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Article

Impact of Phlorotannin Extracts from Fucus vesiculosus on Human Gut Microbiota

by
Marcelo D. Catarino
1,
Catarina Marçal
1,
Teresa Bonifácio-Lopes
2,
Débora Campos
2,
Nuno Mateus
3,
Artur M. S. Silva
1,
Maria Manuela Pintado
2 and
Susana M. Cardoso
1,*
1
LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, 3810-193 Aveiro, Portugal
2
CBQF-Centro de Biotecnologia e Química Fina–Laboratório Associado, Escola Superior de Biotecnologia, Universidade Católica Portuguesa, Rua Diogo Botelho 1327, 4169-005 Porto, Portugal
3
REQUIMTE/LAQV, Department of Chemistry and Biochemistry, Faculty of Sciences, University of Porto, 4169-007 Porto, Portugal
*
Author to whom correspondence should be addressed.
Mar. Drugs 2021, 19(7), 375; https://doi.org/10.3390/md19070375
Submission received: 31 May 2021 / Revised: 18 June 2021 / Accepted: 21 June 2021 / Published: 29 June 2021
(This article belongs to the Special Issue Bioactive Compounds from Brown Algae)
Browse Figures
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Abstract

:
Recent studies indicate that plant polyphenols could be pointed as potential prebiotic candidates since they may interact with the gut microbiota, stimulating its growth and the production of metabolites. However, little is known about the fate of brown seaweeds’ phlorotannins during their passage throughout the gastrointestinal tract. This work aimed to evaluate the stability and bioaccessibility of Fucus vesiculosus phlorotannins after being submitted to a simulated digestive process, as well as their possible modulatory effects on gut microbiota and short-chain fatty acids production following a fermentation procedure using fecal inoculates to mimic the conditions of the large intestine. The stability of phlorotannins throughout the gastrointestinal tract was reduced, with a bioaccessibility index between 2 and 14%. Moreover, slight alterations in the growth of certain commensal bacteria were noticed, with Enterococcus spp. being the most enhanced group. Likewise, F. vesiculosus phlorotannins displayed striking capacity to enhance the levels of propionate and butyrate, which are two important short-chain fatty acids known for their role in intestinal homeostasis. In summary, this work provides valuable information regarding the behavior of F. vesiculosus phlorotannins along the gastrointestinal tract, presenting clear evidence that these compounds can positively contribute to the maintenance of a healthy gastrointestinal condition.

1. Introduction

The human intestinal tract harbors a complex community of microorganisms, collectively termed as intestinal or gut microbiota. The microbial colonization of the gastrointestinal tract starts right after birth and undergoes a symbiotic co-evolution along with their host, importantly contributing to the maintenance of intestinal homeostasis, development and integrity of the mucosal barrier, production of various nutrients, protection against microbial pathogens, maturation of the immune system and many other functions [1]. Throughout adulthood, the intestinal microbiota is regarded as relatively stable, although it may be affected by several extrinsic factors including dietary habits, medication (especially with antibiotics), environmental pollution and exposure to xenobiotics, physical activity and hygiene [2]. When these factors cause significant changes in the composition and/or function of the gut microbiota, the whole microbial ecosystem is perturbed to an extent that exceeds its resistance and resilience capabilities, leading to a condition known as dysbiosis. Consequently, dysbiosis has been associated with an increasing list of diseases, which include inflammatory bowel disease (IBD), irritable bowel syndrome (IBS), coeliac disease and colorectal cancer (CRC) [3]. Additionally, several extra-intestinal disorders such as asthma [4], systemic lupus erythematosus [5], cardiovascular disease [6] or even mental and neurodegenerative diseases including autism, anxiety, depression, chronic pain, Parkinson’s, Alzheimer’s or Huntington’s can be linked to a dysfunctional gut microbiota [7,8,9].
Based on this evidence, it is clear that the manipulation of gut microbiota could be regarded as a promising strategy to treat disease and improve health. In this context, prebiotics appear as important tools capable of manipulating and modifying the gut microbiota composition and promoting the host’s health status. They were first described in 1995 [10] and are currently defined as “a substrate that is selectively utilized by host microorganisms conferring a health benefit” [11]. In other terms, prebiotics are non-digestible dietary components that act as substrates that selectively stimulate the growth and/or biological activity of health-promoting bacteria residing in the host’s colon. Common prebiotics include several non-digestible polysaccharides, such as resistant starch and pectin, as well as oligosaccharides such as fructo-oligosaccharides (FOSs), galacto-oligosaccharides (GOSs), lactulose and inulin, which are found mainly in several land-vegetables, fruits and milk [12]. More recently, increasing evidence has shown that other compounds such as polyphenols and polyunsaturated fatty acids may also display modulatory effects on gut microbiota populations through selective prebiotic effects and antimicrobial activities against gut pathogenic bacteria [13,14]. Indeed, animal studies have demonstrated that the consumption of polyphenols, especially catechins, anthocyanins and proanthocyanidins, not only favors the growth of probiotic bacteria, such as Lactobacillus, Bifidobacterium, Akkermansia, Roseburia and Faecalibacterium spp., but also increases the production of short-chain fatty acids (SCFAs), including butyrate, which is the major energy source for the colonic epithelium and profoundly influences intestinal homeostasis [15]. Likewise, clinical trials have also revealed that the consumption of anthocyanins and ellagic acid promotes increases in Lactobacillus acidophilus, Bifidobacterium and Faecalibacterium spp. abundance in the stool and a reduction of the lipopolysaccharide-binding protein in the plasma of volunteers [16,17].
In contrast, studies regarding the prebiotic potential of seaweeds (particularly brown) are still scarce and essentially focused on the in vitro effects of their polysaccharides, while the fate of phlorotannins when crossing the gastrointestinal tract, remains deeply unexplored subject [18]. These compounds are specific phenolics biosynthesized only by brown seaweeds consisting of polymeric structures composed of several phloroglucinol units [18], and, despite the fact that they have been reported in the literature for their promising and versatile bioactive health benefits, only a limited number of studies have addressed their behavior in the gastrointestinal tract. Recent works have shown that an Ecklonia radiata phlorotannin-enriched extract performed better than inulin as it promoted a higher increase in Lactobacillus, F. prausnitzii, C. coccoides, Firmicutes and E. coli in fermentations conducted with human fecal microbiota [19], while the administration of Lessonia turbeculata polyphenol-rich extract to streptozotocin-induced diabetic rats was found to significantly restore the relative abundance of the overall bacterial diversity and SCFAs to levels similar to the negative control [20]. Interestingly, to the authors knowledge, no studies addressing the stability and bioactivity of phlorotannins throughout the gastrointestinal tract has been performed yet.
In this context, the aim of this work was to evaluate the stability and bioaccessibility of F. vesiculosus phlorotannin-rich extracts when crossing the gastrointestinal tract and ultimately disclose their possible modulatory effects toward the gut microbiota and short-chain fatty acid production.

2. Results and Discussion

2.1. Stability, Bioaccessibility and Antioxidant Activity of F. vesiculosus Extracts throughout the Simulated GIT

To evaluate the stability of F. vesiculosus phlorotannins throughout the digestive tract, both crude (CRD) and ethyl acetate fraction (EtOAc) were submitted to a simulated gastrointestinal (GIT) digestion and evaluated for their total phlorotannin content and antioxidant activity after each gut compartment. The results presented in Table 1 clearly demonstrate that the total phlorotannin content of the EtOAc fraction progressively decreased after each step from the GIT simulation. Interestingly, in the case of CRD, after the initial decrease in the mouth, an increase in the phlorotannin levels was found after the stomach digestion, followed by another decrease in the intestine. The reduction in the total phlorotannin content (TPhC) of the samples after the mouth digestion could be explained by possible interactions occurring between phlorotannins and the salivary proteins. In fact, such interactions are very well described for plant tannins and very relevant for the development of important sensory characteristics of certain foods and beverages such as wine [21]. The extreme pH conditions in the stomach can also explain why the TPhC of the EtOAc kept decreasing in this compartment. However, in the case of CRD, because this sample is more complex and contains other non-phlorotannin compounds, it is possible that such compounds might be interacting with phlorotannins, protecting them from reacting with the mouth proteins and degrading with the low stomach pH. In turn, the stomach pH may also promote the degradation of those non-phlorotannin compounds, promoting the release of the phlorotannins, making them more available to react with the 2,4-dimethoxybenzaldehyde (DMBA). In fact, similar observations have been previously reported for plant phenolics [22,23] and are on the basis of the delivery strategies in which phenolic compounds are encapsulated in order to resist the gastrointestinal conditions and reach intact for absorption in the intestines [24]. Additionally, it was noticed that even though undigested EtOAc had higher TPhC compared to the undigested CRD, after the stomach and intestine digestion, the TPhC of the latter was slightly higher compared with the EtOAc, which is in agreement with the hypothesis that the EtOAc phlorotannins were more exposed to the GIT degradation than those of CRD.
At the end of the simulated GIT, only a small portion of the total phlorotannins loaded in the system was bioaccessible, which is in line with previous studies carried out on land plant tannins. At this point, it is important to clarify that the term “bioavailability” expresses the fraction of an ingested compound/nutrient that reaches the systemic circulation to be distributed to organs and tissues and to manifest its bioactivity. However, before becoming bioavailable, the target compound/nutrient must be released from the food matrix and made available for bloodstream absorption, which is what defines the term “bioaccessibility” [25]. Interestingly, despite the fact that the undigested CRD exhibited lower TPhC compared to the undigested EtOAc, the bioaccessibility index of the former was 14.1%, while the latter was only 2.0%. Once again, this outcome might be in part explained by the fact that EtOAc experienced higher phlorotannin degradation than CRD, and, therefore, when the compounds reach the intestine to be absorbed, the TPhC of the matrix is already lower.
Concerning the antioxidant activity of the samples after each step of the GIT simulation, both NO● and SO●– results were in line with the TPhC of the respective samples, i.e., the samples with higher phlorotannin concentrations exhibited the lowest IC50 values and vice versa. Indeed, strong negative correlations were found between the TPhC and the antioxidant assays with CRD showing R2 of −0.82 and −0.94 and EtOAc showing R2 of −0.91 and −0.82 in NO● and SO●–, respectively, thus indicating a clear association between the phlorotannin content after each step of the simulated digestion and the antioxidant activities observed.

2.2. Prebiotic Effect

The prebiotic activity of digested F. vesiculosus CRD and EtOAc was studied on four strains in basal Man–Rogosa–Sharpe (MRS) broth without glucose, at concentrations of 1–2% (w/v). Figure 1 presents the growth curves of the evaluated Lactobacillus and Bifidobacteria strains over 24 h, as no further alterations were observed between 24 and 48 h. All the probiotic microorganisms were affected by the presence of the F. vesiculosus samples in different manners. Lactobacillus casei exhibited a growth behavior identical for almost all the conditions tested, with no differences observed on the maximum optical density (OD), although the seaweed samples seemed to slightly delay their growth during the first 10 h. The only notable exception was EtOAc at 1%, which caused a slight decrease of the growth curve of this strain. In turn, the incubation of L. acidophilus with either CRD or EtOAc presented a growth curve considerably higher than that of FOS, for all the concentrations tested, thus indicating that both CRD and EtOAc stimulate the growth of this strain.
In contrast, B. animalis growth was the least pronounced of all the strains tested, in the presence of either CRD or EtOAc, suggesting that they might exert a bacteriostatic effect on this strain. The results for B. animalis spp. lactis demonstrated that the CRD at 1% displayed better stimulatory effects than FOS, although the bacterial growth was completely abolished for higher concentrations, indicating that, in such conditions, this extract impairs the growth of this strain. Positive stimulatory effects were noticed for EtOAc at 1 and 1.5% as well, which demonstrated growth curves identical to that of FOS. However, for the concentration of 2%, this sample also exhibited inhibitory effects toward this strain.
The potential prebiotic effect of seaweeds is a subject barely studied so far. Nevertheless, Martelli et al. [26] recently showed that four strains of probiotic bacteria (L. casei, L. paracasei, L. rhamnosus and B. subtilis) all exhibited good capacity to grow in a broth medium containing Himanthalia elongata flour (5%), which is in line with previous works that demonstrated the capacity of different brown algae species (Sargassum siliquanstrum, Laminaria digitata, Laminaria saccharina) to stimulate the growth of several probiotic bacteria including Weissella spp., Lactobacillus spp., Leuconostoc spp., L. plantarum and L. rhamnosus [27,28,29]. However, seaweeds have a very complex matrix and the contribution of phlorotannins for the effects observed by these authors are likely to be negligible. In fact, current knowledge regarding the fate of seaweed polyphenols in the human gastrointestinal tract is scarce. In the work developed by Corona et al. [30], after submitting a polyphenol-rich extract from A. nodosum to a simulated gastrointestinal digestion followed by fecal fermentation, they were able to find seven phlorotannin-derived metabolites, and, although the microbiota composition was not assessed, the presence of these metabolites suggests that phlorotannins might have been used by the colonic bacteria. In turn, in a 24 h in vitro fermentation carried out using Ecklonia radiata phlorotannin extract, a significant increase in the populations of Bacteroidetes, Clostridium coccoides, E. coli and Faecalibacterium prausnitzii was observed, although the levels of Bifidobacterium and Lactobacillus populations were found to be decreased [19]. With these results, we demonstrate for the first time that F. vesiculosus extract and phlorotannin-enriched fraction can stimulate the growth of some probiotic strains in a similar way to that of FOS.

2.3. Evolution of the Gut Microbiota Profile Groups

After GIT simulation, the digested F. vesiculosus CRD and EtOAc were submitted to human feces fermentation during 48 h, and aliquots were taken at 0, 12, 24 and 48 h to study their effect upon the human microbiota. Three of the four dominant phyla in the human gut were evaluated, namely Firmicutes (represented by Clostridium leptum, Enterococcus spp. and Lactobacillus spp.), Bacteroidetes (represented by Bacteroides spp.) and Actinobacteria (represented by Bifidobacterium spp.), and the compositional averages of the copy numbers obtained by real-time PCR of these main groups are depicted in the Table 2.
The numbers were in agreement with those found in healthy volunteers’ feces, with Clostridium, Bacteroides and Bifidobacterium comprising the dominant genera while Lactobacillus spp. and Enterococcus appeared as the subdominant genera [31,32,33]. Figure 2 depicts the relative differences (in %) between the microbiota groups of the tested samples and control feces, along 12, 24 and 48 h of fermentation. Overall, both CRD and EtOAc promoted a modest positive effect on gut microbiota growth, as noticed by the increment in the universal microorganisms compared to the control over time, while FOS exerted a positive effect on the initial 12 h that reversed for the following 24 and 48 h.
The EtOAc fraction caused a positive effect over time on the phyla Firmicutes and Bacteroidetes, which are representative of a healthy microbiota [34], while CRD and FOS exhibited a null or negative effect on these two groups. In turn, as expected, FOS exerted a very positive effect on Lactobacillus spp. and Bifidobacterium spp., two genera that are the markers of prebiosis par excellence. Likewise, despite not having an effect as sharp as FOS, EtOAc fraction also positively stimulated the growth of these two probiotic groups over time, although in the case of Lactobacillus spp., the effect lasted only until 24 h, becoming null at the end of the fermentation (48 h). Identical behavior was noticed for CRD on Bifidobacterium spp., promoting their growth only during the first 24 h. Curiously, no effect was observed on Lactobacillus spp., contrarily to what was expected since L. casei and L. acidophilus responded with a very positive growth behavior in the presence of this sample on the prebiotic studies (Section 2.2).
Interestingly, the group of Enterococcus spp. was the most beneficiated by CRD and EtOAc, although the levels of these organisms progressively decreased over time, contrarily to FOS which promoted their growth at each time point. Poor gut health outcomes have generally been linked to this genus [35], although this is a controversial subject since not all enterococcal strains cause health problems. In fact, strains such as E. faecium SF68® and E. faecalis Symbio-flor® have been marketed as probiotics for two decades without incidence and with very few reported adverse events [36]. Moreover, enterococcal probiotics have been shown to be effective in limiting gastrointestinal infectious burden and in the treatment of gastrointestinal infections and diarrhea [37].
On the contrary, Clostridium leptum, an important butyrate-producing strain, was the least affected by the studied samples, with only CRD causing a slight negative effect on its growth over time.
Regarding Bacteroides spp., the results demonstrated that even though all the samples promoted an increment in this group during the first 12 h, only EtOAc maintained this positive effect throughout the fermentation course. Instead, FOS and CRD turned out to negatively affect the growth of these bacteria after 24 h and until the end of the fermentation. Similar to Enterococcus spp., there is some controversy around the probiotic potential of the genus Bacteroides. On one hand, this group has been associated with the development of intestinal dysfunctions such as diarrhea, inflammatory bowel disease and colorectal cancer, and, on the other hand, it has been recently considered as a next generation probiotic candidate due to its potential role in promoting host health through the regulation of intestinal redox levels or the production of important short-chain fatty acids such as acetate, propionate and butyrate, which in turn can contribute to the regulation of toxin transport from the gut lumen to blood, the prevention of colon cancer and the prevention of inflammatory conditions [38].
Another important aspect to consider is the ratio between Firmicutes and Bacteroidetes (F:B), the most predominant phyla in the human colon. Together they comprise 90% of the total gut microbiota and, thus, their proportion can give us a global idea of the total effect of F. vesiculosus samples on the intestinal flora. Commonly, healthy individuals display a nearly 1:1 ratio of Firmicutes to Bacteroidetes, and significant alterations of this ratio have been associated with pathological states [39]. For instance, increased F:B ratios have been linked to the pathophysiology of obesity [40], while patients of type II diabetes mellitus were found to have their levels of Firmicutes significantly reduced compared to their non-diabetic counterparts and consequently had decreased F:B ratios [41]. In this work, a slight increase of the F:B ratio was noticed for FOS and EtOAc (1.36 ± 0.10 and 1.24 ± 0.14, respectively) compared to the control (1.09 ± 0.05) during the first 12 h of fermentation, which then returned to normal levels over the next 24 and 48 h (Figure 3A). On the contrary, CRD did not cause any significant alterations of this parameter maintaining the F:B ratio values stable and close to one over the course of the fermentation.
Very few studies focusing on the prebiotic potential of phlorotannin-rich extracts have been conducted so far, although there are already some insights on this matter. Interestingly, Charoensiddhi et al. [19] reported that, after the 24 h fermentation period of a phlorotannin-rich extract of E. radiata with human fecal samples, only the group of Bacteroidetes showed an increased growth compared to the negative control, while Firmicutes and Bifidobacterium spp. remained unchanged and Lactobacillus spp. and Enterococcus spp. actually decreased. However, these authors also observed a stimulation of the growth of Faecalibacterium prausnitzii and Clostridium coccoides, which were not analyzed in this study but are two important groups associated to SCFA production (particularly butyrate) and health-promoting effects [42,43]. In a different work, the administration of a polyphenol-rich extract from the brown algae Lessonia trabeculata to streptozotocin-induced diabetic rats under a high-fat diet significantly restored the levels of the three dominant phyla, i.e., Firmicutes, Bacteroidetes and Proteobacteria, as well as the F:B ratio to values identical of the negative control [20]. To the authors knowledge, this work was the first assessing the potential modulatory effects of F. vesiculosus phlorotannin extracts on human gut microbiota and allowed the disclosure of valuable information on how F. vesiculosus phlorotannins may impact on the human gastrointestinal microflora.

2.4. Organic Acids Profile and pH Variation

The changes in the concentration of short-chain fatty acids along the fermentation of FOS, CRD and EtOAc with human feces in basal media were analyzed by HPLC and are presented in Table 3. SCFAs such as acetate, propionate and butyrate are volatile fatty acids that are produced by the gut microbiota in the colon as a result of the fermentation and metabolization of food components that are undigested/unabsorbed in the upper GIT.
In this study, fermentation with FOS caused a remarkable increase in the production of total organic acids, while in the fermentations carried out with F. vesiculosus samples, a tendential increase in the total organic acid levels was noticed despite not being statistically significant when compared with the negative control. These results are also reflected in the pH changes registered during the fermentation (Figure 3B), with FOS producing a significant decrease in the pH values, while the pH registered for CRD and EtOAc remained similar to that of the control, at least for the time window tested. Differences in the SCFA profiles, however, were detected between samples. One of the most evident differences was noticed for lactate, which was the main metabolite produced over the entire fermentation of FOS. This outcome also relates with the high stimulatory effects that FOS produced on Lactobacillus spp. and Bifidobacterium spp. validated above with the 16S rRNA gene analysis (Section 2.3). On the other hand, similar to the negative control, the lactate production in fermentations carried out with CRD and EtOAc were nearly null, and even undetectable, at 48 h. An identical pattern was found for acetate production, which was remarkably stimulated in the presence of FOS but not affected by CRD or EtOAc. Under normal conditions this acid together with propionic and butyric acids comprise the three major SCFAs normally produced in the gut, which are important for the maintenance of intestinal homeostasis [44]. In particular, acetate plays a very important role in energy homeostasis, contributing to appetite regulation, promoting fat oxidation, improving insulin sensitivity and glucose homeostasis, and enhancing the inflammatory status [45].
Interestingly, all three samples promoted an increase in the succinate level, which reached its maximum at 12 h and was kept constant for FOS until the end of the fermentation, while for CRD and EtOAc it decreased over time. On one hand, the accumulation of this organic acid in the gut lumen is usually associated with microbiota disturbances commonly linked to poor gut health states such as antibiotic-induced dysbiosis, motility disturbances and specifically IBD [46]. On the other hand, succinate is also a key intermediate in the production of propionate, which in turn is responsible for modulating lipogenesis, controlling appetite and preventing colon cancer [47]. In fact, the levels of propionate production herein noted seem to follow an identical behavior compared with that of succinate, showing an accentuated increase during the initial phase of the fermentation and a decrease at the end, only for CRD and EtOAc. Indeed, high correlation coefficients between these two organic acids were obtained (R2 = 0.99, 0.88 and 0.97 for FOS, CRD and EtOAc, respectively), which confirms that the production of propionate is indeed associated with the production of succinate.
One of the most important SCFAs produced in the gut is butyrate, which has been repeatedly reported for its positive health-promoting effects. In addition to its function as the primary energy source for colonocytes, butyrate also importantly contributes to the improvement of the gut barrier function, exerts anti-inflammatory and regenerative effects, prevents the formation of colon cancer and helps reduce both type II diabetes and obesity [39]. Therefore, stimulating the production of high levels of this SCFA is of great interest for promoting the healthy function of the gut. The results herein obtained revealed that only the EtOAc led to a significant increase in butyric acid, while, in CRD and FOS, the levels of this SCFA did not differ much from the negative control.
The main butyrate-producing bacteria are Faecalibacterium prausnitzii, Clostridium spp., Eubacterium spp., Roseburia spp. and Anaerostipes spp., which belong to the Firmicutes phylum [44], and, despite the fact that the C. leptum did not show significant positive growth in the presence of EtOAc, an increase in the group Firmicutes was noticed on the EtOAc-fermented samples, which might explain the increased levels of butyrate registered. In turn, the lack of production of butyrate, which was not expected, in the FOS fermentation could be possibly explained by the absence of the common cross-feeding effect among intestinal bacteria that produce acetate, propionate or butyrate as the final product of lactate metabolization [48]. Indeed, the fact that lactate has accumulated so much throughout the fermentation of FOS indicates that it has not been utilized as a substrate by other bacteria. Nevertheless, it must be considered that this experiment was performed without pH control, and, thus, it is likely that the sharp decrease in the pH may have impaired the growth of certain lactate-utilizing bacteria and favored the growth of the lactate-producing ones, therefore contributing to the increasing accumulation of this organic acid at the expense of other SCFAs [49].
When comparing these results with those previously reported by Charoensiddhi et al. [19], the stimulatory effects of F. vesiculosus phlorotannin samples herein tested on the production of SCFAs were much more promising than those of the E. radiata phlorotannin-rich extract used in their study. In fact, the authors reported that the fermentation of the phlorotannin extract caused a reduction on the levels of total SCFAs with a remarkable decrease in the concentration of acetic acid in comparison with the negative control. Contrarily, Yuan et al. [20] found that the administration of a polyphenol-rich extract from the brown algae Lessonia trabeculata to streptozotocin-induced diabetic rats, under a high-fat diet, significantly restored the levels of acetate and butyrate that were depleted in the diabetic control groups. Notably, the levels of butyrate in the treated rats were even higher than those of the control group, i.e., healthy rats. In our study, despite the fact that the total SCFA production was much lower than that observed for FOS, both CRD and EtOAc exhibited interesting alterations in the SCFA profiles stimulating the production of propionate and, in the case of EtOAc, butyrate as well. These SCFAs could exert interesting beneficial health properties not only in the colon and gut microbiota but also in other organs, which could partly explain the health benefits attributed to phlorotannins.

3. Materials and Methods

3.1. Chemicals

Grounded Fucus vesiculosus harvested in July 2017 was purchased from Algaplus Lda. Acetone, methanol, n-hexane, ethyl acetate, DMSO, glacial acetic acid, hydrochloric acid and sodium hydroxide were acquired from Fisher (Pittsburgh, PA, USA). Sodium nitroprusside and sulfanilamide were ordered from Acros Organics (Hampton, NH, USA). Ascorbic acid, gallic acid, NADH, NBT, PMS, FOS, DMBA, α-amylase, paraffin, bile salts, pancreatin, pepsin, sodium hydrogen carbonate, D-glucose, organic acids (succinate, lactate, propionate, butyrate and acetate) and sulfuric acid were obtained from Sigma (St. Louis, MO, USA). Man–Rogosa–Sharpe (MRS) medium and L-cysteine-HCl were purchased from Biokar (Allonne, France) and Merck (Darmstadt, Germany), respectively, while trypticase soya broth (TSB) without dextrose and bactopeptone were acquired from BBL (Cockeysville, Maryland, MD, USA) and Amersham (Buckinghamshire, UK), respectively. Salt solution A (100.0 g/L NH4Cl, 10.0 g/L MgCl2·6H2O, 10.0 g/L CaCl2·2H2O), salt solution B (200.0 g/L K2HPO4·3H2O) and resazurin solution were ordered from ATCC (Manassas, VA, USA). Sodium di-hydrogen phosphate and potassium di-hydrogen phosphate were purchased from Panreac (Barcelona, Spain). Dinitrosalicylic acid and acarbose were purchased from Acros Organics (Hampton, NH, USA), calcium chloride from ChemLab (Eernegem, Belgium) and orlistat from AlfaAesar (Ward Hill, MA, USA). Finally, the Bifidobacterium animalis BB0 were acquired from CSK (Ede, The Netherlands), Bifidobacterium animalis spp. lactis Bb12 and Lactobacillus casei 01 from Chr. Hansen (Hørsholm, Denmark) and Lactobacillus acidophilus La-5 from Lallemand (MontReal, QC, Canada).

3.2. Extraction Procedure

The extracts were prepared following the optimal conditions determined through the response surface method as previously described [50]. For this, 30 g of dried algal powder was dispersed in 2100 mL of 70% acetone solution and incubated for 3 h at room temperature under constant agitation. The mixture was filtered through cotton to remove the solid residues and then through a G4 glass filter. Afterward the extract was concentrated in a rotary evaporator to about 250 mL. The concentrated extract was defatted using n-hexane (1:1, v/v) for several times (until a colorless non-polar fraction was obtained), and the aqueous phase was further submitted to liquid–liquid extraction with ethyl acetate (1:1, v/v) for three times to obtain a phlorotannin-purified fraction (EtOAc). Finally, the solvent was removed from the EtOAc fraction by rotary evaporation. Both CRD and EtOAc were then freeze dried and stored at −20 °C until further use.

3.3. Gastrointestinal Digestion Simulation

The simulation of the gastrointestinal digestion of the F. vesiculosus sample extracts was performed according to the method described by Campos et al. [33]. Oral digestion was started by suspending 1 g of dried sample (CRD or EtOAc) in 20 mL of distilled water followed by the adjustment of the pH between 5.6 and 6.9 with NaHCO3 prior to the addition of 0.6 mL/min of α-amylase at 100 U/mL. Enzymatic digestion was carried out during 2 min of mastication, at 37 °C and 200 rpm. Before moving to the next compartment, the pH of mouth digest was adjusted to 2.0 using 1M HCl and then mixed with a simulated gastric juice consisting of pepsin 25 mg/mL added at a ratio of 0.05 mL/mL of mouth digest. Incubation was carried out over 60 min at 37 °C and 130 rpm. Finally, for intestinal digestion the pH of gastric digest was adjusted to 6.0 using 1M NaHCO3 prior to the addition of a simulated intestinal juice consisting of 2 g/L of pancreatin and 12 g/L bile salts at a ratio of 0.25 mL/mL of gastric digest. The samples were then incubated during 120 min, at 37 °C and 45 rpm, to mimic a long intestine digestion process. In the final step of intestinal digestion, samples were submitted to a dialysis process during 48 h at room temperature using a membrane with a molecular pore size of 3 kDa to reproduce the natural absorption step in the small intestine. At the end of this process, the permeate represented the bioaccessible fraction, while the retentate represented the non-absorbable fraction, both of which were then used for the fermentation experiments. An aliquot of 2 mL was collected before the digestion simulation and after each step of digestion, i.e., mouth digest, gastric digest, intestinal digest, permeate and retentate, and stored at −80 °C until further use for phlorotannin quantification and antioxidant experiments.

3.4. Determination of the Phlorotannin Content and Antioxidant Activities

Quantification of the TPhC was carried out according to the 2,4-dimethoxybenzaldehyde (DMBA) colorimetric method [51]. For this, equal volumes of the stock solutions of DMBA (2%, m/v) and HCl (6%, v/v), both prepared in glacial acetic acid, were mixed prior to use (work solution). Afterwards, 250 µL of this solution was added to 50 µL of each extract in a 96-well plate and the reaction was incubated in the dark, at room temperature. After 60 min, the absorbance was read at 515 nm and the phlorotannin content was determined by using a regression equation of the phloroglucinol linear calibration curve (0.06–0.1 mg/mL). The results were expressed as mg phloroglucinol equivalents/g dry seaweed (mg PGE/g DW).
The NO● scavenging method was adapted from Pereira et al. [52]. For this, 100 µL of six different sample concentrations (0–1 mg/mL) was mixed with 100 µL of sodium nitroprusside (3.33 mM in 100 mM sodium phosphate buffer pH 7.4) and incubated for 15 min under a fluorescent lamp (Tryun 26 W). Next, 100 µL of Griess reagent (0.5% sulfanilamide and 0.05% N-(1-naphthyl)ethylenediamine dihydrochloride in 2.5% H3PO4) was added to the mixture, which was incubated for another 10 min at RT in the dark. The absorbance was then measured at 562 nm, and the NO● scavenging capacity was calculated as the concentration of the sample capable of scavenging 50% of the radical. Ascorbic acid was used as the reference compound.
The O2●– scavenging method was carried out according to the method described by Pereira et al. [53]. In a 96-well plate, 75 µL of six different sample concentrations (0.0–2.0 mg/mL) was mixed with 100 µL of β-NADH (300 µM), 75 µL of NBT (200 µM) and 50 µL of PMS (15 µM). After 5 min, the absorbances at 560 nm were recorded and the inhibition calculated as the concentration capable of scavenging 50% of O2●− (IC50). Gallic acid was used as the reference compound.

3.5. Determination of the Phlorotannin Content and Antioxidant Activities

Potential prebiotic effects of F. vesiculosus phlorotannin-rich samples were determined for Bifidobacterium animalis B0, Bifidobacterium animalis spp. lactis BB12, Lactobacillus casei 01 and Lactobacillus acidophilus LA-5. Strains were stored at −80 °C in MRS broth with 30% (v/v) glycerol. L. casei 01 and L. acidophilus LA-5 inocula were prepared by suspending each bacterial colony into MRS broth, achieving a turbidity equivalent to 0.5 McFarland standard, and then diluting to reach the recommended concentration of probiotic bacteria in the wells, 5 × 105 CFU/mL. Twenty microliters of each inoculum were transferred to a 96-well microplate and every well was fulfilled (to the final volume of 200 µL) with each F. vesiculosus sample, diluted in basal MRS broth without glucose at concentrations of 1, 1.5 and 2% (w/v). The microplate was incubated at 37 °C for 48 h with agitation. Similarly, B. animalis B0 and B. lactis BB12 inocula were prepared under an anaerobic atmosphere, by suspending each bacterial colony into MRS broth supplemented with 0.05% (v/v) L-cysteine-HCl, achieving a final turbidity equivalent to 0.5 McFarland standard, and then diluted to reach the recommended concentration of probiotic bacteria in the wells, 5 × 105 CFU/mL. Twenty microliters of each inoculum were transferred to a 96-well microplate and every well was fulfilled (to the final volume of 200 µL) with each F. vesiculosus sample, diluted in basal MRS broth without glucose at concentrations of 1, 1.5 and 2% (w/v). The microplate was sealed with paraffin and incubated at 37 °C for 48 h with agitation. In all plates, OD measurements at 620 nm were registered every hour. Three controls were also performed: the first one containing inoculum and MRS broth with glucose (positive control), the second one containing inoculum and FOS in MRS broth without glucose (FOS control) and the third one containing only inoculum and MRS broth (negative control).

3.6. In Vitro Fermentation Assays

The human feces were collected into sterile plastic vases and kept under anaerobic conditions, until further notice (maximum of 2 h after collection). The samples were obtained fresh, from healthy human donors, with the premises of not having any known metabolic or gastrointestinal disorder. Moreover, the donors confirmed that they were not taking any probiotic or prebiotic supplements, as well as any form of antibiotics for the previous 3 months. The basal medium was prepared as described previously [33], consisting of a nutrient base medium containing 5.0 g/L trypticase soya broth (TSB) without dextrose (BBL, Cockeysville, Maryland, MD, USA), 5.0 g/L bactopeptone (Amersham, Buckinghamshire, UK), 0.5 g/L L-cysteine-HCl (Merck, Germany), 1.0% (v/v) of salt solution A (100.0 g/L NH4Cl, 10.0 g/L MgCl26H2O, 10.0 g/L CaCl22H2O), 0.2% (v/v) of salt solution B (200.0 g/L K2HPO43H2O) and 0.2% (v/v) of 0.5 g/L resazurin solution, prepared in distilled water and with pH adjustment at 6.8. The basal medium was dispensed into airtight glass anaerobic bottles, sealed with aluminum caps before sterilization by autoclave. Stock solutions of yeast nitrogen base (YNB) were sterilized with 0.2 μm syringe filters (Chromafils, Macherey-Nagel, Düren, Germany) and inserted into the bottles. The serum bottles were incorporated with CRD and EtOAc extract retentate from the in vitro GIT simulation at a final concentration of 2% (w/v) and inoculated with fecal slurries of 2% (v/v) at 37 °C for 48 h without shaking nor pH control. Samples were taken at 0, 12, 24 and 48 h of fermentation. All the experiments were carried out inside an anaerobic cabinet with 5% of H2, 10% of CO2 and 85% of N2 and performed in compliance with the institutional guidelines.

3.7. Gut Microbiota Evaluation

3.7.1. DNA Extraction

Genomic DNA was extracted and purified from stool samples as previously described [33] using NZY Tissue gDNA Isolation Kit (Nzytech, Lisbon, Portugal) with some modifications. Samples were centrifuged at 11,000 g during 10 min to separate the supernatant from the pellet. Around 170–200 mg of pellet was taken from the control and test samples for all times. After, the pellets were homogenized in TE buffer (10 mM Tris/HCl; 1 mM EDTA, pH 8.0) and centrifuged again at 4000 g for 15 min. The supernatant was discarded, and the pellet was resuspended in 350 μL of buffer NT1. After an incubation step at 95 °C for 10 min, the samples were centrifuged at 11,000 g for 1 min. Then, 25 μL of proteinase K was added to 200 μL of supernatant and incubated at 70 °C for 10 min. The remaining steps followed the manufacturer’s instructions. The DNA purity and quantification were assessed with a NanoDrop spectrophotometer (ThermoScientific, Wilmington, DE, USA).

3.7.2. Real-Time PCR for Microbial Analysis of Stool

Real-time PCR was performed as described before in [33] in sealed 96-well microplates using a LightCycler FastStart DNA Master SYBR Green kit and a LightCycler instrument (Roche Applied Science, Indianapolis, ID, USA). PCR reaction mixtures (total of 10 μL) contained 5 μL of 2 × Faststart SYBRGreen (Roche Diagnostics Ltd., Burgess Hill, UK), 0.2 μL of each primer (final concentration of 0.2 μM), 3.6 μL of water and 1 μL of DNA (equilibrated to 20 mg). Primer sequences (Sigma-Aldrich, St. Louis, MO, USA) used to target the 16S rRNA gene of the bacteria and the conditions for PCR amplification reactions are reported in Table 4.
To verify the specificity of the amplicon, a melting curve analysis was performed via monitoring SYBR Green fluorescence in the temperature ramp from 60 to 97 °C. Data were processed and analyzed using the LightCycler software (Roche Applied Science, Penzberg, Germany). Standard curves were constructed using serial tenfold dilutions of bacterial genomic DNA, according to the following webpage http://cels.uri.edu/gsc/cbdna.html (accessed at 31 March 2021). Bacterial genomic DNA used as a standard (Table 4) was obtained from DSMZ (Braunschweig, Germany). Genome size and the copy number of the 16S rRNA gene for each bacterial strain used as a standard was obtained from the NCBI Genome database (http://www.ncbi.nlm.nih.gov, accessed at 31 March 2021). Data are presented as the mean values of duplicate PCR analyses. The F:B ratio was obtained by dividing the number of copies of Firmicutes divisions by the number of copies of Bacteroidetes divisions. Moreover, the relative differences to negative control percentage (only feces fermentation) were calculated using the following equation:
R e l a t i v e   d i f f e r e n c e   t o   c o n t r o l   % = S M C − C M C C M C × 100
where SMC is the mean copy number of the sample at a certain time (12, 24 or 48 h) and CMC is the mean copy number of the control sample at the same time as SMC. Positive % values mean the occurrence of an increase in the number of copies relative to the control sample at that certain time. The higher the value, the higher increase.

3.7.3. Determination of Organic Acids

Supernatants from the batch cultures were filtered through 0.2 μm cellulose acetate membranes. The chromatographic analysis was performed using a Beckman & Coulter 168 series HPLC system with refractive index-RI detector (Knauer, Berlin, Germany). The separation was performed using Aminex HPX-87H column (BioRad, Hercules, CA, USA) operated at 50 °C; mobile phase, 0.003 mol/L H2SO4; flow, 0.6 mL/min. Aliquots of the filtered samples were assayed for organic acids (lactic, acetic, succinic, propionic and butyric) using an Agilent 1200 series HPLC system with an RI detector (Agilent, Germany) and a UV detector.

3.8. Statistical Analysis

Data are expressed as mean ± SD of three similar and independent experiments and analyzed using a one-way ANOVA followed by Tukey’s post hoc test. The statistical tests were applied using GraphPad Prism, version 7.00 (GraphPad Software, San Diego, CA, USA) and the significance level was p < 0.05.

4. Conclusions

Overall, this work provides a great contribution for the understanding of the stability of the phlorotannins of F. vesiculosus along the digestive tract, as well as their bioaccessibility and stimulatory effects toward gut microbiota and SCFA production. Similar to plant polyphenols, phlorotannins seem to be susceptible to gut environmental conditions leading to a decrease in their concentration and antioxidant activity along the digestive tract. Moreover, from the portion of phlorotannins that can reach the intestinal lumen intact, only a small fraction of less than 15% will become bioaccessible and available for absorption, which indicates that the majority of these compounds will accumulate in the large intestine where they will be exposed to the metabolic activity of the gut microbiota. Meanwhile, the fermentation of the digested CRD and EtOAc revealed a slight positive effect on the growth of certain commensal bacteria from the human gut, with Enterococcus spp. showing the most relevant growth. Moreover, both samples demonstrated an interesting capacity to enhance the production of propionate, while EtOAc caused a notable increase in butyrate levels, both representing important short-chain fatty acids known for their health-promoting status.
In summary, the data gathered herein provide valuable information regarding the behavior of F. vesiculosus phlorotannins along their passage through the gastrointestinal tract, and even though the results obtained do not allow to claim F. vesiculosus phlorotannin extracts as prebiotics they present clear evidence that these compounds can still positively contribute to the maintenance of a healthy gastrointestinal condition. From here, it would be important to address whether fermentation with human colonic bacteria could affect the antioxidant and other bioactive properties of F. vesiculosus CRD and EtOAc. Moreover, it would be particularly relevant to disclose the possible formation of phlorotannin metabolites resultant from the biotransformation and bacterial metabolization in the colon.

Author Contributions

M.D.C. contributed to the conceptualization, investigation, data curation, and writing of the original draft; C.M. and T.B.-L. contributed to the investigation, data curation and writing—reviewing and editing; D.C. contributed to the validation and writing—reviewing and editing; N.M. and A.M.S.S. contributed to the supervision and writing—reviewing and editing; M.M.P. contributed to the conceptualization, supervision, resources and writing—reviewing and editing; S.M.C. contributed to the conceptualization, supervision, writing—reviewing and editing, resources and project administration. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by the European Union (FEDER funds through COMPETE POCI-01-0145-FEDER-031015) and national funds (FCT, Fundação para a Ciência e Tecnologia) through project PTDC/BAA-AGR/31015/2017, “Algaphlor—brown algae phlorotannins: from bioavailability to the development of new functional foods”.

Institutional Review Board Statement

Ethical review and approval were waived for this study, as it was conducted according to the internal rules legally established, based on the research ethics recommendations and with the informed consent of all subjects involved in the study.

Informed Consent Statement

Informed consent was obtained from all subjects involved in the study.

Data Availability Statement

Data are available from the corresponding author.

Acknowledgments

Thanks to the University of Aveiro (UA) and the Science and Technology Foundation/Ministry of Education and Science (FCT/MEC) for funding the Associated Laboratory for Green Chemistry (LAQV) of the Network of Chemistry and Technology (REQUIMTE) (UIDB/50006/2020), through national funds and, where applicable, co-financed by FEDER, within Portugal 2020. We would like to thank the scientific collaboration under the FCT project UID/Multi/50016/2019. Marcelo D. Catarino’s PhD grant (PD/BD/114577/2016) was funded by the FCT.

Conflicts of Interest

The authors declare no conflict of interest. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript; or in the decision to publish the results.

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Figure 1. Growth curves of L. casei, L. acidophilus, B. animalis and B. animalis spp. lactis in the presence of different concentrations of digested crude extract (CRD) and ethyl acetate fraction (EtOAc). Data represent the mean ± SD of at least three independent assays.
Figure 1. Growth curves of L. casei, L. acidophilus, B. animalis and B. animalis spp. lactis in the presence of different concentrations of digested crude extract (CRD) and ethyl acetate fraction (EtOAc). Data represent the mean ± SD of at least three independent assays.
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Figure 2. Evolution of the gut microbiota groups (relative differences to negative control in %) along the fermentation. Data represent the mean ± SD of five independent assays.
Figure 2. Evolution of the gut microbiota groups (relative differences to negative control in %) along the fermentation. Data represent the mean ± SD of five independent assays.
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Figure 3. Firmicutes:Bacteroidetes (F:B) ratio (A) and variation of the pH (B) throughout the fermentation of digested FOS, CRD and EtOAC with human microbiota. Data represent the mean ± SD of five independent assays.
Figure 3. Firmicutes:Bacteroidetes (F:B) ratio (A) and variation of the pH (B) throughout the fermentation of digested FOS, CRD and EtOAC with human microbiota. Data represent the mean ± SD of five independent assays.
Marinedrugs 19 00375 g003
Table
Table 1. Total phlorotannin content and antioxidant activity of F. vesiculosus crude and ethyl acetate fraction through the different stages of gastrointestinal digestion.
Table 1. Total phlorotannin content and antioxidant activity of F. vesiculosus crude and ethyl acetate fraction through the different stages of gastrointestinal digestion.
SampleGIT StageTPhC
(mg PGE/g ext)		(1) NO●
(IC50 μg/mL)		(2) O2●–
(IC50 μg/mL)
CRDUndigested9.93 ± 1.48 a161 ± 8.8 a417 ± 164.5 a
Mouth6.33 ± 2.96 b309 ± 105.2 b745 ± 88.2 b
Stomach8.52 ± 1.16 a,b171 ± 27.1 a378 ± 26.6 a
Intestine5.17 ± 0.70 b287 ± 27.2 a,b1105 ± 421.3 b
Retentate *4.60 ± 0.26 b141 ± 9.1 a294 ± 19.3 a
Permeate *1.40 ± 0.19 c2551 ± 30.7 c2580 ± 75.2 c
EtOAcUndigested17.39 ± 1.77 a45 ± 2.5 a118 ± 17.6 a
Mouth13.83 ± 0.74 b73 ± 11.0 a,b221 ± 1.1 a,b
Stomach5.67 ± 0.91 c109 ± 7.1 a,b244 ± 0.4 a,b
Intestine3.28 ± 0.55 c195 ± 38.5 b,c564 ± 19.9 c
Retentate *2.97 ± 0.62 c,d281 ±16.1 c383 ± 18.2 b,c
Permeate *0.37 ± 0.10 d1531 ± 52.2 d3074 ± 32.3 d
Standard compound-36 ± 0.96 ± 0.5
CRD—crude extract; EtOAc—ethyl acetate fraction; GIT—gastrointestinal tract; TPhC—total phlorotannin content. (1) Standard compound for NO• is ascorbic acid; (2) standard compound for O2•− is gallic acid; * results for DMBA expressed in mg PGE/g intestine digest. Data represent the mean ± SD of at least three independent assays. For each sample, different letters indicate significant differences within the same column (p < 0.05).
Table
Table 2. Fecal microbiota composition of volunteer participants.
Table 2. Fecal microbiota composition of volunteer participants.
Division (Genus)Number of Copies (n = 5) a
Universal7.52 ± 0.38
Firmicutes4.76 ± 0.20
Clostridium leptum4.97 ± 0.26
Enterococcus spp.2.07 ± 0.63
Lactobacillus spp.3.27 ± 0.72
Bacteroidetes5.46 ± 0.63
Bacteroides spp.3.76 ± 0.55
Bifidobacterium spp.4.42 ± 0.45
F:B ratio0.97 ± 0.23
a Values are presented as mean ± SD of five independent assays and expressed as log10 16S rRNA gene copies per 20 ng of DNA.
Table
Table 3. Concentration of organic acids (succinic, lactic, acetic, propionic and butyric) throughout fermentation of digested FOS, CRD and EtOAC with human microbiota (mg/mL).
Table 3. Concentration of organic acids (succinic, lactic, acetic, propionic and butyric) throughout fermentation of digested FOS, CRD and EtOAC with human microbiota (mg/mL).
Organic AcidsTime (h)CtrlFOSCRDEtOAc
Total02.38 ± 0.63 a;A2.38 ± 0.63 a;A2.38 ± 0.63 a;A2.38 ± 0.63 a;A
125.24 ± 1.98 a;A10.89 ± 2.79 b;B7.43 ± 2.09 b;A7.76 ± 1.92 b;A,B
244.90 ± 1.59 a;A12.63 ± 2.37 b,c;B7.08 ± 2.45 b;A7.55 ± 1.75 b;A
484.10 ± 2.01 a;A14.78 ± 4.00 c;B5.04 ± 1.57 a,b;A6.38 ± 1.98 b;A
Succinic acid00.45 ± 0.20 a;A0.45 ± 0.20 a;A0.45 ± 0.20 a;A0.45 ± 0.20 a;A
120.77 ± 0.75 a;A1.85 ± 0.92 b;B2.29 ± 1.39 c;B2.15 ± 1.15 b;B
241.12 ± 0.53 a;A1.97 ± 0.58 b;B2.02 ± 0.93 b,c;A,B1.35 ± 0.50 a,b;A,B
480.74 ± 0.71 a;A2.03 ± 0.85 b;B1.12 ± 0.20 a,b;A,B1.40 ± 0.89 a,b;A,B
Lactic acid0NDNDNDND
121.21 ± 0.93 a;A3.91 ± 1.94 a;B0.87 ± 0.22 a;A0.87 ± 0.23 a;A
240.34 ± 0.14 a;A4.81 ± 0.75 a,b;B0.76 ± 0.58 a;A0.26 ± 0.16 a;A
48ND5.49 ± 2.14 bNDND
Acetic acid00.16 ± 0.04 a;A0.16 ± 0.04 a;A0.16 ± 0.04 a;A0.16 ± 0.04 a;A
120.81 ± 0.10 b;A1.36 ± 0.75 b;A1.03 ±0.09 b;A1.02 ± 0.19 b;A
240.82 ± 0.17 b;A1.65 ± 0.52 b;B0.92 ± 0.22 b;A0.96 ± 0.30 b;A
480.78 ± 0.20 b;A2.77 ± 1.21 c;B0.78 ± 0.20 b;A0.93 ± 0.28 b;A
Propionic acid00.34 ± 0.09 a;A0.34 ± 0.09 a;A0.34 ± 0.09 a;A0.34 ± 0.09 a;A
120.53 ± 0.23 a;A1.48 ± 0.32 b;B1.14 ± 0.49 b;B1.43 ± 0.87 b;B
240.65 ± 0.35 a;A1.89 ± 0.75 b;C1.25 ± 0.58 b;B0.85 ± 0.27 a,b;A,B
480.50 ± 0.24 a;A1.64 ± 0.60 b;B0.77 ± 0.20 a,b;A0.90 ± 0.24 a,b;A
Butyric acid01.41 ± 0.25 a;A1.41 ± 0.25 a;A1.41 ± 0.25 a;A1.41 ± 0.25 a;A
121.92 ± 0.69 a;A2.29 ± 0.99 a;A2.10 ± 0.79 a;A2.71 ± 0.94 a;A
242.24 ± 0.67 a;A2.23 ± 0.86 a;A2.54 ± 1.05 a;A4.12 ± 0.37 b;B
482.23 ± 1.35 a;A2.70 ± 1.43 a;A2.31 ± 0.85 a;A4.31 ± 0.62 b;B
Ctrl—negative control; FOS—fructo-oligosaccharides; CRD—crude extract; EtOAc—ethyl acetate fraction; ND—not detected. Different letters indicate significant differences (p < 0.05). The capital letters indicate the differences among the Ctrl, FOS, CRD and EtOAc for organic acid concentration at the same time (same row), and the lowercase letters indicate the differences for the same sample over time for each organic acid concentration (same column within an organic acid). Data represent the mean ± SD of five independent assays.
Table
Table 4. Primer sequences and real-time PCR conditions used for gut microbiota analysis.
Table 4. Primer sequences and real-time PCR conditions used for gut microbiota analysis.
Target GroupMaximum Growth Rate (µmax.h−1)
Primer Sequence (5′–3′)Genomic DNA StandardPCR Product Size (bp)AT (°C)
UniversalAAA CTC AAA GGA ATT GAC GG
ACT TCA CGA GCT GAC		Bacteroides vulgatus
ATCC 8482 (DSMZ 1447)		18045
FirmicutesATG TGG TTT AAT TCG AAG CA
AGC TGA CGA CAA CCA TGC AC		Lactobacillus gasseri
ATCC 33323 (DSMZ 20243)		12645
Enterococcus spp.CCC TTA TTG TTA GTT GCC ATC ATT
ACT CGT TGT ACT TCC CT TGT		Enterococcus gilvus
ATCC BAA-350 (DSMZ 15689)		14445
Lactobacillus spp.GAG GCA GCA GTA GGG AAT CTT C
GGC CAG TTA CTA CCT CTA TCC TTC TTC		Lactobacillus gasseri
ATCC 33323 (DSMZ 20243)		12655
BacteroidetesCAT GTG GTT TAA TTC GAT GAT
AGC TGA CGA CAA CCA TGC AG		Bacteroides vulgatus
ATCC 8482 (DSMZ 1447)		12645
Bacteroides spp.ATA GCC TTT CGA AAG RAA GAT
CCA GTA TCA ACT GCA ATT TTA		Bacteroides vulgatus
ATCC 8482 (DSMZ 1447)		49545
Bifidobacterium spp.CGC GTC TGG TGT GAA AG
CCC CAC ATC CAG CAT CCA		Bifidobacterium longum subsp. infantis
ATCC 15697 (DSMZ 20088)		24450
AT—annealing temperature; bp—base pairs; PCR—polymerase chain reaction.
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Catarino, M.D.; Marçal, C.; Bonifácio-Lopes, T.; Campos, D.; Mateus, N.; Silva, A.M.S.; Pintado, M.M.; Cardoso, S.M. Impact of Phlorotannin Extracts from Fucus vesiculosus on Human Gut Microbiota. Mar. Drugs 2021, 19, 375. https://doi.org/10.3390/md19070375

AMA Style

Catarino MD, Marçal C, Bonifácio-Lopes T, Campos D, Mateus N, Silva AMS, Pintado MM, Cardoso SM. Impact of Phlorotannin Extracts from Fucus vesiculosus on Human Gut Microbiota. Marine Drugs. 2021; 19(7):375. https://doi.org/10.3390/md19070375

Chicago/Turabian Style

Catarino, Marcelo D., Catarina Marçal, Teresa Bonifácio-Lopes, Débora Campos, Nuno Mateus, Artur M. S. Silva, Maria Manuela Pintado, and Susana M. Cardoso. 2021. "Impact of Phlorotannin Extracts from Fucus vesiculosus on Human Gut Microbiota" Marine Drugs 19, no. 7: 375. https://doi.org/10.3390/md19070375

APA Style

Catarino, M. D., Marçal, C., Bonifácio-Lopes, T., Campos, D., Mateus, N., Silva, A. M. S., Pintado, M. M., & Cardoso, S. M. (2021). Impact of Phlorotannin Extracts from Fucus vesiculosus on Human Gut Microbiota. Marine Drugs, 19(7), 375. https://doi.org/10.3390/md19070375

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