced ARF mRNA levels by only 50–80%. The phenotype observed here in M. truncatula contrasts with that previously described by Marin et al. (2010) in Arabidopsis, where the authors showed that plants expressing an artificial miRNA that simultaneously knock down the three ARFs (aMIR-ARFs) exhibited longer lateral roots. In addition, individual arf2, arf3, and arf4 Arabidopsis mutants showed a mild enhancement in primary and lateral root length as compared to WT plants, whereas arf3 and arf4 mutants had reduced lateral root density (Marin et al., 2010). On the other hand, expression of an RNAi that targets PtARF4 in P. trichocarpa increased both lateral root length and density under normal or salt stress conditions (He et al., 2018), whereas overexpression of OsTAS3 in O. sativa, which results in a reduction in ARF levels, yielded denser lateral roots (Lu et al., 2018). Thus, it seems that distinct plant species respond with different alteration of root architecture to the reduction or loss of ARF2, ARF3, and/or ARF4. These species-specific determination mechanisms have been previously observed in leaf development, where alteration in the production of tasiARFs results in highly variable phenotypic response depending on the species such as wiry leaves in tomato (Yifhar et al., 2012), cylindrical leaves in O. sativa (Douglas et al., 2010), reduced number of leaflets in L. japonicus (Yan et al., 2010), and lobed leaf margin and widely spaced lateral shoot organs in M. truncatula (Zhou et al., 2013). Species-specific phenotypic variation in root architecture has also been observed in response to the lack or reduction of ARF10/16/17 levels. In Arabidopsis, an arf10/arf16 double mutant or a miR160-overexpressing line exhibited more lateral roots and reduced primary root growth (Mallory et al., 2005; Wang et al., 2005), whereas reduction of MtARF10/16/17 levels by overexpression of miR160 in M. truncatula did not alter lateral root formation or elongation but instead affected primary root growth by altering the organization of the root apical meristem (Bustos-Sanmamed et al., 2013).

In the root nodule symbiosis, members of the ARF family exert either positive or negative roles on nodule number and rhizobial infection. GmARF8a and GmARF8b function as negative regulators of nodule formation in G. max (Wang et al., 2015). On the other hand, GmARF10, GmARF16, and GmARF17, which are post-transcriptionally repressed by miR160, acts as positive regulators of nodule formation in both determinate and indeterminate nodule-forming species G. max (Turner et al., 2013; Nizampatnam et al., 2015) and M. truncatula (Bustos-Sanmamed et al., 2013), respectively. Here, we showed that the MtARF2, MtARF3, MtARF4a, and MtARF4b members of the B clade of the ARF family are required for proper nodule formation and development in M. truncatula (Table 1 and Figures 4B,C). This indicates that in addition to members of the C clade, such as MtARF10, MtARF16, and MtARF17, MtARF2, MtARF3, and MtARF4 can act as positive regulators of indeterminate nodule formation. These results are in agreement with those previously obtained by overexpression of miR390 in M. truncatula (Hobecker et al., 2017). Although our RNAi strategy effectively silenced MtARF2, MtARF3, and MtARF4a/b, expression data indicated that MtARF4a was the main ARF transcriptionally activated by rhizobia among these three ARF members (Figure 2 and Supplementary Figure 3). Unfortunately, the high similarity of nucleotide sequences of MtARF2, MtARF3, MtARF4a, and MtARF4b transcripts made it unfeasible to design RNAi constructs specific for each member, preventing us to dissect the individual contribution of MtARF2, MtARF3, and MtARF4b to the root architecture and nodulation phenotype. However, the single arf4a mutant showed a very similar nodulation phenotype than that observed by simultaneous silencing of ARF2/3/4a/4b (Figures 4B, 5B), suggesting that MtARF4a has a preponderant function in nodule formation. This reduction in nodule number observed in ARF2/3/4a/4b RNAi roots or in the arf4a mutant might be due to a decrease in auxin signaling and response, which is also correlated with the reactivation of cell divisions in the root cortex that promote nodule organogenesis (Kohlen et al., 2018). Intriguingly, it has been suggested that LjARF2, LjARF3, and LjARF4 can potentially act as negative regulators of nodulation in L. japonicus, since their expression is enhanced in reduced leaflet3/argonaute7 (rel3/ago7) mutants, which are impaired in nodule formation (Li et al., 2014). If this is the case, the contrasting results found in L. japonicus (Li et al., 2014) and M. truncatula (Hobecker et al., 2017 and this study) suggest that the role of these ARFs in nodulation might be also subjected to species-specific determinant mechanisms. Further analysis in other legume species will certainly help to elucidate whether the mode of action of these ARFs is different in determinate and indeterminate nodule-forming species.

As for other ARF genes involved in both lateral root architecture and nodule formation (e.g., ARF8 and ARF10/16/17), the possibility that the symbiotic phenotype observed in arf4a mutants might be a consequence of alteration in root architecture and/or shoot development cannot be excluded. However, the nodulation phenotype of arf4a mutants—with over 70% reduction in nodule number as compared to WT (Figure 5B)—was more severe than the root architecture phenotype, where lateral root length was reduced by 20% but the number of lateral roots increased by 35% as compared to WT (Figure 8). Considering that nodules formed mainly in lateral roots, the total lateral root system for nodule formation is not drastically altered in arf4a mutants; thus, it seems unlikely that root architecture was the cause of the symbiotic phenotype. Remarkably, infection by rhizobia, which can be genetically separated from nodule organogenesis (Oldroyd et al., 2011), was also severely impaired in arf4a mutants (Figures 5C,D), supporting a role for MtARF4a in the root nodule symbiosis.

ARFs and Their Role in Rhizobial Infection

Infection by rhizobia can be arrested either at the initiation stage or during the progression of the infection events toward the dividing cortical cells that will form the nodule primordium. Here, we found that silencing of MtARF2, MtARF3, MtARF4a, and MtARF4b or mutation of MtARF4a in M. truncatula, resulted in a moderate reduction in the density of infection events, but a severe impairment of the progression of these events to root cortex (Figures 4D,E, 5C,D). The infection phenotype observed here using an RNAi strategy or the arf4a mutant was more pronounced than that observed by Hobecker et al. (2017), since overexpression of miR390 reduced the density of infection events but not their progression. This might be explained considering that the RNAi is more effective in reducing ARF transcript levels than overexpression of miR390 (70–90 vs. 50–80% depending on the ARF). Previously, Breakspear et al. (2014) have shown that mutations in MtARF16a also affected infection by rhizobia in M. truncatula, mostly caused by a decrease in the formation of pockets containing microcolonies and elongating ITs. Thus, MtARF16 seems to be required for the initiation of infection rather than for elongation and ramification of ITs. Our results indicate that MtARF4a participate not only in the initiation but also in the elongation and ramification of ITs, since the majority of infection events were arrested at the microcolony stage and only a minor proportion of the ITs reached the dividing cortex (Figure 5D). A recent study in L. japonicus using a DR5:GUS reporter or a LjDII auxin sensor—consisting of the DII domain of Arabidopsis AtIAA28 and nuclear−localized triple YFP—has demonstrated that auxins accumulate specifically in rhizobium-infected root hairs and, moreover, that this accumulation is dependent on the NF signaling (Nadzieja et al., 2018). In addition, the same study revealed that components of the auxin biosynthetic pathway are up-regulated specifically in the rhizobia infected root hairs. In M. truncatula, inoculation with S. meliloti induced DR5:GUS reporter in both infected and uninfected root hairs over the entire infection zone and up-regulated a number of genes involved in auxin signaling and response such as MtGH3, MtSAUR1, and MtARF16a (Breakspear et al., 2014). The promoter:GFP analysis presented here has shown that MtARF4a, but not MtARF3, is expressed in the infected root hairs and in epidermal surrounding cells (Figure 2), supporting the notion that auxin signaling and response have a crucial role in promoting infection events in epidermal cells. This requirement for auxin signaling might be related to changes in cell-cycle progression that increase extensibility of the cell wall during IT formation in the root hairs (Breakspear et al., 2014; Lin et al., 2020).

ARFs and the Nod Factor Signaling Pathway

We have found that the expression of MtARF2, MtARF3, and MtARF4/b was activated in response to NFs, and that this activation requires the Nod Factor Receptor MtNFP and the MtNF-YA1 transcription factor (Figure 3), suggesting that this set of ARFs might act downstream of NF-Y in the NF signaling pathway. MtNFP was also required for timely activation of miR160 in M. truncatula, which targets MtARF10, MtARF16, and MtARF17 (Bustos-Sanmamed et al., 2013). Conversely, NF perception-dependent expression has been described for the miR167 in G. max, which targets GmARF8a/b, since accumulation of this miRNA in response to rhizobia was impaired in the non-nodulating mutant defective in the NF receptor GmNFR1α (Wang et al., 2015). Thus, it seems that modulation of the expression of different members of the ARFs family is dependent on NF signaling pathway in legumes. In addition, silencing of MtARF2, MtARF3, MtARF4a, and MtARF4b did not affect the up-regulation of MtNF-YA1 and MtNF-YC1 in response to rhizobia (Figure 6), supporting the notion that these ARF members act downstream of the NF-Y complex. On the other hand, we have found that MtARF2, MtARF3, MtARF4a, and MtARF4b are required for full induction of MtNSP2 in response to S. meliloti (Figure 6), indicating that these ARFs might intercept the Nod signaling pathway acting upstream of MtNSP2. This agrees with previous results that showed that roots overexpressing miR390, which have reduced levels of MtARF2, MtARF3, MtARF4a, and MtARF4b, failed to up-regulate MtNSP1 and MtNSP2 in M. truncatula in response to rhizobia (Hobecker et al., 2017). In G. max, GmARF8a/b can potentially act as negative regulators of GmNSP1 and other symbiotically related genes (Wang et al., 2015). On the other hand, G. max roots with reduced levels of miR160, which targets ARF10/16/17, exhibited greater induction of GmNSP1 upon inoculation with its symbiotic partner Bradyrhizobium japonicum, indicating that GmARF10, GmARF16, and GmARF17 can act as positive regulators of GmNSP1 (Nizampatnam et al., 2015). These results indicate that different ARF members intercept the nodulation signaling pathway acting either as positive or negative regulators of distinct components required for nodulation, such as NSP1 and NSP2. Further analysis will help to elucidate whether ARFs can act as direct activators or repressors of NSP1 and NSP2. Interestingly, recent studies on the Arabidopsis AtARF5 revealed a new paradigm to explain the ARF-mediated transcriptional response to auxin. In addition to the auxin−mediated degradation of Aux/IAA proteins that releases ARF repression, ARFs can potentially act as pioneer transcription factors by recruiting chromatin remodeling proteins that promote a chromatin permissive configuration at auxin-regulated loci (e.g., PLETHORA), allowing proximal cis−AuxREs to become accessible to form higher-order transcriptional complexes, and adding a new layer of complexity to the auxin transcriptional response (Kornet and Scheres, 2009; Wu et al., 2015; Chandler, 2016). Undoubtedly, more research is needed to clarify which loci are targeted by MtARF2, MtARF3, MtARF4a, and MtARF4b and the mechanisms by which these ARFs mediate auxin response in the root nodule symbiosis. The results presented here regarding the positive role of these ARF members in nodulation and its crosstalk with the nodulation signaling pathway represent an initial step toward the elucidation of such mechanisms.

Data Availability Statement

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

Author Contributions

MZ and FB conceived the research, conceptualized the study, and supervised the study. CK, KH, MZ, FB, and AN designed the experiments. CK, KH, and AN performed the experiments. JW, KM, and AN contributed to the biological material. CK, KH, FB, and MZ analyzed the data. CK, MZ, and FB wrote the original draft of the article. CK, KH, AN, FB, and MZ reviewed and edited the article. AN, FB, and MZ acquired funding. All authors contributed to the article and approved the submitted version.

Funding

This study was financially supported by the Agencia Nacional de Promoción Científica y Tecnológica, Argentina through PICT2016-0582 and PICT2017-0581 granted to MZ and PICT2016-0333 and PICT2017-0069 granted to FB. The study was also funded by a IAL (International Associated Laboratory) NOCOSYM project funded by Centre National de la Recherche Scientifique (CNRS) granted to AN and MZ. Development of M. truncatula Tnt1 mutant population was, in part, funded by the National Science Foundation, United States (DBI-0703285 and IOS-1127155) to KM. MZ and FB are members of Consejo Nacional de Investigaciones Científicas y Técnicas (CONICET). CK and KH were recipients of CONICET fellowships.

Conflict of Interest

JW and KM were employed by the company Noble Research Institute LLC.

The remaining authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

We would like to thank Claudio Mazzo for assistance with the preparation of transgenic roots and Mauricio Reynoso for advice on growing arf4a mutants and critical reading of the manuscript. We would also like to thank the CNRS of France for funding visiting programs between France and Argentina.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fpls.2021.659061/full#supplementary-material

Footnotes

1. ^ http://www.montpellier.inra.fr
2. ^ https://www.arabidopsis.org/
3. ^ https://medicago.toulouse.inra.fr/MtrunA17r5.0-ANR/
4. ^ https://www.ebi.ac.uk/Tools/msa/clustalo/
5. ^ http://sourceforge.net/projects/boxshade/

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