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Article

The Lotus japonicus AFB6 Gene Is Involved in the Auxin Dependent Root Developmental Program

by
Alessandra Rogato
1,†,
Vladimir Totev Valkov
1,†,
Marcin Nadzieja
2,
Jens Stougaard
2 and
Maurizio Chiurazzi
1,*
1
Institute of Biosciences and Bioresources (IBBR), CNR, 80131 Napoli, Italy
2
Department of Molecular Biology and Genetics, Aarhus University, 8000 Aarhus, Denmark
*
Author to whom correspondence should be addressed.
†
These authors have contributed equally to this work.
Int. J. Mol. Sci. 2021, 22(16), 8495; https://doi.org/10.3390/ijms22168495
Submission received: 5 May 2021 / Revised: 30 July 2021 / Accepted: 3 August 2021 / Published: 6 August 2021
(This article belongs to the Special Issue Transcriptomic Basis and Nutrient Dependent Signaling Pathways in Plant Development 2.0)
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Abstract

:
Auxin is essential for root development, and its regulatory action is exerted at different steps from perception of the hormone up to transcriptional regulation of target genes. In legume plants there is an overlap between the developmental programs governing lateral root and N2-fixing nodule organogenesis, the latter induced as the result of the symbiotic interaction with rhizobia. Here we report the characterization of a member of the L. japonicus TIR1/AFB auxin receptor family, LjAFB6. A preferential expression of the LjAFB6 gene in the aerial portion of L. japonicus plants was observed. Significant regulation of the expression was not observed during the symbiotic interaction with Mesorhizobium loti and the nodule organogenesis process. In roots, the LjAFB6 expression was induced in response to nitrate supply and was mainly localized in the meristematic regions of both primary and lateral roots. The phenotypic analyses conducted on two independent null mutants indicated a specialized role in the control of primary and lateral root elongation processes in response to auxin, whereas no involvement in the nodulation process was found. We also report the involvement of LjAFB6 in the hypocotyl elongation process and in the control of the expression profile of an auxin-responsive gene.

1. Introduction

The major form of auxin in vascular plants, indole-3-acetic acid (IAA), is mainly biosynthesized in aerial tissue and directionally transported to its responsive sink sites, resulting in modulation of local auxin distribution that regulates most aspects of plant growth, development and acclimation [1]. In the root, auxin accumulates at the root tip and afterwards is transported shootward via the lateral root cap and epidermis with a “reverse fountain” transport mechanism [2]. A sophisticated network of signaling pathways is involved in the control of the amount of auxin perceived at the subcellular, cellular, tissue and organ scales.
Changes of auxin levels control cellular responses in part via modulation of transcriptional regulation. Increasing auxin levels promotes physical interactions between Transport Inhibitor1/Auxin-Signaling (TIR1/AFB) receptors and the auxin coreceptors Auxin/Indole-3-Acetic Acid (Aux/IAA) repressor proteins [3,4]. The latter are consequently polyubiquitinated and degraded through the 26S-mediated proteasome action. Degradation of the repressor results in the release of auxin response transcriptional factors (ARFs), which bind to specific Auxin Response Elements (ARE) with the consensus TGTCTC [5], to activate the transcription of the auxin-responsive genes [6,7].
The auxin signaling pathways are extremely diversified in plants, and this may be at least partially due to different combination of TIR1/AFBs and Aux/IAA (29 members in Arabidopsis thaliana) proteins characterized by different affinities [8]. The nuclear signaling pathway controlling gene transcription regulates auxin-dependent growth of the shoot toward the light [9] and it is also involved in the root growth inhibition pathway triggered by high auxin concentrations [10,11,12]. However, a more recent model proposes that very rapid auxin perception occurs through an instant cell wall depolarization mediated by calcium influx. This results in root growth inhibition that is then reinforced by the TIR1-dependent transcriptional regulation pathway [10,13,14].
The TIR/AFB family is composed of seven members in A. thaliana [15], including the divergent Coronatine Insensitive 1 (AtCOI1), a protein required for efficient response to the plant hormone jasmonic acid [16]. Phylogenetic analysis led to the identification of three pairs of paralogues in A. thaliana, TIR1/AFB1, AFB2/AFB3 and AFB4/AFB5 sub-grouped in three distinct clades [17], whereas a fourth clade, AFB6 was lost early in Brassicaceae and Poaceae [17]. Single TIR/AFB mutants have been isolated and phenotypically characterized in A. thaliana. Tir1, afb1, afb2, afb3, afb4, afb5 mutants appear similar to wild type plants in standard laboratory conditions of growth, whereas these display different level of resistant phenotypes to natural and synthetic auxins. These phenotypes are amplified in double and triple mutant backgrounds, indicating functional redundancy and additive actions [18]. In species other than A. thaliana, the investigation of the TIR1/AFB auxin receptor family has been quite limited. Very recently the functional characterization of the Oryza sativa TIR1/AFB family was reported [19]. The O. sativa members maintain the capacity to physically interact with IAA proteins, and single mutants display a mild resistance to exogenous auxin and partially redundant phenotypes in grain yield, tillering, plant height, root system and germination [19].
In legume plants, most studies have aimed to identify the link between auxin and the nodulation process, whereas the auxin signaling pathways governing root development have been poorly investigated. So far, auxin has been implicated in the control of early steps of nodulation including cell division and rhizobial infection, as well as nodular vascular tissue differentiation [20]. Addition of external auxin at low concentration triggers a slight increase of nodule number in both L. japonicus and Medicago truncatula-inoculated plants, whereas higher concentrations inhibit nodule formation progressively [21,22]. An inhibitory effect on nodule formation has been also reported by application of transport inhibitors [21,22,23], and all these observations can be associated with the reported physiological local accumulation of auxin at the site of incipient emerging nodule primordium, where cortical cell division take place [23,24,25,26,27]. Auxin biosynthesis and accumulation, induced by perception of rhizobial nodulation (Nod) factors, has been reported in L. japonicus root hairs infected by Mesorhizobium loti [28]. Furthermore, auxin responses monitored through the analysis of auxin-reporter GH3 and DR5-fused markers were detected in nodule vascular tissues [23,24,26,29,30], and application of auxin transport inhibitors and antagonists led to inhibition of nodule vascular development [23].
Despite the increased amount of information about auxin signal distribution in roots and nodules, relatively little is known about the roles played by the different molecular actors controlling auxin signaling in legume plants. Interestingly, modulation of nodule formation capacity can be triggered in soybean through over-expression of miRNAs controlling the expression of ARFs [26,31]. A transcriptomic analysis revealed that different M. truncatula ARF genes are induced during the early steps of rhizobial infection, and an insertion mutant of M. truncatula, Mtarf16a, displayed a reduced number of infection events when compared to controls [27]. The involvement of the TIR/AFB auxin receptors in the nodulation process has been investigated only through RNAi and over-expression approaches to control auxin signaling components in transgenic hairy roots of composite plants [32]. In soybean and M. truncatula, over-expression of miRNA393 triggers a reduced expression of TIR1/AFB members, leading to hyposensitivity to external auxin [26], which in M. truncatula results in reduced nodulation [33].
Here we report the functional characterization of a member of the L. japonicus TIR1/AFB auxin receptor family, LjAFB6. To our knowledge this is the first protein belonging to the AFB6 clade to be investigated in plants. The analyses of gene expression profiles and the phenotypic characterization of independent null mutants indicate its specialized function in the pathway governing the auxin signaling pathways involved in root development of legume plants.

2. Results

2.1. Identification of the L. japonicus TIR1/AFB Family

In order to explore and compare the role played by auxin signaling pathways on root and nodule development in legume plants, we retrieved the L. japonicus TIR1/AFB family through a blast search of the Lotus japonicus genome (http://www.kazusa.or.jp/lotus/summary3.0.html (accessed on 1 July 2021); https://lotus.au.dk/ (accessed on 1 July 2021) [34,35], using as queries the A. thaliana TIR1/AFB sequences. In A. thaliana a small subfamily of seven genes was identified among the 700 F-box-containing proteins, including the divergent Coronatine Insensitive 1 (AtCOI1) [15,16]. We found an equivalent group of seven F-box containing members, sharing a significant level of amino acid identities in both the L. japonicus GIFU and MG20 accessions. Significant pair-wise similarities with the A. thaliana proteins were scored for the seven L. japonicus proteins (Table S1). The phylogenetic relationship of the TIR1/AFB members identified in different plant genomes was obtained and the resulting tree subgrouped in the five clades previously identified in vascular plants (Figure 1) [17].
The seven L. japonicus proteins are distributed in the five clades with two members located in the TIR1 and COI clades (Figure 1). LotjaGi4g1v0048600.1 falls in the clade AFB6, where no A. thaliana sequences are found, as this clade was lost early in the brassicaceae family [17]. To the best of our knowledge, no members of the AFB6 clade have been characterized in plants, and we started our characterization of the L. japonicus family with LotjaGi4g1v0048600.1, hereafter termed LjAFB6. LjAFB6 has a predicted sequence containing three exons and two introns, encoding for a 623 amino acid protein with a predicted molecular mass of 70.05 kDa. Residues involved in the protein AtTIR1 protein oligomerization and auxin binding [36], are conserved in LjAFB6 and highlighted in Figure S1A as well as the N-terminal F-box motif (amino acids 22–60) that is required for the assembly of the F-box protein onto the core of the SCF complex. The three-dimensional structure model obtained using as template the X-ray structure of A. thaliana TIR1 (PDB code:2P1M) [37] is shown in Figure S1B.

2.2. Regulatory Profiles of Transcription

Expression data retrieved from the Lotus gene atlas (https://lotus.au.dk/expat/ (accessed on 1 July 2021)) [38] indicate a low level of transcriptional regulation in different organs for the seven L. japonicus TIR1/AFB genes with a preferential expression in the aerial portions of the plant (Figure S2). In particular, none of the five Lotus TIR/AFB auxin receptors genes display a significant up or down-regulated expression in the nodule organ as compared to roots (Figure S2). To investigate the physiological function of the LjAFB6 gene and to confirm the expression data retrieved from the L. japonicus gene atlas, we analyzed the LjAFB6 transcript abundances in different organs of L. japonicus by qRT-PCR. Seedlings germinated on the Gamborg-B5 derived medium without nitrogen sources were inoculated with M. loti and amount of LjAFB6 transcript tested on RNAs extracted from different organs at three weeks after inoculation. The LjAFB6 gene was mainly expressed in shoot tissues (leaf and stem) and was not significantly modulated in root and nodule organs (Figure 2A). The lack of transcriptional regulation during the nodule organogenesis process was also confirmed in a time course experiment where we compared the LjAFB6 expression in uninoculated and inoculated roots (Figure 2B).
In order to investigate a distinctive transcriptional regulatory trait reported for the A. thaliana TIR1/AFB family [40,41], we also analyzed the expression profiles of the L. japonicus members in response to nitrate supply. L. japonicus wild type plants grown for 10 days on B5-derived medium with glutamine 1 mM as the sole nitrogen source were transferred for 4 and 8 h on B5-derived medium with 1 mM KNO3 as sole nitrogen source and the LjTIR1/AFB transcript levels were tested in the roots by qRT-PCR (Figure 3). An increased amount of transcript after nitrate supply (about 2.5 fold) was identified for two out of the five members of the L. japonicus family, LjAFB6 and LotjaGi5g1v0262400.1. However, as control plants were not transferred on new plates with glutamine at four and ten hours, we cannot completely rule out the possibility that the observed changes of expression were due to the experimental manipulation and plant perturbation.

2.3. Spatial Profile of LjAFB6 Expression and Protein Subcellular Localization

To gain further information about the profile of LjAFB6 expression in roots and nodules, the PCR fragment containing the 5′ region of the gene extending up to 1222 bp upstream of the ATG and including the first 11 LjAFB6 codons, was subcloned in the pBI101.1 binary vector to obtain a translational fusion with the gusA reporter gene [42]. Lotus composite plants obtained upon transformation with Agrobacterium rhizogenes were inoculated with M. loti and GUS activity tested in hairy roots. Strong GUS activity was detected in the apical meristem of primary and elongated lateral roots and in the developing lateral root primordia (Figure 4A–D). Staining was also detected with lower intensity in root vascular bundle (Figure 4A,B), whereas no activity could be observed in mature nodules (Figure 4B).
To determine the subcellular localization, we generated a construct that fused YFP to the C-terminus of LjAFB6 under the control of the cauliflower mosaic virus 35S promoter and introduced this construct into tobacco protoplasts. Confocal microscopy indicated that the 35S-LjAFB6-YFP fusion was exclusively localized to the nucleus of transformed protoplasts (Figure S3A–C).

2.4. Isolation of LORE1-Insertion Null Mutants and Root Elongation Phenotypic Analyses

To investigate the involvement of LjAFB6 in the auxin response, we isolated two independent LORE1 insertion mutants from the L. japonicus GIFU LORE1 collection lines [43,44,45]. Lines 30003519 and 30004527, bearing retrotransposon insertions in the first, and second exon (Figure 5A), were genotyped by PCR to identify homozygous plants for the insertion events. Endpoint RT-PCR analyses of homozygous plants from lines 30003519 and 30004527 revealed no detectable LjAFB6 mRNA in shoots, and hence were considered null mutants and hereafter called Ljafb6-1 and Ljafb6-2, respectively (Figure 5B). Two individual homozygous mutant lines for both LORE1 insertions were selected for analyses, and because their growth phenotypes did not significantly differ, the data obtained with the selected individual mutants were pooled in the phenotypical analyses.
The auxin signaling pathways controlling root elongation have not been studied adequately in legume plants as most of the studies have been focused on the correlation with the nodulation process [22,27,46]. With only limited information describing the experimental conditions to highlight the root response to external hormone applications in the Ljafb6 genetic background, we first determined the optimal range of concentrations. In A. thaliana, the root elongation phenotype in response to external auxin has been mainly tested with the synthetic auxin 2,4-D provided at concentrations ranging from 0.01 to 0.15 μM [17,18,36,47,48]. Therefore, three days old wild type synchronized L. japonicus seedlings with comparable primary root lengths were transferred on B5 medium supplemented with 0.01 μM and 0.1 μM 2,4-D to test the effects on shoot and root elongation up to 20 days from the transfer (Figure 6 and Figure 7). The primary root length of wild type plants, scored at 10 days, displayed a progressive decrease in the presence of 0.01 μM and 0.1 μM 2,4-D as compared to control plants, whereas the shoot elongation was slightly inhibited by the addition of the synthetic auxin (Figure 6A).
The emerged lateral roots were still too short to be feasibly measured at 10 days of exposure to auxin, and the data reported in Figure 7 refer to the scoring of the lateral root length at 20 days. The wild type lateral roots displayed a clear-cut progressive reduction of length in the presence of 0.01 μM and 0.1 μM 2,4-D (Figure 7A and Figure S4A–F).
As the effects triggered on plant growth by the external addition of natural and synthetic auxins may differ each other quantitatively and qualitatively, we also scored the L. japonicus root response phenotype after exposure to a wide range of IAA concentrations. The lowest 0.05 μM concentration did not affect significantly the root architecture response in wild type L. japonicus plants (Figure 6B and Figure 7B), whereas the presence of 0.5 μM and 5 μM IAA caused a significant reduction of the primary root length, scorable at 10 days after the exposure (Figure 6B). At 5 μM IAA concentration we observed a significant reduction of the shoot elongation response (Figure 6B). The lateral roots elongation was also significantly reduced at 0.5 μM IAA, although not as severely as in the presence of 2,4-D (Figure 7B).
Interestingly, primary and lateral root elongation responses of both Ljafb6 mutants were also progressively affected by increasing concentrations of 2,4-D and IAA, but these effects were significantly reduced compared to wild type plants (Figure 6 and Figure 7). In particular, the Ljafb6 primary roots were about 20% (0.01 μM 2,4-D) and 38% (0.1 μM 2,4-D) longer than wild type after 10 days of exposure (Figure 6A). The same phenotypic response was also displayed by the Ljafb6 plants after 10 days of exposure to 0.5 μM IAA and 5 μM IAA (Figure 6B). Concerning the lateral root elongation, the average increase scored after 20 days of exposure to 0.01 μM 2,4-D and 0.1 μM 2,4-D, was about 31% and 65% in the Ljafb6 mutants as compared to wild type plants, respectively (Figure 7A and Figure S4A–F). A reduced response of the lateral root elongation phenotype in the Ljafb6 genotype, was also observed in the presence of 0.5 μM IAA (Figure 7B; Figure S5A,B).
These results demonstrate an alteration of the auxin-dependent responses in the Ljafb6 genetic background. Furthermore, it is remarkable that, although expected, growth in the presence of auxin stimulated lateral root formation, we did not observe in the L. japonicus afb6 mutants, the reduced density of lateral roots reported for the A. thaliana tir1 and afb1 mutants [3,17] (Figure S6).

2.5. LjAFB6 Is Involved in the Hypocotyl Elongation Process

We also compared another auxin-dependent phenotype represented by the hypocotyl elongation. Etiolated wild type and mutant seedlings were obtained after germination in the dark for two weeks at 23 °C. As expected, a dramatic increase of the hypocotyl length was observed for both genotypes, but reduced length of the hypocotyl was scored in the mutant seedlings (Figure 8; Figure S5C). The causal relationship between KO mutations in the LjAFB6 gene and the reported phenotypes were confirmed by cosegregation analyses conducted on the progeny of plants heterozygous for the LORE1 insertion event into the LjAFB6 gene. All the segregants genotyped as homozygous for the insertion event showed the short hypocotyl phenotype, whereas such a phenotype was not exhibited by heterozygous and wild type plants.

2.6. Auxin Responsive Profiles of Expression

The phenotypic characterization of the two null mutants clearly indicated the contribution of LjAFB6 to auxin responses in both primary and lateral root elongation processes (Figure 6 and Figure 7). Therefore, to determine whether auxin regulates expression of the LjAFB6 gene, we analyzed its expression in L. japonicus wild type roots exposed for 12 and 24 h to 1 and 5 μM IAA. The results shown in Figure 9A indicate no changes of the LjAFB6 transcript level under both IAA treatments. We have further tested the involvement of LjAFB6 in auxin response signaling by comparing the expression of a GRETCHEN HAGEN 3 (GH3) auxin-responsive gene in the wild type and Ljafb6 genetic backgrounds. The profiles of expression of the IAA Amido Synthetase (LotjaGi2g1v0405900.1) were analyzed in roots of wild type and Ljafb6 plants, transferred at ten days after sowing, on a medium supplemented with 1 μM and 5 μM IAA. The early transcriptional induction of this ARF marker in the roots of L. japonicus plants exposed to IAA was previously reported [49]. The transcription of the GH3 auxin responsive gene was strongly induced at both IAA concentrations, and the level of induction was reduced of about four-fold in the Ljafb6-1 and Ljafb6-2 mutants compared to wild type (Figure 9B).

2.7. Analyses of the Symbiotic Phenotypes

In order to test whether LjAFB6 is also involved in the auxin signaling pathways controlling different steps of the nodulation process, we set up the conditions for the symbiotic phenotypic characterization by identifying the range of auxin concentrations needed to highlight symbiotic phenotypes in our experimental conditions. Addition of IAA at low concentration (0.01 μM) has been reported to trigger a slight increase of nodule number in both L. japonicus and M. truncatula inoculated plants, whereas higher concentrations (0.2–1 μM) inhibited nodule formation progressively [21,22]. Synchronised L. japonicus wild type seedlings were transferred 6 days after sowing on B5 Gamborg-derived medium without nitrogen sources supplied with different IAA concentrations ranging from 0.25 μM to 1 μM and inoculated with M. loti. The inhibitory effect of 0.25 μM IAA resulted in halving the nodule formation capacity and this action was further increased at 0.5 and 1 μM (Figure 10A). Therefore, we compared the nodulation capacity of the different L. japonicus genotypes in the presence of 0.25 and 0.5 μM IAA. No significant difference was observed (Figure 10B). Furthermore, in agreement with the profile of expression shown in Figure 1A,B and Figure 2B, we did not detect any difference in the development of mature nodule and vascular bundle structures (Figure 10D). Noteworthy is the confirmation of increased lateral root elongation displayed by the Ljafb6 plants in the presence of 0.25 μM and 0.5 μM IAA compared to wild type plants (Figure S7). Finally, in order to investigate the possible involvement of LjAFB6, whose expression is induced by KNO3 (Figure 3), in the cross-talk between nitrate and auxin signals controlling the nodulation process, we tested whether the nitrate-dependent inhibitory pathway triggered by high external KNO3 concentration was altered in the Ljafb6 backgrounds. Synchronized wild type and Ljafb6 seedlings were transferred after germination in Petri dishes with B5 derived media without nitrogen sources or in the presence of 5 and 10 mM KNO3 and inoculated with M. loti. As shown in Figure 10C the curve of nitrate-dependent nodulation inhibition is conserved among the different genotypes.

3. Discussion

In legume plants unraveling the roles played by factors involved in the auxin signaling pathways governing root and nodule development is crucial to establish functional boundaries between two organogenic processes that display similarities [24,50,51,52]. Both lateral roots and nodule development are regulated by a complex hormonal network, with the auxin involved in the control of organ primordia initiation, emergence and vasculature differentiations. We report here the characterization of a member of the L. japonicus TIR1/AFB family based on the analyses of temporal and spatial profiles of expression and phenotypes of independent null mutants.
The spatial pattern of expression exhibited by the prLjAFB6-gusA fusion in the root tissues, with GUS activity detected in the meristematic regions of primary and lateral roots as well as lateral root primordia and vascular structures (Figure 4A–D) and the reported LjAFB6 nuclear localization (Figure S3), are comparable to results reported for most of the A. thaliana TIR1/AFB genes [17,18,53]. In legume plants, a similar pattern of promoter activity has been reported for the four GmTIR1A/B/C/D and the two GmAFB3A/B predicted genes retrieved in the allotetraploid soybean genome [32]. In particular, in soybean hairy roots GUS activity was displayed in the main and lateral root tips and lateral root primordia, with weaker GUS staining exhibited by the prGmAFB3-gusA fusion [32]. Interestingly, the root meristem and columella cell root cap expression were also reported for an auxin-responsive DR5 promoter fusion in M. truncatula [26]. The preferential GUS expression exhibited in the primary and lateral root tips is consistent with LjAFB6 involvement in the auxin-dependent signaling pathways governing root elongation. All the A. thaliana TIR1/AFB members were demonstrated to act as auxin receptors by promoting the degradation of the Aux/IAA transcriptional repressors resulting in the release of the ARFs transcriptional factors. The involvement of LjAFB6 in this auxin response signaling pathway was confirmed by the significantly reduced expression of the GH3 auxin responsive gene in the roots of Ljafb6 as compared to wild type plants grown in the presence of IAA (Figure 9B). The lack of the transcriptional LjAFB6 auxin responsiveness reported in Figure 9A is also consistent with the expression profiles reported for the A. thaliana TIR1/AFB genes [17], but different from responses observed in soybean, where GmTIR1A, GmTIR1C and GmAFB3A are induced by 2,4-D treatment in roots [32].
The main phenotypic trait reported in the A. thaliana tir1, afb1, afb2, afb3, afb4 and afb5 single mutant backgrounds was increased primary root growth in the presence of auxin, whereas they appeared similar to wild type plants in standard laboratory conditions of growth [11,17,18,36,47,48,53]. An increased root elongation tolerance in the presence of 2,4-D was recently reported also in O. sativa tir1/afb single mutants [19].
In legumes, the experimental setup for testing root responsiveness to phytohormone treatments is not an easily predictable matter, as those physiological traits that have been associated to the acquisition of symbiotic predisposition appear to be peculiar in this plant family [54]. Therefore, the optimal range of 2,4-D and IAA concentration exploited to highlight clear-cut root phenotypes as well as the timing of the plant exposure to the hormone had to be tailored for L. japonicus root responsiveness. In particular, L. japonicus primary roots displayed a sensitivity response to 0.01 μM and 0.1 μM 2,4-D similar to those reported in A. thaliana (Figure 6A), although in the latter a short time of exposure was exploited for scoring the root elongation phenotype [17,18,36,47,48]. On the other side, L. japonicus primary roots appeared to be more tolerant than A. thaliana to IAA, where 25% and 50% growth inhibition were reported in the presence of 0.03 μM and 0.1 μM concentrations (Figure 6B). However, these quantitatively different primary root responses need to be further investigated to narrow the curve of sensitivity.
Importantly, the analyses conducted on the two Ljafb6 knock out LORE1 mutants revealed a significant increased tolerance of the primary root growth in plants exposed for 10 days to 2,4-D and IAA as compared to wild type plants (Figure 6A–D). Furthermore, etiolated mutant seedlings displayed a significant hypocotyl length reduction compared to wild type seedlings, indicating the involvement of LjAFB6 in another auxin dependent elongation process (Figure 8). A similar phenotype was reported in A. thaliana only for Attir1 single mutants that displayed a short hypocotyl length compared to wild type after incubation at 28 °C [11,47]. Therefore, our analysis reveals that a member of the AFB6 clade such as LjAFB6, apparently shares the involvement in the primary root elongation response to auxin reported for the A. thaliana and O. sativa TIR1/AFB genes. Furthermore, a very interesting phenotype revealed by the comparison of Ljafb6 and wild type plants is the striking increased tolerance of the lateral root elongation to both 2,4-D and IAA in the mutated genotypes (Figure 7; Figures S4–S6). These results suggest a functional correlation of the LjAFB6 and AtAFB3 genes, as the latter was the only member of the A. thaliana family to display alterations of both primary and lateral root growth in the mutated background [40]. AtAFB3, whose nitrate-dependent induction of expression was correlated in the root tips with an increased auxin activity, has been reported to be a master regulator of the nitrate dependent signaling cascade controlling the root system architecture [40,41]. This nitrate-dependent pathway depends on the nitrate transport function of AtNPF6.3, a nitrate transporter that also functions as an auxin transport facilitator [55,56] and acts through the transcription factor AtNAC4 target [40,41,57,58].
In the case of LjAFB6, the correlation with a nitrate dependent signaling was suggested by the transcriptional induction shown in Figure 3, where a transient peak of expression is observed at 4 h after the transfer in 1 mM KNO3 conditions, a profile very similar to the one reported for AtAFB3 [40]. However, the involvement of LjAFB6 in a nitrate dependent signaling pathway controlling root architecture must be further investigated because the main phenotypic trait reported for Atafb3, which is the rescue of the inhibitory effect exerted by high concentration of nitrate (5 mM) on root development [40], could not be tested in the Ljafb6 background since such an inhibitory effect of nitrate on root development in L. japonicus plants has never been reported, even in the presence of 20 mM KNO3 [59].
On the other hand, a nitrate dependent signaling pathway responsible of the inhibition of nodule organogenesis in the presence of external high concentrations of KNO3 is well-known for legume plants [60,61,62], but the result shown in Figure 10C with the overlapping curves of inhibition of nodulation in the presence of progressively increased concentrations of KNO3 in wild type and Ljafb6 plants, seems to exclude this functional link. A functional link of LjAFB6 with the nodulation process is also excluded by the profile of expression of LjAFB6 shown in Figure 2A,B, which did not indicate a transcriptional regulation temporally associated with root infection, nodule development or functioning processes. This unregulated pattern of expression is shared with all the other members of the Lotus family (Figure S2). Consistently, the spatial profile of expression shown in Figure 4, rules out the possible involvement of LjAFB6 in the nodulation process, as GUS activity was not detected in nodules developed in the inoculated hairy roots transformed with the prLjAFB6-gusA fusion (Figure 4B). The phenotypic characterization reported in Figure 10 further confirmed that conclusion, as no differences were scored between wild type and nodule plants for the nodule formation capacity, as well as nodule development with and without addition of auxin in the media. These results indicating the lack of any obvious functional link with the nodulation process for LjAFB6 are distinct from the ones reported in soybean for the four GmTIR1 and GmAFB3 predicted sequences, which displayed significant promoter activity in the nodules of the inoculated hairy roots, with the exception of GmAFB3B that did not exhibit a significant expression [31]. Their potential roles in the perception of auxin during nodulation in soybean were confirmed by reduced or increased nodule numbers displayed by hairy roots transformed with GmTIR1A, GmTIR1B, GmAFB3A RNAi and over-expressing constructs, respectively [31]. However, a complete characterization of the L. japonicus TIR1/AFB family is necessary to establish putative orthologous relationships between the different members in the two legume plants.

4. Materials and Methods

4.1. Plant Material and Growth Conditions

All experiments were carried out with Lotus japonicus ecotype B-129 F12 GIFU [63,64]. Plants were cultivated in a controlled growth chamber with a light intensity of 200 μmol m−2 s−1 at 23 °C with a 16 h:8 h, light:dark cycle. Seeds sterilization was performed as described in [65]. Five days after sowing in axenic conditions on H2O agar Petri dishes, unsynchronized seedlings were discarded. Seedlings were transferred on sterile filter paper placed on agar slants of B5 [66] or B5 derived growth media with/out 2,4-D (D8407; Sigma Aldrich, St. Louis, MO, USA) and IAA (I0901; Duchefa, Haarlem, The Netherlands). Filter papers (070115; DIAPATH) with growing plants were transferred on fresh media with/out hormones every 8 days. The root system was shielded from light access (even overhead light) by fitting the plates into a blacked-out container and by shielding the roots with autoclaved aluminium foil. Mesorhizobium loti inoculation was performed at 7 d after sowing as described in [67]. The strain R7A used for the inoculation experiments was grown in liquid TYR-medium supplemented with rifampicin (20 mg L−1). In the case of M. loti inoculation plants were transferred on medium with the same composition as Gamborg B5 medium [66], except that (NH4)2SO4 and KNO3 were omitted. KCl was added, when necessary, to the medium to replace the same concentrations of potassium source. The media containing vitamins (G0415; Duchefa) were buffered with 2.5 mM 2-(N-morpholino)ethanesulfonic acid (MES, M1503.0250; Duchefa) and pH-adjusted to 5.7 with KOH. Plant length parameters were measured with the ImageJ software [68].

4.2. Lotus Japonicus Transformation Procedures

Binary vectors were conjugated into the Agrobacterium rhizogenes 15834 strain [69]. A. rhizogenes-mediated L. japonicus transformations and inoculation of composite plants were performed as described in [70].

4.3. Protoplast Transformation

Leaf protoplasts were prepared and transformed according to [71] using 3-wk-old N. tabacum plants. DNA (40 μg of each construct) was introduced into 1 × 106 protoplasts by polyethylene glycol (PEG)-mediated transfection. After 16 h incubation in the dark at 25 °C, yellow fluorescent protein (YFP) fluorescence in protoplast cells was detected by confocal microscopy.

4.4. Plasmids Preparation

prLjAFB6-gusA, the PCR-amplified fragment containing 1222 bp upstream of the ATG, was obtained on genomic DNA with forward and reverse oligonucleotides containing SalI and BamHI sites, respectively (Table S2). The amplicon was subcloned as SalI-BamHI fragment into the pBI101.1 vector [42] to obtain the T-DNA construct. Finally, the prLjTIR1/AFB-gusA cassette was subcloned as an EcoRI–HindIII fragment into the pIV10 plasmid for cointegration into the pAR1193 [69]. LjAFB6-YFP, the PCR-amplified fragment obtained on leaf cDNA with forward and reverse oligonucleotides containing BglII and KpnI sites, respectively (Table S2), was subcloned into the pENTRTM1A plasmid (A10462; ThermoFisher, Waltham, MA, USA). The resulting donor plasmid was mixed with the pEarleyGate 104 destination vector to obtain the YPF-LjAFB6 fusion [72].

4.5. Quantitative Real-Time qRT-PCR

qRT-PCR was performed with a DNA Engine Opticon 2 System, MJ Research (Waltham, MA, USA) using SYBR to monitor dsDNA synthesis. The procedure is described in [73]. The UBIQUITIN (UBI) gene (AW719589) was used as an internal standard. The oligonucleotides used for the qRT-PCR are listed in Table S2.

4.6. LORE1 Lines Analyses

LORE1 lines 30003519 and 30004527 were obtained from the LORE1 collection [43,44,45]. Plants in the segregating populations were genotyped, and expression of homozygous plants tested with oligonucleotides listed in the Table S2. After PCR genotyping, shoot cuts of the homozygous plants were cultured and amplified in axenic conditions as described in [74].

4.7. Histochemical β-Glucuronidase (GUS) Analysis

Histochemical GUS was performed as described in [75]. Sections 80 μm thick were obtained with the vibratome (Leica VT1000S; Wetzlar, Germany) as reported in [76].

4.8. Confocal Imaging

Confocal microscope analyses were performed using a LeicaDMi8 (Leica Biosystems, Wetzlar, Germany) laser scanning confocal imaging system. For YFP detection, the excitation was at 488 nm and detection was between 515 and 530 nm. For chlorophyll detection, excitation was at 488 nm and detection over 570 nm.

4.9. Statistical Analyses

Statistical analyses were performed using the VASSARSTATS two way factorial ANOVA for independent samples program (http://vassarstats.net/ (accessed on 5 July 2021).

4.10. Phylogenetic Study

Evolutionary history was inferred using the Neighbor-Joining method [39], the optimal tree having a sum of branch length = 8.90683588. The percentage of replicate trees in which the associated taxa clustered together in the bootstrap test (500 replicates) are shown next to the branches [77]. The evolutionary distances were computed using the JTT matrix-based method [78] and given in the units of the number of amino acid substitutions per site. The analysis involved 50 amino acid sequences. All positions with less than 65% site coverage were eliminated. That is, fewer than 35% alignment gaps, missing data, and ambiguous bases were allowed at any position. There were a total of 564 positions in the final dataset. Evolutionary analyses were conducted in MEGA7 [79]. Sequence data for the proteins described in the phylogenetic tree shown in Figure 1 can be found at the following databases: L. japonicus, https://lotus.au.dk/ (accessed on 1 April 2021); S. lycopersicon, ftp://ftp.solgenomics.net/tomato_genome/annotation/ITAG4.0_release/ (accessed on 1 April 2021); A. thaliana, https://www.arabidopsis.org (accessed on 1 April 2021); M. truncatula, https://www.genome.jp/kegg-bin/get_htext?mtr00001 (accessed on 1 April 2021); O. sativa, http://rice.plantbiology.msu.edu/index.shtml (accessed on 1 April 2021); V. vinifera, http://www.plantgdb.org/VvGDB/ (accessed on 1 April 2021); P. trichocarpa, http://www.plantgdb.org/PtGDB/ (accessed on 1 April 2021).

4.11. Protein Modeling

The model was obtained online at the SWISS MODEL server, (swissmodel.expasy.org, accessed on 1 April 2021) by using tools of the Deep view Swiss PDB Viewer program [80]. The picture was generated by PyMOL program (Schrödinger, Inc., New York, NY, USA).

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/ijms22168495/s1. Figure S1. (A) The LjAFB6 amino acid sequence. Conserved amino acid residues are highlighted (red, F-box; green, conserved auxin binding residues; blue, residues involved in the oligomerization). (B) Three-dimensional structure model obtained using as template the X-ray structure of A. thaliana TIR1 (PDB code:2P1M) [37]. F-box and LRRs are indicated in red and blue, respectively. The model was obtained online at the SWISS MODEL server by using tools of the Deep view Swiss PDB Viewer program (Guex and Peitsch, 1997). The picture was generated by PyMOL program. Figure S2. Relative expression levels of the TIR1/AFB genes in different organs, normalized to the tissue with the highest transcript abundance. The heatmap was generated using the ExpAt tool available online at https://lotus.au.dk/expat/ (accessed on 5 May 2021) [38]. Figure S3. Lotus japonicus AFB6 localization at the nucleus. The LjAFB6-YFP translational fusion was transiently expressed in protoplast of tobacco mesophyll cells under the control of the 35S promoter. (A) YFP nuclear localization (B) DAPI nuclear localization (C) Merged image of chlorophyll autofluorescence and DAPI-stained nucleus. White bar = 20 μm. Figure S4. Phenotypic characterization of Ljafb6 plants. Representative images of wild type and Ljafb6 plants at 20 days after transfer on 2,4-D media. (A) Roots of wild type and Ljafb6-1 plants grown on B5 Gamborg medium without 2,4-D. (B) Roots of wild type and Ljafb6-1 grown in the presence of 0.01 μM 2,4-D. (C) Roots of wild type and Ljafb6-1 plants grown in the presence of 0.1 μM 2,4-D. (D) Same plants as in C. (E) Roots of wild type and Ljafb6-2 plants grown in the presence of 0.1 μM 2,4-D. (F) Same plants as in E. Figure S5. Phenotypic characterization of Ljafb6 plants. (A) Representative images of the roots of wild type and Ljafb6-1 plants at 20 days after transfer on 0.5 μM IAA media. (B) Same plants as in A. (B) Etiolated wild type and Ljafb6 seedlings maintained for 2 weeks in the dark. Plant different genotypes are indicated. Figure S6. Number of lateral roots formed in wild type and Ljafb6 plants. Plants were scored at 20 days after transfer on media supplemented with IAA. Bars represent means and SE of measures from three experiments (12 plants per experiment per condition). Figure S7. Mean of lateral root elongation of inoculated plants. Wild type and Ljafb6 plants were grown in a B5 derived medium without nitrogen sources and inoculated with M. loti. Roots length were scored at 3 weeks after inoculation. The different concentrations of IAA are indicated. Bars represent means and SE of measures from three experiments (15 plants per experiment per condition). Asterisks indicate significant differences with wild type measures. * p < 0.001. Table S1. List of the L. japonicus TIR1/AFB members. Amino acid length and identity values with the A. thaliana members are indicated (the significant peaks of identity are highlighted in bold). Table S2. Oligonucleotides used in the present work. References [37,38] are cited in the supplementary materials.

Author Contributions

All the authors gave a critical contribution to the experimental design and manuscript preparation. V.T.V., A.R., M.N. designed, performed and analyzed the experiments; J.S. designed the experiments and edited the manuscript; M.C. designed the experiments and wrote the article. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by grant from CNR project FOE-2019 DBA.AD003.139 and by the European Community, Horizon 2020, PRIMA (Partnership for Research and Innovation in the Mediterranean Area), Section 2, 2019–2021, Legumes in biodiversity-based farming systems in Mediterranean basin—LEGU-MED.

Data Availability Statement

Sequence data for the genes described in this article can be found in the Lotus database https://lotus.au.dk/ (accessed on 1 July 2021).

Acknowledgments

We thank G. Manco for helping with the protein modeling, Marco Petruzziello and Giuseppina Zampi for technical assistance and Finn Pedersen for professional plant care.

Conflicts of Interest

The authors declare no conflict of interest.

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Figure 1. The evolutionary relationship between plant TIR/AFB members. The evolutional history was inferred using the Neighbor-Joining method [39]. The optimal tree with the sum of branch length = 8.90683588 is shown. The tree is drawn to scale, with branch lengths in the same units as those of the evolutionary distances used to infer the phylogenetic tree. The evolutionary distances were computed using the JTT matrix-based method and are in the units of the number of amino acid substitutions per site. The five distinct clades of the TIR/AFB family are indicated by different bar colours on the right. L. japonicus and A. thaliana members are highlighted by colours. The LjAFB6 member is framed. Abbreviations: Lotja, Lotus japonicus; AT, Arabidopsis thaliana; MTR, Medicago truncatula; Os, Oryza sativa, Solyc, Solanum lycopersicon; GSVIV, Vitis vinifera; POPTR, Populus trichocarpa.
Figure 1. The evolutionary relationship between plant TIR/AFB members. The evolutional history was inferred using the Neighbor-Joining method [39]. The optimal tree with the sum of branch length = 8.90683588 is shown. The tree is drawn to scale, with branch lengths in the same units as those of the evolutionary distances used to infer the phylogenetic tree. The evolutionary distances were computed using the JTT matrix-based method and are in the units of the number of amino acid substitutions per site. The five distinct clades of the TIR/AFB family are indicated by different bar colours on the right. L. japonicus and A. thaliana members are highlighted by colours. The LjAFB6 member is framed. Abbreviations: Lotja, Lotus japonicus; AT, Arabidopsis thaliana; MTR, Medicago truncatula; Os, Oryza sativa, Solyc, Solanum lycopersicon; GSVIV, Vitis vinifera; POPTR, Populus trichocarpa.
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Figure 2. (A) LjAFB6 expression in different organs. RNAs were extracted from wild-type plants grown on Gamborg B5 derivative medium without nitrogen source at 3 weeks post inoculation (wpi). Mature flowers were obtained from L. japonicus plants propagated in the growth chamber. (B) Time course of expression of LjAFB6 in root and nodule tissues after M. loti inoculation. RNAs were extracted from roots of wild-type seedlings grown in nitrogen starvation conditions at different times after inoculation (R0, 24 h, 48 h, 72 h, 28 days), from nodule primordia (6 days) and mature nodules (14 days and 28 days post inoculation). Expression levels are normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of leaf (A) and R0 (B). Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments.
Figure 2. (A) LjAFB6 expression in different organs. RNAs were extracted from wild-type plants grown on Gamborg B5 derivative medium without nitrogen source at 3 weeks post inoculation (wpi). Mature flowers were obtained from L. japonicus plants propagated in the growth chamber. (B) Time course of expression of LjAFB6 in root and nodule tissues after M. loti inoculation. RNAs were extracted from roots of wild-type seedlings grown in nitrogen starvation conditions at different times after inoculation (R0, 24 h, 48 h, 72 h, 28 days), from nodule primordia (6 days) and mature nodules (14 days and 28 days post inoculation). Expression levels are normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of leaf (A) and R0 (B). Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments.
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Figure 3. Nitrate dependent expression of the LjTIR1/AFB genes. RNAs were extracted from roots of wild-type plants grown for 10 days on Gamborg B5 derivative medium with glutamine 1 mM as the sole nitrogen source and transferred on 1 mM KNO3 for the indicated range of times. Expression levels are normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of T0. Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments. Asterisks indicate significant differences with T0 levels. * p < 0.01.
Figure 3. Nitrate dependent expression of the LjTIR1/AFB genes. RNAs were extracted from roots of wild-type plants grown for 10 days on Gamborg B5 derivative medium with glutamine 1 mM as the sole nitrogen source and transferred on 1 mM KNO3 for the indicated range of times. Expression levels are normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of T0. Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments. Asterisks indicate significant differences with T0 levels. * p < 0.01.
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Figure 4. Representative β-glucuronidase (GUS) activity in L. japonicus hairy roots transformed with the prLjAFB6-gusA construct. (A,B) Arrows and arrowheads indicate staining in the meristems of primary/lateral elongated roots and in the lateral root primordia, respectively. (C) GUS activity in the root stele, in the emergence region of the lateral root and in the apical meristem (arrow). (D) GUS activity in the apical region of a primary root. Black bars on the left = 50 μm.
Figure 4. Representative β-glucuronidase (GUS) activity in L. japonicus hairy roots transformed with the prLjAFB6-gusA construct. (A,B) Arrows and arrowheads indicate staining in the meristems of primary/lateral elongated roots and in the lateral root primordia, respectively. (C) GUS activity in the root stele, in the emergence region of the lateral root and in the apical meristem (arrow). (D) GUS activity in the apical region of a primary root. Black bars on the left = 50 μm.
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Figure 5. Structure of the L. japonicus AFB6 gene and analysis of the expression in the LORE1 segregants. (A) Gene model of LjAFB6. Insertion sites and relative orientations of the LORE1 retrotransposon element in the 30003519 and 30004527 lines are indicated. (B) Expression of the LjAFB6 gene in the Ljafb6-1 and Ljafb6-2 plants. Total RNAs isolated from leaves was used for qRT-PCR analyses.
Figure 5. Structure of the L. japonicus AFB6 gene and analysis of the expression in the LORE1 segregants. (A) Gene model of LjAFB6. Insertion sites and relative orientations of the LORE1 retrotransposon element in the 30003519 and 30004527 lines are indicated. (B) Expression of the LjAFB6 gene in the Ljafb6-1 and Ljafb6-2 plants. Total RNAs isolated from leaves was used for qRT-PCR analyses.
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Figure 6. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. Wild type and Ljafb6 plants were grown in the presence of different concentrations of 2,4-D and IAA. (A) Shoots and primary roots length of wild type and Ljafb6 plants, 10 days after transfer on 2,4-D media. (B) Shoots and primary roots length of wild type and Ljafb6 plants 10 days after transfer on IAA media. Ct indicates control plants grown without addition of hormones. Bars represent means and SE of measures from three experiments (12 plants per experiment per condition). Asterisks indicate significant differences between plant genotypes in the same conditions of growth. * p < 0.05; ** p < 0.002; *** p < 0.0001.
Figure 6. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. Wild type and Ljafb6 plants were grown in the presence of different concentrations of 2,4-D and IAA. (A) Shoots and primary roots length of wild type and Ljafb6 plants, 10 days after transfer on 2,4-D media. (B) Shoots and primary roots length of wild type and Ljafb6 plants 10 days after transfer on IAA media. Ct indicates control plants grown without addition of hormones. Bars represent means and SE of measures from three experiments (12 plants per experiment per condition). Asterisks indicate significant differences between plant genotypes in the same conditions of growth. * p < 0.05; ** p < 0.002; *** p < 0.0001.
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Figure 7. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. (A) Mean of lateral roots length of wild type and Ljafb6 plants 20 days after transfer on 2,4-D media. (B) Mean of lateral roots length of wild type and Ljafb6 plants 20 days after transfer on IAA media. Bars represent means and SE of measures from three experiments (12 plants per experiment per condition). Asterisks indicate significant differences between plant genotypes in the same conditions of growth. ** p < 0.002; *** p < 0.0001.
Figure 7. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. (A) Mean of lateral roots length of wild type and Ljafb6 plants 20 days after transfer on 2,4-D media. (B) Mean of lateral roots length of wild type and Ljafb6 plants 20 days after transfer on IAA media. Bars represent means and SE of measures from three experiments (12 plants per experiment per condition). Asterisks indicate significant differences between plant genotypes in the same conditions of growth. ** p < 0.002; *** p < 0.0001.
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Figure 8. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. Hypocotyl length of wild type and Ljafb6 etiolated seedlings maintained for 2 weeks in the dark. Asterisks indicate significant differences between plant genotypes. *** p < 0.0001.
Figure 8. Phenotypic characterization of Ljafb6-1 and Ljafb6-2 mutants. Hypocotyl length of wild type and Ljafb6 etiolated seedlings maintained for 2 weeks in the dark. Asterisks indicate significant differences between plant genotypes. *** p < 0.0001.
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Figure 9. Auxin responsive profiles of expression. (A) Wild type plants were treated with 1 and 5 μM IAA for 12 and 24 h. (B) Wild type and Ljafb6 plants were treated with 1 and 5 μM IAA for 12 and 24 h. Genotypes and growth conditions are indicated. Bars with oblique and horizontal motifs indicate 12 h and 24 h samples, respectively. RNAs were extracted from roots and qRT-PCR performed using primers listed in Table S2. Expression levels were normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of T0. Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments.
Figure 9. Auxin responsive profiles of expression. (A) Wild type plants were treated with 1 and 5 μM IAA for 12 and 24 h. (B) Wild type and Ljafb6 plants were treated with 1 and 5 μM IAA for 12 and 24 h. Genotypes and growth conditions are indicated. Bars with oblique and horizontal motifs indicate 12 h and 24 h samples, respectively. RNAs were extracted from roots and qRT-PCR performed using primers listed in Table S2. Expression levels were normalized with respect to the internal control UBIQUITIN (UBI) gene and plotted relative to the expression of T0. Data bars represent means and SD of data obtained with RNA extracted from three different sets of plants and three qRT-PCR experiments.
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Figure 10. Symbiotic phenotypes of wild type and Ljafb6 plants. (A) Kinetic of nodulation in wild type plants grown in the presence of different concentrations of IAA. IAA concentrations are indicated. (B) Kinetic of nodulation in wild type and Ljafb6 plants grown in the presence of 0.25 and 0.5 μM IAA. (C) Kinetic of nodulation in wild type and Ljafb6 plants grown in permissive conditions (without nitrate) and inhibitory conditions (5 and 10 mM KNO3). Nodules were scored weekly after inoculation, up to three weeks. KNO3 concentrations are indicated. (D) 80 μm vibratome sections of wild type and Ljafb6-1 nodules. Higher magnification images refer to zones of the nodular sections where vascular bundle structures are visible (arrows).
Figure 10. Symbiotic phenotypes of wild type and Ljafb6 plants. (A) Kinetic of nodulation in wild type plants grown in the presence of different concentrations of IAA. IAA concentrations are indicated. (B) Kinetic of nodulation in wild type and Ljafb6 plants grown in the presence of 0.25 and 0.5 μM IAA. (C) Kinetic of nodulation in wild type and Ljafb6 plants grown in permissive conditions (without nitrate) and inhibitory conditions (5 and 10 mM KNO3). Nodules were scored weekly after inoculation, up to three weeks. KNO3 concentrations are indicated. (D) 80 μm vibratome sections of wild type and Ljafb6-1 nodules. Higher magnification images refer to zones of the nodular sections where vascular bundle structures are visible (arrows).
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Rogato, A.; Valkov, V.T.; Nadzieja, M.; Stougaard, J.; Chiurazzi, M. The Lotus japonicus AFB6 Gene Is Involved in the Auxin Dependent Root Developmental Program. Int. J. Mol. Sci. 2021, 22, 8495. https://doi.org/10.3390/ijms22168495

AMA Style

Rogato A, Valkov VT, Nadzieja M, Stougaard J, Chiurazzi M. The Lotus japonicus AFB6 Gene Is Involved in the Auxin Dependent Root Developmental Program. International Journal of Molecular Sciences. 2021; 22(16):8495. https://doi.org/10.3390/ijms22168495

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Rogato, Alessandra, Vladimir Totev Valkov, Marcin Nadzieja, Jens Stougaard, and Maurizio Chiurazzi. 2021. "The Lotus japonicus AFB6 Gene Is Involved in the Auxin Dependent Root Developmental Program" International Journal of Molecular Sciences 22, no. 16: 8495. https://doi.org/10.3390/ijms22168495

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