Growth Inhibition of Phaeocystis Globosa Induced by Luteolin-7-O-glucuronide from Seagrass Enhalus acoroides

Enhalus acoroides (E. acoroides) is one of the most common species in seagrass meadows. Based on the application of allelochemicals from aquatic plants to inhibit harmful algal blooms (HABs), we used E. acoroides aqueous extract against harmful algae species Phaeocystis globosa (P. globosa). The results showed that E. acoroides aqueous extract could significantly inhibited the growth of P. globosa, decrease the chlorophyll-a content and photosynthetic efficiency (Fv/Fm) values of P. globosa, followed by vacuolization, plasmolysis, and the destruction of organelles. Twelve types of major chemical constituents were identified in E. acoroides aqueous extracts by ultraperformance liquid chromatography-high resolution mass spectrometry (UPLC-HRMS), including six flavonoids, two homocyclic peptides, two long-chain aliphatic amides, one tannin, and one nitrogen heterocyclic compound. Flavonoids were the characteristic chemical constituents of E. acoroides aqueous extract. Furthermore, the antialgal activity of luteolin-7-O-glucuronide (68.125 μg/mL in 8 g/L E. acoroides aqueous extract) was assessed. The EC50–96 h value was 34.29 μg/mL. In conclusion, the results revealed that luteolin 7-O-glucuronide was one of the antialgal compounds of E. acoroides aqueous extract, with potential application as novel algaecide.


Introduction
Harmful algal blooms (HABs) cause a series of ecological problems. They contribute to the death of fish, birds, and mammals (including humans), cause respiratory or digestive tract problems, as well as losses of coastal resources [1]. Phaeocystis globosa (P. globosa) is regarded as an unwanted algal species. It is associated with shellfish mortality and acid rain, and can produce hemolytic toxins, bad odors, and form foam through high biomass accumulation [2,3]. P. globosa blooms not only destroy marine ecosystem but also are hazardous to human health and aquaculture. One of the most striking characteristics of P. globosa is that they have a heteromorphic life cycle, with solitary cells as well as colonies. P. globosa blooms are frequently found in China, Viet Nam, and the eastern English Channel [4][5][6]. This inspired scientists to develop effective methods to inhibit and prevent the P. globosa blooms.
Biological methods, which rely on allelochemicals from aquatic plants to constrain harmful algal blooms, have become a research hotspot for their high biodegradability, low toxicity, and low cost [7][8][9]. Seagrasses are submerged marine aquatic plants that play an important role in coastal ecosystems such as providing food and habitat for animals, taking up metals, and contributing to the primary production [10]. Seagrasses are abundant in secondary metabolites, which is thought to be a defense mechanism that provides the plant with the capability to survive and resist different stress types, such as larvae feeding, fungal and bacterial infection [11]. Many studies reported that secondary metabolites from seagrasses have antibacterial, antiviral, anti-fungal, anti-inflammatory, and antioxidant activities, but only a few studies have examined the antialgal activity of seagrasses for biological application [12,13]. Consequently, there is a need to explore the antialgal activity of seagrasses.
Enhalus acoroides (E. acoroides) is a morphologically large, long-lived, and common seagrass [14]. In addition to being edible, E. acoroides has been used as a remedy against stings, and is also effective for muscle pains, wounds, and stomach problems [13]. Interestingly, red tides rarely occur in places where E. acoroides grows, and the seawater is very clear in such places [15]. Previous studies reported that E. acoroides synthesized flavonoids to resist larvae feeding and bacterial infection, which implied that the seagrass may have inhibitory effects on algae [16]. Hence, further studies are needed to examine whether E. acoroides produces secondary metabolites with antialgal activity leading to the rarity of red tides in places where E. acoroides grows. In order to develop antialgal compounds from E. acoroides, we investigated the inhibitory effects of E. acoroides aqueous extracts on the growth of P. globosa, identified the chemical constituents, and uncovered the antialgal compounds.

Materials and Culture Conditions
E. acoroides were collected from Xincun bay, ling shui county, Hainan province (18 • 23 N, 109 • 59 E), and stored in a heat insulated box at room temperature (about 4 • C). P. globosa were obtained from the Research Center of Hydrobiology, Jinan University, Guangzhou, China. Algal cells were incubated in F/2 medium under a photoperiod of 12 h (light):12 h (dark) at 22-24 • C and an irradiance of 100 µmol photons m −2 s −1 .

Preparation of E. acoroides Aqueous Extract
The seagrass was cleaned with distilled water and scrubbed with a soft brush to remove algae and other microorganisms attached to its surface as much as possible. Then, the cleaned seagrass was dried in a drying oven at 65 • C to constant weight. After drying, the seagrass was ground into powder, filtered by a 40-mesh sieve, mixed with seawater (1:50 w/v), and placed in a constant temperature water bath electromagnetic stirring pot of 25 • C for 48 h at middle-speed. The aqueous extract was then centrifuged for 15 min at 5000 rpm. The supernatant was filtered with 0.22 µm filter to remove all microorganisms and was stored at 4 • C before use.

Treatments with E. acoroides Aqueous Extract
To study the inhibitory effects of different concentrations of E. acoroides aqueous extract on the growth of P. globosa, conical flasks (50 mL) were prepared and autoclaved. Each group of flasks contained 20 mL culture media. The aqueous extract concentration in the culture medium in each group was 0, 2, 4, 6, and 8 g/L. The group without aqueous extract served as the control sample. The initial algal density (IAD) in each flask was 1 × 10 5 cells/mL, and each flask was inoculated with P. globosa culture in the exponential growth phase. Each treatment was replicated three times. The cultures were incubated under the conditions mentioned above. To obtain the algal growth curve under treatments with different concentrations of aqueous extract, the algal cells were counted from 0 to 96 h under a light microscope with a hemocytometer.
The inhibition rate (IR) of P. globosa growth under treatment of different concentrations of E. acoroides aqueous extract was calculated by the following equation: where N is the Algal density of the treatment group (cell/mL); N 0 is the Algal density of the control group (cell/mL).

Chlorophyll-a Concentration and Photosynthetic Efficiency (Fv/Fm) Assays
Chlorophyll-a is the primary photosynthetic pigment. Chlorophyll-a concentration was measured according to previous methods [17]. Briefly, the algal cells were collected and centrifuged. The pigments were extracted using 95% ethanol at 4 • C in the dark for 48 h. After extraction, the samples were centrifuged for 30 min at 2500× g. The supernatant was used to measure absorbance values at 665 nm and 645 nm. The pigments were calculated according to the following formula: The chlorophyll fluorescence parameter, Fv/Fm is used to reflect the maximum quantum efficiency of PSII photochemistry. A Plant Efficiency Analyzer (PEA MK2, Hansatech Instrument LTD, Norfolk, UK) was used to measure Fv/Fm. The algal cultures (2 mL) were incubated in the dark for 20 min and then Fv/Fm was measured.

Transmission Electron Microscopy (TEM) Analysis
The algal cells were collected (2000× g, 15 min) and then fixed overnight at 4 • C in PBS buffer containing 2.5% glutaraldehyde (v/v). The fixed algal cells were washed three times in PBS buffer (50 mM, pH 7.4) and post-fixed for 2 h in 1% OsO 4 in the same buffer at room temperature. After being washed three times, the samples were dehydrated through a graded ethanol series (30,50,70,80,85,90, and 100% (v/v in ddH 2 O); 15-20 min at each concentration), then permeated and embedded in araldite resin. Sections (80-100 nm), obtained with an ultramicrotome, were stained in 3% acetic acid uranium-citric acid and viewed using TEM.
The quantification of luteolin-7-O-glucuronide was performed using external calibration. Compound was dissolved in methanol using a vortex mixer to prepare standard solutions (1 µg/mL) and the 8 g/L E. acoroides aqueous extract was diluted to accurately measure the compound. The injection volume was 1.0 µL. UPLC-HRMS conditions were as described above. The results are presented as µg per mL.

Data Analysis
Statistical analysis of data was performed using GraphPad Prism 7 software. The means and standard deviations (SD) of all data were determined and graphed. Students' t-test was used, and p < 0.05 and p < 0.01 were considered significant.

Effects of E. acoroides Aqueous Extract on the Growth of P. globosa
The relationship between the concentration of aqueous extract and the growth of P. globosa is shown in Figure 1A. After 48 h, the inhibitory effects of E. acoroides aqueous extract concentrations from 2 g/L to 8 g/L on P. globosa were significant (p < 0.01). Also, the IR increased with the increase in aqueous extract concentration and exposure time ( Figure 1B). At 96 h, the IR of P. globosa exposed to 2, 4, 6, and 8 g/L of E. acoroides aqueous extract peaked, which were 27.52% (p < 0.01), 40.32% (p < 0.01), 71.10% (p < 0.01), and 98.02% (p < 0.01), respectively.

Data Analysis
Statistical analysis of data was performed using GraphPad Prism 7 software. The means and standard deviations (SD) of all data were determined and graphed. Students' t-test was used, and p < 0.05 and p < 0.01 were considered significant.

Effects of E. acoroides Aqueous Extract on the Growth of P. globosa
The relationship between the concentration of aqueous extract and the growth of P. globosa is shown in Figure 1A. After 48 h, the inhibitory effects of E. acoroides aqueous extract concentrations from 2 g/L to 8 g/L on P. globosa were significant (p < 0.01). Also, the IR increased with the increase in aqueous extract concentration and exposure time ( Figure 1B). At 96 h, the IR of P. globosa exposed to 2, 4, 6, and 8 g/L of E. acoroides aqueous extract peaked, which were 27.52% (p < 0.01), 40.32% (p < 0.01), 71.10% (p < 0.01), and 98.02% (p < 0.01), respectively.

Effects of E. acoroides Aqueous Extract on Chlorophyll-a Concentration and Fv/Fm of P. globosa
As shown in Figure 1C, there was significant difference (p < 0.01) between the treatment groups of 2, 4, 6, and 8 g/L and the controls after 72 h. The chlorophyll-a content reached the highest in the experimental groups of 2, 4, and 6 g/L after 96 h, and were 79.60% (p < 0.01), 69.47% (p < 0.01), and 27.91% (p < 0.01) compared to the controls, respectively. The chlorophyll-a content in the group of 8 g/L remained at a low level, and was 4.96% (p < 0.01) as compared to the control after 96 h. The Fv/Fm values in the treatment groups of 2, 4, 6, and 8 g/L showed a downward trend with prolonged exposure time ( Figure 1D). At 96 h, the values reached the lowest, and were 96.92% (p < 0.01), 80.32%

Effects of E. acoroides Aqueous Extract on Chlorophyll-a Concentration and Fv/Fm of P. globosa
As shown in Figure 1C, there was significant difference (p < 0.01) between the treatment groups of 2, 4, 6, and 8 g/L and the controls after 72 h. The chlorophyll-a content reached the highest in the experimental groups of 2, 4, and 6 g/L after 96 h, and were 79.60% (p < 0.01), 69.47% (p < 0.01), and 27.91% (p < 0.01) compared to the controls, respectively. The chlorophyll-a content in the group of 8 g/L remained at a low level, and was 4.96% (p < 0.01) as compared to the control after 96 h. The Fv/Fm values in the treatment groups of 2, 4, 6, and 8 g/L showed a downward trend with prolonged exposure time ( Figure 1D). At 96 h, the values reached the lowest, and were 96.92% (p < 0.01), 80.32% (p < 0.01), 71.41% (p < 0.01), and 60.95% (p < 0.01) compared to the controls after exposure to the E. acoroides aqueous extract at concentrations of 2, 4, 6, and 8 g/L, respectively.

Effects of E. acoroides Aqueous Extract on Subcellular Structure of P. globosa
Transmission electron microscopy (TEM) revealed modifications in the ultrastructure of P. globosa due to the effects of E. acoroides aqueous extract. Figure 2A shows that the algal cells in the control had intact cellular morphology and microscopic structure. Figure 2B shows obvious plasmolysis and vacuolization. Many organelles were severely damaged at this time point. Considerable changes appeared in the chloroplasts, especially in the loose lamellar structures, which was not as compact as before. After 96 h exposure, the plasma membrane was severely damaged and cellular inclusions were released from cells, indicating the death of algal cells ( Figure 2C). Transmission electron microscopy (TEM) revealed modifications in the ultrastructure of P. globosa due to the effects of E. acoroides aqueous extract. Figure 2A shows that the algal cells in the control had intact cellular morphology and microscopic structure. Figure 2B shows obvious plasmolysis and vacuolization. Many organelles were severely damaged at this time point. Considerable changes appeared in the chloroplasts, especially in the loose lamellar structures, which was not as compact as before. After 96 h exposure, the plasma membrane was severely damaged and cellular inclusions were released from cells, indicating the death of algal cells ( Figure 2C).

Chemical Constituent Analysis of Aqueous Extract from E. acoroides
In order to identify the compounds in E. acoroides aqueous extract, positive and negative ionization modes were used. Table 1 and Figure 3 indicated that fourteen peaks were detected from E. acoroides aqueous extract, excluding the compounds in the sterilized artificial seawater ( Figure 3C and D). Briefly, a total of 12 major chemical constituents were identified (Figure 4), and mass spectrograms of all identified compounds are presented in Figures S2-S15. Compounds 1 and 2 were identified as polypeptides, but the specific structures could not be accurately inferred due to their low contents in E. acoroides aqueous extract and the poor information of secondary ion mass spectrometry. Among the 12 identified compounds, there were six flavonoids, two homocyclic peptides, two long-chain aliphatic amides, one tannin, and one nitrogen heterocyclic compound.

Chemical Constituent Analysis of Aqueous Extract from E. acoroides
In order to identify the compounds in E. acoroides aqueous extract, positive and negative ionization modes were used. Table 1 and Figure 3 indicated that fourteen peaks were detected from E. acoroides aqueous extract, excluding the compounds in the sterilized artificial seawater ( Figure 3C,D). Briefly, a total of 12 major chemical constituents were identified (Figure 4), and mass spectrograms of all identified compounds are presented in Figures S2-S15. Compounds 1 and 2 were identified as polypeptides, but the specific structures could not be accurately inferred due to their low contents in E. acoroides aqueous extract and the poor information of secondary ion mass spectrometry. Among the 12 identified compounds, there were six flavonoids, two homocyclic peptides, two long-chain aliphatic amides, one tannin, and one nitrogen heterocyclic compound.

Antialgal Activity of Luteolin-7-O-glucuronide
Six of twelve major chemical constituents were flavonoids, indicating that flavonoids were the characteristic chemical constituents of E. acoroides aqueous extract. Many studies have demonstrated that flavonoids have great antialgal activity [18]. Therefore, we were mainly focused on flavonoids in our study. Among the flavonoids, the peak area of luteolin-3′,7-O-diglucuronide was the largest (430,617) in Table 2, followed by luteolin-7-O-glucuronide (268,581). There was no direct relation between concentrations and peak area, because the ionization difficulty and ionic stability of different compounds were different. However, we could compare concentrations of flavonoid compounds in aqueous extract based on peak area, because similar classes of compounds may possess similar chemical features and ionization potential [19]. Therefore, we speculated that luteolin-3′,7-Odiglucuronide and luteolin-7-O-glucuronide may have relatively higher concentrations compared to other flavonoids in aqueous extract, which might have inhibitory effects on P. globosa.

Antialgal Activity of Luteolin-7-O-glucuronide
Six of twelve major chemical constituents were flavonoids, indicating that flavonoids were the characteristic chemical constituents of E. acoroides aqueous extract. Many studies have demonstrated that flavonoids have great antialgal activity [18]. Therefore, we were mainly focused on flavonoids in our study. Among the flavonoids, the peak area of luteolin-3 ,7-O-diglucuronide was the largest (430,617) in Table 2, followed by luteolin-7-O-glucuronide (268,581). There was no direct relation between concentrations and peak area, because the ionization difficulty and ionic stability of different compounds were different. However, we could compare concentrations of flavonoid compounds in aqueous extract based on peak area, because similar classes of compounds may possess similar chemical features and ionization potential [19]. Therefore, we speculated that luteolin-3 ,7-O-diglucuronide and luteolin-7-O-glucuronide may have relatively higher concentrations compared to other flavonoids in aqueous extract, which might have inhibitory effects on P. globosa. Luteolin-7-O-glucuronide has good prospects for application compared to luteolin-3 ,7-O-diglucuronide. Luteolin-7-O-glucuronide can treat diseases related to reactive species production and oxidative stress and can resist to bacterial infections, thus it may have inhibitory effects on P. globosa [20,21]. Yet, there are no studies on the activity of luteolin-3 ,7-O-diglucuronide. Therefore, luteolin-7-O-glucuronide was selected as the novel algaecide to control P. globosa blooms and the inhibitory effects of luteolin-7-O-glucuronide on P. globosa were investigated in our research. Figure 5A shows that the algal density of P. globosa was significantly decreased (p < 0.01) after 48 h exposure to different concentrations of luteolin-7-O-glucuronide. The IR increased with the increase of luteolin-7-O-glucuronide concentration and exposure time ( Figure 5B). After 96 h, the IR was 26.92%

Discussion
Many studies have used the plant aqueous extract, organic extract, thalli, culture filtrate, fresh tissue, dry tissue, and dry powder to control HABs [22][23][24][25][26]. However, only a few studies have uncovered antialgal compounds from plants [27][28][29]. In the present study, E. acoroides aqueous extract had a notable inhibitory effect on P. globosa, which was concentration-dependent. Therefore, the antialgal activities of E. acoroides aqueous extract were believed to indicate the existence of antialgal active substances. To explore any damage to the photosynthetic system and subcellular structure of P. globosa, further experiments were conducted. Chlorophyll-a content can be used to reflect potential photosynthesis capacity and estimate the biomass of algae, and Fv/Fm was used to evaluate photosynthesis efficiency [30]. Based on the decrease in chlorophyll-a concentration and Fv/Fm values, we concluded that the growth and reproduction of P. globosa was inhibited and its photosynthetic system was destroyed, which was also confirmed by the seriously damaged chloroplast. Under TEM, the lamellar structures of chloroplasts became looser with exposure time, finally breaking up. Other obvious differences could be observed between the treated and untreated cells, such as vacuolization, organelle decomposition, and plasmolysis, finally leading to the death of treated cells. Previous studies have reported that prodigiosin and the supernatant of bacterium inhibited the growth of P. globosa and destructed photosynthetic system and subcellular structure, which were consistent with our findings [17,31,32].
Our research indicated that E. acoroides aqueous extract could be used to control HABs. Nevertheless, considering that E. acoroides grows along the coastline, between 40 and 160m from the shore, these plants are not easily assessed [33]. Thus, the following step is to investigate whether the antialgal compounds from E. acoroides could be found in other plants that are easier to access. In this study, we used UPLC-HRMS to identify the chemical constitutes in E. acoroides aqueous extract, including six flavonoids, two homocyclic peptides, two long-chain aliphatic amides, one tannin, and one nitrogen heterocyclic compound. There were many types of flavonoids in E. acoroides aqueous

Discussion
Many studies have used the plant aqueous extract, organic extract, thalli, culture filtrate, fresh tissue, dry tissue, and dry powder to control HABs [22][23][24][25][26]. However, only a few studies have uncovered antialgal compounds from plants [27][28][29]. In the present study, E. acoroides aqueous extract had a notable inhibitory effect on P. globosa, which was concentration-dependent. Therefore, the antialgal activities of E. acoroides aqueous extract were believed to indicate the existence of antialgal active substances. To explore any damage to the photosynthetic system and subcellular structure of P. globosa, further experiments were conducted. Chlorophyll-a content can be used to reflect potential photosynthesis capacity and estimate the biomass of algae, and Fv/Fm was used to evaluate photosynthesis efficiency [30]. Based on the decrease in chlorophyll-a concentration and Fv/Fm values, we concluded that the growth and reproduction of P. globosa was inhibited and its photosynthetic system was destroyed, which was also confirmed by the seriously damaged chloroplast. Under TEM, the lamellar structures of chloroplasts became looser with exposure time, finally breaking up. Other obvious differences could be observed between the treated and untreated cells, such as vacuolization, organelle decomposition, and plasmolysis, finally leading to the death of treated cells. Previous studies have reported that prodigiosin and the supernatant of bacterium inhibited the growth of P. globosa and destructed photosynthetic system and subcellular structure, which were consistent with our findings [17,31,32].
Our research indicated that E. acoroides aqueous extract could be used to control HABs. Nevertheless, considering that E. acoroides grows along the coastline, between 40 and 160m from the shore, these plants are not easily assessed [33]. Thus, the following step is to investigate whether the antialgal compounds from E. acoroides could be found in other plants that are easier to access. In this study, we used UPLC-HRMS to identify the chemical constitutes in E. acoroides aqueous extract, including six flavonoids, two homocyclic peptides, two long-chain aliphatic amides, one tannin, and one nitrogen heterocyclic compound. There were many types of flavonoids in E. acoroides aqueous extract compared to other types of compounds, which was similar to a previous report [16]. Our research revealed that flavonoids were the characteristic chemical constituents of E. acoroides aqueous extract and according to the literature flavonoids usually have good antialgal activity [18]. Thus, in this study, luteolin-7-O-glucuronide was selected as the representative flavonoids to investigate the potential antialgal activity. The EC 50-96h of luteolin-7-O-glucuronide was 34.29 µg/mL, indicating that it was an effective algaecide. The concentration of luteolin-7-O-glucuronide was 68.125 µg/mL in 8 g/L E. acoroides aqueous extract (Table 3), which means that approximately 80.03% P. globosa was constrained at this concentration at 96 h ( Figure S1). Combined with the IR of 8 g/L E. acoroides aqueous extract, which was 99.78% at 96 h ( Figure 1B), we concluded that luteolin-7-O-glucuronide played a role in the inhibitory effects of E. acoroides aqueous extract on the growth of P. globosa. However, it was difficult to attribute the antialgal activity to a specific compound in such a complex aqueous extract, because of the existence of synergistic and antagonistic effects [34]. This is the first study that reported on the antialgal activity of luteolin-7-O-glucuronide, which can be used as an algicide to control P. globosa blooms. It is widely present in lots of plants and has significant inhibitory effects on P. globosa [35,36]. Zhang reported that 5 µg/mL prodigiosin, from bacterium Hahella, produced 84% algicidal activity in 72 h [37]. Although the inhibitory effects of prodigiosin are superior, it is insoluble in water and expensive. It is also difficult to be used to control P. globosa blooms in natural water bodies. The application of secondary metabolites, from algicidal bacteria, against P. globosa has been reported [32]. However, it remains unclear whether secondary metabolites can have negative effects on higher trophic levels. In general, antialgal activity compounds from aquatic plants may have little effect on other organisms and aquatic ecosystems. Previous reports have shown that luteolin-7-O-glucuronide had antioxidant, anti-mutagenic, anti-genotoxic, anti-inflammatory, and anti-arthritic activities, which are beneficial for humans [38][39][40]. Therefore, the application of luteolin-7-O-glucuronide may be safer.

Conclusions
In summary, this study revealed that E. acoroides aqueous extract had significant inhibitory effects on P. globosa. E. acoroides aqueous extract inhibited algal growth by decreasing its chlorophyll-a content, Fv/Fm values, and by damaging its subcellular structure. UPLC-HRMS analysis revealed that flavonoids were the characteristic chemical constituents. Among the flavonoids, luteolin-7-O-glucuronide was found to have significant inhibitory effects on the growth of P. globosa. The antialgal compound can be used as a novel algicide to control P. globosa blooms, which is widely present in lots of plants and non-toxic for other organisms.
However, our research is limited, thus additional studies are required. The cost of adding luteolin-7-O-glucuronide for a typical treatment for P. globosa blooms is still unknown. The antialgal mechanism need to be further elucidated in order to reveal the practical utilization values.
Supplementary Materials: The following are available online at http://www.mdpi.com/1660-4601/16/14/2615/s1, Figure S1: Correlation relationships between the contents of luteolin-7-O-glucuronide and the inhibition rate at 96 h, Figure S2: Mass spectrogram of polypeptide (unknown) at 2.83 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S3: Mass spectrogram of polypeptide (unknown) at 2.90 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S4: Mass spectrogram of luteolin-3',7-O-diglucuronides at 3.00 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S5: Mass spectrogram of diphlorethohydroxycarmalol at 3.22 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S6: Mass spectrogram of cyclo (L-leucyl-L-leucyl-L-leucyl-L-leucyl-L-leucyl) at 3.27 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S7: Mass spectrogram of cyclo (L-leucyl-L-leucyl-L-leucyl-L-leucyl-L-leucyl-L-leucyl) at 3.42 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S8: Mass spectrogram of luteolin-7-O-glucuronide at 3.55 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S9: Mass spectrogram of chrysoeriol-7-O-glucuronide at 3.66 min negative ionization mode at low energy channels, Figure S10: Mass spectrogram of 6-hydroxy-1,3-divinyldihydropyrimidine-2,4,5(3H)-trione at 3.95 min (A) positive ionization mode at low energy channels; (B) postive ionization mode at high energy channels, Figure S11: Mass spectrogram of luteolin at 4.07 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S12: Mass spectrogram of apigenin at 4.48 min (A) positive ionization mode at low energy channels; (B) negative ionization mode at low energy channels; (C) positive ionization mode at high energy channels; (D) negative ionization mode at high energy channels, Figure S13: Mass spectrogram of chrysoeriol at 5.18 min (A) negative ionization mode at low energy channels; (B) negative ionization mode at high energy channels, Figure S14: Mass spectrogram of (9E,12Z)-octadeca-9,12-dienamide at 9.36 min (A) positive ionization mode at low energy channels; (B) positive ionization mode at low energy channels, Figure