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Article

Strain-Specific Biostimulant Effects of Chlorella and Chlamydomonas Green Microalgae on Medicago truncatula

by
Margaret Mukami Gitau
1,
Attila Farkas
1,
Benedikta Balla
1,
Vince Ördög
2,3,
Zoltán Futó
4 and
Gergely Maróti
1,5,*
1
Institute of Plant Biology, Biological Research Center, 6726 Szeged, Hungary
2
Department of Plant Sciences, Faculty of Agricultural and Food Sciences, Széchenyi István University, 9246 Mosonmagyaróvár, Hungary
3
Research Centre for Plant Growth and Development, School of Life Sciences, Campus Pietermaritzburg, University of KwaZulu-Natal, 3201 Scottsville, Pietermaritzburg, South Africa
4
Department of Irrigation Development and Melioration, Hungarian University of Agriculture and Life Sciences, 5540 Szarvas, Hungary
5
Department of Water Sciences, University of Public Service, 6500 Baja, Hungary
*
Author to whom correspondence should be addressed.
Plants 2021, 10(6), 1060; https://doi.org/10.3390/plants10061060
Submission received: 30 April 2021 / Revised: 17 May 2021 / Accepted: 21 May 2021 / Published: 25 May 2021
(This article belongs to the Special Issue Biostimulants as Growth Promoting and Stress Protecting Compounds)
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Abstract

:
Microalgae have been identified to produce a plethora of bioactive compounds exerting growth stimulating effects on plants. The objective of this study was to investigate the plant-growth-promoting effects of three selected strains of eukaryotic green microalgae. The biostimulatory effects of two Chlorella species (MACC-360 and MACC-38) and a Chlamydomonas reinhardtii strain (cc124) were investigated in a Medicago truncatula model plant grown under controlled greenhouse conditions. The physiological responses of the M. truncatula A17 ecotype to algal biomass addition were characterized thoroughly. The plants were cultivated in pots containing a mixture of vermiculite and soil (1:3) layered with clay at the bottom. The application of live algae cells using the soil drench method significantly increased the plants’ shoot length, leaf size, fresh weight, number of flowers and pigment content. For most of the parameters analyzed, the effects of treatment proved to be specific for the applied algae strains. Overall, Chlorella application led to more robust plants with increased fresh biomass, bigger leaves and more flowers/pods compared to the control and Chlamydomonas-treated samples receiving identical total nutrients.

1. Introduction

The human population has significantly increased over the past few decades. This increase has raised the demand for food but reduced land for crop production because of urbanization and clearance for human settlement. To increase food supply, chemical fertilizers have been used for various crops including forage and food crops. Unfortunately, chemical fertilizers have detrimental effects on the environment as they cause accumulation of nitrogen and phosphorous to harmful levels. The accumulated nutrients alter the balance in most ecosystems and hence reduce biodiversity. Additionally, chemical fertilizers no longer have a significant impact on crop yield unless when used at high concentrations, which is not economical for farmers.
Since the global demand for food is projected to double by 2050 [1], it is imperative to find alternatives to increase crop production. There is a need for novel agricultural methods that promote sustainable use of natural resources, such as salty water, and allow reclamation of polluted lands. Biostimulants from seaweeds [2,3,4,5,6,7,8,9], plants [10,11,12] and microorganisms (monocultures and co-cultures) [13,14,15,16,17,18] have been found to improve plant growth and yield in several plant species under normal as well as stressful conditions. However, preparation of these biostimulants requires high energy and is labor intensive in most cases. While seaweeds are abundant in the seas, continuous harvesting alters the water ecosystems, and at some point the seaweed population might be depleted. Plants, on the other hand, require fertile land for cultivation and may take a long time to grow sufficient biomass for biostimulant processing. In contrast, microorganisms multiply rapidly but may require special media and facilities for mass cultivation and biomass processing.
Microalgae (MA) represent a group of photosynthetic microorganisms that grow rapidly not only in clean but also in wastewater in natural association with bacteria and fungi. Studies have shown that most eukaryotic green microalgae produce a plethora of bioactive compounds with a wide range of applications in several sectors such as animal feed, human food, pharmaceuticals, aquaculture and hydroponic crop production [19,20,21,22,23]. Thus, MA represent a viable alternative for biostimulant/biofertilizer production since they can be incorporated into various systems such as wastewater management or aquaculture and hydroponic crop production. To increase the environmental impact of MA use in agriculture, live cell suspension or whole algae cultures cultivated in wastewater can be used for application to soil (or plants) [10,24,25], eliminating the need for expensive clean water and mineral addition for farming. This process also eradicates energy expenditure in extraction procedures or wastewater management. Algae biomass can be concentrated by flocculation (using bacterial or fungal co-culture, which also promotes biomass accumulation) [26,27,28]. Overall, using live MA cells in agriculture saves water, chemicals/fertilizers, energy, time and space.
Medicago truncatula is a model plant of the Fabaceae family, the third largest angiosperm family, which, after the Gramineae (Poaceae) family, is the most important to humans [29]. Several commercial crops such as soybean, garden pea, peanut and alfalfa, the world’s most cultivated and most valuable forage plant, belong to this family. These plants can fix nitrogen and are, therefore, important sources of oil and protein for animals and humans. In addition, they sequester carbon, which makes them promising candidates for fuelwood. Although most studies on legumes focus on their interaction with plant-growth-promoting rhizobacteria (PGPR), a few studies evaluate the effect of seaweed and MA biostimulants on these plants including Phaseolus vulgaris [7,30], Vigna radiata [6,31,32], Glycine max [33,34] and Medicago sativa [35,36,37]. In plant biostimulant studies, MA were administered to plants in the form of extracts [32,38,39,40], dry biomass [41,42,43,44,45], spent medium/supernatant [46,47], whole cultures [46] as well as cell suspensions [47,48], and desirable results were achieved. Application of the same MA strain’s dry biomass, liquid fertilizer and foliar application all led to positive results, although foliar application had greater effects [49]. Overall, the desirable results relative to the controls were observed irrespective of the application method of MA. This implies that MA indeed had positive effects on plants, although the effects may be dependent on species, cultivar, concentration and mode of application [29]. Monocultures [41] as well as co-cultures of eukaryotic green algae with other green algae, bacteria, cyanobacteria, fungi and all together have all shown plant growth stimulation [34,50,51,52,53,54]. However, to the best of our knowledge, no study sought to elucidate the effects of axenic monocultures of Chlorophyta microalgae without any other accompanying microbes on M. truncatula plants.
In most studies on the effect of MA on plants, Chlorella [42,47,48,49,55,56,57,58,59], Scenedesmus [32,34,39] and the cyanobacterium Arthrospira (Spirulina) [60,61,62] species have been investigated for their potential biostimulatory effect on a whole range of plants including corn, spinach, Chinese chives, onions, lettuce and tomatoes. Chlorella is the most popular because of its rapid growth and ability to thrive in a wide range of environmental conditions including adverse ones such as drought, saline, cold and hot habitats. In contrast, Chlamydomonas species remain unstudied and underutilized in agriculture despite being some of the most abundant microalgae species in natural soil ecosystems. This is despite the species’ rapid biomass accumulation and capacity to produce phytohormones such as auxins, ethylene, brassinosteroids, cytokinin and trehalose [63,64,65,66].
To fill the above identified gaps in research on MA as biostimulants, our study aimed to investigate the specific effects of selected green eukaryotic MA on M. truncatula grown under controlled greenhouse conditions. We conducted a comparative study of the growth-promoting effects of two Chlorella strains and one Chlamydomonas strain on M. truncatula when administered as live cells via the soil drench method. Our main focus was on parameters that additively determined yield and quality. These included plant structure/morphology, height, flower number, biomass and pigment content.

2. Results

2.1. Characterization of the Selected Microalgae Strains

2.1.1. Algae Growth and Morphology

All investigated green algae strains had reached a stationary phase by the 5th day according to optical density measurements (Figure 1a).
However, the cell numbers indicated that Chlorella MACC-360 had reached a plateau much earlier than the two other strains. Chlorella MACC-360 also had the highest number of cells, approximately 8-fold that of C. reinhardtii cc124 and 3-fold that of Chlorella MACC-38 (Figure 1b). The differences in cell numbers are attributable to the fact that Chlorella MACC-360 had a higher initial cell number value for the same optical density owing to its small cell size. In addition, Chlorella MACC-360 has a shorter cell division cycle compared to the other strains.
Scanning electron microscopy was applied to investigate the morphology and size of the applied green microalgae cells. The pictures revealed that the three strains were different with regards to size and surface texture. Chlorella MACC-38 (Figure 2a) had a rough surface, while C. reinhardtii cc124 and Chlorella MACC-360 appeared smooth (Figure 2b–d).
C. reinhardtii cc124 had the largest size followed by Chlorella MACC-38, and Chlorella MACC-360 was the smallest. Neither extracellular material nor cellular aggregations were present in Chlorella MACC-38 and C. reinhardtii cc124 cultures. In contrast, strong aggregations appeared in Chlorella MACC-360; the cells in these aggregations were joined to each other by filament-like extracellular material.

2.1.2. Extracellular Polysaccharide Production of the Selected Microalgae

Confocal laser scanning microscopy (CLSM) was used to investigate the potential production of the extracellular matrix. Seven-day-old MA cells were stained with calcofluor white (CFW) and concanavalin A (Con A) dyes (Figure 3). CFW dye binds to the β-D glucopyranose polysaccharides, while Con A binds to the α-D glucopyranose polysaccharides [67,68].
C. reinhardtii cc124 was not only larger in cell size than Chlorella species, but it was also different with respect to cell wall composition since CFW dye did not stain the Chlamydomonas cells. Chlorella species MACC-38 and MACC-360 had similar cell wall composition indicated by the blue fluorescence (Figure 3a,c, respectively). However, Chlorella MACC-38 was significantly larger in cell size than Chlorella MACC-360. In addition, MACC-38 did not form strong aggregates like Chlorella MACC-360 (Figure 3c).
Both Chlorella species were stained with dyes specific for polysaccharides. However, Chlorella MACC-38 produced polysaccharides that are localized in the cell wall, while Chlorella MACC-360 produced polysaccharides, which were secreted out of the cells. The CLSM pictures confirmed that the extracellular material observed under the scanning electron microscope was extracellular polysaccharides.
The most striking difference was the ability of Chlorella MACC-360 to produce EPS (green fluorescence from the third day (Figure S1, 360 C) of inoculation with the signal getting stronger with time as shown on day 5 (Figure 3c and Figure S1, 360 E). This implies that Chlorella MACC-360 accumulated EPS with time. Although the green fluorescence appeared on the C. reinhardtii cc124 cell walls, it is likely to bind to the sugars present in cell walls. This phenomenon highlighted another difference of C. reinhardtii cc124 and Chlorella MACC-360. Chlorella MACC-38 did not stain with Con A, implying that it neither produced EPS nor possessed cell wall sugars with affinity for Con A (Figure 3a).

2.2. Effect of Microalgae Application on Plant Architecture and Canopy Cover

Pictures taken on the 45th day of growth from an aerial view allowed visualization of canopy cover in terms of area covered by green plant material, while those of 50-day-old uprooted plants showed the root structure (Figure 4). Pots in which the plant tissue appeared dense were considered to have high biomass. In contrast, pots which appeared to have sparse plant/leaf tissue were considered to have less biomass.
It seemed that the same number (20) of control plants (Figure 4a) had less canopy cover than that of algae-treated plants (Figure 4b–d). C. reinhardtii cc124 and Chlorella MACC-360-treated (Figure 4c,d) plants were profusely branched and leafier than the control (Figure 4a). C. reinhardtii cc124 and Chlorella MACC-38-treated plants had slightly more canopy cover compared to the control. The images of the uprooted plants from C. reinhardtii cc124 and Chlorella MACC-360 regimes appeared to have more leaves and axillary branches compared to the control. In addition, C. reinhardtii cc124 and Chlorella MACC-360 treatments resulted in longer roots compared to the control plants. Plants from the C. reinhardtii cc124 regime had the longest roots based on the images (Figure 4c); the roots from Chlorella MACC-360-treated samples (Figure 4d) were moderately long, while the DW/Control (Figure 4a) and Chlorella MACC-38-treated samples (Figure 4b) appeared to have the least root biomass.

2.3. Effect of Microalgae Application on Leaf Parameters

Algae application caused changes in the leaf dimensions of plants (Figure 5). The leaf dimensions measured were petiole length, leaf blade length and leaf blade width (Figure 5a–f). These were measured according to Figure 5g, following the numerical nomenclature coding of M. truncatula [69]. According to this nomenclature, metamers are labelled from the bottom to the top along the main axis as M1, M2, M3 and so on (Figure 5g). A metamer is the plant part including an internode, a bud and a leaf. The developmental stage of the plant parts is denoted with a decimal code from the bud stage to the fully open blue-green leaf that ranges between 0.1 to 0.9. In our study, we assessed measurements from 50-day-old plants. Consequently, all the leaves were fully matured at this time and hence the ‘0.9′ code on all measurements.
All the strains reduced the petiole length of the first true leaf. The effects on the second and third leaves were negligible. In contrast, the MA increased leaf petiole length on the older leaves (M4.9 and M5.9). Chlorella MACC-38 and C. reinhardtii cc124 effects were stronger (12–32% increase) than those of 360 (2–9% increase). Overall, none of the strains significantly affected petiole length (Figure 5a,b).
Both Chlorella MACC-38 and C. reinhardtii cc124 decreased the blade length on plants during early development. However, they increased the blade length from the third leaf onwards. In contrast, Chlorella MACC-360 increased leaf blade length from the first leaf onwards (Figure 5c,d). The biggest change was observed on M4.9 at 11% and the smallest on M1.9 at 2%. Strain Chlorella MACC-38 slightly exceeded Chlorella MACC-360′s effect on M4.9 and M5.9 by increasing leaf blade length by 11% and 5%, respectively. Overall, the effects of algae treatment on blade length were strong during the development period between the third and fourth leaf (Figure 5d). Chlorella species had stronger effects on blade length than the Chlamydomonas sp. Overall, Chlorella MACC-360 is the only strain whose effects proved to be statistically significant.
All the algae treatments had a positive impact on leaf blade width throughout the growth period except for Chlorella MACC-38 during late development (Figure 5e,f). This effect was more pronounced during early development where it ranged between 2% in Chlorella MACC-38 to 16% in Chlorella MACC-360-treated plants for M2.9 to M4.9. C. reinhardtii cc124′s effect was strongest on the fourth leaf and dropped down in subsequent leaves. Overall, Chlorella MACC-360 had the most pronounced effect on leaf width; it significantly increased width of the fourth, fifth and sixth leaf by 15%, 12% and 9%, respectively (Figure 5f).
Thus, the different algae strains had different effects on leaf parameters. Their effects also differed at different developmental stages. Overall, their additive effects imply that they increased the leaf size/leaf area with Chlorella MACC-360 showing the most striking difference, which was even visible during data collection.

2.4. Effect of Microalgae Application on Plant Height, Flowers, Fresh Weight, Chlorophylls and Carotenoids

In addition to leaf dimensions, we assessed more phenotypic data to capture visible differences between treatments. We measured the following physiological parameters: plant height, fresh biomass, dry biomass and flower number. We also measured chlorophyll and carotenoid levels as the representative biochemical parameters (Figure 6).
C. reinhardtii cc124 and Chlorella MACC-360 increased plant height by 2% and 11%, respectively. In contrast, Chlorella MACC-38 decreased plant height by 2%. Only Chlorella MACC-360 had a significant impact on plant height (Figure 6a).
All the algae strains increased flower number per plant by 15%, 24% and 36% in Chlorella MACC-38, C. reinhardtii cc124 and Chlorella MACC-360 regimes, respectively. The increase resulting from Chlorella MACC-360 was statistically significant (Figure 6b).
All the algae treatments increased shoot fresh weight by a range of 3% to 31%. Chlorella MACC-38 had the least effect with a 3% increase followed by C. reinhardtii cc124 with 15% and Chlorella MACC-360 with 31%. Only Chlorella MACC-360 had significantly higher shoot fresh weight compared to the control (Figure 6c).
Strains C. reinhardtii cc124 and Chlorella MACC-360 increased root fresh weight by 18% and 31%, respectively. In contrast, Chlorella MACC-38 decreased root fresh weight by 8% (Figure 6c).
Overall, all the algae strains increased total fresh weight, Chlorella MACC-38 by 4%, C. reinhardtii cc124 by 21% and Chlorella MACC-360 by 36%. Nevertheless, only Chlorella MACC-360’s increase was statistically significant (Figure 6c).
Chlorella MACC-360 treatment increased shoot dry weight (18%) and total dry weight (14%) (Figure 4d). The treatments with the other two algae strains did not significantly influence dry weight. Interestingly, all algae treatments decreased root dry weight by 9%, 14% and 18% for Chlorella MACC-38, C. reinhardtii cc124 and Chlorella MACC-360 treatments, respectively. Overall, none of the algae strains had a significant effect on total dry weight of plants (Figure 4d).
C. reinhardtii cc124 remarkably increased chlorophyll levels, showing a 32%, 35% and 32% increase in chlorophyll a, b and total chlorophyll, respectively. In contrast, Chlorella MACC-38 had a negligible impact on chlorophyll a (0.3% increment), a moderate effect on chlorophyll b (15% increment) and little effect on total chlorophyll (3.7% increment). In contrast, Chlorella MACC-360 treatment decreased both chlorophyll a and total chlorophyll by 5% and 4%, respectively, while it slightly increased chlorophyll b content by 1% (Figure 6e).
All the algae strains remarkably increased carotenoid content in plants. Interestingly, Chlorella MACC-38 and Chlorella MACC-360 extremely increased carotenoids by 31%. The effect of C. reinhardtii cc124 (15% increase) on carotenoid levels was half that of the chlorella strains, although it was the most significantly different from the control (Figure 6f).
Overall, Chlorella MACC-360 and C. reinhardtii cc124 strains had a more striking effect on the M. truncatula than Chlorella MACC-38 (Figure 6).

3. Discussion

The vast majority of studies of growth promotion in M. truncatula and its relatives such as M. sativa concentrate on the effects of growth-promoting bacteria [18,70,71,72]. These studies especially focus on the mechanisms of these microorganisms in root development and nodulation but pay little attention to the plant architecture and leaf morphology. A few studies exist on plant growth stimulating seaweed extracts applied under normal [36] and salt stressed [35] conditions. However, no study has used living green microalgae cells for growth stimulation of legumes.
Microalgae application altered the development and shoot growth of M. truncatula in this study compared to the control conditions. The plant height, phyllotaxy and leaf size were significantly altered in response to microalgae treatment in an algae-strain-specific manner. Chlorella MACC-38-treated plants had similar phyllotaxy to the control. On the contrary, bifurcation (splitting into two branches) occurred on some C. reinhardtii cc124-treated plants, while Chlorella MACC-360-treated plants had extremely enhanced axillary shoot development. C. reinhardtii cc124-treated plants had deformities during the vegetative phase; they lost the main shoot and developed two long branches in comparison to the control. In addition, most of the plants lacked the unifoliate leaf and flowered significantly later. These plants also had reduced axillary shoot development, a characteristic of Headless (HDL1) mutants. This result could be attributed to changes in the HDL1 gene, which plays a role in the maintenance of shoot apical meristems (SAM) and leaf blade length determination. The phenotypes we observed are similar to those of HDL 1 mutants; they have heart-shaped leaves, stems are missing (dwarf plants) and impaired flower production was observed [73]. HDL1 was found to participate in auxin-dependent leaf morphogenesis [74] which implies that the C. reinhardtii cc124 treatment had an influence on auxin homeostasis in plants.
All applied microalgae species decreased leaf petiole and blade length at the early growth phase (M1.9) with the exception of Chlorella MACC-360, which increased blade length and width throughout the plant life. Chlorella MACC-38 and C. reinhardtii cc124 decreased blade length during juvenile stage but increased this parameter later on. Similar to Chlorella MACC-360, C. reinhardtii cc124 increased blade width throughout plant growth. In contrast, Chlorella MACC-38 treatment resulted in a slight decrease of blade length during the reproductive phase. Overall, all microalgae treatments increased the leaf size/area relative to control. This observation implies that the treated plants had more light-trapping capacity than the control and corresponds to the increased biomass. Another affected developmental milestone was flowering, where Chlorella MACC-360 induced early blooming while C. reinhardtii cc124 delayed flowering.
The observed results could be attributed to the possibility of differential regulation of specific plant genes involved in leaf development in M. truncatula. For example, Single leaf (SGL 1) and fused compound leaf (FCL1) genes have been found to regulate petiole development in M. truncatula, and mutations of both genes caused drastically reduced petioles [75]. Phantastica (MtPhan) has also been identified as a key regulator of petiole length. MtPhan suppresses elongated petiolule (ELP 1), which is responsible for organ mortality [76]. From our phenotypic results, it seems that algae reduced expression of MtPhan at the very first leaf, which consequently increased that ectopic expression of ELP1 in the rachis or petioles. Thus, the plants had reduced petiole length. It is possible that the reduced petioles could have become motor; this implies that the leaves could fold and unfold to control light intensity and reduce water loss. Thus, the young plants could be more efficient at photosynthesis than their control counterparts. The later increase in petiole length could be a strategy to reach out into open space to avoid shade as the plants become bushy. Overall, it is likely that algae treatment interfered with the expression of genes involved in petiole development especially the MtPhan. Also notable is the fact that development of the first unifoliate leaf was completely aborted, and some leaflets were occasionally mismatched in most of the algae-treated plants irrespective of strain. This could be linked to the possible interference with the expression of MtPIN 10, an auxin efflux transporter that plays a critical role in dissected leaf and flower development [76].
Stenofolia (STF) is another gene involved in leaf and floral lateral development [77]. Because the leaves from algae-treated plants had altered leaf dimensions in comparison to the control, it is possible that they had a similar effect on this gene. Just like HDL1, STF regulates leaf growth by controlling auxin levels [78,79,80]. Current literature suggests that STF modulates auxin and cytokinin homeostasis as well the hormonal crosstalk that coordinates developmental signals at the adaxial–abaxial interface of leaf primordial [81].
Microalgae application increased plant height in all cases, although only the increase resulting from Chlorella MACC-360 was significant. The plant biomass and flower number also showed a clear increase. Another significant observation was the remarkable increase in pigments (chlorophylls and carotenoids). These results are consistent with previous studies on the effect of biostimulants on both monocot and dicot plants [5,41,47,51,82,83,84].
The enlarged leaves in algae-treated plants could be due to the enhanced cell division and cell elongation by the phytohormones in the MA treatments. Microalgae application could be expected to directly impact shoot and root elongation since eukaryotic green microalgae produce auxins and cytokinins. Our results are consistent with what has been reported on auxin producing microorganisms such as bacteria and endophytic fungi, which were found to promote plant growth [18,70,71,72,85,86,87,88]. The difference observed in the different algae treatments could be attributed to the ratios of auxins/cytokinins or different concentrations of specific phytohormones. One particular study revealed that even strains from the same genus could have huge differences in cytokinin production [89]. Moreover, various microalgae might produce different types of auxins and cytokinins as well as other hormones, which were not quantified in this study. Stirk [66] showed that most algae strains produce the indole-3-acetic acid (IAA) form of auxin in higher proportions than the indole-3-acetamide (IAM). The same author goes on to reveal that three different forms of cytokinins are prevalent in microalgae implying differential hormone producing capacities among strains. All the same, Chlorella MACC-360 was found to endogenously produce a plethora of plant-growth-promoting phytohormones [90].
The cell size of the microalgae might also play a significant role in the interaction with other microbes and plant surface at the root interphase. Small size could mean that the algal cells fit in a smaller space and interact with more microbes and larger plant surface. Thus, based on cell size, it is possible to hypothesize that Chlorella MACC-360 has more interactions/contacts with other microbes and with the plants in the soil than Chlorella MACC-38 and C. reinhardtii cc124.
Exopolysaccharides (EPS) released by one of the applied microalgae strains could explain the pronounced effect of Chlorella MACC-360 on plants in comparison to the other two algae. The presence of a significant number of extracellular polysaccharides in the vicinity of Chlorella MACC-360 implies that this strain has the capacity to alter its immediate environment. The secreted metabolites might either attract or repel microorganisms and trigger biological responses from organisms including the plants. The material could also aid in water and air circulation in the soil. Consequently, MA influence the physical, chemical and the biological properties of the rhizosphere.
EPS have been found to be indispensable in rhizobium–legume symbiosis and hence in nitrogen fixation. The presence of algal EPS could help in recruitment of beneficial bacteria and fungi to the plant rhizosphere. Furthermore, the presence of EPS in soil has also been found to improve soil drainage and nutrient availability by increasing the content of ions in soil [91]. EPS isolated from a Chlorella species were found to possess immunomodulatory and antioxidant capacity too; the former refers to modulating biological response, while the latter implies a role in response to reactive oxygen species (ROS) [92]. These properties imply that EPS participate in designing microbial interactions and response to stress. Furthermore, EPS contain sugars, which the plants may directly absorb and use for growth. Studies to evaluate the biostimulatory effect of Chlorella derived polysaccharides showed that they improve plant growth, pigment content and fresh biomass [93].
EPS also strongly facilitate biofilm development. Biofilms have been identified to contribute towards growth promotion in plants. Biofilms improve soil characteristics by absorbing atmospheric moisture and trapping water in the topsoil layers thus making it more available to plants especially in sandy soils. They also reduce water infiltration and hence prevent soil erosion [94]. Biofilmed biofertilizers (BFBFs) prepared with microbial consortia have proved to be a sustainable means of increasing crop yield [95]. Addition of cyanobacteria into areas undergoing desertification was found to stimulate biocrust formation, which improved soil properties and triggered plant succession [96]. In an independent study, biocrusts were found to reduce loss of soil organic carbon content via soil erosion [97]. These studies revealed the role of biofilm forming microorganisms in maintenance of soil fertility and their potential as tools for soil resources conservation and restoration of fertility to dry land. Chlorella MACC-360 is a strong EPS producer and can form biofilms as evidenced by the cell aggregations shown in the microscopy pictures. This phenomenon could explain the observed strong growth promotion effects it exerted on M. truncatula.

4. Materials and Methods

4.1. Algae Strains

Two microalgae species belonging to the Chlorella genus (Chlorella MACC-360 and Chlorella MACC-38) taken from the Mosonmagyaróvár Algal Culture Collection (MACC) and the Chlamydomonas reinhardtii cc124 strain were selected for plant biostimulant studies based on their rapid biomass accumulation.

4.1.1. Determination of Algal Growth

Under aseptic conditions, the surface of a 7-day lawn algae culture in a tris-acetate-phosphate (TAP)-agar plate was scrubbed with a sterile rod and dipped into a 10 mL falcon tube containing 5mL of TAP media. The mouth of the falcon tube was flamed before capping. The tubes were placed in an incubator with the following conditions; 25 °C, 16/8 h light/dark regime, white light and shaker set at 180 rpm. After 3 days, the cultures’ optical density was determined by measuring absorbance at 750 nm with a spectrophotometer. The cultures were then used for inoculation into 1500 μL TAP media in 24-well plates to make cultures with a final optical density (O.D) of 0.2 at 750 nm. Each strain was replicated 6 times. A blank was also maintained and replicated 6 times as well. The plate was placed in the incubator, and optical density was determined by a Hidex plate reader once per day.

4.1.2. Determination of Cell Numbers

Three-day-old starter cultures were inoculated into 25 mL of TAP media to an initial O.D of 0.2. Two flasks per strain were prepared. The flasks were incubated in the same incubator described above. To determine the cell numbers, 100 μL was drawn from the flasks and made up to a volume of 1 mL using water. Then, 10 μL of the diluted culture was placed in the Luna slides, and cell numbers were determined with the fluorescent algae protocol in the Luna Automated cell counter (Luna FL-Logos Biosystems). Cell counts were determined once at the same time every day for 5 days. Cell numbers per day from each flask were individually plotted using GraphPad Prism.

4.2. Microscopy

4.2.1. SEM—Scanning Electron Microscopy

Eight μL of algae samples was spotted onto a silicon disc coated with 0.01% (w/v) poly-l-lysine (Merck Millipore, Billerica, MA, USA). Cells were fixed with 2.5% (v/v) glutaraldehyde and 0.05 M cacodylate buffer (pH 7.2) in PBS overnight at 4 °C. The discs were washed twice with potassium buffered saline (PBS) and dehydrated with a graded ethanol series (30%, 50%, 70%, 80%, 100% ethanol (v/v), for 1.5 h each at 4 °C). The samples were dried with a critical point dryer, followed by 12 nm gold coating (Quorum Technologies, Laughton, East Sussex, UK) and observed under a JEOL JSM-7100F/LV scanning electron microscope (JEOL Ltd., Tokyo, Japan).

4.2.2. CLSM—Confocal Laser Scanning Microscopy

From the flasks with cultures, 50 μL was drawn out into an Eppendorf tube and stained with CFW and Con A both at a concentration of 10 µg/μL. After 30 min incubation in dark, the cells (8 μL) were spotted on microscope slides and covered with 2% (w/v) agar slices and observed with an Olympus Fluoview FV 1000 confocal laser microscope with 60× magnification objective. Sequential scanning was used to avoid crosstalk of the fluorescent dyes and chlorophyll autofluorescence.

4.3. Preparation of the Algae for Plant Treatment

Broth cultures of the algae strains in TAP media, pH 7, were cultivated for preparation of plant treatment. Under aseptic conditions, the surface of a fully grown lawn algae culture from a TAP-agar plate was scrubbed with a sterile rod. The rod was dipped in a 50 mL Erlenmeyer flask containing 15 mL of TAP media. The mouth of the flask was flamed before capping. The flasks were then placed in an algae growth chamber with the following conditions: 25 °C, 16/8 h light/dark regime, white light and shaker set at 180 rpm. After 5 days, 5 mL of the culture was transferred into a 100 mL Erlenmeyer flask containing 50 mL TAP media and placed in the aforementioned growth conditions. The cultures were left to grow for 7 days. On the 7th day, 5 mL of the culture was transferred into a new conical flask containing 50 mL of TAP media to start culture for the next application. The remaining 50 mL was used to prepare the algae treatment.
The 7-day-old cultures were transferred into 50 mL falcon tubes and centrifuged at 4600 rpm for 15 min. The supernatant was discarded, and the cells were resuspended in 50 mL of sterile distilled water. The suspension was centrifuged again at 4600 rpm for 15 min, and the supernatant was discarded. The pellet was then resuspended in sterile distilled water at a concentration of 1 g/L. Total carbon and nitrogen content of the 1 g algae pellet was determined using an elemental analyzer. Control solution (referred to control/distilled water throughout the manuscript) contained respective amounts of sodium acetate and ammonium-chloride dissolved in distilled water.

4.4. Greenhouse-Based Bioassays

Medicago truncatula seeds of line A17 Jemalong, were used for the studies. Planting and phenotyping were done according to Bucciarelli [69]. Plants were surface scarified with concentrated sulfuric acid for 5 min and thoroughly washed with sterile ice-cold water. Seeds were consequently surface sterilized for 3 min with 0.01% HgCl2 and then washed 5 times with sterile distilled water. The seeds were allowed to germinate for 2 days at 4 °C then transferred to Petri dishes with moistened filter paper and given a 21-day vernalization period at 4 °C. The plates were then transferred to a growth chamber for 2–3 days.
Vernalized seeds with a radical length of 1 to 1.5 cm were treated with each of the treatments (distilled water/DW, Chlorella MACC-38, C. reinhardtii cc124 and Chlorella MACC-360 algae suspensions) for 20 min. The seedlings were then rinsed with water and planted in pots containing soil mixed with vermiculate in the ratio of 3:1. Pot size was 10 × 10 × 35 cm3. Each pot contained 4 plants, and each treatment had 5 pots placed in one box. Plants were fertilized during transplantation with 100mL of Solution I (Sol I) diluted 40× from the stock solution prepared as follows: First, the following macronutrient stock solutions were prepared separately: 20.2 g/L KNO3, 73 g/L CaCl2 × 2H2O, 24.6 g/L MgSO4, 43.5 g/L K2SO4, 8.2 g/L Fe-Na-EDTA and 27.2 g/L KH2PO4 and 0.05 M H3BO3. Secondly, a microelement stock solution was prepared by adding 6.2g MnSO4, 10 g KCl, 1 g ZnSO4 × 7H2O, 1g (NH4) Mo7O2 × 4H2O, 0.5 g CuSO4 and 0.5 mL H2SO4 into water and topping it up to 1 L. The stock solutions and 800 mL distilled water were autoclaved separately. Finally, 25 mL of each of the macronutrient solutions and 1.35 mL micronutrient stock solution were added into 800 mL of sterile water to make Sol 1 stock solution. Plants were grown in the greenhouse at 24 to 26 °C and with a 16 h photoperiod. Plants were watered weekly with the water-based algae suspensions (0.05 g/L) for the algae regimes and control solution for the control/distilled water regime, with the last treatment being on the 35th day of growth.
After 45 days, aerial pictures of the plants were taken with a camera to capture the plant cover. After 50 days, the growth experiments were terminated. Ten plants from each treatment were used for phenotyping. Leaf parameters were measured for the leaves associated with the first to the fifth metamer (M1–M5) for leaf petiole and leaf blade length. Leaf blade width was measured up to the sixth metamer (Figure 5g). Leaf blade length was measured along the midrib, from the tip of the middle leaflet to the end of leaf petiole. Leaf blade width was determined as the distance between the two opposite leaflets of a trifoliate leaf. Plant height (height of main axis or one of the axis in bifurcated plants) and flower number were also recorded. All measurements were taken with a flexible handheld ruler.
Plants were gently uprooted and the roots thoroughly washed with distilled water to remove all the soil debris. Five plants were laid out on a black background and pictures taken with a camera. Shoots and roots were separated and weighed separately to record fresh biomass. The plants were then dried in a dry air oven for 48 h at 70 °C, and the dry weight was recorded. Dry weight was recorded as an average of the pooled sample for each treatment regime.
Another set of 10 plants per treatment was collected and processed for determination of plant pigment content determination. For each treatment, 2 pooled samples from 5 plants were put into separate tubes. About 0.1 g of this fresh leaf material was placed in a test tube, and 10 mL of 80% acetone was added. The tubes were placed in a water bath set at 60 °C for 30 min and cooled in ice. Then, 200 μL of the extract was transferred into two wells in a 96-well plate, and absorbance values were measured with a HIDEX plater reader. The content of chlorophylls was calculated according to Arnon equations, and the formula for carotenoids was adopted from Lichtenthaler et al. equation specific for acetone extracts [98,99].

4.5. Statistical Analysis

Data from 3 independent experiments were used for statistical analysis; the data represented parameters measured from 30 plants from each treatment and in total 120 plants. The collected data were tested for normality and homoscedasticity. Multiple comparisons of the groups or treatments were performed with analysis of variance (one-way ANOVA) for plant height, flower number, biomass and pigment parameters. Two-way ANOVA was applied for the comparison of leaf parameters data, which were in the format of grouped data. Tukey’s multiple comparison test with the alpha 0.05 was used to analyze the significance of differences. All statistical analyses were executed using GraphPad Prism 8.

5. Conclusions

The tested eukaryotic green microalgae exerted growth stimulating effects on Medicago truncatula, a phenomenon attributable to phytohormones and algal EPS production. The algae application on plants influenced leaf size, biomass accumulation, pigment content and pod/flower production. Chlorella MACC-360 had the most significant impact on Medicago plants. However, the treatment with C. reinhardtii cc124 persistently increased both chlorophyll and carotenoid contents of the plant contrary to the applied Chlorella species. These results inspire insightful studies to elucidate the mechanism of the different microalgae on plants at the molecular level.
Future studies will employ microscopy techniques to elucidate the status of the interaction between the microalgae and plant roots. The differential expression of the described genes will also be studied via targeted molecular techniques such as quantitative polymerase chain reaction (qPCR) to obtain better insight into the effects of microalgae treatments on plants at the molecular level.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/plants10061060/s1, Figure S1: Confocal laser scanning microscopy (CLSM) pictures of live microalgae cells over a period of 5 days.

Author Contributions

M.M.G. wrote the manuscript and performed the experiments; A.F. performed the confocal and electron microscopy analyses; B.B. participated in the plant phenotyping; V.Ö. and Z.F. provided useful practical hints and participated in the critical discussions and G.M. designed the study, wrote the manuscript and discussed the relevant literature. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by the following international and domestic funds: NKFI-FK-123899 (GM), GINOP-2.2.1-15-2017-00042, 2020-1.1.2-PIACI-KFI-2020-00020 and the Lendület-Programme (GM) of the Hungarian Academy of Sciences (LP2020-5/2020).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Medicago truncatula plants were used in this study. M. truncatula ecotype A17 were kindly provided by Dr. Attila Kereszt (Biological Research Center (BRC), Szeged, Hungary).

Data Availability Statement

The data presented in this study are available in the main text and in Figure S1.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Singh, R.P. Improving Seed Systems Resiliency at Local Level through Participatory Approach for Adaptation to Climate Change. Adv. Plants Agric. Res. 2016, 6, 00-200. [Google Scholar] [CrossRef] [Green Version]
  2. Brain, K.R.; Chalopin, M.C.; Turner, T.D.; Blunden, G.; Wildgoose, P.B. Cytokinin activity of commercial aqueous seaweed extract. Plant Sci. Lett. 1973, 1, 241–245. [Google Scholar] [CrossRef]
  3. Melo, P.C.; Collela, C.F.; Sousa, T.; Pacheco, D.; Cotas, J.; Gonçalves, A.M.; Bahcevandziev, K.; Pereira, L. Seaweed-Based Products and Mushroom β-Glucan as Tomato Plant Immunological Inducers. Vaccines 2020, 8, 524. [Google Scholar] [CrossRef] [PubMed]
  4. Digruber, T.; Sassa, L.; Cseria, A.; Paula, K.; Nagya, A.V.; Remenyikc, J.; Molnárb, I.; Vassa, I.; Toldid, O.; Gyuriczae, C.; et al. Stimulation of energy willow biomass with triacontanol and seaweed extract. Ind. Crop. Prod. 2018, 120, 104–112. [Google Scholar] [CrossRef]
  5. Fayzi, L.; Dayan, M.; Cherifi, O.; Boufous, E.H.; Cherifi, K. Biostimulant effect of four moroccan seaweed extracts applied as seed treatment and foliar spray on maize. Asian J. Plant Sci. 2020, 19. [Google Scholar] [CrossRef]
  6. Kavipriya, R.; Dhanalakshmi, P.K.; Jayashree, S.; Thangaraju, N. Seaweed extract as a biostimulant for legume crop, green gram. J. Ecobiotechnol. 2011, 3, 16–19. [Google Scholar]
  7. Kocira, S.; Kocira, A.; Kornas, R.; Koszel, M.; Szmigielski, M.; Krajewska, M.; Szparaga, A.; Krzysiak, Z. Effects of seaweed extract on yield and protein content of two common bean (Phaseolus vulgaris L.) cultivars. Legume Res. 2018, 41, 589–593. [Google Scholar] [CrossRef]
  8. Michalak, I.; Tuhy, Ł.; Chojnacka, K. Seaweed extract by microwave assisted extraction as plant growth biostimulant. Open Chem. 2015, 13, 1183–1195. [Google Scholar] [CrossRef]
  9. Pomin, V.H. Seaweeds: Agricultural Uses, Biological and Antioxidant Agents; Nova Science Publishers, Inc.: Hauppauge, NY, USA, 2014. [Google Scholar]
  10. Francesca, S.; Carmen, A.; Mele, B.H.; Schettini, C.; Ambrosinom, P.; Barone, A.; Rigano, M.M. The use of a plant-based biostimulant improves plant performances and fruit quality in tomato plants grown at elevated temperatures. Agronomy 2020, 10, 363. [Google Scholar] [CrossRef] [Green Version]
  11. Godlewska, A.; Ciepiela, G.A. Assessment of the effect of various biostimulants on medicago X varia T. Martyn yielding and content of selected organic components. Appl. Ecol. Environ. Res. 2018, 16, 5571–5581. [Google Scholar] [CrossRef]
  12. Gramss, G.; Voigt, K.D.; Bergmann, H. Irrigation with plant extracts in ecofarming increases biomass production and mineral and organic nitrogen content of plants. J. Plant Nutr. Soil Sci. 2003, 166, 612–620. [Google Scholar] [CrossRef]
  13. Coban, G.A.; Dasgan, H.Y.; Akhoundnejad, Y.; Cimen, B.A. Use of microalgae (Chlorella vulgaris) to save mineral nutrients in soilless grown tomato. Acta Hortic. 2020, 1273. [Google Scholar] [CrossRef]
  14. Dineshkumar, R.; Kumaravel, R.; Gopalsamy, J.; Sikder, M.N.A.; Sampathkumar, P. Microalgae as Bio-fertilizers for Rice Growth and Seed Yield Productivity. Waste Biomass Valorization 2018, 9, 793–800. [Google Scholar] [CrossRef]
  15. Dineshkumar, R.; Subramanian, J.; Gopalsamy, J.; Jayasingam, P.; Arumugam, A. The Impact of Using Microalgae as Biofertilizer in Maize (Zea mays L.). Waste Biomass Valorization 2019, 10, 1101–1110. [Google Scholar] [CrossRef]
  16. Iriti, M.; Scarafoni, A.; Pierce, S.; Castorina, G.; Vitalini, S. Soil application of effective microorganisms (EM) maintains leaf photosynthetic efficiency, increases seed yield and quality traits of bean (Phaseolus vulgaris L.) plants grown on different substrates. Int. J. Mol. Sci. 2019, 20, 2327. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  17. Kublanovskaya, A.A.; Khapchaeva, S.A.; Zotov, V.S.; Zaytsev, P.A.; Lobakova, E.S.; Solovchenko, A.E. The Effect of the Microalga Chlorella vulgaris Ippas C-1 Biomass Application on Yield, Biological Activity, and the Microbiome of the Soil during Bean Growing. Mosc. Univ. Biol. Sci. Bull. 2019, 74. [Google Scholar] [CrossRef]
  18. Viaene, T.; Langendries, S.; Beirinckx, S.; Maes, M.; Goormachtig, S. Streptomyces as a plant’s best friend? FEMS Microbiol. Ecol. 2016, 92, 1–10. [Google Scholar] [CrossRef] [Green Version]
  19. Ahmad, M.T.; Shariff, M.; Yusoff, F.; Goh, Y.M.; Banerjee, S. Applications of microalga Chlorella vulgaris in aquaculture. Rev. Aquac. 2020, 12. [Google Scholar] [CrossRef]
  20. Hakim, M.; Thaher, M.; Aljabri, H.; Alghasal, G.; Das, P. Microalgae biomass production in municipal wastewater and use of the produced biomass as sustainable biofertilizer. QScience Proc. 2016, 4. [Google Scholar] [CrossRef]
  21. Sassi, K.K.B.; da Silva, J.A.; Calixto, C.D.; Sassi, R.; Sassi, C.F.d.C. Metabolites of interest for food technology produced by microalgae from the Northeast Brazil. Rev. Cienc. Agron. 2019, 50, 54–65. [Google Scholar] [CrossRef]
  22. Skjånes, K.; Rebours, C.; Lindblad, P. Potential for green microalgae to produce hydrogen, pharmaceuticals and other high value products in a combined process. Crit. Rev. Biotechnol. 2013, 33, 172–215. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Suganya, T.; Varman, M.; Masjuki, H.H.; Renganathan, S. Macroalgae and microalgae as a potential source for commercial applications along with biofuels production: A biorefinery approach. Renew. Sustain. Energy Rev. 2016, 55, 909–941. [Google Scholar] [CrossRef]
  24. Elhafiz, A.A.; Elhafiz, A.A.; Gaur, S.S.; Hamdany, N.; Osman, M.; Lakshmi, T.V.R. Chlorella vulgaris and Chlorella pyrenoidosa live cells appear to be promising sustainable biofertilizer to grow rice, lettuce, cucumber and eggplant in the UAE soils. Recent Res. Sci. Technol. 2015, 7, 14–21. [Google Scholar] [CrossRef]
  25. Marks, E.A.N.; Montero, O.; Rad, C. The biostimulating effects of viable microalgal cells applied to a calcareous soil: Increases in bacterial biomass, phosphorus scavenging, and precipitation of carbonates. Sci. Total Environ. 2019, 692. [Google Scholar] [CrossRef]
  26. Kumar, R.; Sharma, A.K.; Ahluwalia, S.S. Advances in Environmental Biotechnology; Springer: Singapore, 2017; pp. 1–288. [Google Scholar] [CrossRef]
  27. Ramanan, R.; Kim, B.H.; Cho, D.H.; Oh, H.M.; Kim, H.S. Algae-bacteria interactions: Evolution, ecology and emerging applications. Biotechnol. Adv. 2016, 34, 4–29. [Google Scholar] [CrossRef] [Green Version]
  28. Toyama, T.; Kasuya, M.; Hanaoka, T.; Kobayashi, N.; Tanaka, Y.; Inoue, D.; Sei, K.; Morikawa, M.; Mori, K. Biotechnology for Biofuels Growth promotion of three microalgae, Chlamydomonas reinhadtii, Chlorella vulgaris, and Euglena gracilis, by in situ indigenous bacteria in wastewater effluent. Biotechnol. Biofuels 2018, 11, 1–12. [Google Scholar] [CrossRef] [Green Version]
  29. Ciepiela, G.A.; Godlewska, A.; Jankowska, J. The effect of biostimulant on yields of mixed grass/red clover stands and chlorophyll content in crop plant leaves under different nitrogen fertilisation regimes. Fresenius Environ. Bull. 2013, 22, 3700–3708. [Google Scholar]
  30. Paulert, R.; Talamini, V.; Cassolato, J.E.; Duarte, M.E.; Noseda, M.D.; Smania, A.; Stadnik, M.J. Effects of sulfated polysaccharide and alcoholic extracts from green seaweed Ulva fasciata on anthracnose severity and growth of common bean (Phaseolus vulgaris L.). J. Plant Dis. Prot. 2009, 116, 263–270. [Google Scholar] [CrossRef]
  31. Rengasamy, K.R.; Kulkarni, M.G.; Stirk, W.A.; Van Staden, J. Eckol-a new plant growth stimulant from the brown seaweed Ecklonia maxima. J. Appl. Phycol. 2015, 27, 581–587. [Google Scholar] [CrossRef]
  32. Navarro-López, E.; Ruíz-Nieto, A.; Ferreira, A.; Acién, F.G.; Gouveia, L. Biostimulant Potential of Scenedesmus obliquus Grown in Brewery Wastewater. Molecules 2020, 25, 664. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Rathore, S.S.; Chaudhary, D.R.; Boricha, G.N.; Ghosh, A.; Bhatt, B.P.; Zodape, S.T.; Patolia, J.S. Effect of seaweed extract on the growth, yield and nutrient uptake of soybean (Glycine max) under rainfed conditions. S. Afr. J. Bot. 2009, 75, 351–355. [Google Scholar] [CrossRef] [Green Version]
  34. Gatamaneni Loganathan, B.; Orsat, V.; Lefsrud, M. Utilizing the microalgal biomass of Chlorella variabilis and Scenedesmus obliquus produced from the treatment of synthetic dairy wastewater as a biofertilizer. J. Plant Nutr. 2020, 1–12. [Google Scholar] [CrossRef]
  35. El-Sharkawy, M.; El-Beshsbeshy, T.; Al-Shal, R.; Missaoui, A. Effect of Plant Growth Stimulants on Alfalfa Response to Salt Stress. Agric. Sci. 2017, 8, 267–291. [Google Scholar] [CrossRef] [Green Version]
  36. Sosnowski, J.; Jankowski, K.; Malinowska, E.; Truba, M. The effect of Ecklonia maxima extract on Medicago x varia T. Martyn biomass. J. Soil Sci. Plant Nutr. 2017, 17, 770–780. [Google Scholar] [CrossRef] [Green Version]
  37. Brahmbhatt, N.H.; Kalasariya, H.S. Effect of algae on seedling growth of “Queen of Forages”. Int. J. Eng. Res. Gen. Sci. 2015, 3, 827–833. [Google Scholar]
  38. Satish, L.; Ramesh, M. Algae-based extracts as a natural biostimulant for plant growth and development: Current and future prospects. In Photobioreactors: Advancements, Applications and Research; Nova Science Publishers, Inc.: Hauppauge, NY, USA, 2017; pp. 1–13. [Google Scholar]
  39. Puglisi, I.; Barone, V.; Fragalà, F.; Stevanato, P.; Baglieri, A.; Vitale, A. Effect of microalgal extracts from Chlorella vulgaris and Scenedesmus quadricauda on germination of beta vulgaris seeds. Plants 2020, 9, 675. [Google Scholar] [CrossRef] [PubMed]
  40. Dineshkumar, R.; Subramanian, J.; Arumugam, A.; Rasheeq, A.A.; Sampathkumar, P. Exploring the microalgae biofertilizer effect on onion cultivation by field experiment. Waste Biomass Valorization 2020, 11, 77–87. [Google Scholar] [CrossRef]
  41. Faheed, F.A.; Abd-el Fattah, Z. Effect of Chlorella vulgaris as Bio-fertilizer on Growth Parameters and Metabolic Aspects of Lettuce Plant. J. Agric. Soc. Sci. 2008, 4, 165–169. [Google Scholar]
  42. Agwa, O.K.; Ogugbue, C.J.; Williams, E.E. Field Evidence of Chlorella vulgaris Potentials as a Biofertilizer for Hibiscus esculentus. Int. J. Agric. Res. 2017, 12, 181–189. [Google Scholar] [CrossRef] [Green Version]
  43. Suleiman, A.K.; Lourenço, K.S.; Clark, C.; Luz, R.L.; da Silva, G.H.; Vet, L.E.; Cantarella, H.; Fernandes, T.V.; Kuramae, E.E. Fertilization with microalgal biomass from wastewater impacts the soil and rhizosphere active microbiomes, greenhouse gas emissions and plant growth. Resour. Conserv. Recycl. 2020, 161. [Google Scholar] [CrossRef]
  44. De Siqueira Castro, J.; Calijuri, M.L.; Mattiello, E.M.; Ribeiro, V.J.; Assemany, P.P. Algal biomass from wastewater: Soil phosphorus bioavailability and plants productivity. Sci. Total Environ. 2020, 711. [Google Scholar] [CrossRef]
  45. Rasheed, R.; Bounnit, T.; Al Jabri, H.; Saadaoui, I. Algae-based biofertilizer for date palm cultivation in Qatar. In Proceedings of the Qatar University Annual Research Forum and Exhibition (QUARFE 2020), Qatar, Doha, 28 October 2020. [Google Scholar] [CrossRef]
  46. Jo, S.W.; Do, J.M.; Na, H.; Hong, J.W.; Kim, I.S.; Yoon, H.S. Assessment of biomass potentials of microalgal communities in open pond raceways using mass cultivation. PeerJ 2020, 8. [Google Scholar] [CrossRef] [PubMed]
  47. Kholssi, R.; Marks, E.A.; Miñón, J.; Montero, O.; Debdoubi, A.; Rad, C. Biofertilizing effect of Chlorella sorokiniana suspensions on wheat growth. J. Plant Growth Regul. 2019, 38, 644–649. [Google Scholar] [CrossRef]
  48. Bumandalai, O.; Tserennadmid, R. Effect of Chlorella vulgaris as a biofertilizer on germination of tomato and cucumber seeds. Int. J. Aquat. Biol. 2019, 7, 95–99. [Google Scholar] [CrossRef]
  49. Özdemİr, S.; Sukatar, A.; Öztekin, G.B. Production of Chlorella vulgaris and its effects on plant growth, yield and fruit quality of organic tomato grown in greenhouse as biofertilizer. Tarim Bilim. Derg. 2016, 22, 596–605. [Google Scholar] [CrossRef]
  50. Schwarz, D.; Gross, W. Algae affecting lettuce growth in hydroponic systems. J. Hortic. Sci. Biotechnol. 2004, 79, 554–559. [Google Scholar] [CrossRef]
  51. Kopta, T.; Pavlikova, M.; Sękara, A.; Pokluda, R.; Maršálek, B. Effect of bacterial-algal biostimulant on the yield and internal quality of lettuce (Lactuca sativa L.) produced for spring and summer crop. Not. Bot. Horti Agrobot. Cluj-Napoca 2018, 46, 615–621. [Google Scholar] [CrossRef] [Green Version]
  52. Grzesik, M.; Romanowska-Duda, Z. Ability of Cyanobacteria and Green Algae to Improve Metabolic Activity and Development of Willow Plants. Pol. J. Environ. Stud. 2015, 24, 1003–1012. [Google Scholar] [CrossRef]
  53. Zayadan, B.K.; Matorin, D.N.; Baimakhanova, G.B.; Bolathan, K.; Oraz, G.D.; Sadanov, A.K. Promising microbial consortia for producing biofertilizers for rice fields. Microbiology 2014, 83, 391–397. [Google Scholar] [CrossRef]
  54. Renuka, N.; Guldhe, A.; Prasanna, R.; Singh, P.; Bux, F. Microalgae as multi-functional options in modern agriculture: Current trends, prospects and challenges. Biotechnol. Adv. 2018, 36, 1255–1273. [Google Scholar] [CrossRef]
  55. Odgerel, B.; Tserendulam, D. Effect of Chlorella as a biofertilizer on germination of wheat and barley grains. Proc. Mong. Acad. Sci. 2016, 26–31. [Google Scholar] [CrossRef] [Green Version]
  56. Dineshkumar, R.; Subramanian, J.; Sampathkumar, P. Prospective of Chlorella vulgaris to Augment Growth and Yield Parameters Along with Superior Seed Qualities in Black Gram, Vigna mungo (L.). Waste Biomass Valorization 2020, 11. [Google Scholar] [CrossRef]
  57. Ergun, O.; Dasgan, H.Y.; Isik, O. Effects of microalgae Chlorella vulgaris on hydroponically grown lettuce. Acta Hortic. 2020, 1273. [Google Scholar] [CrossRef]
  58. Kim, M.J.; Shim, C.K.; Kim, Y.K.; Ko, B.G.; Park, J.H.; Hwang, S.G.; Kim, B.H. Effect of biostimulator Chlorella fusca on improving growth and qualities of chinese chives and spinach in organic farm. Plant Pathol. J. 2018, 34, 567–574. [Google Scholar] [CrossRef] [PubMed]
  59. De Lima, J.F. Utilization of Chlorella sp. as biostimulant in the germination of melon seeds (Cucumis melo L.). J. Agric. Stud. 2020, 8, 750–773. [Google Scholar] [CrossRef]
  60. Yanni, Y.G.; Elashmouny, A.A.; Elsadany, A.Y. Differential Response of Cotton Growth, Yield and Fiber Quality to Foliar Application of Spirulina platensis and Urea Fertilizer. Asian J. Adv. Agric. Res. 2020, 29–40. [Google Scholar] [CrossRef] [Green Version]
  61. Uddin, A.F.M.J.; Rakibuzzaman, M.; naher Wasin, E.W.; Husna, M.A.; Mahato, A.K. Foliar application of Spirulina and Oscillatoria on growth and yield of okra as bio-fertilizer. J. Biosci. Agric. Res. 2019, 22, 1840–1844. [Google Scholar] [CrossRef]
  62. Wuang, S.C.; Khin, M.C.; Chua, P.Q.D.; Luo, Y.D. Use of Spirulina biomass produced from treatment of aquaculture wastewater as agricultural fertilizers. Algal Res. 2016, 15, 59–64. [Google Scholar] [CrossRef]
  63. Carillo, P.; Ciarmiello, L.F.; Woodrow, P.; Corrado, G.; Chiaiese, P.; Rouphael, Y. Enhancing sustainability by improving plant salt tolerance through macro-and micro-algal biostimulants. Biology 2020, 9, 253. [Google Scholar] [CrossRef]
  64. Singh, R.; Parihar, P.; Singh, M.; Bajguz, A.; Kumar, J.; Singh, S.; Singh, V.P.; Prasad, S.M.; Singh, R.; Parihar, P. Uncovering potential applications of cyanobacteria and algal metabolites in biology, agriculture and medicine: Current status and future prospects. Front. Microbiol. 2017, 8, 515. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  65. Stirk, W.A.; Ördög, V.; Van Staden, J.; Jäger, K. Cytokinin- and auxin-like activity in Cyanophyta and microalgae. J. Appl. Phycol. 2002, 14, 215–221. [Google Scholar] [CrossRef]
  66. Stirk, W.A.; Ördög, V.; Novák, O.; Rolčík, J.; Strnad, M.; Bálint, P.; van Staden, J. Auxin and cytokinin relationships in 24 microalgal strains1. J. Phycol. 2013, 49, 459–467. [Google Scholar] [CrossRef]
  67. Kuhn, D.M.; Chandra, J.; Mukherjee, P.K.; Ghannoum, M.A. Comparison of biofilms formed by Candida albicans and Candida parapsilosis on bioprosthetic surfaces. Infect. Immun. 2002, 70, 878–888. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  68. Chen, M.Y.; Lee, D.J.; Tay, J.H. Distribution of extracellular polymeric substances in aerobic granules. Appl. Microbiol. Biotechnol. 2007, 73, 1463–1469. [Google Scholar] [CrossRef] [PubMed]
  69. Bucciarelli, B.; Hanan, J.; Palmquist, D.; Vance, C.P. A standardized method for analysis of Medicago truncatula phenotypic development. Plant Physiol. 2006, 142, 207–219. [Google Scholar] [CrossRef] [Green Version]
  70. Chinnaswamy, A.; Coba de la Peña, T.; Stoll, A.; de la Peña Rojo, D.; Bravo, J.; Rincón, A.; Lucas, M.M.; Pueyo, J.J. A nodule endophytic Bacillus megaterium strain isolated from Medicago polymorpha enhances growth, promotes nodulation by Ensifer medicae and alleviates salt stress in alfalfa plants. Ann. Appl. Biol. 2018, 172, 295–308. [Google Scholar] [CrossRef]
  71. Defez, R.; Andreozzi, A.; Romano, S.; Pocsfalvi, G.; Fiume, I.; Esposito, R.; Angelini, C.; Bianco, C. Bacterial IAA-delivery into medicago root nodules triggers a balanced stimulation of C and N metabolism leading to a biomass increase. Microorganisms 2019, 7, 403. [Google Scholar] [CrossRef] [Green Version]
  72. Kępczyńska, E.; Karczyński, P. Medicago truncatula root developmental changes by growth-promoting microbes isolated from Fabaceae, growing on organic farms, involve cell cycle changes and WOX5 gene expression. Planta 2020, 251, 1–19. [Google Scholar] [CrossRef]
  73. Wang, H.; Xu, Y.; Hong, L.; Zhang, X.; Wang, X.; Zhang, J.; Ding, Z.; Meng, Z.; Wang, Z.Y.; Long, R.; et al. HEADLESS Regulates Auxin Response and Compound Leaf Morphogenesis in Medicago truncatula. Front. Plant Sci. 2019, 10, 1024. [Google Scholar] [CrossRef] [Green Version]
  74. Ge, L.; Peng, J.; Berbel, A.; Madueño, F.; Chen, R. Regulation of compound leaf development by PHANTASTICA in Medicago truncatula. Plant Physiol. 2014, 164, 216–228. [Google Scholar] [CrossRef] [Green Version]
  75. Ge, L.; Chen, R. PHANTASTICA regulates leaf polarity and petiole identity in Medicago truncatula. Plant Signal. Behav. 2014, 9, e28121. [Google Scholar] [CrossRef] [Green Version]
  76. Peng, J.; Chen, R. Auxin efflux transporter MtPIN10 regulates compound leaf and flower development in Medicago truncatula. Plant Signal. Behav. 2011, 6, 1537–1544. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  77. Meng, Y.; Liu, H.; Wang, H.; Liu, Y.; Zhu, B.; Wang, Z.; Hou, Y.; Zhang, P.; Wen, J.; Yang, H.; et al. HEADLESS, a WUSCHEL homolog, uncovers novel aspects of shoot meristem regulation and leaf blade development in Medicago truncatula. J. Exp. Bot. 2019, 70, 149–163. [Google Scholar] [CrossRef] [Green Version]
  78. Tadege, M.; Lin, H.; Bedair, M.; Berbel, A.; Wen, J.; Rojas, C.M.; Niu, L.; Tang, Y.; Sumner, L.; Ratet, P.; et al. STENOFOLIA regulates blade outgrowth and leaf vascular patterning in Medicago truncatula and Nicotiana sylvestris. Plant Cell 2011, 23, 2125–2142. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  79. Zhang, F.; Wang, Y.; Li, G.; Tang, Y.; Kramer, E.M.; Tadege, M. STENOFOLIA recruits TOPLESS to repress ASYMMETRIC LEAVES2 at the leaf margin and promote leaf blade outgrowth in Medicago truncatula. Plant Cell. 2014, 26, 650–664. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  80. Zhang, F.; Wang, H.; Tadege, M. Mechanistic insights into STENOFOLIA-mediated leaf blade outgrowth in Medicago truncatula. Model Legume Med. Truncatula 2019, 173–182. [Google Scholar] [CrossRef]
  81. Niu, L.; Lin, H.; Zhang, F.; Watira, T.W.; Li, G.; Tang, Y.; Wen, J.; Ratet, P.; Mysore, K.S.; Tadege, M.L. LOOSE FLOWER, a WUSCHEL-like Homeobox gene, is required for lateral fusion of floral organs in Medicago truncatula. Plant J. 2015, 81, 480–492. [Google Scholar] [CrossRef] [PubMed]
  82. Dineshkumar, R.; Duraimurugan, M.; Sharmiladevi, N.; Lakshmi, L.P.; Rasheeq, A.A.; Arumugam, A.; Sampathkumar, P. Microalgal liquid biofertilizer and biostimulant effect on green gram (Vigna radiata L) an experimental cultivation. Biomass Convers. Biorefinery 2020, 1–21. [Google Scholar] [CrossRef]
  83. Puglisi, I.; La Bella, E.; Rovetto, E.I.; Lo Piero, A.R.; Baglieri, A. Biostimulant effect and biochemical response in lettuce seedlings treated with a Scenedesmus quadricauda extract. Plants 2020, 9, 123. [Google Scholar] [CrossRef] [Green Version]
  84. Umamaheswari, J.; Shanthakumar, S. Paddy-soaked rice mill wastewater treatment by phycoremediation and feasibility study on use of algal biomass as biofertilizer. J. Chem. Technol. Biotechnol. 2021, 96, 394–403. [Google Scholar] [CrossRef]
  85. Bianco, C.; Defez, R. Improvement of phosphate solubilization and Medicago plant yield by an indole-3-acetic acid-overproducing strain of Sinorhizobium meliloti. Appl. Environ. Microbiol. 2010, 76, 4626–4632. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  86. Maymon, M.; Martínez-Hidalgo, P.; Tran, S.S.; Ice, T.; Craemer, K.; Anbarchian, T.; Sung, T.; Hwang, L.H.; Chou, M.; Fujishige, N.A.; et al. Mining the phytomicrobiome to understand how bacterial coinoculations enhance plant growth. Front. Plant Sci. 2015, 6, 784. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  87. Rey, T.; Dumas, B. Plenty Is No Plague: Streptomyces Symbiosis with Crops. Trends Plant Sci. 2017, 22, 30–37. [Google Scholar] [CrossRef]
  88. Varma, A.; Tripathi, S.; Prasad, R. (Eds.) Plant Microbe Interface; Springer: Berlin/Heidelberg, Germany, 2019; pp. 219–253. [Google Scholar]
  89. Ördög, V.; Stirk, W.A.; Van Staden, J.; Novák, O.; Strnad, M. Endogenous cytokinins in three genera of microalgae from the chlorophyte. J. Phycol. 2004, 40, 88–95. [Google Scholar] [CrossRef]
  90. Stirk, W.A.; Bálint, P.; Tarkowská, D.; Novák, O.; Maróti, G.; Ljung, K.; Turečková, V.; Strnad, M.; Ördög, V.; Van Staden, J. Effect of light on growth and endogenous hormones in Chlorella minutissima (Trebouxiophyceae). Plant Physiol. Biochem. 2014, 79, 66–76. [Google Scholar] [CrossRef] [PubMed]
  91. Ortiz-Moreno, M.L.; Sandoval-Parra, K.X.; Solarte-Murillo, L.V. Chlorella, a potential biofertilizer? Orinoquia 2019, 23, 71–78. [Google Scholar] [CrossRef]
  92. Yuan, Q.; Li, H.; Wei, Z.; Lv, K.; Gao, C.; Liu, Y.; Zhao, L. Isolation, structures and biological activities of polysaccharides from Chlorella: A review. Int. J. Biol. Macromol. 2020, 163, 2199–2209. [Google Scholar] [CrossRef] [PubMed]
  93. El-Naggar, N.E.; Hussein, M.H.; Shaaban-Dessuuki, S.A.; Dalal, S.R. Production, extraction and characterization of Chlorella vulgaris soluble polysaccharides and their applications in AgNPs biosynthesis and biostimulation of plant growth. Sci. Rep. 2020, 10, 1–19. [Google Scholar] [CrossRef] [Green Version]
  94. Colica, G.; Li, H.; Rossi, F.; Li, D.; Liu, Y.; De Philippis, R. Microbial secreted exopolysaccharides affect the hydrological behavior of induced biological soil crusts in desert sandy soils. Soil Biol. Biochem. 2014, 68, 62–70. [Google Scholar] [CrossRef]
  95. Zakeel, M.C.M.; Safeena, M.I.S. Biofilmed Biofertilizer for Sustainable Agriculture. In Plant Health under Biotic Stress; Springer: Singapore, 2019; pp. 65–82. [Google Scholar]
  96. Lan, S.; Zhang, Q.; Wu, L.; Liu, Y.; Zhang, D.; Hu, C. Artificially accelerating the reversal of desertification: Cyanobacterial inoculation facilitates the succession of vegetation communities. Environ. Sci. Technol. 2014, 48, 307–315. [Google Scholar] [CrossRef]
  97. Chamizo, S.; Rodríguez-Caballero, E.; Román, J.R.; Cantón, Y. Effects of biocrust on soil erosion and organic carbon losses under natural rainfall. Catena 2017, 148, 117–125. [Google Scholar] [CrossRef]
  98. Manolopoulou, E.; Varzakas, T.; Petsalaki, A. Chlorophyll determination in green pepper using two different extraction methods. Curr. Res. Nutr. Food Sci. J. 2016, 4, 52–60. [Google Scholar] [CrossRef]
  99. Lichtenthaler, H.; Wellburn, A.R. Determinations of total carotenoids and chlorophylls a and b of leaf extracts in different solvents. Adv. Photosynth. Res. 1984, 11, 591–592. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Growth parameters showing optical density and cell numbers of the algae strains grown under light/dark conditions over 7 days: (a) growth curve; (b) cell numbers. MACC-38 = Chlorella MACC-38; cc124 = C. reinhardtii cc124 and MACC-360 = Chlorella MACC-360 on both graphs.
Figure 1. Growth parameters showing optical density and cell numbers of the algae strains grown under light/dark conditions over 7 days: (a) growth curve; (b) cell numbers. MACC-38 = Chlorella MACC-38; cc124 = C. reinhardtii cc124 and MACC-360 = Chlorella MACC-360 on both graphs.
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Figure 2. Scanning electron microscopy pictures of the three strains: (a) Chlorella MACC-38; (b) C. reinhardtii cc124; (c) Chlorella MACC-360 at 5000× magnification; (d) Chlorella MACC-360 at 10,000× magnification. Black arrows on (b) show flagella; black arrows on (c) show aggregation or clustering of cells while black arrows on (d) show the extracellular material connecting one cell to another in the cell aggregations/matrix.
Figure 2. Scanning electron microscopy pictures of the three strains: (a) Chlorella MACC-38; (b) C. reinhardtii cc124; (c) Chlorella MACC-360 at 5000× magnification; (d) Chlorella MACC-360 at 10,000× magnification. Black arrows on (b) show flagella; black arrows on (c) show aggregation or clustering of cells while black arrows on (d) show the extracellular material connecting one cell to another in the cell aggregations/matrix.
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Figure 3. CLSM pictures of live microalgae cells on the 7th day after inoculation; (a) Chlorella MACC-38; (b) C. reinhardtii cc124; (c) Chlorella MACC-360 stained with calcofluor white (CFW) and concanavalin A (Con A). The blue fluorescence is CFW dye, which stains the cell walls, red is the chloroplast autofluorescence of live cells and green fluorescence is Con A dye, which binds to extracellular polysaccharides (EPS).
Figure 3. CLSM pictures of live microalgae cells on the 7th day after inoculation; (a) Chlorella MACC-38; (b) C. reinhardtii cc124; (c) Chlorella MACC-360 stained with calcofluor white (CFW) and concanavalin A (Con A). The blue fluorescence is CFW dye, which stains the cell walls, red is the chloroplast autofluorescence of live cells and green fluorescence is Con A dye, which binds to extracellular polysaccharides (EPS).
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Figure 4. Aerial pictures of the plants (five pots per treatment placed in a box) at 45 days after planting: (a) DW/Control plants; (b) Chlorella MACC-38-treated plants; (c) C. reinhardtii cc124-treated plants and (d) Chlorella MACC-360-treated plants. For all figure panels, the left image shows the aerial view, while the right one shows the front view of uprooted plants.
Figure 4. Aerial pictures of the plants (five pots per treatment placed in a box) at 45 days after planting: (a) DW/Control plants; (b) Chlorella MACC-38-treated plants; (c) C. reinhardtii cc124-treated plants and (d) Chlorella MACC-360-treated plants. For all figure panels, the left image shows the aerial view, while the right one shows the front view of uprooted plants.
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Figure 5. Effect of algae application on the leaf size of 50-day-old Medicago truncatula leaves; 10 replicates were measured per experiment. (a) Leaf petiole; (b) petiole length relative to control; (c) leaf blade length; (d) leaf blade length relative to control; (e) leaf blade width; (f) leaf blade width relative to control; (g) Illustrative diagram of M. truncatula, created with BioRender.com, showing the different phenotypic parameters that were measured. Metamers (internode, leaf and bud) and their associated leaves are labelled from the bottom to the top along the main axis in ascending order. The red arrow on the first leaf depicts blade width, the dark blue arrow depicts blade length and the brackets show the petiole length. Different letters on the bars indicate significant differences between groups (p < 0.05) according to Tukey’s multiple comparison test. Two-way ANOVA was used for all parameters.
Figure 5. Effect of algae application on the leaf size of 50-day-old Medicago truncatula leaves; 10 replicates were measured per experiment. (a) Leaf petiole; (b) petiole length relative to control; (c) leaf blade length; (d) leaf blade length relative to control; (e) leaf blade width; (f) leaf blade width relative to control; (g) Illustrative diagram of M. truncatula, created with BioRender.com, showing the different phenotypic parameters that were measured. Metamers (internode, leaf and bud) and their associated leaves are labelled from the bottom to the top along the main axis in ascending order. The red arrow on the first leaf depicts blade width, the dark blue arrow depicts blade length and the brackets show the petiole length. Different letters on the bars indicate significant differences between groups (p < 0.05) according to Tukey’s multiple comparison test. Two-way ANOVA was used for all parameters.
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Figure 6. Effects of microalgae applications on plants (50-day-old plants); (a) plant height; (b) flower number; (c) fresh weight; (d) dry weight; (e) chlorophyll; (f) carotenoids. Data represent means and standard errors (error bars) of 10 biological replicates per experiment. Different letters on bars indicate significant differences between groups (p < 0.05), according to Tukey’s test. One-way ANOVA was used for all parameters.
Figure 6. Effects of microalgae applications on plants (50-day-old plants); (a) plant height; (b) flower number; (c) fresh weight; (d) dry weight; (e) chlorophyll; (f) carotenoids. Data represent means and standard errors (error bars) of 10 biological replicates per experiment. Different letters on bars indicate significant differences between groups (p < 0.05), according to Tukey’s test. One-way ANOVA was used for all parameters.
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Gitau, M.M.; Farkas, A.; Balla, B.; Ördög, V.; Futó, Z.; Maróti, G. Strain-Specific Biostimulant Effects of Chlorella and Chlamydomonas Green Microalgae on Medicago truncatula. Plants 2021, 10, 1060. https://doi.org/10.3390/plants10061060

AMA Style

Gitau MM, Farkas A, Balla B, Ördög V, Futó Z, Maróti G. Strain-Specific Biostimulant Effects of Chlorella and Chlamydomonas Green Microalgae on Medicago truncatula. Plants. 2021; 10(6):1060. https://doi.org/10.3390/plants10061060

Chicago/Turabian Style

Gitau, Margaret Mukami, Attila Farkas, Benedikta Balla, Vince Ördög, Zoltán Futó, and Gergely Maróti. 2021. "Strain-Specific Biostimulant Effects of Chlorella and Chlamydomonas Green Microalgae on Medicago truncatula" Plants 10, no. 6: 1060. https://doi.org/10.3390/plants10061060

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