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Article

Accumulation of Secondary Metabolites of Rhodiola semenovii Boriss. In Situ in the Dynamics of Growth and Development

by
Nina V. Terletskaya
1,2,*,
Nazym K. Korbozova
1,2,
Alexander E. Grazhdannikov
3,
Gulnaz A. Seitimova
1,2,
Nataliya D. Meduntseva
1 and
Nataliya O. Kudrina
1,2,*
1
Faculty of Biology and Biotechnology and Faculty of Chemistry and Chemical Technology, Al-Farabi Kazakh National University, Al-Farabi Avenue 71, 050040 Almaty, Kazakhstan
2
Institute of Genetic and Physiology, Al-Farabi Avenue 93, 050040 Almaty, Kazakhstan
3
N.N. Vorozhtsov Novosibirsk Institute of Organic Chemistry, Siberian Branch of Russian Academy of Science, 630090 Novosibirsk, Russia
*
Authors to whom correspondence should be addressed.
Metabolites 2022, 12(7), 622; https://doi.org/10.3390/metabo12070622
Submission received: 8 June 2022 / Revised: 29 June 2022 / Accepted: 30 June 2022 / Published: 6 July 2022
(This article belongs to the Special Issue Metabolism of Plant Secondary Metabolites under Stress Conditions)
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Versions Notes

Abstract

:
Rhodiola semenovii Boriss. (Regel and Herder) might be a promising replacement for the well-known but endangered Rhodiola rosea L. In this research, the metabolic profile of R. semenovii, including drug-active and stress-resistant components, was studied in the context of source–sink interactions in situ in the dynamics of growth and development. Gas chromatography with mass spectrometric detection and liquid chromatography methods were used. The data obtained allow for assumptions to be made about which secondary metabolites determine the level of stress resistance in R. semenovii at different stages of ontogeny in situ. For the first time, an expansion in the content of salidroside in the above-ground organs, with its maximum value during the period of seed maturation, and a significant decrease in its content in the root were revealed in the dynamics of vegetation. These results allow us to recommend collecting the ground component of R. semenovii for pharmaceutical purposes throughout the seed development stage without damaging the root system.

1. Introduction

Rhodiola semenovii Boriss. (Regel and Herder) plants have long been used in Central Asian traditional medicine as a source of adaptogenic, choleretic, tonic, anti-inflammatory, hypoglycemic, and antioxidant qualities [1,2,3,4]. R. semenovii has the potential to replace the well-known Rhodiola rosea L., which is now listed in the Red Book due to its medicinal properties. However, the metabolic profile of R. semenovii and its prospective alterations, including drug-active and stress-resistant components, has yet to be depicted in detail, including focusing on the dynamics of vegetation at various phases of growth.
It was established that the synthesis of secondary metabolites, including those valuable for pharmacy, significantly varies by plant organs depending on the stage of ontogeny [5]. In the context of physiological, biological, and functional regulation, plant metabolites are the biochemical “levers” by which the plant organism solves numerous issues throughout its life [6]. In addition, the synthesis of metabolites in a plant is a system mediated both by external influences (temperature, precipitation, solar insolation, and other environmental factors) and internal factors (stages of plant ontogeny) [7,8]. The chemotypes are more variable than phylogeny due to the presence of a delicate balance between sink and source during plant development [9,10,11]. An adjustment in chemical profiles suggests that various biosynthetic pathways are activated during development [12]. Secondary metabolite synthesis involves some ecological effects, such as a redistribution of the plant’s internal resources between growth and defense. The theory of optimal defense assumes that distinct tissues of a plant during its growth are protected from several abiotic and biotic stressors based on their value to the plant at this stage of development [13]. During ontogeny, stressors and their intensity vary, and the concentrations of secondary metabolites (SM) depending on the availability of carbon resources also vary. The very structure of a vegetative plant is a consequence of the gradual complication of the source–sink interaction [14,15,16,17,18].
The carbohydrates are the primary substrates used in the processes of photosynthesis and respiration, supplying the plant with energy. They likewise provide a carbon skeleton for the synthesis of protective compounds, including SM, such as flavonoids, stilbenes, lignins, etc. It is possible that carbohydrate complexes regulate the response to light, the concentration of soil nutrients, and stress, whereas internal development programs are controlled by plant hormones [19,20]. The hypothesis “general control” states that the distribution of carbon to diverse sink organs is controlled both by the demand for “sinks” (their activity and size) and by the control of “sources” of photosynthates production [21]. The assimilation of carbon in the plant, in coordination with the absorption of nitrogen, ensures the overall production of biomass, as well as the construction of carbon skeletons of biomolecules and amino acid balance with the corresponding transport processes from source to sink. The dynamic regulation of metabolism ensures an optimal targeted delivery of SM—the right “building blocks”—to emerging and developing organs and tissues [22]. A vast arrangement of plant metabolite transporters provides flexibility and adaptability in coordinating between pathways and source–sink interactions [23,24]. Plant secondary metabolites and their degradation products can also work as plant growth modulators and integrated components of metabolic networks that are dynamically formed during ontogenesis under the pressure of many environmental factors [25,26,27,28].
The integration of phenotyping and metabolic studies in the context of the source–sink interaction is emerging as a promising technique for studying genotype–environment interactions in order to identify critical factors for increasing productivity and the optimal timing of medicinal plant material collection when the content of bioactive compounds is at its highest level [29,30]. Nevertheless, despite the fact that researchers have made significant efforts to investigate the “source–sink” connection, we are still far from a thorough understanding of the source–sink interaction in plants, as well as the rational application of “source–sink interaction” results [31].
As a result, the goal of this work was to investigate the synthesis of secondary metabolites, specifically p-hydroxyphenylethyl-O—D-glucopyranoside (salidroside), which is valuable from a therapeutic standpoint and can be considered as a generic trait of Rhodiola species [32] in the dynamics of vegetation in situ in the foothills of the Trans-Ili Alatau (Northern Tien Shan, Kazakhstan). We expect that studying the accumulation of valuable medicinal SMs in R. semenovii in the context of source–acceptor interactions will reveal patterns of stress tolerance formation in this species at different stages of in situ ontogeny, as well as the optimal time for collecting R. semenovii as a medicinal raw material.

2. Results

2.1. Determination of Organic Compounds in Root and Shoot of R. semenovii during Vegetation

The comparative quantitative analysis based on GC-MS spectra from the Wiley 7th edition and NIST’02 libraries made it possible to identify 35 metabolites from different classes as significantly different components in immature plant tissues of R. semenovii, 68 metabolites in flowering plant tissues, and 40 metabolites in adult plant tissues at p < 0.05 (Tables S1–S3).
The metabolic profile of the root and shoot of R. semenovii (Figure 1, Figure 2, Figure 3 and Figure 4) under natural vegetation circumstances demonstrated quantitative variations in the classes of organic molecules at different phases of ontogenesis.
According to the data (Figure 1, Figures S1 and S2, Table S1), immature plants have a higher concentration of SM in the root, with the largest proportion found in fatty acid esters (15.9%), ketones (13.1%, including cyclic ketones), lactones (17.2%), hydrocarbons (11.6%), dioxolane derivatives (11.8%), and terpenes (10.5%).
However, they have a comparatively low level of beneficial secondary metabolites in the shoot at this stage of development, with the exception of ketones (18.4%, including cyclic ketones), carbohydrates and their derivatives (45.1%), six-membered aromatic heterocycles (4.9%), and pyrroles (0.6%), which are only present in the shoot.
The spectrum of SMs detected in the root and shoot of plants in the flowering phase broadened (Figure 2, Figure 3 and Figures S3–S5, Table S2). At the same time, the amount of fatty acid esters (up to 4.9%), ketones and cyclic ketones (up to 10%), and dioxolanone derivatives (up to 6.6%) decreased, while hydrocarbons and terpenes were absent. The amount of lactones (including furan derivatives) increased to 20.5%. In addition, a rather substantial number of monocarboxylic acid esters (23.2%) and oximes (11.4%) were identified, which had not before been observed in the root.
It was indicated that the shoot spectrum is both quantitatively and qualitatively more diverse and affluent than the root spectrum at this stage of the growing season. The maximum in the shoot falls on lactones (including derivatives of furan) (45.6%), fatty acid esters (15.8%), ketones and cyclic ketones (15.2%), and carbohydrates and its derivatives (29.4%). At the same time, a large number of the identified metabolites in the shoot fell on flowers, such as, and in particular, hydrocarbons (24.3%), carbohydrates and its derivatives (17.0%), aldehydes (15.4%), lactones (including derivatives of furan) (9.7%), and ketones (8.1 %). The hydroxypyridines (alkaloids) (6.2%), salicylates (1.6%), and aliphatic nitriles (2.4%) were identified only in flowers.
The data illustrated in Figure 4 (Figures S6 and S7, Table S3) present organic compounds classes in the metabolic profile of adult plants R. semenovii under the ripening of seeds.
According to the information provided, at this stage of development in the root, quantitative GC-MS analysis allows for the identification of a reasonably substantial content of class of components (16), with oximes (12.3%), lactones (9.3%), and ketones being the most prevalent (8.7% including cyclic ketones), whereas only fatty acids esters (95.3%) and terpenes (4.7%) were identified in the shoot and seeds.
Some regularities were discovered that are subject to the main groups of SM, which are present throughout the growth season in both the root and shoot, with a sufficiently high degree of correlation (Figure 5).
Thus, over the growing season, the accumulation of fatty acid esters in root declines and the proportion of their content in shoot grows (r = −0.5), but the accumulation of phenols has an inverse dependency (r = −0.8), with a maximum concentration in the root at the stage of seed maturation.
The highest concentration of ketones, terpenes, and ubiquinones was observed in the root and shoot of immature R. semenovii plants, with a further reduction over the growth season (correlation coefficient in the root and shoot r = 0.7, r = 0.9, and r = 1, respectively), whereas the peak of lactone accumulation in both the root and shoot of R. semenovii was seen during the blooming period (r = 0.8).
The remaining SM classes are absent at all phases of vegetative development in the root and shoot, with different dynamics. This implies that source–sink interactions have an unequivocal impact on the synthesis and redistribution of SM in R. semenovii plants during the growth season.

2.2. Determination of Salidrosid in Root and Shoot of R. semenovii during Vegetation

The liquid chromatography technique was used to detect the presence of the valuable medicine glycoside salidroside in the organs of R. semenovii. Additionally, it was found that salidroside during the growing season can be localized both in the root and shoot of R. semenovii in concentrations that vary depending on the stage of development (Figure 6 and Figure S8–S16).
The highest content of salidroside was noted in the root during flowering and in the shoot during seed maturation. At the same time, a positive dynamic of the accumulation of salidroside was exposed in the shoot during the growing season, whereas, after the peak level during flowering in the root, a further decrease in the concentration of this substance was indicated.

3. Discussion

The experiment demonstrated changes in the synthesis and redistribution of SM in R. semenovii plants over the growth season, indicating the impact of source–sink interactions on metabolism. In doing so, the “source” and “sink” modifications are rather conditional on the type and growth stage of the plant [31]. Therefore, the comparatively low amount of beneficial secondary metabolites, particularly in the shoots of immature plants, was clearly reflected in our experiment on the detection of SM, indicating that young plants have an increased requirement for primary metabolites and nutrients [33,34]. Meanwhile, an increased expression of the majority of detected SMs in the root may indicate other activities of the compounds, such as stimulation of the root’s capacity to absorb micronutrients [35], including in situations of insufficient water supply. This is particularly evidenced by our identification in the roots of immature plants of lipophilic alkane hydrocarbons, such as geneucosan and tetratetracontan (11.6%), which, according to the literature, are characteristic of arid regions [36].
The root is the solitary source of inorganic nitrogen, the basis of proteins and nucleic acids. Organic forms of nitrogen are frequently shaped by incorporating the ammonium ion into the composition of amino groups and amide groups through reactions already catalyzed by numerous enzymes in the early stages of plant development. Nitrogen can then pass into several carbon compounds, having been included in the composition of an organic compound. The carbon compounds accumulating in various sink organs play a significant role both as structural components of cells and as participants in respiratory metabolism [37]. This is attested by the amino acids and its derivatives identified by us in the root and shoot and six-membered nitrogen heterocycles (1.8% in the shoot) and pyrroles (0.6%) in the shoot.
We observed the highest terpene concentration in R. semenovii plants during the initial stages of development. The biosynthesis of isoprenoids (terpenoids) occurs in the plant under intense insolation, a high temperature, and a low concentration of carbon dioxide in the air by combining five-carbon fragments. Without its participation, the processes of plant growth and development are impossible, since many phytohormones belong to this class of compounds [37,38,39]. Thus, 3,7,11,15-tetramethyl-2-hexadecen-1-ol (9.8%), identified by us in the shoot, which can be considered as a hydrogenated diterpene alcohol, is a part of chlorophyll. We assume that the shifting of squalene synthetase in photosynthetic immature plants at the phase of squalene and supraene (10.5%) identified in the root and shoot activates a specific isoprenoid pathway for sterol synthesis in R. semenovii. Sterols, in turn, affect the mobility of the bilayer of cell membranes, reduce their fluidity and permeability, adjust the phase transitions of phospholipids, and influence the movement of dissolved substances and cell components through the bilayer [33]. In the meantime, the main role of terpenoids is to protect plants from various adverse environmental effects, including macro- and micro-pests [28,40,41]. However, we believe that the additional reduction in sterol synthesis during ontogenesis indicated by our study is connected with the regulation of squalene synthetase activity. This is presumably a key moment in the control of carbon flux and the formation of end products [42].
We identified ubiquinones, such as tocopherols, exclusively in the root and shoot of R. semenovii immature plants. Tocopherols in immature plants, as previously said, can serve as antioxidants in oxidative reactions under diverse abiotic conditions [4], producing phenoxyl radicals and interacting with peroxide radicals to create quinones, dimers, and trimers [43]. The same processes appear to work in natural unstable natural environments, leading to the transition of ubiquinones.
As our experimental data reveal, there is a shift in the attractor activity of organs through the ontogenesis process, which represents the stages of the execution of the morphogenetic program of development. This is clearly demonstrated by the discovered negative association between the concentration of fatty acid esters in the root and shoot of R. semenovii. While FAs are essential components of all plant cells [44] and precursors of the key plant hormones involved in stress tolerance [45], the significance of their highest concentration in the immature root and shoot during seed development in mature plants is undeniable.
In herbaceous perennials, such as R. semenovii, the transition to a new level of source–sink interaction underlies essential processes and characteristics, such as flowering, reproductive ability, and, of course, resistance to multiple stressors, since the movement of carbohydrates from “source” organs provides the substrates required for the growth of “sink” organs [46,47,48]. In this way, phosphoric acid esters were detected in immature plants R. semenovii in the shoot (0.39%) and in flowering plants in the shoot and in flowers (1.42 and 1.36%, respectively). In our opinion, this fact suggests that, when the primary products of photosynthesis are spent on respiration, the energy stored in the form of high-energy ester bonds of phosphoric acid is used in growth processes to maintain the status quo.
Photosynthesis and carbon and nitrogen metabolism, as well as pyruvate and glycolysis/gluconeogenesis, are considered to be the processes that have the most impact on source–sink interactions and the modifications connected with them [49]. We can assume from the experimental data that the highest levels of carbohydrates and its derivatives (12.4%) and hydrocarbons (1.4%), as well as aldehydes (5.9%) and ketones, including cyclic ketones (15.2%), are in the leaves of flowering plants R. semenovii, because the functioning photosynthetic leaves and other green tissues during reproductive growth are a main source of carbon and organic nitrogen. In the meantime, as we can see, the roots accumulating carbon in the form of carbohydrates and its derivatives (5.8%), mono- and dicarboxylic acid esters (25.2%), phenols (1.4%), and nitrogen in the form of oximes (11.1%) become one of the competing colors of sink photosynthates. The cells of the parenchyma and phloem of the root at this stage of ontogenesis can perform as a reserve pool for the temporary storage of C and N. If, before seed setting, they act as a sink, then, during seed setting, they frequently play the role of a source [50,51]. Thus, it was indicated in the literature that histochemical studies revealed phenolic substances in the rhizomes and roots of R. rosea that were localized not only in parenchymal, but in vascular tissues as well [52].
If the main function of leaves during the flowering stage is to fix CO2 through photosynthesis (source), then flowers (as a sink) are largely dependent on organic molecules synthesized in leaves and roots [53]. Nevertheless, flowers are not just a sink of carbohydrates and amino acids. As presented in the literature, they utilize them as a basis for the synthesis of enzymes and structural proteins, as well as precursors of nitrogen-rich secondary metabolites and signaling molecules [54,55,56]. We are aware of the possibility of increasing the level of amino acids in flowers in response to heat stress [57]. However, a detailed analysis of the metabolism of nitrogenous compounds at the flowering stage does not exist yet. According to our results, a relatively high content of hydroxypyridines (alkaloids) (6.2%) and aliphatic nitriles (2.4%) in R. semenovii flowers is presented. These alkaloids can be involved in a “sourcesink interaction” in a certain balance between distribution and degradation in the production of amino acids [58]. Moreover, aliphatic nitriles decompose under physiological conditions with the formation of the corresponding carbonyl compound and hydrocyanic acid, which induces the toxicity of plants and their protection from being consumed by animals.
Fundamentally, flower nectar is an aqueous solution of sucrose, glucose, and fructose [52]. Among other things, this is likewise confirmed by our experimental data demonstrating an almost 17% sucrose level in the R. semenovii flower. According to Southwick, nectar is an extremely powerful sink [59]. The energy used to produce flower nectar is almost double that stored in seeds. It is known that the level of complexity of communication between pollen and pistil makes the pollination process extremely susceptible to numerous stress factors [60]. However, the role of metabolism and hormonal signaling in conferring tolerance to abiotic stresses at this stage of ontogeny has not been fully studied so far [61]. We assume that the level of stress tolerance of a R. semenovii flower can primarily determine the presence of terpenoids (1.4%), lactones (9.7%), phenols (1.8%), and alcane such as heneicosane (21.3%) detected by this experiment, which, according to the literature, quantitatively depends on the type of habitat [61]. Furthermore, signaling molecules formed from the group of polyunsaturated fatty acids are involved in the formation of body responses to various environmental signals [4,62].
With a sufficient long-term supply of assimilates, particularly nitrogen, from the roots at the late stages of vegetation, a mild stimulating effect on developing seeds may occur. The seeds perform the function of the main sink, which activates the formation of the endosperm [63]. The enhanced sink strength in late grain filling stages can eventually lead to the higher conversion efficiency of stem and shell stocks for grain filling as well [64]. Our experiments revealed an increased content of fatty acids esters (95.3%) and terpenes (4.7%) in shoot and seeds at this stage of ontogenesis. The obtained results also confirm the opinion that, by the end of the seed formation phase (as the power of absorption of the latter increases), the supply of assimilates to the roots reduces [65]. On this metabolic spectrum, biologically active oximes (12.3%), lactones (9.3%), cyclic ketones (7.2%), alcohols (6%), and furan derivatives (5.1%) dominate in the root. We have previously detected elevated concentrations of some of them under the influence of induced cold stress [4]. Thus, we can refer to the active formation of the stored SM pool, since cold exposure in situ is a natural phenomenon at this stage of ontogeny and the active vegetation of terrestrial organs is terminated.
According to Suzich et al. [66], up to 25% of the total carbon flux in higher plants passes through the shikimate pathway. A significant part of one of the final products of this metabolic pathway is consumed in the formation of the carbon skeleton of phenols and the accumulation of phenolic compounds [5]. Meanwhile, temperature, precipitation, or solar insolation do not directly influence the content of phenolic compounds in plant tissues. However, they can influence the signaling substances that regulate the transitions of ontogeny stages, which, in turn, causes an adjustment in the biochemical composition [67]. In general, we ascertained a change in the content of phenols in the organs of R. semenovii in the dynamics of vegetation, with their maximum content in the root at the stage of seed maturation. At the same time, we identified them in the shoot of immature plants (0.83%); in the root, the shoot, and flowers (1.39, 0.93, and 1. 81%, respectively) of flowering plants, and in the root (3.01%) of adult plants during seed maturation.
Molecules of the valuable phenolic chemical “salidroside,” which contains a benzene ring, are also products of a specific metabolism along the shikimate pathway. According to the literature, the high content of phenolic compounds, which include salidroside, and their most dramatic quantitative changes are observed during periods of the greatest intensity of plant life functions [68,69]. It is observed in the literature that the maximum level of accumulation of such SMs as essential oils and steroidal glycosides often falls in the period of budding and flowering [68]. Kiryanov et al. [70] and Kurkin et al. [71] hence recorded the maximum accumulation of salidroside in the root of R. rosea in the flowering phase, which is consistent with the data of our study on the accumulation of salidroside in the root of R. semenovii during this period. Our results are likewise consistent with those of Kim [72] and Rybakova [59] on the presence of salidroside in the shoot of R. rosea during flowering, with amounts ranging from 0.08 to 0.74% based on the dry weight.
At the same time, we discovered positive dynamics of salidroside accumulation in the shoot of R. semenovii during the growing season, with a maximum during seed maturation, which can serve as a basis for recommending plant material collection during this period without damaging the plant’s root system.
Consequently, the analysis of multidirectional and coordinated source–sink interactions determines the correctness of this approach toward the complex study of the integral metabolism of a plant organism in the dynamics of vegetation in situ. This approach may lead to a further comprehension of the source–sink interaction and, in turn, contribute to the more optimal timing of the collection of medicinal plant materials. In the future, this method may contribute to the rational manipulation of “source–sink” mechanisms to identify new alternative opportunities for obtaining valuable herbal medicines.

4. Materials and Methods

4.1. Plant Material

Rhodiola semenovii (Regel and Herder) Boriss. plants are immobile tap-rooted vegetative short-rhizome perennials. The inflorescence is a long, dense spiky raceme. Flowering occurs 3 to 4 years after sowing [73,74,75]. R. semenovii prefers high soil moisture and a sunlight location [76]. Experimental plants were selected at an altitude of 2350 m above sea level in the foothills of the Trans-Ili Alatau (latitude: 43°04′21″ N, longitude: 76°59′07″ E) in the dynamics of vegetation (10 May, 10 July, 5 September). The average annual air temperature at this altitude was +3.12 °C and precipitation was, on average, 881 mm per year [77].
Plant material of R. semenovii was identified in the Republican State Enterprise at the Institute of Botany and Phytointroduction of the Ministry of Education and Science of the Republic of Kazakhstan. Plant number of R. semenovii in the seed bank—3885.
Each analyzed group of plant tissues consisted of one shoot and a part of the rhizome from each of the three plants of the same age growing close to each other to ensure the reliability of the data obtained and minimal damage to the living plants.

4.2. Determination of Organic Compounds in Extracts

One of the best methods for identifying SM is gas chromatography–mass spectrometry (GC-MS), which allows for the isolation and analysis of compounds in a single step using a mass detector and available GC-MS libraries [78]. Gas chromatography with mass spectrometric detection (Agilent 6890 N/5973 N, Santa Clara, CA, USA) was used for determination of organic compounds. For this experiment, plant tissue samples were fixed in 96% ethanol at a ratio of 100 g of tissue: 500 mL of ethanol. The extraction was carried out in an orbital shaker in two stages (72 h each) with the same solvent until a clear colorless solvent was obtained. Sample volume 1.0 µL, sample injection temperature 260 °C, without flow division. Each sample was injected into the GC-MS system one time (three technical repetitions in total). Separation was carried out using a chromatographic capillary column DB-35 MS with a length of 30 m, an inner diameter of 0.25 mm, and a film thickness of 0.25 µm at a constant carrier gas (helium) velocity of 1 mL/min. The chromatographic temperature was programmed from 40 (exposure 0 min) to 150 °C with a heating rate of 10 °C/min (exposure 0 min) and up to 300 °C with a heating rate of 5 °C/min (exposure 10 min). Detection was carried out in the SCAN m/z 34–850 mode. Agilent MSD ChemStation software (version 1701EA) (Santa Clara, CA, USA) was used to control the gas chromatography system and to register and process the obtained results and data. For data processing, the average values of the obtained data were taken. Data processing included determination of retention times and peak areas, as well as processing; spectral information was obtained using a mass spectrometric detector. The Wiley 7th edition and NIST’02 libraries were used to decode the obtained mass spectra (the total number of spectra in the libraries is more than 550 thousand). The chromatograms and tables are presented in the Supplementary Materials (Tables S1–S3, Figures S1–S7).

4.3. Determination of Salidrosid

Liquid chromatography (LC) is a highly selective, but extremely flexible and very sparing method for isolating secondary metabolites from plants with weak chromophores [79]. Water–alcohol extracts of R. semenovii organs were kept at a temperature of +40–50 °C. The extracts were evaporated to a constant weight of dry residues (within 10–12 h). Liquid chromatography was carried out on a Milichrom-A-02 liquid chromatograph (“EcoNova” JSC, Novosibirsk, Russian Federation) with a chromatographic column 75 × 2 mm filled with a ProntoSIL-120-5-C18 sorbent. A total of 20 μL of the dried extract solution (solvent MeOH-H2O, 2:1) was collected into the needle of the sample injection device; the sample was injected into the device. Chromatography was performed in gradient mode. The eluent feed rate was 200 µL/min. Detection was under-taken at a wavelength of 220, 280 nm. Gradient composition: 300 µL methanol–0.05 N H3PO4 mixture (1:9, v/v)—2200 µL methanol–0.05 N H3PO4 mixture (11:9, v/v); further, a gradual increase in the concentration of methanol to pure. The duration of the analysis was 20 min. The retention time of tyrosol was 6.5 to 7.5 min. The limit of detection of tyrosol in the described experiments was 0.005% (for the dry part of the extract). The location of the tyrosol peak on the chromatogram was determined by the addition method. The concentration of tyrosol was determined in comparison with the chromatogram of pure tyrosol (tyrosol produced by NIOCH SB RAS, SOV 98% by GLC) (Figures S8–S16). No ion chromatograms were recorded.
The dry residue content in the extract was calculated by the formula:
1: (100 × mdry residue)/mextract 1
The tyrosol content in the dry part of extract 1 was calculated by the formula:
1: 100 × S tyrosol on chrom. of extr. × Ctyrosol in calibr. sol./
S tyrosol on chrom. of calibr. sol. × Ctyrosol in calibr. sol.
The content of salidroside in the dry part of extract 2 was calculated by the formula:
C tyrosol in the dry part of extr.1 × 2.17

4.4. Statistical Analyses

All experiments were conducted in three replicates (biological and technical). The processing of data and graphing was performed using Microsoft Excel (Microsoft Corp., Redmond, Washington, DC, USA). Atypical values were excluded from the data based on t-tests, and the standard error of the average sample was calculated. Correlations between expressed metabolites in the root and shoot in the dynamics of vegetation were analyzed using the Spearman coefficient. Differences were considered significant at p < 0.05.

5. Conclusions

In this work, the features of the accumulation of some secondary metabolites of the R. semenovii plant were exposed in the dynamics of growth and development in the context of source–sink interactions in situ. Assumptions were made about which secondary metabolites determine the level of resistance to stress in R. semenovii at different stages of ontogeny in situ. For the first time, the presence of seasonal changes in the content of glycosides was demonstrated, due to a significant decrease in the content of salidroside in the root during the reproductive development of plants. At the same time, the dynamics of the enlargement in the content of salidroside during the growing season in the aerial organs, with a maximum during seed ripening, was observed. As a result, it allows for recommendations on collecting medicinal raw materials in this phase without damaging the root system.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/metabo12070622/s1, Table S1: Content of SM in immature plants of R. semenovii, Figure S1: Chromatogram of immature plants extract (roots of R. semenovii), Figure S2: Chromatogram of immature plants extract (shoots of R. semenovii), Table S2: Content of SM in flowering plants of R. semenovii, Figure S3: Chromatogram of flowering plants extract (roots of R. semenovii), Figure S4: Chromatogram of flowering plants extract (shoots of R. semenovii), Figure S5: Chromatogram of flowering plant extract (flowers of R. semenovii), Table S3: Content of SM in ripening of seeds of R. semenovii, Figure S6: Chromatogram of adult plants extract (roots of R. semenovii), Figure S7: Chromatogram of adult plants extract (shoots of R. semenovii), Figure S8: Chromatogram of tyrosol calibration solution-3 (220nm), Figure S9: Determination of salidroside content in the shoot of an immature plants of R. semenovii, Figure S10: Determination of salidroside content in the root of an immature plants of R. semenovii, Figure S11: Chromatogram of tyrosol calibration solution (280nm), Figure S12: Determination of salidroside content during the flowering in the shoot of the plants of R. semenovii, Figure S13: Chromatogram of tyrosol calibration solution-2 (220nm), Figure S14: Determination of salidroside content during the flowering in the root of the plants of R. semenovii, Figure S15: Determination of salidroside content during ripening of seeds in the shoot of the plants of R. semenovii, Figure S16: Determination of salidroside content during ripening of seeds in the root of the plants of R. semenovii.

Author Contributions

Conceptualization, N.V.T.; methodology, N.V.T. and A.E.G.; formal analysis, N.V.T., N.O.K. and G.A.S.; investigation, N.K.K. and A.E.G.; data curation, N.V.T. and N.O.K.; writing—original draft preparation, N.V.T., A.E.G. and N.D.M.; writing—review and editing N.V.T.; visualization, A.E.G. and N.D.M.; supervision, N.V.T. and N.O.K.; resource, N.O.K.; project administration, N.V.T.; funding acquisition, N.V.T. All authors have read and agreed to the published version of the manuscript.

Funding

This research was carried out in the framework of the project AP08855699 “The impact of abiotic stresses on the morphophysiological and phytochemical aspects of adaptation and biological activity of Kazakhstan plant Rhodiola semenovii Boriss.” (2020–2022). This grant is funded by the Ministry of Education and Science of the Republic of Kazakhstan.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

Authors declare that they have no conflict of interest.

References

  1. Kurmakov, A.G.; Belolipov, I.V. Wild Medicinal Plants of Uzbekistan (Botany, Chemistry, Pharmacology, Medicine); Extremum Press: Tashkent, Uzbekistan, 2012; 221p. (In Russian) [Google Scholar]
  2. Kuliev, R.Z.; Akhmedov, U.; Khalmatov, K.K.; Kuliev, Z.A. Dimeric Proanthocyanidins from Rhodiola semenovii. Chem. Nat. Compd. 2004, 40, 94–95. [Google Scholar] [CrossRef]
  3. Kuliev, Z.A.; Kim, K.K.; Vdovin, A.D.; Abdullaev, N.; Khushbaktova, Z.A.; Syrov, V.N. Oligomeric proanthocyanidin glycosides ofClementsia semenovii and their biological activity. III. Chem. Nat. Compd. 2000, 36, 60–67. [Google Scholar] [CrossRef]
  4. Terletskaya, N.V.; Korbozova, N.K.; Kudrina, N.O.; Kobylina, T.N.; Kurmanbayeva, M.S.; Meduntseva, N.T.; Tolstikova, T.G. The Influence of Abiotic Stress Factors on the Morphophysiological and Phytochemical Aspects of the Acclimation of the Plant Rhodiola semenowii Boriss. Plants 2021, 10, 1196. [Google Scholar] [CrossRef] [PubMed]
  5. Koricheva, J.; Barton, K.E. Temporal changes in plant secondary metabolite production: Patterns, causes and consequences. In The Ecology of Plant Secondary Metabolites: From Genes to Global Processes; Iason, G., Dicke, M., Hartley, S., Eds.; Cambridge University Press: Cambridge, UK, 2012; pp. 34–55. [Google Scholar] [CrossRef]
  6. Płonka, J.; Górny, A.; Kokoszka, K.; Barchanska, H. Metabolic profiles in the course of the shikimic acid pathway of Raphanus sativus var. longipinnatus exposed to mesotrione and its degradation products. Chemosphere 2020, 245, 125616. [Google Scholar] [CrossRef]
  7. Akula, R.; Ravishankar, G.A. Influence of abiotic stress signals on secondary metabolites in plants. Plant Signal. Behav. 2011, 6, 1720–1731. [Google Scholar] [CrossRef]
  8. Holeski, L.M.; Hillstrom, M.L.; Whitham, T.G.; Lindroth, R.L. Relative importance of genetic, ontogenetic, induction, and seasonal variation in producing a multivariate defense phenotype in a foundation tree species. Oecologia 2012, 170, 695–707. [Google Scholar] [CrossRef]
  9. Kursar, T.A.; Dexter, K.G.; Lokvam, J.; Pennington, R.T.; Richardson, J.E.; Weber, M.G.; Murakami, E.T.; Drake, C.; McGregor, R.; Coley, P.D. The evolution of antiherbivore defenses and their contribution to species coexistence in the tropical tree genus Inga. Proc. Natl. Acad. Sci. USA 2009, 106, 18073–18078. [Google Scholar] [CrossRef] [Green Version]
  10. Endara, M.-J.; Soule, A.J.; Forrister, D.L.; Dexter, K.G.; Pennington, R.T.; Nicholls, J.A.; Loiseau, O.; Kursar, T.A.; Coley, P.D. The role of plant secondary metabolites in shaping regional and local plant community assembly. J. Ecol. 2021, 110, 34–45. [Google Scholar] [CrossRef]
  11. Tollenaar, M.; Daynard, T.B. Effect of source-sink ratio on dry matter accumulation and leaf senesence of Maize. Can. J. Plant Sci. 2022, 62, 855–860. [Google Scholar] [CrossRef]
  12. Gaia, A.M.; Yamaguchi, L.F.; Guerrero-Perilla, C.; Kato, M.J. Ontogenetic Changes in the Chemical Profiles of Piper Species. Plants 2021, 10, 1085. [Google Scholar] [CrossRef]
  13. Marak, H.B.; Biere, A.; Van Damme, J.M.M. Fitness costs of chemical defense in Plantago lanceolata L.: Effects of nutrient and competition stress. Evolution 2003, 57, 2519–2530. [Google Scholar] [CrossRef] [PubMed]
  14. Stamp, N. Out Of The Quagmire Of Plant Defense Hypotheses. Q. Rev. Biol. 2003, 78, 23–55. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Hartmann, T. From waste products to ecochemicals: Fifty years research of plant secondary metabolism. Phytochemistry 2007, 68, 2831–2846. [Google Scholar] [CrossRef]
  16. Barton, K.E.; Koricheva, J. The Ontogeny of Plant Defense and Herbivory: Characterizing General Patterns Using Meta-Analysis. Am. Nat. 2010, 175, 481–493. [Google Scholar] [CrossRef] [Green Version]
  17. Mirajkar, S.J.; Suprasanna, P.; Vaidya, E.R. Spatial distribution and dynamics of sucrose metabolising enzymes in radiation induced mutants of sugarcane. Plant Physiol. Biochem. 2016, 100, 85–93. [Google Scholar] [CrossRef]
  18. Walters, D.; Heil, M. Costs and trade-offs associated with induced resistance. Physiol. Mol. Plant Pathol. 2007, 71, 3–17. [Google Scholar] [CrossRef]
  19. Sheen, J.; Zhou, L.; Jang, J.-C. Sugars as signaling molecules. Curr. Opin. Plant Biol. 1999, 2, 410–418. [Google Scholar] [CrossRef]
  20. Andersen, C.P. Source–sink balance and carbon allocation below ground in plants exposed to ozone. New Phytol. 2003, 157, 213–228. [Google Scholar] [CrossRef]
  21. Farrar, J.F.; Jones, D.L. The control of carbon acquisition by roots. New Phytol. 2000, 147, 43–53. [Google Scholar] [CrossRef]
  22. Cara, C.; Gauvin-Lepage, J.; Lefebvre, H.; Létourneau, D.; Alderson, M.; LaRue, C.; Beauchamp, J.; Gagnon, L.; Casimir, M.; Girard, F.; et al. Le Modèle humaniste des soins infirmiers -UdeM: Perspective novatrice et pragmatique. Rech. Soins Infirm. 2016, 125, 20–31. [Google Scholar] [CrossRef]
  23. Griffiths, C.A.; Paul, M.; Foyer, C.H. Metabolite transport and associated sugar signalling systems underpinning source/sink interactions. Biochim. Biophys. Acta-Bioenerg. 2016, 1857, 1715–1725. [Google Scholar] [CrossRef] [Green Version]
  24. Zakhozhiy, I.G.; Dalke, I.V.; Nizovtsev, A.N.; Golovko, T.K. Bioaccumulation and physiological responses of plants to man-made contamination of the environment by mercury. Theor. Appl. Ecol. 2011, 2, 37–44. (In Russian) [Google Scholar]
  25. Li, B.; Förster, C.; Robert, C.A.M.; Züst, T.; Hu, L.; Machado, R.A.R.; Berset, J.-D.; Handrick, V.; Knauer, T.; Hensel, G.; et al. Convergent evolution of a metabolic switch between aphid and caterpillar resistance in cereals. Sci. Adv. 2018, 4, eaat6797. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  26. Aslani, L.; Gholami, M.; Mobli, M.; Sabzalian, M.R. The influence of altered sink-source balance on the plant growth and yield of greenhouse tomato. Physiol. Mol. Biol. Plants 2020, 26, 2109–2123. [Google Scholar] [CrossRef] [PubMed]
  27. Zhao, B.; Ma, B.-L.; Hu, Y.; Liu, J. Source–Sink Adjustment: A Mechanistic Understanding of the Timing and Severity of Drought Stress on Photosynthesis and Grain Yields of Two Contrasting Oat (Avena sativa L.) Genotypes. J. Plant Growth Regul. 2021, 40, 263–276. [Google Scholar] [CrossRef]
  28. Erb, M.; Kliebenstein, D.J. Plant Secondary Metabolites as Defenses, Regulators, and Primary Metabolites: The Blurred Functional Trichotomy. Plant Physiol. 2020, 184, 39–52. [Google Scholar] [CrossRef]
  29. Cirak, C.; Radusiene, J.; Camas, N.; Caliskan, O.; Odabas, M.S. Changes in the contents of main secondary metabolites in two Turkish Hypericum species during plant development. Pharm. Biol. 2012, 51, 391–399. [Google Scholar] [CrossRef] [Green Version]
  30. Martínez-Peña, R.; Schlereth, A.; Höhne, M.; Encke, B.; Morcuende, R.; Nieto-Taladriz, M.T.; Araus, J.L.; Aparicio, N.; Vicente, R. Source-Sink Dynamics in Field-Grown Durum Wheat Under Contrasting Nitrogen Supplies: Key Role of Non-Foliar Organs During Grain Filling. Front. Plant Sci. 2022, 13, 869680. [Google Scholar] [CrossRef]
  31. Chang, T.-G.; Zhu, X.-G. Source–sink interaction: A century old concept under the light of modern molecular systems biology. J. Exp. Bot. 2017, 68, 4417–4431. [Google Scholar] [CrossRef]
  32. Chang, Y.; Yao, H.; Hsieh, S.; Lu, T.; Yeh, T. Quantitative determination of salidroside in rat plasma by on-line solid-phase extraction integrated with high-performance liquid chromatography/electrospray ionization tandem mass spectrometry. J. Chromatogr. B 2007, 857, 164–169. [Google Scholar] [CrossRef]
  33. Meldau, S.; Erb, M.; Baldwin, I.T. Defence on demand: Mechanisms behind optimal defence patterns. Ann. Bot. 2012, 110, 1503–1514. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Barton, K.E.; Boege, K.; Barton, K.E.; Boege, K. Future directions in the ontogeny of plant defence: Understanding the evolutionary causes and consequences. Ecol. Lett. 2017, 20, 403–411. [Google Scholar] [CrossRef] [PubMed]
  35. Hu, L.; Mateo, P.; Ye, M.; Zhang, X.; Berset, J.D.; Handrick, V.; Radisch, D.; Grabe, V.; Köllner, T.G.; Gershenzon, J.; et al. Plant iron acquisition strategy exploited by an insect herbivore. Science 2018, 361, 694–697. [Google Scholar] [CrossRef] [Green Version]
  36. van Miltenburg, J.C.; Oonk, H.A.J.; Ventola, L. Heat Capacities and Derived Thermodynamic Functions of 1-Octadecanol, 1-Nonadecanol, 1-Eicosanol, and 1-Docosanol between 10 K and 370 K. J. Chem. Eng. Data 2000, 46, 90–97. [Google Scholar] [CrossRef]
  37. Borisova, G.G.; Ermoshin, A.A.; Maleva, M.G.; Chukina, N.V. Fundamentals of biochemistry of the secondary metabolism of plants. In Learning Method. Allowance; Borisova, G.G., Ed.; Publishing House Ural.: Yekaterinburg, Russia, 2014; 128p. (In Russian) [Google Scholar]
  38. Rohmer, M.; Seemann, M.; Horbach, S.; Bringer-Meyer, S.; Sahm, H. Glyceraldehyde 3-Phosphate and Pyruvate as Precursors of Isoprenic Units in an Alternative Non-mevalonate Pathway for Terpenoid Biosynthesis. J. Am. Chem. Soc. 1996, 118, 2564–2566. [Google Scholar] [CrossRef]
  39. Temelli, F.; Saldaña, M.D.A.; Comin, L. Application of Supercritical Fluid Extraction in Food Processing. In Comprehensive Sampling and Sample Preparation; Pawliszyn, J., Ed.; Academic Press: Cambridge, MA, USA, 2012; pp. 415–440. [Google Scholar]
  40. Baldwin, I.T.; Halitschke, R.; Paschold, A.; von Dahl, C.C.; Preston, C.A. Volatile Signaling in Plant-Plant Interactions: "Talking Trees" in the Genomics Era. Science 2006, 311, 812–815. [Google Scholar] [CrossRef] [Green Version]
  41. Bouwmeester, H.; Schuurink, R.C.; Bleeker, P.M.; Schiestl, F. The role of volatiles in plant communication. Plant J. 2019, 100, 892–907. [Google Scholar] [CrossRef] [Green Version]
  42. Piironen, V.; Lindsay, D.G.; Miettinen, T.A.; Toivo, J.; Lampi, A.-M. Plant sterols: Biosynthesis, biological function and their importance to human nutrition. J. Sci. Food Agric. 2000, 80, 939–966. [Google Scholar] [CrossRef]
  43. Rontani, J.-F.; Nassiry, M.; Mouzdahir, A. Free radical oxidation (autoxidation) of α-tocopherol (vitamin E): A potential source of 4,8,12,16-tetramethylheptadecan-4-olide in the environment. Org. Geochem. 2007, 38, 37–47. [Google Scholar] [CrossRef]
  44. Lyutikova, M.N.; Turov, Y.P.; Botirov, E.H. Application of chromatography-mass spectrometry to determine free and esterified fatty acids in their combined presence in plant raw materials. Fine Chem. Technol. 2013, 8, 52–57. (In Russian) [Google Scholar]
  45. Iba, K. Acclimative response to temperature stress in higher plants: Approaches of Gene Engineering for Temperature Tolerance. Annu. Rev. Plant Biol. 2002, 53, 225–245. [Google Scholar] [CrossRef] [Green Version]
  46. Aluko, O.O.; Li, C.; Wang, Q.; Liu, H. Sucrose Utilization for Improved Crop Yields: A Review Article. Int. J. Mol. Sci. 2021, 22, 4704. [Google Scholar] [CrossRef] [PubMed]
  47. Nuccio, M.L.; Wu, J.; Mowers, R.; Zhou, H.-P.; Meghji, M.; Primavesi, L.F.; Paul, M.; Chen, X.; Gao, Y.; Haque, E.; et al. Expression of trehalose-6-phosphate phosphatase in maize ears improves yield in well-watered and drought conditions. Nat. Biotechnol. 2015, 33, 862–869. [Google Scholar] [CrossRef] [PubMed]
  48. Lee, J.; Dong, X.; Choi, K.; Song, H.; Yi, H.; Hur, Y. Identification of source-sink tissues in the leaf of Chinese cabbage (Brassica rapa ssp. pekinensis) by carbohydrate content and transcriptomic analysis. Genes Genom. 2020, 42, 13–24. [Google Scholar] [CrossRef] [PubMed]
  49. Lv, X.; Zhang, Y.; Zhang, Y.; Fan, S.; Kong, L. Source-sink modifications affect leaf senescence and grain mass in wheat as revealed by proteomic analysis. BMC Plant Biol. 2020, 20, 257. [Google Scholar] [CrossRef]
  50. Foulkes, M.J.; Slafer, G.A.; Davies, W.J.; Berry, P.M.; Sylvester-Bradley, R.; Martre, P.; Calderini, D.F.; Griffiths, S.; Reynolds, M.P. Raising yield potential of wheat. III. Optimizing partitioning to grain while maintaining lodging resistance. J. Exp. Bot. 2011, 62, 469–486. [Google Scholar] [CrossRef] [Green Version]
  51. Ho, L.C. Metabolism and Compartmentation of Imported Sugars in Sink Organs in Relation to Sink Strength. Annu. Rev. Plant Phys. 1988, 39, 355–378. [Google Scholar] [CrossRef]
  52. Erst, A.A.; Petruk, A.A.; Zibareva, L.N.; Erst, A.S. Morphological, Histochemical and Biochemical Features of Cultivated Rhodiola rosea (Altai Mountains Ecotype). Contemp. Probl. Ecol. 2021, 14, 701–710. [Google Scholar] [CrossRef]
  53. Borghi, M.; Fernie, A.R. Outstanding questions in flower metabolism. Plant J. 2020, 103, 1275–1288. [Google Scholar] [CrossRef]
  54. Ruan, Y.-L.; Patrick, J.W.; Bouzayen, M.; Osorio, S.; Fernie, A.R. Molecular regulation of seed and fruit set. Trends Plant Sci. 2012, 17, 656–665. [Google Scholar] [CrossRef] [Green Version]
  55. Borghi, M.; Fernie, A.R. Floral Metabolism of Sugars and Amino Acids: Implications for Pollinators’ Preferences and Seed and Fruit Set. Plant Physiol. 2017, 175, 1510–1524. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  56. Tegeder, M.; Hammes, U.Z. The way out and in: Phloem loading and unloading of amino acids. Curr. Opin. Plant Biol. 2018, 43, 16–21. [Google Scholar] [CrossRef] [PubMed]
  57. Southwick, E.E. Photosynthate Allocation to Floral Nectar: A Neglected Energy Investment. Ecology 1984, 65, 1775–1779. [Google Scholar] [CrossRef]
  58. Borghi, M.; De Souza, L.P.; Yoshida, T.; Fernie, A.R. Flowers and climate change: A metabolic perspective. New Phytol. 2019, 224, 1425–1441. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  59. Rybakova, G.R.; Tikhomirov, A.A.; Chepeleva, G.G. Research and study of the spectral composition of light when grown in light conditions at the exit of salidroside in Rhodiola rosea. Chem. Plant Raw Mater. 2002, 3, 77–83. (In Russian) [Google Scholar]
  60. Aniszewski, T. Alkaloids—Secrets of Life; Elsevier: Amsterdam, The Netherlands, 2007; 335p. [Google Scholar] [CrossRef]
  61. Jovanović, S.; Zlatković, B.K.; Stojanović, G.S. The chemical composition of Sedum rupestre L. ssp. rupestre epicuticular waxes: Horticultural versus the natural plant habitat. Facta Univ.-Ser. Phys. Chem. Technol. 2015, 13, 77–82. [Google Scholar] [CrossRef] [Green Version]
  62. Terletskaya, N.V.; Seitimova, G.A.; Kudrina, N.O.; Meduntseva, N.D.; Ashimuly, K. The Reactions of Photosynthetic Capacity and Plant Metabolites of Sedum hybridum L. in Response to Mild and Moderate Abiotic Stresses. Plants 2022, 11, 828. [Google Scholar] [CrossRef]
  63. Yang, J.; Zhang, J.; Huang, Z.; Wang, Z.; Zhu, Q.; Liu, L. Correlation of Cytokinin Levels in the Endosperms and Roots with Cell Number and Cell Division Activity during Endosperm Development in Rice. Ann. Bot. 2002, 90, 369–377. [Google Scholar] [CrossRef] [Green Version]
  64. Mohapatra, P.K.; Panigrahi, R.; Turner, N.C. Physiology of Spikelet Development on the Rice Panicle: Is manipulation of apical dominance crucial for grain yield improvement? Adv. Agron. 2011, 110, 333–359. [Google Scholar] [CrossRef]
  65. Chikov, V.; Abdrakhimov, F.; Bakirova, G.; Batasheva, S. The role of sink-source relationships between different organs in regulation of photosynthesis and productivity. In Proceedings of the International Symposium on Source-Sink Relationships in Plants, Kaliningrad, Russia, 21–26 May 2007; pp. 87–98. [Google Scholar] [CrossRef]
  66. Suzich, J.A.; Dean, J.F.D.; Herrmann, K.M. 3-Deoxy-d-arabino-Heptulosonate 7-Phosphate Synthase from Carrot Root (Daucus carota) Is a Hysteretic Enzyme. Plant Physiol. 1985, 79, 765–770. [Google Scholar] [CrossRef] [Green Version]
  67. Zakhozhiy, I.G. The chemical composition of the underground organs of the plant Rhodiola rosea L., cultivated in the middle-taiga subzone of the Komi Republic. Bull. Inf. Secur. 2009, 8, 9–12. (In Russian) [Google Scholar]
  68. Sleptsov, I.V.; Zhuravskaya, A.N. Dynamics of flavonoid accumulation in the leaves of Amaranthus retroflexus, Agastache rugosa and Thlaspi arvense collected in Central Yakutia. Chem. Plant Raw Mater. 2016, 3, 67–72. (In Russian) [Google Scholar] [CrossRef]
  69. Andysheva, E.V.; Khramova, E.P. A chemotaxonomic study of phenolic compounds in the species of the genus Dasiphora (Rosaceae) from the Russian Far East and Eastern Siberia. Bot. Pacifica 2020, 9, 77–83. [Google Scholar] [CrossRef] [Green Version]
  70. Kiryanov, A.A.; Bondarenko, L.T.; Kurkin, V.A.; Zapesochnaya, G.G. Dynamics of accumulation of rosavidin and salidroside in the raw materials of Rhodiola rosea cultivated in the Moscow region. Chem.-Farm. J. 1989, 4, 449–452. (In Russian) [Google Scholar]
  71. Kurkin, V.A.; Kurkina, T.V.; Zapesochnaya, G.G. Study of the dynamics of accumulation of active substances in the rhizomes of Rhodiola rosea, introduced in the Samara region. In Proceedings of the Scintific Conference “Biodiversity. Plant Introduction”, Saint-Petersburg, Russia, 12–15 December 1995; pp. 154–155. (In Russian). [Google Scholar]
  72. Kim, E.F. The content and age dynamics of the accumulation of salidroside in the aerial organs of Rhodiola rosea in connection with its introduction in different altitudinal zones of Altai. In Flora and vegetation of Siberia and the Far East; Krasnoyarsk Pedagogical University: Krasnoyarsk, Russia, 1996; pp. 255–257. (In Russian) [Google Scholar]
  73. Borisova, A.G. Abstract of the Crassulaceae DC family system. flora of the USSR (additions and changes). News Taxon. High. Plants 1969, 6, 112–121. (In Russian) [Google Scholar]
  74. Alekseeva, V.A.; Golotova, T.P.; Mikhailova, G.S. State Pharmacopoeia, 11th ed.; Medicine: Moskow, Russia, 1990; Volume 2, pp. 143–159. (In Russian) [Google Scholar]
  75. Kuliev, R.Z. Anatomical diagnosis of rhizomes and roots of Rhodiola Semenovii. Pharm. J. 2004, 2, 32–34. (In Russian) [Google Scholar]
  76. Mazurenko, M.; Andreeva, A. Succulents in the Kolyma. In The World of Plants; Capstone: Mankato, MN, USA, 2002; Volume 12, p. 14. (In Russian) [Google Scholar]
  77. Salnikov, V.; Turulina, G.; Polyakova, S.; Petrova, Y.; Skakova, A. Climate change in Kazakhstan during the past 70 years. Quat. Int. 2015, 358, 77–82. [Google Scholar] [CrossRef]
  78. Gomathi, D.; Kalaiselvi, M.; Ravikumar, G.; Devaki, K.; Uma, C. GC-MS analysis of bioactive compounds from the whole plant ethanolic extract of Evolvulus alsinoides (L.) L. J. Food Sci. Technol. 2015, 52, 1212–1217. [Google Scholar] [CrossRef] [Green Version]
  79. Theodoridis, G.A.; Gika, H.G.; Plumb, R.; Wilson, I.D. Liquid chromatographic methods combined with mass spectrometry in metabolomics. In Proteomic and Metabolomic Approaches to Biomarker Discovery, 2nd ed.; Issaq, H.J., Veenstra, T.D., Eds.; Academic Press: Cambridge, MA, USA, 2020; pp. 149–169. [Google Scholar] [CrossRef]
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Figure 1. (a) Content of secondary metabolites classes of immature plants R. semenovii, %. Values presented are means (± SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) immature plants R. semenovii.
Figure 1. (a) Content of secondary metabolites classes of immature plants R. semenovii, %. Values presented are means (± SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) immature plants R. semenovii.
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Figure 2. (a) Content of secondary metabolites classes in root and shoot of flowering plants R. semenovii, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) flowering plants R. semenovii.
Figure 2. (a) Content of secondary metabolites classes in root and shoot of flowering plants R. semenovii, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) flowering plants R. semenovii.
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Figure 3. (a) Content of secondary metabolites classes in flowers of R. semenovii, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) flower of R. semenovii.
Figure 3. (a) Content of secondary metabolites classes in flowers of R. semenovii, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) flower of R. semenovii.
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Figure 4. (a) Content of secondary metabolites classes of adult plants R. semenovii under ripening of seeds, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) adult plants R. semenovii with seeds.
Figure 4. (a) Content of secondary metabolites classes of adult plants R. semenovii under ripening of seeds, %. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments; (b) adult plants R. semenovii with seeds.
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Figure 5. Influence of the vegetation phase on the correlation relationships of the accumulation of individual groups of SM in the root and shoot of R. semenovii.
Figure 5. Influence of the vegetation phase on the correlation relationships of the accumulation of individual groups of SM in the root and shoot of R. semenovii.
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Figure 6. The content of salidroside in the tissues of R. semenovii in ontogenesis. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments.
Figure 6. The content of salidroside in the tissues of R. semenovii in ontogenesis. Values presented are means (±SD). Different letters above the bars represent significant differences at p ≤ 0.05, n = 3 plants in each of 3 replicates for all treatments.
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Terletskaya, N.V.; Korbozova, N.K.; Grazhdannikov, A.E.; Seitimova, G.A.; Meduntseva, N.D.; Kudrina, N.O. Accumulation of Secondary Metabolites of Rhodiola semenovii Boriss. In Situ in the Dynamics of Growth and Development. Metabolites 2022, 12, 622. https://doi.org/10.3390/metabo12070622

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Terletskaya NV, Korbozova NK, Grazhdannikov AE, Seitimova GA, Meduntseva ND, Kudrina NO. Accumulation of Secondary Metabolites of Rhodiola semenovii Boriss. In Situ in the Dynamics of Growth and Development. Metabolites. 2022; 12(7):622. https://doi.org/10.3390/metabo12070622

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Terletskaya, Nina V., Nazym K. Korbozova, Alexander E. Grazhdannikov, Gulnaz A. Seitimova, Nataliya D. Meduntseva, and Nataliya O. Kudrina. 2022. "Accumulation of Secondary Metabolites of Rhodiola semenovii Boriss. In Situ in the Dynamics of Growth and Development" Metabolites 12, no. 7: 622. https://doi.org/10.3390/metabo12070622

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