Research Article | Open Access
Influence of Biostimulants on Important Traits of Zinnia elegans Jacq. under Open Field Conditions
The efficacy of microbial treatment on growth, yield, and nutrient uptake is very well acknowledged for field crops. However, the use of microbes for Zinnia elegans has rarely been exploited under field trials. Therefore, in this study, we have evaluated the efficacy of different microbial bioinoculants on sixteen morphological and nine biochemical traits of Z. elegans. We used two arbuscular mycorrhizal fungi (AMF) (Glomus mosseae (G) and Acaulospora laevis (A)) along with Trichoderma viride (T) and Pseudomonas florescence (P) as five different treatments under open field conditions, in a randomized complete block design. There were significant differences for all of the traits studied. Treatment 5 (G + A + T + P) was noted as the best treatment for the improvement of morphological characters, whereas Treatment 4 (G + A + P) was most significant for the biochemical trait improvement in Z. elegans. Overall, this study provides useful insight into the bioinoculant treatment that can be applied to improve the yield and flower quality of Z. elegans under open field conditions.
Zinnia elegans Jacq., a member of family Asteraceae, is an important summer garden flower with diverse shade of colours . Z. elegans can accumulate heavy metals like cadmium in its shoots; therefore, it can be used as an eradication treatment for soils contaminated with heavy metals [2, 3]. Z. elegans can tolerate harsh environmental conditions, and its production on marginal lands during harsh summer is preferred under north Indian conditions . In order to get above average production, the use of heavy dosages of chemical fertilizers is not uncommon. But, chemical fertilizers alter the soil nutrient profile and could result in water and air pollution . Hence, there is a need to identify sustainable and eco-friendly practices for higher production, and the use of microbial inoculants is one of the commonly used sustainable approaches .
Microbes especially the arbuscular mycorrhizal fungi (AMF) has a significant influence on the terrestrial ecosystem where they perform a key role in providing ecosystem services and species richness [7, 8]. AMF is the obligate association of plant roots with beneficial fungi (belonging to either basidiomycetes and ascomycetes clades), and it is well recognized that vascularophytes get up to 86% of their nutrients and water requirements via mycorrhization, whereas their host plant supports fungal partner in its carbon requirement [9, 10]. This mycorrhizal association along with different kinds of soil microbiota like Trichoderma viride and Pseudomonas fluorescens acts as biostimulants, in order to significantly improve the uptake of even less mobile elements like phosphorous [11, 12]. Biostimulants treatment as compared to soil fertilizers improves floral traits as well as soil nutrient profile, even with its small quantities [13, 14].
Over a course of time, AMF has established a healthy relationship in several plant hosts, for example, Pelargonium peltatum showed an increased shoot phosphorous/potassium concentrations and flower numbers when inoculated by AMF culture . Another study reported that microbial inoculation in hyacinth has resulted in the higher concentration of N, P, and K in hyacinth flower . Likewise, Pseudomonas fluorescens is a Gram-negative rhizobacterium well known for its role in plant development . Trichoderma viride is popular for its use in floriculture practices, in order to obtain better plant growth by assisting the AMF species already present in the soil .
Pseudomonas fluorescence and Trichoderma viride work as the mycorrhizal helper, and these are well demonstrated to promote mycorrhizal development as well as to provide immunity against plant pathogens like Pythium sp. . Several microbial treatments are known for their positive effect in different flowering plants [20–22]. However, the effect of AMF treatment alone or in combination with Pseudomonas fluoresces and Trichoderma viride on the roots of Z. elegans under open field condition has not been explored. Although, we have shown the effects of these microbes for Zinnia elegans under polyhouse conditions . Nonetheless, the behaviour of microbial treatment under open field conditions is still unknown Therefore, the main objective of our study was to select the best and efficient microbial amalgamation among Glomus mosseae (Funelliformis mosseae), Acaulospora laevis, Pseudomonas fluoresces, and Trichoderma viride for Z. elegans under open field conditions.
2. Materials and Methods
2.1. Study Area and Experimental Design
The experiment was conducted at Botanical Garden of Kurukshetra University, Haryana, India. The site soil was sandy loam in texture with a pH of 8.2. However, the soil nutrients were determined as 0.35 mg nitrogen kg−1, 1.68 mg phosphorous kg−1, and 22.98 mg potassium kg−1 following the package and practices provided elsewhere . Further, the indigenous density of AMF spores was 26 ± 5 spores 10−1 g soil which was counted by the gridline intersect method of Adholeya and Gaur , whereas the soil diversity of AMF species was assessed and the major constituents identified were Glomus mosseae, G. convolutum, Acaulospora elegans, A. laevis, and Scutellospora calospora using different manuals [25–27].
The experiment was laid out from April 2018 to July 2018 in a random complete block design (RCBD) with a total of six treatments grown across six separate flowerbeds (thoroughly ploughed) with ten plantlets per treatment. The plot size was 1 × 2 m, that was parted by a 0.25 m wide alleyway. In our previous work, a pot experiment was performed in polyhouse condition and five treatments were identified promising, i.e., Glomus mosseae + Acaulospora laevis (Treatment 1), G. mosseae + Trichoderma viride (Treatment 2), G. mosseae + A. laevis + T. viride (Treatment 3), G. mosseae + A. laevis + Pseudomonas florescence (Treatment 4), and G. mosseae + A. laevis + T. viride + P. florescence (Treatment 5). Hence, these treatments were selected for the open field trail along with the control (Treatment 0), to assess the best treatment for growers as these microbes are also naturally present in the soil . Therefore, to validate the effect of bioinoculant formulation under open field conditions, this experiment was carried out using the treatments provided in Table 1.
2.2. Plant Inoculation
For treatments (T1–T5), each plantlet was supplemented with uniform supply of AMF inoculum at the rate of 100 g/plant around the roots of plantlets containing 670–700 AMF spores counted by Adholeya and Gaur  method and at least 80–85% of AM infection assessed by “Rapid Clearing and Staining Method” of Phillips and Hayman ; this treatment was followed by immediate watering. Roots were dipped for 10 minutes for P. florescence treatment, that was cultured in nutrient broth medium. Pseudomonas fluorescens for the inoculation was applied at a concentration of 1 × 109 colony mL−1. In case where T. viride treatment (density 3.4 108 CFU g−1 per treatment) was applied, CFU/g (colony-forming units per Gram) determination was based on the following formula: CFU/g = (no. of colonies × dilution factor)/weight of the culture plate.
2.3. Plant Characterization and Data Analysis
After 120 days, 6–7 plants were randomly selected and used for the measurement of traits. Morphological parameters were measured as root length (cm), shoot length (cm), and total leaf area (cm2) at the harvest stage. Initial values of root fresh weight (g), shoot fresh weight (g), and leaf fresh weight (g) were used to determine the dry weight after over drying at 70°C. Whereas the number of floral heads and number of floret layers were measured at the full bloom stage. Floral heads were harvested at maturity for measuring the diameter and for fresh and dry weight. AMF diversity and AM spore quantification were noted from the rhizosphere of an uprooted plant, and a soil sample (∼20 g) was analyzed based on the method defined elsewhere . The AMF root colonization (%) was determined using the following formula: 100 × (number of root segments colonized/the total number of root segments).
Physiological parameters were analyzed as leaves samples were used to determine the total chlorophyll and carotenoid contents . Anthocyanin content was estimated from the floral head using the method given by Tsushida and Suzuki . Whereas root and shoot phosphatase activities were evaluated by the method of Tabatabai and Bremmer . Whereas the phosphorus content was determined based on “Jackson’s vanadomolybdo phosphoric acid yellow colour method” .
Means of each treatment were exposed to analyses of variance (ANOVA) to detect differences among the six groups. The significance of differences among group means was evaluated using the least significant differences (LSD) test. All these analyses were performed with the SPSS (11.5 version) software package . The correlation coefficients (r) and their values were estimated and plotted with the help of the package corrplot in the R environment .
The analysis of variance (ANOVA) revealed the presence of highly significant differences (<0.001) among all of the six treatment groups. The result pertaining to growth, yield, and physiological parameters is illustrated in Tables 2 and 3.
Means within rows separated by different letters are significantly different based on the least significant difference test (LSD).
Means within rows separated by different letters are significantly different based on the least significant difference test (LSD).
3.1. Morphological, Mycorrhization, and Yield Parameters
In the experiment, morphological growth parameters, namely, plant length, root length, and shoot and root weight as well as yield was found increased over control plants (Table 2). Up to 76% increment was noticed for the growth when inoculated by biostimulants. Plant height was noticed prominent in case of T5 (56 ± 5.8) having G. mosseae, A. laevis, T. viride, and P. fluorescens, altogether followed by T4 (50 ± 3.4) having G. mosseae, A. laevis and P. fluorescens (Table 2). The same pattern was observed in the case of root length, where the longest was T5 (17.09 ± 1.35) followed by T4 (16 ± 1.3) (Table 2). Similarly, fresh shoot (17.25 ± 1.358) and root (11.757 ± 1.082) weight, as well as dry shoot (2.294 ± 0.489) and root (1.044 ± 0.345) weight were found highest in T5 followed by T4 (Table 2). Whereas the total leaf area was found largest in T4 (35.33 ± 0.054) followed by T5 (32.31 ± 0.03) (Table 2).
Though there was a slight difference in both the treatments, T4 proved to be the leading treatment for yield and biochemical attributes (Table 2). T4 was found with the extreme mycorrhizal infection (63 ± 3.87) and the largest number of AM spore (153 ± 13.4) followed by T5 with 58% (±6.68) mycorrhization and 140 (±10.3) AM spore count (Table 2). The floral head weight (fresh weight: 5.4 ± 0.469; dry weight: 1.66 ± 0.315; floral head number: 10 ± 1.15) was too noted maximum in T4 followed by T5 (fresh weight: 5.02 ± 0.312; dry weight: 1.17 ± 0.176; floral head number: 9 ± 1.63) (Table 2). Although the floral head diameter was measured largest in T5 (10.24 ± 0.665) followed by T4 (9.8 ± 0.421), the number of floret layers was maximum in T4 (7 ± 0.816) as compared to T5 (Table 2). The shoot length and root length changes across different treatments are represented in Table 2 and Figure 1. Root colonization (%) was around six times higher in the consortium treatment T5 (G + A + T + P) as compared to control (T0) (Figure 1). Interestingly, root lengths were almost similar in case of treatment T2 and T5 (Figure 1).
3.2. Plant Physiological Responses
The morphological outcomes of a plant are also determined by physiological and biochemical traits . Plants with bioinoculants were observed with an improvement in all the physiological parameters considered for the experiment. Microbial colonization increased the total chlorophyll and carotenoid pigment content. Flower bed containing Treatment 4 (2.207 ± 0.236) was recorded with higher total chlorophyll and carotenoid content followed by T3 (1.797 ± 0.19) as compared to control T0 (0.059 ± 0.031) (Table 3). Similarly, anthocyanin content was found the maximum in the Treatment 4 (2.363 ± 0.285) followed by T3 (2.008 ± 0.121) (Table 3). Likewise, the phosphatase activity was at par in the T4 (acidic phosphatase: 0.708 ± 0.159; alkaline phosphatase: 0.961 ± 0.123). Correspondingly, phosphorous content was highest in the same treatment, i.e., T4 (root phosphorous: 3.746 ± 0.278; shoot phosphorous: 3.292 ± 0.197) (Table 3). Overall, for the biochemical traits, there were several fold differences among the treatments and T4 (G + A + P) was the best treatment for all of the biochemical traits (Table 3). The correlation analysis showed the presence of significant () and positive correlation for all of the traits studied (Figure 2).
In order to determine the microbial inoculant treatment, it is important to know the practicality and feasibility of microbes, especially of their combined formulation, as different microbes have a different degree of colonization and specificity . As anticipated, we have observed a significant improvement with bioinoculants treatment in Z. elegans for important morphological and biochemical traits in Zinnia elegans. AMF is a well-known enhancer of water absorption along with macro and micronutrients uptake via extraradical hyphae emerging from infected their host plants root system . This ought to be the reason for a significant increase in all important morphological traits of Z. elegans in our field study. Previously, with AMF treatment improvement for several morphological traits were recorded for other flower crops like Lilium, rose, and gazania [12, 38–40]. Likewise, an investigation carried out by Lazzara et al.  reported that inoculation with AMF noticeably increased the flower size and number, in Snapdragon and Hypericum perforatum.
AMF is a well-known regulator of plant auxins and gibberellins content and both are crucial for promotes flower development; this supports our finding of increased flower weight and diameter in Zinnia elegans . Increased phytohormones especially the auxins stimulate the lateral roots formation owing to absorb more water and minerals . A significant increase in total chlorophyll and carotenoid content was found to be increased which could be due to improved stomatal conductance . Earlier, it was suggested that AMF treatment considerably improves the host growth by proving an important iron chelating low molecular weight “siderophores” which are beneficial for the photosynthesis and respiration in plants, ultimately enhancing the floral quantitative and qualitative characteristics [37, 45, 46].
Caser et al.  and Saini et al.  studied that AMF-inoculated plants showed an increase in secondary metabolites and various pharmacologically active compounds which is why the amount of anthocyanin had increased considerably in treated plants of saffron and Gazania elegans, respectively, probably the reason for increases in anthocyanin content. Lingua et al.  also confirmed that on inoculating AMF and Pseudomonas sp., useful secondary metabolites like anthocyanin along with phosphatase activity got increased.
Somewhat surprisingly, there were positive correlations among all of the traits studied, confirming that bioinoculants have an overall positive effect on all important traits for Z. elegans. Findings of Rouphael et al.  are in accordance with our results that biostimulants produce hydrolases and phosphatases enzymes more efficiently as compared to noninoculated treatments, and this could be the reason of improved phosphatase activity. Furthermore, an increased phosphatase activity results in the rise of phosphorous content in the root and shoot even under nutrient deficit condition . Fonte et al.  also concluded that biostimulants trigger phosphatase enzyme which solubilizes and mobilizes inorganic phosphorous in root microbiota. Inorganic phosphorous has a slow rate of solubilization; hence, its absorption is slow but the application of AMF during floricultural practices increased the mobilization of phosphorous allowing co-transport of phosphorous toward host root . It is already documented that AMF improves the phosphorous uptake even under phosphorous stress conditions .
AMF like Glomus and Acaulospora is the most dominant foremost mycorrhizal fungi almost ubiquitous in nature are now being used in the agriculture system around the world as phosphorus biostimulants . So it is advisable that AM fungi can be seen as an exciting alternative to minimize crop dependency on phosphorous fertilizers, and their actual impact is currently strongly debated by several groups since contrasting effects of AM colonization on plant phosphorous nutrition have been reported [54–56].
In our experiment, inoculation treatment with biofertilizers of field-grown Zinnia elegans and conglomerate treatment of AMF and Pseudomonas fluorescence gave the best results in terms of plant growth and flower yield. As a result of the amalgamation of these biofertilizers, all the biochemical parameters do get increased. So it can be concluded that mycorrhizal fungi can increase the flower development by stimulating phytohormones and nutrient availability. Therefore, it is advised that the application of AMF during cultivation of floral products should be considered for the betterment of plant as well as soil ecosystem.
The data used to support the findings of this study are included in the article.
Conflicts of Interest
The authors declare that there are no conflicts of interest regarding the publication of this paper.
- Y. Gu, “Cut flower productivity and economic analysis, polyploidy induction in two Zinnia varieties, Zinnia pollination mechanisms and DNA content of Zinnia species,” pp. 75–88, 2015.
- W.-T. Chen, C.-C. Chen, Y.-C. Wang, and Y.-R. Chen, “Distribution of cadmium and its effect on growth of Zinnia elegans,” Taiwania, vol. 46, no. 4, pp. 295–306, 2001.
- D. Thamayanthi and P. S. Sharavanan, “Phytoaccmulation of cadmium polluted soil using Zinnia plants (Zinnia elegans L.),” International Journal of Current Science, pp. 311–315, 2012.
- C. Gabaldón, L. V. G. Ros, M. A. Pedreño, and A. R. Barceló, “Nitric oxide production by the differentiating xylem of Zinnia elegans,” New Phytologist, vol. 165, no. 1, pp. 121–130, 2005.
- M. N. Khan, M. Mobin, Z. K. Abbas, and S. A. Alamri, “Fertilizers and their contaminants in soils, surface and groundwater,” in Reference Module in Earth Systems and Environmental Sciences, D. A. Dellasala and M. I. Goldstein, Eds., pp. 225–240, Elsevier, Oxford, UK, 2018, Encyclopedia of the Anthropocene.
- J. S. Singh, V. C. Pandey, and D. P. Singh, “Efficient soil microorganisms: a new dimension for sustainable agriculture and environmental development,” Agriculture, Ecosystems & Environment, vol. 140, no. 3-4, pp. 339–353, 2011.
- M. G. A. van der Heijden, R. D. Bardgett, and N. M. van Straalen, “The unseen majority: soil microbes as drivers of plant diversity and productivity in terrestrial ecosystems,” Ecology Letters, vol. 11, no. 3, pp. 296–310, 2008.
- E. Barrios, “Soil biota, ecosystem services and land productivity,” Ecological Economics, vol. 64, no. 2, pp. 269–285, 2007.
- N. Corradi and P. Bonfante, “The arbuscular mycorrhizal symbiosis: origin and evolution of a beneficial plant infection,” PLoS Pathogens, vol. 8, no. 4, Article ID e1002600, 2012.
- M. Chen, M. Arato, L. Borghi, E. Nouri, and D. Reinhardt, ““Beneficial services of arbuscular mycorrhizal fungi from ecology to application,” Frontiers in Plant Science, vol. 9, 2018.
- I. Saini, K. Yadav, and A. Aggarwal, “Effect of bioinoculants on morphological and biochemical parameters of Zinnia elegans Jacq,” Journal of Applied Horticulture., vol. 19, no. 2, 2017.
- I. Saini, A. Aggarwal, P. Kaushik, I. Saini, A. Aggarwal, and P. Kaushik, “Inoculation with mycorrhizal fungi and other microbes to improve the morpho-physiological and floral traits of Gazania rigens (L.) gaertn,” Agriculture, vol. 9, no. 3, p. 51, 2019.
- H.-J. Kim, K.-M. Ku, S. Choi et al., “Vegetal-derived biostimulant enhances adventitious rooting in cuttings of basil, tomato, and Chrysanthemum via brassinosteroid-mediated processes,” Agronomy, vol. 9, no. 2, p. 74, 2019.
- A. Bargaz, K. Lyamlouli, M. Chtouki, Y. Zeroual, and D. Dhiba, “Soil microbial resources for improving fertilizers efficiency in an integrated plant nutrient management system,” Frontiers in Microbiology, vol. 9, 2018.
- H. Perner, D. Schwarz, C. Bruns, P. Mäder, and E. George, “Effect of arbuscular mycorrhizal colonization and two levels of compost supply on nutrient uptake and flowering of pelargonium plants,” Mycorrhiza, vol. 17, no. 5, pp. 469–474, 2007.
- M. M. Xie and Q. S. Wu, “Mycorrhiza modulates morphology, color and duration of flowers in hyacinth,” Biotechnology, vol. 16, no. 3, pp. 116–122, 2017.
- B. V. David, G. Chandrasehar, and P. N. Selvam, “Pseudomonas fluorescens: a plant-growth-promoting rhizobacterium (PGPR) with potential role in biocontrol of pests of crops,” in Crop Improvement Through Microbial Biotechnology, pp. 221–243, 2018.
- A. Yadav, K. Yadav, and A. Aggarwal, “Impact of arbuscular mycorrhizal fungi withTrichoderma virideandPseudomonas fluorescenson growth, yield and oil content inHelianthus annuusL,” Journal of Essential Oil Bearing Plants, vol. 18, no. 2, pp. 444–454, 2015.
- P. Frey‐Klett, J. Garbaye, and M. Tarkka, “The mycorrhiza helper bacteria revisited,” New Phytologist, vol. 176, no. 1, pp. 22–36, 2007.
- M. Saleem, N. Meckes, Z. H. Pervaiz, and M. B. Traw, “Microbial interactions in the phyllosphere increase plant performance under herbivore biotic stress,” Frontiers in Microbiology, vol. 8, 2017.
- J. Schirawski and M. H. Perlin, “Plant–Microbe interaction 2017—the good, the bad and the diverse,” International Journal of Molecular Sciences, vol. 19, no. 5, p. 1374, 2018.
- A. C. Abreu, A. Coqueiro, A. R. Sultan et al., “Looking to nature for a new concept in antimicrobial treatments: isoflavonoids from Cytisus striatus as antibiotic adjuvants against MRSA,” Scientific Reports, vol. 7, no. 1, p. 3777, 2017.
- K. Bandyopadhyay, P. Aggarwal, D. Chakraborty, S. Pradhan, R. Narayan Garg, and R. Singh, Practical Manual on Measurement of Soil Physical Properties Practical, 2012.
- A. Adholeya and A. Gaur, “Estimation of VAM fungal spores in soil,” Mycorrhiza News, vol. 6, no. 1, pp. 10-11, 1994.
- N. C. Schenck and Y. Pérez, Manual for the Identification of VA Mycorrhizal Fungi, Synergistic Publications, Gainesville, FL, USA, 1990.
- C. Walker, “Taxonomic concepts in the Endogonaceae: spore wall characteristics in species descriptions,” Mycotaxon, vol. 18, pp. 443–455, 1983.
- J. B. West, V. U. Morton, and G. L. Benny, Revised classification of arbuscular mycorrhizal fungi (Zygomycetes): a new Order, Glomales, two new suborders, Glomineae and Gigasporineae, and two new families, Acaulosporaceae and Gigasporaceae, with an emendation of Glomaceae, Mycotaxon, Ithaca, NY, USA, 1990.
- J. M. Phillips and D. S. Hayman, “Improved procedures for clearing roots and staining parasitic and vesicular-arbuscular mycorrhizal fungi for rapid assessment of infection,” Transactions of the British Mycological Society, vol. 55, no. 1, pp. 158–161, 1970.
- J. W. Gerdemann and T. H. Nicolson, “Spores of mycorrhizal Endogone species extracted from soil by wet sieving and decanting,” Transactions of the British Mycological Society, vol. 46, no. 2, pp. 235–244, 1963.
- T. Tsushida and M. Suzuki, “Flavonoid in fruits and vegetables part I. Isolation of flavonoid-glycosides in onion and identification by chemical synthesis of the glycosides,” Nippon Shokuhin Kagaku Kogaku Kaishi, vol. 42, no. 2, pp. 100–108, 1995.
- M. A. Tabatabai and J. M. Bremner, “Use of p-nitrophenyl phosphate for assay of soil phosphatase activity,” Soil Biology and Biochemistry, vol. 1, no. 4, pp. 301–307, 1969.
- M. L. Jackson, “Vanadomolybdo phosphoric yellow colour method for determination of phosphorus,” in Soil Chemical Analysis, pp. 151–154, Prentice Hall of India Pvt. Ltd., New Delhi, India, 1973.
- N. H. Nie, D. H. Bent, and C. H. Hull, SPSS: Statistical Package for the Social Sciences, McGraw-Hill, New York, NY, USA, 1975.
- T. Wei, V. Simko, M. Levy, Y. Xie, Y. Jin, and J. Zemla, Corrplot: Visualization of a Correlation Matrix, 2017.
- C. Guo, L. Ma, S. Yuan, and R. Wang, “Morphological, physiological and anatomical traits of plant functional types in temperate grasslands along a large-scale aridity gradient in northeastern China,” Scientific Reports, vol. 7, no. 1, Article ID 40900, 2017.
- A. Ambrosini, R. de Souza, and L. M. P. Passaglia, “Ecological role of bacterial inoculants and their potential impact on soil microbial diversity,” Plant and Soil, vol. 400, no. 1-2, pp. 193–207, 2016.
- M. Agnolucci, F. Battini, C. Cristani, and M. Giovannetti, “Diverse bacterial communities are recruited on spores of different arbuscular mycorrhizal fungal isolates,” Biology and Fertility of Soils, vol. 51, no. 3, pp. 379–389, 2015.
- A. Varshney, M. P. Sharma, A. Adholeya, V. Dhawan, and P. S. Srivastava, “Enhanced growth of micropropagated bulblets ofLiliumsp. inoculated with arbuscular mycorrhizal fungi at different P fertility levels in an alfisol,” Journal of Horticultural Science and Biotechnology, vol. 77, no. 3, pp. 258–263, 2002.
- R. Kapoor, D. Sharma, and A. K. Bhatnagar, “Arbuscular mycorrhizae in micropropagation systems and their potential applications,” Scientia Horticulturae, vol. 116, no. 3, pp. 227–239, 2008.
- I. Garmendia and V. J. Mangas, “Application of arbuscular mycorrhizal fungi on the production of cut flower roses under commercial-like conditions,” Spanish Journal of Agricultural Research, vol. 10, no. 1, pp. 166–174, 2012.
- S. Lazzara, M. Militello, A. Carrubba, E. Napoli, and S. Saia, “Arbuscular mycorrhizal fungi altered the hypericin, pseudohypericin, and hyperforin content in flowers of Hypericum perforatum grown under contrasting P availability in a highly organic substrate,” Mycorrhiza, vol. 27, no. 4, pp. 345–354, 2017.
- L. Zhang, J. Fan, X. Ding, X. He, F. Zhang, and G. Feng, “Hyphosphere interactions between an arbuscular mycorrhizal fungus and a phosphate solubilizing bacterium promote phytate mineralization in soil,” Soil Biology and Biochemistry, vol. 74, pp. 177–183, 2014.
- D. Duca, J. Lorv, C. L. Patten, D. Rose, and B. R. Glick, “Indole-3-acetic acid in plant-microbe interactions,” Antonie Van Leeuwenhoek, vol. 106, no. 1, pp. 85–125, 2014.
- K. Boldt, Y. Pörs, B. Haupt et al., “Photochemical processes, carbon assimilation and RNA accumulation of sucrose transporter genes in tomato arbuscular mycorrhiza,” Journal of Plant Physiology, vol. 168, no. 11, pp. 1256–1263, 2011.
- A. Jilling, M. Keiluweit, A. R. Contosta et al., “Minerals in the rhizosphere: overlooked mediators of soil nitrogen availability to plants and microbes,” Biogeochemistry, vol. 139, no. 2, pp. 103–122, 2018.
- T. Kobayashi and N. K. Nishizawa, “Iron uptake, translocation, and regulation in higher plants,” Annual Review of Plant Biology, vol. 63, no. 1, pp. 131–152, 2012.
- M. Caser, Í. M. M. Victorino, S. Demasi et al., “Saffron cultivation in marginal alpine environments: how AMF inoculation modulates yield and bioactive compounds,” Agronomy, vol. 9, no. 1, p. 12, 2019.
- G. Lingua, E. Bona, P. Manassero et al., “Arbuscular mycorrhizal fungi and plant growth-promoting pseudomonads increases anthocyanin concentration in strawberry fruits (Fragaria x ananassa var. Selva) in conditions of reduced fertilization,” International Journal of Molecular Sciences, vol. 14, no. 8, pp. 16207–16225, 2013.
- Y. Rouphael, P. Franken, C. Schneider et al., “Arbuscular mycorrhizal fungi act as biostimulants in horticultural crops,” Scientia Horticulturae, vol. 196, pp. 91–108, 2015.
- S. J. Fonte, M. Nesper, D. Hegglin et al., “Pasture degradation impacts soil phosphorus storage via changes to aggregate-associated soil organic matter in highly weathered tropical soils,” Soil Biology and Biochemistry, vol. 68, pp. 150–157, 2014.
- M. Toro, R. Azcon, and J. Barea, “Improvement of arbuscular mycorrhiza development by inoculation of soil with phosphate-solubilizing rhizobacteria to improve rock phosphate bioavailability ((sup32)P) and nutrient cycling,” Applied and Environmental Microbiology, vol. 63, no. 11, pp. 4408–4412, 1997.
- H. Li, S. E. Smith, R. E. Holloway, Y. Zhu, and F. A. Smith, “Arbuscular mycorrhizal fungi contribute to phosphorus uptake by wheat grown in a phosphorus-fixing soil even in the absence of positive growth responses,” New Phytologist, vol. 172, no. 3, pp. 536–543, 2006.
- J.-E. Lee and A.-H. Eom, “Effect of organic farming on spore diversity of arbuscular mycorrhizal fungi and glomalin in soil,” Mycobiology, vol. 37, no. 4, pp. 272–276, 2009.
- W. Liu, Y. Zhang, S. Jiang et al., “Arbuscular mycorrhizal fungi in soil and roots respond differently to phosphorus inputs in an intensively managed calcareous agricultural soil,” Scientific Reports, vol. 6, no. 1, 2016.
- M. Sharma, P. Kaushik, and P. Chaturvedi, “Enumeration, antagonism and enzymatic activities of microorganisms isolated from railway station soil,” Article ID 454595, 2018, bioRxiv.
- I. Saini, K. Yadav, and A. Aggarwal, “Response of arbuscular mycorrhizal fungi along with Trichoderma viride and Pseudomonas fluorescens on the growth, biochemical attributes and vase life of Chrysanthemum indicum,” Journal of Environmental Biology, vol. 40, no. 2, pp. 183–191, 2018.
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