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Article

The Pyla-1 Natural Accession of Arabidopsis thaliana Shows Little Nitrate-Induced Plasticity of Root Development

by
Silvana Porco
1,
Loïc Haelterman
1,
Jérôme De Pessemier
1,
Hugues De Gernier
1,2,3,
Florence Reyé
1 and
Christian Hermans
1,*
1
Crop Production and Biostimulation Laboratory, Brussels Bioengineering School, Université libre de Bruxelles, Campus Plaine CP 245, Bd du Triomphe, 1050 Brussels, Belgium
2
Department of Plant Biotechnology and Bioinformatics, Ghent University, 9052 Ghent, Belgium
3
Center for Plant Systems Biology, VIB, Technologiepark 927, 9052 Ghent, Belgium
*
Author to whom correspondence should be addressed.
Nitrogen 2022, 3(3), 444-454; https://0-doi-org.brum.beds.ac.uk/10.3390/nitrogen3030029
Submission received: 30 June 2022 / Revised: 5 August 2022 / Accepted: 6 August 2022 / Published: 8 August 2022
(This article belongs to the Special Issue Nitrogen Metabolism: From Plant Cell to Field and Vice Versa)
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Abstract

:
Optimizing root system architecture is a strategy for coping with soil fertility, such as low nitrogen input. An ample number of Arabidopsis thaliana natural accessions have set the foundation for studies on mechanisms that regulate root morphology. This report compares the Columbia-0 (Col-0) reference and Pyla-1 (Pyl-1) from a coastal zone in France, known for having the tallest sand dune in Europe. Seedlings were grown on vertical agar plates with different nitrate concentrations. The lateral root outgrowth of Col-0 was stimulated under mild depletion and repressed under nitrate enrichment. The Pyl-1 produced a long primary root and any or very few visible lateral roots across the nitrate supplies. This could reflect an adaptation to sandy soil conditions, where the primary root grows downwards to the lower strata to take up water and mobile soil resources without elongating the lateral roots. Microscopic observations revealed similar densities of lateral root primordia in both accessions. The Pyl-1 maintained the ability to initiate lateral root primordia. However, the post-initiation events seemed to be critical in modulating the lateral-root-less phenotype. In Pyl-1, the emergence of primordia through the primary root tissues was slowed, and newly formed lateral roots stayed stunted. In brief, Pyl-1 is a fascinating genotype for studying the nutritional influences on lateral root development.

1. Introduction

Nitrogen (N) mineral fertilization is used to sustain crop production, but excessive concentrations of nitrate have harmful effects on the environment and human health by causing soil nitrate leaching, groundwater pollution and greenhouse gas emissions [1,2]. Improving decision tools for agricultural management and breeding crops for better nitrogen use efficiency (NUE) are implemented to reduce N fertilizer input [3,4,5]. The optimization of the root system architecture of crops for a more efficient N capture is a key determinant to reaching that goal. The root organ has plasticity to adapt to the nitrate supply: local nitrate patches stimulate lateral root outgrowth, whereas globally high external nitrate concentrations have a systemic inhibitory effect [6,7]. Increasing lateral root branching of a crop species would serve to explore a larger soil volume and to enhance nitrate capture [8,9,10].
In plant biology research, Arabidopsis thaliana has a long history of being used as a model for studying root organogenesis. The formation of a lateral root is a post-embryonic event that originates from the asymmetric division of the pericycle cell pair—a step referred to as the lateral root initiation [11,12,13]. The dividing pericycle cells develop into a lateral root primordium that emerges through the overlying tissues (subsequently, the endodermis, cortex and epidermis) of the parent root [14,15,16]. Next, the apical meristem is activated, and the newly formed lateral root elongates. Genetic screens have isolated a plethora of Arabidopsis mutants with lateral root developmental defects [17]. Additionally, the Arabidopsis model represents a step forward in understanding the nitrate influences on root growth [18]. The variability of root morphologies, offered by abundant natural accessions, is exploited to mine for the genes and alleles that regulate root traits in response to the nitrate supply [19]. This knowledge may provide new targets to breed genetically related crops with larger genomes (e.g., cultivated Brassica), which could be more efficient at capturing N in the soil.
This study provides a detailed root phenotype characterization of Pyla-1 (Pyl-1), one natural Arabidopsis accession that is part of a core collection that maximizes the genetic diversity of the species [20]. The Pyl-1 originates from the coastal zone of Arcachon Bay in France, known for having the tallest sand dune in Europe. Following previous phenotyping screens conducted in vitro [21,22], the accession shows any or very few visible lateral roots at a young developmental stage. This report provides (i) a comparison of a two-dimensional root morphology between the Columbia-0 (Col-0) reference and Pyl-1 in response to a nitrate supply, and together with four accessions collected from the Arcachon urban area, (ii) a quantification of the total number and developmental stages of lateral root primordia, and (iii) a temporal sequence of the lateral root formation after a gravitropic curvature. These findings underline Pyl-1 as a prevailing genotype for studying the mechanisms of repression exerted by nitrate on lateral root growth.

2. Materials and Methods

2.1. Plant Material

The Arabidopsis thaliana Columbia-0 (Col-0) accession was obtained from the Nottingham Arabidopsis Stock Centre, and Pyla-1 (Pyl-1) was obtained from the INRAE Versailles Genomic Resource Center. The four Arcachon (Arc-1, Arc-2, Arc-3, Arc-4) accessions were collected in the Arcachon-Pyla area, France. The geographical map of the harvesting sites and coordinates is shown in Figure S1.

2.2. In Vitro Culture

The in vitro culture procedure is described in [22]. Briefly, sterilized seeds were plated on a 1× Murashige and Skoog medium, modified with nitrate as the only N source, 1% (w/v) sucrose and 0.8% (w/v) plant agar (Duschefa Biochemie, Haarlem, the Netherlands). The pH was adjusted to 5.7. Five media with different nitrate concentrations were prepared: 0.1 mM KNO3 + 9.9 mM KCl (added to prevent potassium depletion), 1 mM KNO3 + 9 mM KCl, 10 mM KNO3, 25 mM KNO3 or 50 mM KNO3. A volume of 50 mL of medium was poured into one square Petri plate (12 cm × 12 cm). Five seeds of one genotype were sown on a Petri plate and were stratified for two days at 4 °C in the dark. The plates were vertically incubated in a culture chamber with a constant temperature of 20 °C and a photoperiod of 16 h light (45 µmol photons m−2 s−1) /8 h darkness.

2.3. Two-Dimensional Root Morphology Analysis

Eleven days after germination, the root systems were scanned with an EPSON Scan Perfection V30 at a resolution of 400 dpi. The scans were annotated using the RootNav image analysis software [23]. The length of the primary root (LPR), the number of lateral roots that visibly emerged from the primary root longer than 1 mm (NLR) and the sum of the length of lateral roots (ΣLLR) were quantified [22].

2.4. Quantification of Lateral Root Primordium Developmental Stages

The roots were cleared following the protocol detailed in [24]. The developmental stages of lateral root primordia were observed with an Optika B-350 microscope. Nine categories were established: I (initiating primordium), II–III (up to three cell layers structure), IV–VII (primordium dome formation and emergence through parental tissues), E (lateral root emerged from the epidermis and of less than 1 mm) and LR (lateral root strictly longer than 1 mm). The total number of lateral root primordia (NLRP) and the density of lateral root primordia per primary root length (DLRP) were measured 11 days after germination.

2.5. Lateral Root Bending

The seeds were plated on a medium containing 10 mM KNO3. The seedlings were grown for three days under continuous light (45 µmol photons m−2 s−1) conditions. The plates positioned vertically were turned 90°, as described in [25]. The roots were collected at eight different time points (18 h, 24 h, 30 h, 36 h, 42 h, 48 h, 54 h and 60 h) after rotation. The root bends were cleared (see Section 2.4), and the development stages of the lateral root primordia (from initiation to emergence) were scored.

2.6. Statistical Treatment

All statistical analyses were done with R software [26] and XLSTAT [27]. An analysis of variance was performed for the variables LPR, NLR, ΣLLR, NLRP and DLRP, using the lme4 R package [28]. The phenotypic models were fitted on the Col-0 and Pyl-1 genotypes using the REML method, according to the equation Pijk = μ + Gi + Nj + Gi × Nj + eijk, where Pijk is the phenotypic value, µ is the general mean, Gi is the genotype i, Nj is the nitrate supply j, and eijk is the residual. All effects were declared as random. Moreover, multiple t-tests were performed using the tidyverse and rstatix R packages [29,30] to compare the mean values of the root morphological traits under each genotype x nitrate combination.

3. Results

3.1. The Pyla-1 Accession Exhibited Little Macroscopic Variation of Root Morphology in Response to Nitrate Supply

The seedlings of Col-0 and Pyl-1 grew vertically on media supplemented with 0.1, 1, 10, 25 or 50 mM nitrate. The morphological variation of the whole root organs is shown in Figure 1. The length of the primary root (LPR), the number of visible lateral roots > 1 mm (NLR) and the sum of the length of lateral roots (ΣLLR) reached the greatest values in the Col-0 seedlings supplied with 1 mM nitrate (Figure 2). The modulation of the root morphology by nitrate availability followed the previous observations in the reference accession [31,32]. A low but moderate nitrate supply (1 mM) promoted the growth of both the primary and lateral roots, while a severe nitrate shortage (0.1 mM) and elevated nitrate supply (>25 mM) repressed the number and the length of lateral roots in Col-0 (Figure 2). By contrast, Pyl-1 was slightly responsive to the nitrate supply and produced very few short lateral roots, solely at 0.1 mM nitrate. For every nitrate concentration tested, the LPR values were significantly (p < 0.05) greater in Pyl-1 than in Col-0, while NLR and ΣLLR were lower (Figure 2). We assessed the extent to which a variation in the root morphological traits was due to the genetic differences between accessions (G), nitrate treatment differences (N), genetic differences in the level of response to nitrate treatment (G × N) and unexplained experimental errors (residuals) (Figure S2). Most of the variations for LPR and NLR were due to G (35% and 65%, respectively). The ΣLLR trait showed a nearly equal dependence on G (47%) and G × N (44%). This highlighted a larger genotype-dependent plasticity to the nitrate treatment for ΣLLR than for LPR or NLR.
All four Arcachon accessions showed similar root morphologies at 10 mM nitrate (Figure 1). The LPR, NLR and ΣLLR values were significantly (p < 0.05) lower compared to Col-0 (Figure 2). Only LPR was identical between Arc-4 and Col-0. Contrastingly, these accessions did not mimic the Pyl-1 root phenotype; rather, they presented shorter LPR and more important NLR and ΣLLR values than Pyl-1.

3.2. The Initiation of Lateral Root Primordium Was Not Impaired in Pyla-1

One possible explanation for the lateral-root-less phenotype harbored by Pyl-1 (Figure 1) could be an impairment of lateral root initiation. Hence, we examined the lateral root development at the microscopic level (Figure 3). In both genotypes, the number of lateral root primordia (NLRP) globally decreased with the nitrate concentration increasing. The NLRP was significantly (p < 0.05) more important in Pyl-1 compared to Col-0 at 0.1, 1 and 50 mM nitrate (Figure 3a). No significant difference in the density of lateral root primordia (DLRP) was observed between the genotypes across all nitrate concentrations; however, DLRP was greater in Pyl-1 than Col-0 at 50 mM nitrate (Figure 3b). By contrast, with the macroscopic root morphological traits (Figure 2), NLRP and DLRP showed a large N treatment effect (44% and 71%, respectively) (Figure S2).
The lateral root formation follows a precise developmental program during which successive phases, from the initiation to the emergence, arise to penetrate the parent root tissue layers [33] (Figure 3c). At 1 mM nitrate, almost three-quarters of the lateral root primordia emerged from the primary root in Col-0 (Figure 3d). That proportion decreased when the seedlings were subjected to lower or greater nitrate concentrations. The percentages of the emerged (<1 mm) and visible (>1 mm) lateral roots were 54 % and 13%, respectively, at 0.1 mM nitrate, while these values reached 28% and 33% at 50 mM nitrate. By comparison, three-thirds of the Pyl-1 primordia had not emerged from the primary root at 1 mM nitrate. The percentages of the emerged and visible lateral roots reached 23% and 19%, respectively, at 0.1 mM nitrate, while only 7% emerged at 50 mM nitrate. Across all nitrate concentrations, Pyl-1 had greater cumulated percentages at stages III, IV and V compared to Col-0 (Figure 3d). At 50 mM nitrate, more than one-third of the primordia stayed at stage IV. This indicates that the intermediate stages of progression through the cortex tissue were affected rather than at the initiation.

3.3. Lateral Root Primordia Exhibit Slower Organ Emergence in Pyla-1

A root bending assay was conducted to follow the temporal sequence of lateral root formation. By applying a 90° gravitropic stimulus, the lateral root initiation was synchronically induced at the outer edges of the bending roots. Then, the developmental stages of the lateral root primordia at the root bends were scored every 6 h between 18 h and until their emergence from the primary root. In Col-0, the lateral root initiation (stage I) was detected 18 h post gravity induction, and the emergence (stage E) happened after 42 h (Figure 4a). These observations matched with previous reports on the reference accession [25]. In Pyl-1, the lateral root initiation happened at the same time compared to Col-0. However, stages I and II accumulated during the first hours, and the progression to stages III and IV was drastically delayed (Figure 4b). After 42 h, most Pyl-1 primordia were still blocked around these stages. Eventually, the primordia progressed to the later stages, VI and VII, with the majority of them emerging from the parent root after 60 h. The newly emerged lateral roots did not elongate after that time (data not shown). These data indicated that Pyl-1 had a slower lateral root developmental program with a bottleneck around stages III–V. The accumulation of these specific stages pointed to a defect in the transition from a flat to dome-shaped lateral root primordium [15,34]. This prompted us to examine the shapes of primordia (length, height and area) at stages II, III and IV in the two genotypes (Figure S2). The length and/or the area of the primordia were significantly (p < 0.05) increased by 5–15% in Pyl-1 compared to Col-0. This is documenting that the Pyl-1 lateral root primordium is misshaped.

4. Discussion

The Arabidopsis thaliana species has a vast geographical distribution. Natural populations growing in a wide range of soil conditions around the world are showing a large variation in the expression of numerous phenotypic traits and also at the root organ level [35,36]. These accessions provide a rich and diverse genetic resource for studying NUE processes [37,38,39,40] and the N-related adaptive differences in root morphology [41,42]. The Pyl-1 accession shows a fascinating root phenotype that is slightly responsive to nitrate availability (Figure 1).
The developmental and morphological defects are largely documented during the lateral root organogenesis of the Arabidopsis model [17,43]. For instance, the alf4-1, arf7arf19, gata23, and slr-1 mutants [44,45,46,47] are unable to trigger the initiation cascade, resulting in a lateral-root-less phenotype. In terms of the macroscopic root architecture, Pyl-1 looks very similar to these mutants. However, this natural accession has identical or even greater densities of lateral root primordia compared to the Col-0 wild-type (Figure 3a). This clearly indicates that Pyl-1 maintains the ability to initiate lateral root primordia. Thus, the post-initiation events seem to be critical in modulating the Pyl-1 macroscopic root morphology. A biomechanical constraint may be exerted on the primordia breaking through overlying tissues. Such a mechanical constraint is documented to cause a change in primordium shape [14,17]. The contours of some Pyl-1 primordia are altered (Figure S2), further pointing to such mechanical properties of the cortex. Further studies on the tensile properties of tissues need to be carried out.
During the lateral root formation sequence (Figure 3d), the progression occurring from early primordium development is slowed down, with a bottleneck arising around stages III–V, followed by a later constraint on the elongation out of the parent root. These defects likely involve the phytohormone auxin, which is a key regulator of lateral root formation [48]. The auxin accumulation in the cells overlying the primordium depends on transcription factor LATERAL ORGAN BOUNDARIES-DOMAIN 29 (LBD29) regulating the auxin influx carrier LIKE-AUX1 3 (LAX3) [15,49]. The loss-of-function of these two genes results in a slowdown from stages III to V [15,49], as observed in Pyl-1. Moreover, this hormone alters cell wall properties by inducing wall loosening [50], and auxin-dependent cell separation promotes lateral organ emergence [15]. Furthermore, auxin regulates the root tissue hydraulic properties and aquaporin function to facilitate emergence [25]. Altering PLASMA MEMBRANE INTRINSIC PROTEIN 2;1 (PIP2;1) causes a flattened dome-shape primordia and delays emergence [25]. Another case was reported on the overexpression of MYB DOMAIN PROTEIN 93 (MYB93) negatively impacting the primordium progression [51,52]. Likewise, the loss of the MYB36 function results in the accumulation of stages IV–V [34]. A thorough analysis of the genetic and developmental background of the Pyl-1 root phenotype will be essential in the future.
The natural Arabidopsis populations undergo various selective environmental pressures. Developmental and physiological adaptations are likely to occur in order to optimize plant performance in different habitats [53,54]. The Pyl-1 accession was initially collected in the Pyla area, Arcachon Bay, France. There, the tallest sand dune in Europe is found. The Pyl-1 root phenotype observed in vitro (Figure 1) may reflect an adaptation to sandy soil conditions, where the primary root grows downwards to the lower strata to take up water without elongating the lateral roots. However, the lack of data on local soil conditions makes it difficult to support this hypothesis further. Therefore, we launched a prospection campaign in the Arcachon Bay area. No accession was found in the Dune of Pilat, but four of them were collected in the Arcachon urban environment (Figure S1). These accessions were growing on sidewalks in the city, and soil sampling was impossible. Thus, the hypothesis of an adaptation to a sand habitat is still lacking to support field evidence at this stage. Additional observations of root morphology upon growth conditions in rhizotrons filled with sand could provide more indications of the Pyl-1 phenotype.

5. Conclusions

Pyl-1 is a fascinating plant material for studying root organogenesis. The next step will be to identify the alleles(s) responsible for the lateral-root-less phenotype. After generating one F2 (Col-0 × Pyl-1)-segregating population, a mapping-by-sequencing strategy [55] could be employed on two pooled genomes showing contrasting lateral root outgrowth. A further molecular characterization could involve monitoring the expression of the genes involved in cell separation and lateral root emergence. The molecular dissection of the lateral root development in Pyl-1 could greatly contribute to drawing strategies for optimizing the root system architecture and improving N capture in plants.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/nitrogen3030029/s1, Table S1: Variance components extracted from mixed linear models, Figure S1: Arabidopsis accessions in the Arcachon Bay area, France, Figure S2: Comparison of the shape of lateral root primordia in Columbia-0 and Pyla-1 accessions.

Author Contributions

Conceptualization: C.H.; Original draft preparation: C.H. and S.P.; Investigation, methodology: C.H., F.R., J.D.P., H.D.G. and L.H. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by Fonds de la Recherche Scientifique (F.R.S.-FNRS) (MIS and CDR J.0106.20).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The data presented in this study are available on request from the corresponding author.

Acknowledgments

L.H. and C.H. are, respectively, a PhD fellow and research associate from F.R.S.-FNRS.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Walling, E.; Vaneeckhaute, C.J. Greenhouse gas emissions from inorganic and organic fertilizer production and use: A review of emission factors and their variability. J. Environ. Manage. 2020, 276, 111211. [Google Scholar] [CrossRef]
  2. Picetti, R.; Deeney, M.; Pastorino, S.; Miller, M.R.; Shah, A.; Leon, D.A.; Dangour, A.D.; Green, R. Nitrate and nitrite contamination in drinking water and cancer risk: A systematic review with meta-analysis. Environ. Res. 2022, 210, 112988. [Google Scholar] [CrossRef]
  3. Lebedev, V.G.; Popova, A.A.; Shestibratov, K.A. Genetic engineering and genome editing for improving nitrogen use efficiency in plants. Cells 2021, 10, 3303. [Google Scholar] [CrossRef]
  4. Javed, T.; Indu, I.; Singhal, R.K.; Shabbir, R.; Shah, A.N.; Kumar, P.; Jinger, D.; Dharmappa, P.M.; Shad, M.A.; Saha, D.; et al. Recent advances in agronomic and physio-molecular approaches for improving nitrogen use effiency in crop plants. Front. Plant. Sci. 2022, 13, 877544. [Google Scholar] [CrossRef]
  5. Whetton, R.L.; Harty, M.A.; Holden, N.M. Communicating nitrogen loss mechanisms for improving nitrogen use efficiency management, focused on global wheat. Nitrogen 2022, 3, 213–246. [Google Scholar] [CrossRef]
  6. Walch-Liu, P.; Ivanov, I.I.; Filleur, S.; Gan, Y.; Remans, T.; Forde, B.G. Nitrogen regulation of root branching. Ann. Bot. 2006, 97, 875–881. [Google Scholar] [CrossRef]
  7. Asim, M.; Ullah, Z.; Xu, F.; An, L.; Aluko, O.O.; Wang, Q.; Liu, H. Nitrate signaling, functions, and regulation of root system architecture: Insights from Arabidopsis thaliana. Genes 2020, 11, 633. [Google Scholar] [CrossRef]
  8. Louvieaux, J.; Spanoghe, M.; Hermans, C. Root morphological traits of seedlings are predictors of seed yield and quality in winter oilseed rape hybrid cultivars. Front. Plant. Sci. 2020, 11, 568009. [Google Scholar] [CrossRef]
  9. Kupcsik, L.; Chiodi, C.; Moturu, T.R.; De Gernier, H.; Haelterman, L.; Louvieaux, J.; Tillard, P.; Sturrock, C.J.; Bennett, M.; Nacry, P.; et al. Oilseed rape cultivars show diversity of root morphologies with the potential for better capture of nitrogen. Nitrogen 2021, 2, 491–505. [Google Scholar] [CrossRef]
  10. Wang, H.; Wu, Y.; An, T.; Chen, Y.J. Lateral root elongation enhances nitrogen-use efficiency in maize genotypes at the seedling stage. J. Sci. Food Agric. 2022. [Google Scholar] [CrossRef]
  11. Casimiro, I.; Marchant, A.; Bhalerao, R.; Beeckman, T.; Dhooge, S.; Swarup, R.; Graham, N.; Inzé, D.; Sandber, G.; Casero, P.; et al. Auxin transport promotes Arabidopsis lateral root initiation. Plant. Cell 2001, 13, 843–852. [Google Scholar] [CrossRef] [Green Version]
  12. Dubrovsky, J.G.; Rost, T.L.; Colón-Carmona, A.; Doerner, P. Early primordium morphogenesis during lateral root initiation in Arabidopsis thaliana. Planta 2001, 214, 30–36. [Google Scholar] [CrossRef]
  13. Du, Y.; Scheres, B. Lateral root formation and the multiple roles of auxin. J. Exp. Bot. 2018, 69, 155–167. [Google Scholar] [CrossRef]
  14. Lucas, M.; Kenobi, K.; von Wangenheim, D.; Voβ, U.; Swarup, K.; De Smet, I.; Van Damme, D.; Lawrence, T.; Péret, B.; Moscardi, E.; et al. Lateral root morphogenesis is dependent on the mechanical properties of the overlaying tissues. Proc. Natl. Acad. Sci. USA 2013, 110, 5229–5234. [Google Scholar] [CrossRef] [Green Version]
  15. Porco, S.; Larrieu, A.; Du, Y.; Gaudinier, A.; Goh, T.; Swarup, K.; Swarup, R.; Kuempers, B.; Bishopp, A.; Lavenus, J.; et al. Lateral root emergence in Arabidopsis is dependent on transcription factor LBD29 regulation of auxin influx carrier LAX3. Development 2016, 143, 3340–3349. [Google Scholar]
  16. Malamy, J.E.; Benfey, P.N. Down and out in Arabidopsis: The formation of lateral roots. Trends Plant. Sci. 1997, 2, 390–396. [Google Scholar] [CrossRef]
  17. Szymanowska-Pulka, J. Form matters: Morphological aspects of lateral root development. Ann. Bot. 2013, 112, 1643–1654. [Google Scholar] [CrossRef]
  18. Fredes, I.; Moreno, S.; Díaz, F.P.; Gutiérrez, R.A. Nitrate signaling and the control of Arabidopsis growth and development. Curr. Opin. Plant. Biol. 2019, 47, 112–118. [Google Scholar] [CrossRef]
  19. Pélissier, P.-M.; Motte, M.; Beeckman, T. Lateral root formation and nutrients: Nitrogen in the spotlight. Plant. Physiol. 2021, 187, 1104–1116. [Google Scholar] [CrossRef]
  20. McKhann, H.I.; Camilleri, C.; Bérard, A.; Bataillon, T.; David, J.L.; Reboud, X.; Le Corre, V.; Caloustian, C.; Gut, I.G.; Brunel, D. Nested core collections maximizing genetic diversity in Arabidopsis thaliana. Plant. J. 2004, 38, 193–202. [Google Scholar] [CrossRef]
  21. De Pessemier, J.; Chardon, F.; Juraniec, M.; Delaplace, P.; Hermans, C. Natural variation of the root morphological response to nitrate supply in Arabidopsis thaliana. Mech. Dev. 2013, 130, 45–53. [Google Scholar] [CrossRef]
  22. De Pessemier, J.; Moturu, T.R.; Nacry, P.; Ebert, R.; De Gernier, H.; Tillard, P.; Swarup, K.; Wells, D.M.; Haseloff, J.; Murray, S.C.; et al. Root system size and root hair length are key phenes for nitrate acquisition and biomass production across natural variation in Arabidopsis. J. Exp. Bot. 2022, 73, 3569–3583. [Google Scholar] [CrossRef]
  23. Pound, M.P.; French, A.P.; Atkinson, J.A.; Wells, D.M.; Bennett, M.J.; Pridmore, T. RootNav: Navigating images of complex root architectures. Plant. Physiol. 2013, 162, 1802–1814. [Google Scholar] [CrossRef] [Green Version]
  24. Dubrovsky, J.G.; Gambetta, G.A.; Hernández-Barrera, A.; Shishkova, S.; González, I. Lateral root initiation in Arabidopsis: Developmental window, spatial patterning, density and predictability. Ann. Bot. 2006, 97, 903–915. [Google Scholar] [CrossRef] [Green Version]
  25. Péret, B.; Li, G.; Zhao, J.; Band, L.R.; Voβ, U.; Postaire, O.; Luu, D.-T.; Da Ines, O.; Casimiro, I.; Lucas, M.; et al. Auxin regulates aquaporin function to facilitate lateral root emergence. Nature Cell Biol. 2012, 14, 991–998. [Google Scholar] [CrossRef]
  26. R Core Team. R: A Language and Environment for Statistical Computing; R Foundation for Statistical Computing: Vienna, Austria, 2020; Available online: https://www.R-project.org/ (accessed on 30 June 2022).
  27. XLSTAT. Statistical Software for Excel. 2007. Available online: https://www.xlstat.com (accessed on 30 June 2022).
  28. Bates, D.; Mächler, M.; Bolker, B.; Walker, S. Fitting linear mixed-effects models using lme4. J. Stat. Softw. 2015, 67, 1–48. [Google Scholar] [CrossRef]
  29. Wickham, H.; Averick, M.; Bryan, J.; Chang, W.; McGowan, L.; François, R.; Grolemund, G.; Hayes, A.; Henry, L.; Hester, J.; et al. Welcome to the Tidyverse. JOSS 2019, 4, 1686. [Google Scholar] [CrossRef]
  30. Kassambara, A. Rstatix: Pipe-Friendly Framework for Basic Statistical Tests. R Package Version 0.7.0. 2021. Available online: https://rpkgs.datanovia.com/rstatix/ (accessed on 30 June 2022).
  31. Sun, C.H.; Yu, Q.; Hu, D.G. Nitrate: A crucial signal during lateral roots development. Front. Plant. Sci. 2017, 8, 485. [Google Scholar] [CrossRef]
  32. Louvieaux, J.; De Gernier, H.; Hermans, C. Exploiting genetic variability of root morphology as a lever to improve nitrogen use efficiency in oilseed rape. In Engineering Nitrogen Utilization in Crop Plants; Springer: Berlin/Heidelberg, Germany, 2018; pp. 185–201. [Google Scholar]
  33. Malamy, J.E.; Benfey, P.N. Organization and cell differentiation in lateral roots of Arabidopsis thaliana. Development 1997, 124, 33–44. [Google Scholar] [CrossRef]
  34. Fernández-Marcos, M.; Desvoyes, B.; Manzano, C.; Liberman, L.M.; Benfey, P.N.; Del Pozo, J.C.; Gutierrez, C. Control of Arabidopsis lateral root primordium boundaries by MYB36. New Phytol. 2017, 213, 105–112. [Google Scholar] [CrossRef] [Green Version]
  35. Deja-Muylle, A.; Parizot, B.; Motte, H.; Beeckman, T. Exploiting natural variation in root system architecture via genome-wide association studies. J. Exp. Bot. 2020, 71, 2379–2389. [Google Scholar] [CrossRef]
  36. Deja-Muylle, A.; Opdenacker, D.; Parizot, B.; Motte, H.; Lobe, G.; Storme, V.; Clauw, P.; Njo, M.; Beeckman, T. Genetic variability of Arabidopsis thaliana mature root system architecture and genome-wide association study. Front. Plant. Sci. 2022, 12, 814110. [Google Scholar] [CrossRef]
  37. North, K.A.; Ehlting, B.; Koprivova, A.; Rennenberg, H.; Kopriva, S. Natural variation in Arabidopsis adaptation to growth at low nitrogen conditions. Plant. Physiol. Biochem. 2009, 47, 912–918. [Google Scholar] [CrossRef]
  38. Chardon, F.; Barthélémy, J.; Daniel-Vedele, F.; Masclaux-Daubresse, C. Natural variation of nitrate uptake and nitrogen use efficiency in Arabidopsis thaliana cultivated with limiting and ample nitrogen supply. J. Exp. Bot. 2010, 61, 2293–2302. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  39. Masclaux-Daubresse, C.; Chardon, F. Exploring nitrogen remobilization for seed filling using natural variation in Arabidopsis thaliana. J. Exp. Bot. 2011, 62, 2131–2142. [Google Scholar] [CrossRef] [Green Version]
  40. Meyer, R.C.; Gryczka, C.; Neitsch, C.; Müller, M.; Bräutigam, A.; Schlereth, A.; Schön, H.; Weigelt-Fischer, K.; Altmann, T. Genetic diversity for nitrogen use efficiency in Arabidopsis thaliana. Planta 2019, 250, 41–57. [Google Scholar] [CrossRef] [Green Version]
  41. Gifford, M.L.; Banta, J.A.; Katari, M.S.; Hulsmans, J.; Chen, L.; Ristova, D.; Tranchina, D.; Purugganan, M.D.; Coruzzi, G.M.; Birnbaum, K.D. Plasticity regulators modulate specific root traits in discrete nitrogen environments. PLoS Genet. 2013, 9, e1003760. [Google Scholar] [CrossRef]
  42. Jia, Z.; Giehl, R.F.H.; von Wirén, N. The root foraging response under low nitrogen depends on DWARF1-mediated brassinosteroid biosynthesis. Plant. Physiol. 2020, 183, 998–1010. [Google Scholar] [CrossRef]
  43. Satbhai, S.B.; Ristova, D.; Busch, W. Underground tuning: Quantitative regulation of root growth. J. Exp. Bot. 2015, 66, 1099–1112. [Google Scholar] [CrossRef] [Green Version]
  44. Celenza Jr., J. L.; Grisafi, P.L.; Fink, G.R. A pathway for lateral root formation in Arabidopsis thaliana. Genes Dev. 1995, 9, 2131–2142. [Google Scholar] [CrossRef] [Green Version]
  45. Okushima, Y.; Fukaki, H.; Onoda, M.; Theologis, A.; Tasaka, M. ARF7 and ARF19 regulate lateral root formation via direct activation of LBD/ASL genes in Arabidopsis. Plant Cell. 2007, 19, 118–130. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  46. De Rybel, B.; Vassileva, V.; Parizot, B.; Demeulenaere, M.; Grunewald, W.; Audenaert, D.; Van Campenhout, J.; Overvoorde, P.; Jansen, L.; Vanneste, S.; et al. A novel aux/IAA28 signaling cascade activates GATA23-dependent specification of lateral root founder cell identity. Curr. Biol. 2010, 20, 697–706. [Google Scholar] [CrossRef]
  47. Fukaki, H.; Tameda, S.; Masuda, H.; Tasaka, M. Lateral root formation is blocked by a gain-of-function mutation in the SOLITARY-ROOT/IAA14 gene of Arabidopsis. Plant. J. 2022, 29, 153–168. [Google Scholar] [CrossRef]
  48. Lavenus, J.; Goh, T.; Roberts, I.; Guyomarc'h, S.; Lucas, M.; De Smet, I.; Fukaki, H.; Beeckman, T.; Bennett, M.; Laplaze, L. Lateral root development in Arabidopsis: Fifty shades of auxin. Trends Plant. Sci. 2013, 18, 450–458. [Google Scholar] [CrossRef]
  49. Swarup, K.; Benková, E.; Swarup, R.; Casimiro, I.; Péret, B.; Yang, Y.; Parry, G.; Nielsen, E.; De Smet, I.; Vanneste, S.; et al. The auxin influx carrier LAX3 promotes lateral root emergence. Nat. Cell Biol. 2008, 10, 946–954. [Google Scholar] [CrossRef] [PubMed]
  50. Majda, M.; Robert, S. The role of auxin in cell wall expansion. Int. J. Mol. Sci. 2018, 19, 951. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  51. Gibbs, D.; Voss, U.; Harding, S.; Fannon, J.; Moody, L.; Yamada, E.; Swarup, K.; Nibau, C.; Bassel, G.; Choudhary, A.; et al. AtMYB93 is a novel negative regulator of lateral root development in Arabidopsis. New Phytol. 2014, 4, 1194–1207. [Google Scholar] [CrossRef] [Green Version]
  52. Gibbs, D.; Coates, J. AtMYB93 is an endodermis-specific transcriptional regulator of lateral root development in Arabidopsis. Plant. Signal. Behav. 2014, 9, e970406. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  53. Lev-Yadun, S.; Berleth, T. Expanding ecological and evolutionary insights from wild Arabidopsis thaliana accessions. Plant. Signal. Behav. 2009, 4, 796–797. [Google Scholar] [CrossRef] [Green Version]
  54. Baxter, I.; Brazelton, J.N.; Yu, D.; Huang, Y.S.; Lahner, B.; Yakubova, E.; Li, Y.; Bergelson, J.; Borevitz, J.O.; Nordborg, M.; et al. A coastal cline in sodium accumulation in Arabidopsis thaliana is driven by natural variation of the sodium transporter AtHKT1;1. PLoS Genet. 2010, 6, e1001193. [Google Scholar] [CrossRef] [Green Version]
  55. James, G.V.; Patel, V.; Nordström, K.J.; Klasen, J.R.; Salomé, P.A.; Weigel, D.; Schneeberger, K. User guide for mapping-by-sequencing in Arabidopsis. Genome Biol. 2013, 14, R61. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Root phenotypes of Arabidopsis accessions in response to nitrate supply. Pyla-1 (Pyl-1), Columbia-0 (Col-0) accessions are germinated on media containing 0.1, 1, 10, 25 or 50 mM nitrate and Arcachon accessions (Arc-1, Arc-2, Arc-3, Arc-4) on 10 mM nitrate. Pictures were taken 11 days after germination. Scale bar: 1 cm.
Figure 1. Root phenotypes of Arabidopsis accessions in response to nitrate supply. Pyla-1 (Pyl-1), Columbia-0 (Col-0) accessions are germinated on media containing 0.1, 1, 10, 25 or 50 mM nitrate and Arcachon accessions (Arc-1, Arc-2, Arc-3, Arc-4) on 10 mM nitrate. Pictures were taken 11 days after germination. Scale bar: 1 cm.
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Figure 2. Root morphological traits of Columbia-0, Pyla-1 and Arcachon accessions in response to nitrate supply. Plants were grown as described in the legend of Figure 1. (a) Length of the primary root (LPR); (b) number of lateral roots longer than 1 mm length (NLR); (c) sum of the length of lateral roots (∑LLR). Black columns: Col-0, white columns: Pyl-1, gray columns: Arc-1, Arc-2, Arc-3 and Arc-4. n = 20–48 root organs ± std. Data are analyzed with multiple t-tests, and the different letters allow for visualizing the significant differences. Values sharing the same letter are not significantly different (p-value > 0.05). Phenotypic models are shown in Table S1.
Figure 2. Root morphological traits of Columbia-0, Pyla-1 and Arcachon accessions in response to nitrate supply. Plants were grown as described in the legend of Figure 1. (a) Length of the primary root (LPR); (b) number of lateral roots longer than 1 mm length (NLR); (c) sum of the length of lateral roots (∑LLR). Black columns: Col-0, white columns: Pyl-1, gray columns: Arc-1, Arc-2, Arc-3 and Arc-4. n = 20–48 root organs ± std. Data are analyzed with multiple t-tests, and the different letters allow for visualizing the significant differences. Values sharing the same letter are not significantly different (p-value > 0.05). Phenotypic models are shown in Table S1.
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Figure 3. Lateral root primordium quantification of Pyla-1 and Columbia-0 accessions in response to nitrate supply. The total number of lateral root primordia (NLRP) (a) and the density of lateral root primordia (DLRP) (b) were measured under 0.1, 1, 10, 25 and 50 mM nitrate supplies 11 days after germination. Growth conditions are described in Figure 1. Black columns: Col-0, white columns: Pyl-1. n = 12 observations ± std. Data are analyzed with multiple t-tests, and the different letters allow for visualizing the significant differences. Values sharing the same letter are not significantly different (p-value > 0.05). (c) Microscopic pictures illustrate nine stages of lateral root primordium development in Col-0, indicated by Roman numbers I–VII (initiation to emergence through parental tissues) and E (primordium emerged from the epidermis). Scale bar: 20 µm. (d) The distribution of lateral root primordia (LRP) between developmental stages I–VIII, E and LR (mature lateral root of strictly more than 1 mm). n = 12 observations.
Figure 3. Lateral root primordium quantification of Pyla-1 and Columbia-0 accessions in response to nitrate supply. The total number of lateral root primordia (NLRP) (a) and the density of lateral root primordia (DLRP) (b) were measured under 0.1, 1, 10, 25 and 50 mM nitrate supplies 11 days after germination. Growth conditions are described in Figure 1. Black columns: Col-0, white columns: Pyl-1. n = 12 observations ± std. Data are analyzed with multiple t-tests, and the different letters allow for visualizing the significant differences. Values sharing the same letter are not significantly different (p-value > 0.05). (c) Microscopic pictures illustrate nine stages of lateral root primordium development in Col-0, indicated by Roman numbers I–VII (initiation to emergence through parental tissues) and E (primordium emerged from the epidermis). Scale bar: 20 µm. (d) The distribution of lateral root primordia (LRP) between developmental stages I–VIII, E and LR (mature lateral root of strictly more than 1 mm). n = 12 observations.
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Figure 4. Time course of lateral root primordium development in Columbia-0 and Pyla-1 accessions. Developmental stages (from I to VIII) were determined every 6 h post-stimulus and were represented as a percentage of the total number of induced lateral root primordia (LRP) in Col-0 (a) and Pyl-1 (b). Bending assays were conducted on media containing 10 mM nitrate. n = 25–30 observations.
Figure 4. Time course of lateral root primordium development in Columbia-0 and Pyla-1 accessions. Developmental stages (from I to VIII) were determined every 6 h post-stimulus and were represented as a percentage of the total number of induced lateral root primordia (LRP) in Col-0 (a) and Pyl-1 (b). Bending assays were conducted on media containing 10 mM nitrate. n = 25–30 observations.
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Porco, S.; Haelterman, L.; De Pessemier, J.; De Gernier, H.; Reyé, F.; Hermans, C. The Pyla-1 Natural Accession of Arabidopsis thaliana Shows Little Nitrate-Induced Plasticity of Root Development. Nitrogen 2022, 3, 444-454. https://0-doi-org.brum.beds.ac.uk/10.3390/nitrogen3030029

AMA Style

Porco S, Haelterman L, De Pessemier J, De Gernier H, Reyé F, Hermans C. The Pyla-1 Natural Accession of Arabidopsis thaliana Shows Little Nitrate-Induced Plasticity of Root Development. Nitrogen. 2022; 3(3):444-454. https://0-doi-org.brum.beds.ac.uk/10.3390/nitrogen3030029

Chicago/Turabian Style

Porco, Silvana, Loïc Haelterman, Jérôme De Pessemier, Hugues De Gernier, Florence Reyé, and Christian Hermans. 2022. "The Pyla-1 Natural Accession of Arabidopsis thaliana Shows Little Nitrate-Induced Plasticity of Root Development" Nitrogen 3, no. 3: 444-454. https://0-doi-org.brum.beds.ac.uk/10.3390/nitrogen3030029

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