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Strain engineering and metabolic flux analysis of a probiotic yeast Saccharomyces boulardii for metabolizing l-fucose, a mammalian mucin component

Microbial Cell Factories volume 21, Article number: 204 (2022) Cite this article

Abstract

Background

Saccharomyces boulardii is a probiotic yeast that exhibits antimicrobial and anti-toxin activities. Although S. boulardii has been clinically used for decades to treat gastrointestinal disorders, several studies have reported weak or no beneficial effects of S. boulardii administration in some cases. These conflicting results of S. boulardii efficacity may be due to nutrient deficiencies in the intestine that make it difficult for S. boulardii to maintain its metabolic activity.

Results

To enable S. boulardii to overcome any nutritional deficiencies in the intestine, we constructed a S. boulardii strain that could metabolize l-fucose, a major component of mucin in the gut epithelium. The fucU, fucI, fucK, and fucA from Escherichia coli and HXT4 from S. cerevisiae were overexpressed in S. boulardii. The engineered S. boulardii metabolized l-fucose and produced 1,2-propanediol under aerobic and anaerobic conditions. It also produced large amounts of 1,2-propanediol under strict anaerobic conditions. An in silico genome-scale metabolic model analysis was performed to simulate the growth of S. boulardii on l-fucose, and elementary flux modes were calculated to identify critical metabolic reactions for assimilating l-fucose. As a result, we found that the engineered S. boulardii consumes l-fucose via (S)-lactaldehyde-(S)-lactate-pyruvate pathway, which is highly oxygen dependent.

Conclusion

To the best of our knowledge, this is the first study in which S. cerevisiae and S. boulardii strains capable of metabolizing l-fucose have been constructed. This strategy could be used to enhance the metabolic activity of S. boulardii and other probiotic microorganisms in the gut.

Background

Saccharomyces boulardii is a probiotic yeast known to interact with its host and exhibits antimicrobial activity [1, 2], antitoxin effects [3, 4], and immunoregulatory effects in the human intestine [5]. S. boulardii has a genome similar to that of S. cerevisiae but has a distinct phenotype [6]. For example, S. boulardii can readily grow at 37 °C, the normal human body temperature, and attach to human [7] or mouse intestinal epithelial cells [7, 8]. In addition, S. boulardii is more resistant to environmental stressors such as heat and acid than S. cerevisiae [9]. Because of these growth advantages, S. boulardii has higher metabolic activity in the intestine than S. cerevisiae and provides various health benefits in humans [6]. In particular, S. boulardii has prophylactic and therapeutic effects for many gastrointestinal diseases caused by pathogens such as pathogenic Escherichia coli [10, 11], Salmonella enterica serotype Typhimurium [12], Campylobacter jejuni [13, 14], and Clostridium difficile [3, 15]. These therapeutic effects have been reported in numerous clinical trials, and S. boulardii has been used for decades as an over-the-counter medicine to treat or prevent diarrhea in Europe, Africa, and America [16,17,18].

Although the therapeutic effects of S. boulardii administration have been validated in many studies, several studies have reported that S. boulardii administration had weak or no beneficial effects [19]. For example, Canani et al. reported that the administration of Lactobacillus rhamnosus GG or a mixture of probiotic bacteria reduced disease duration in children suffering from acute diarrhea, but the administration of S. boulardii had no effect [20]. In addition, Lewis et al. reported that S. boulardii administration to the elderly suffering from diarrhea was not effective in reducing the levels of the C. difficile toxin or treating general diarrhea [21]. Furthermore, Surawicz et al. reported that the administration of low-dose vancomycin and S. boulardii was ineffective in the treatment of C. difficile infection, although administration of high-dose vancomycin and S. boulardii was more effective than vancomycin alone [22]. These conflicting reports on the therapeutic effects of S. boulardii administration may be due to its limited ability to grow or maintain its normal metabolic activity in the intestine. In general, S. boulardii can remain in human and mouse intestines only after oral administration at a high dose, and it is completely excreted 3–7 days post-administration [23,24,25]. Interestingly, S. boulardii has been reported to colonize intestinal epithelial cells in antibiotic-treated humans or gnotobiotic mice [7, 8, 22, 26]. This suggests that although S. boulardii can grow and exhibit various metabolic activities in the intestine, it can be easily inhibited by competition with other gut microorganisms [6]. The reduced viability or metabolic activity of S. boulardii in the intestinal environment may cause the probiotic yeast to be degraded or excreted from the intestine before its therapeutic effects can be realized.

After colonizing the host, gut microorganisms metabolize molecules that are either secreted by the host or part of its diet [27]; however, dietary nutrients are competitively consumed by the host and other gut microorganisms [28, 29]. To overcome insufficient nutrient supply, some microorganisms metabolize mucins secreted by mammalian hosts [27]. Mucin is mainly composed of l-fucose, d-galactose, N-acetylgalactosamine, N-acetylglucosamine, d-glucuronic acid, and sialic acid [30]. Of these, gut microorganisms most frequently use l-fucose as a carbon source [31, 32]. Microorganisms such as Bacteroides thetaiotaomicron, Bacteroides fragilis, and Bifidobacterium bifidum secrete fucosidase to cleave l-fucose from the glycoprotein terminus of mucin molecules [33, 34]. The free l-fucose is then metabolized by other microbes via the fucose kinase pathway [35]. In this pathway, fucose mutarotase (fucU) converts β-l-fucose to α-l-fucose at the initial phase. Then, fucose isomerase (fucI) converts α-l-fucose to l-fuculose, which is then phosphorylated to l-fuculose-1-phosphate by fuculose kinase (fucK); this is followed by the conversion of fuculose-1-phosphate to lactaldehyde (LAD) and dihydroxyacetophenone (DHAP) by the action of fuculose phosphate aldolase (fucA) [35]. DHAP is used to synthesize building blocks for cell growth, while LAD is converted to 1,2-propanediol (1,2-PDO), which is converted to propionate by other microorganisms such as Eubacterium hallii [29]. 1,2-PDO is safe to humans as it is registered as generally recognized as safe (GRAS), and propionate is a short-chain fatty acid that is beneficial to humans [29]. This survival strategy can be applied to S. boulardii to ensure that it has access to an energy source in the intestine.

Our goal was to construct an engineered S. bouladii strain that can metabolize l-fucose for improved survival and metabolic activities in the intestine. Although the same genetic engineering techniques may be used for S. boulardii and S. cerevisiae, their efficiency is at least 30- to 50-fold lower in S. boulardii [36]; hence, we first introduced a fucose metabolic pathway using S. cerevisiae as a testbed. To investigate whether fucose metabolism in yeast strains can support cell growth, we performed in silico simulations using a genome-scale metabolic model (GEM) of S. cerevisiae (yeast-GEM; version 8.5.0) [37]. In addition, we used elementary flux mode analysis (EFMA) [38] to infer more details about the metabolic fluxes that involve l-fucose and generate energy under aerobic and anaerobic conditions.

Results and discussion

Growth simulation of S. cerevisiae that can metabolize l-fucose based on GEM analysis

Microorganisms that metabolize l-fucose must synthesize biological building blocks from lower glycolysis intermediates such as DHAP; thus, they are characterized by low energy levels and a slow growth rate [39]. To confirm that yeast can synthesize sufficient amounts of biological building blocks for cell growth while metabolizing l-fucose, we simulated in silico growth using a S. cerevisiae GEM (Fig. 1 and Additional file 1). During the growth simulation under aerobic conditions (objective function: biomass synthesis; oxygen supply unlimited), S. cerevisiae metabolized l-fucose at a rate of 1 mmol/g dried cell weight (DCW)/h and showed a specific growth rate of 0.08145/h (Fig. 1B). DHAP, which is an important intermediate in fucose metabolism and is also a part of the pentose phosphate pathway and glycolysis, is used for the synthesis of biological building blocks (Fig. 1A). LAD, another key intermediate in fucose metabolism, is known to be converted to 1,2-PDO [39]; however, in the growth simulation, all of the LAD was converted to pyruvate by lactaldehyde dehydrogenase and lactic acid dehydrogenase and used for the production of biological building blocks (Fig. 1A). In addition, the simulated S. cerevisiae secreted ethanol while metabolizing d-glucose but did not secrete extracellular metabolites such as ethanol, glycerol, and acetate while metabolizing l-fucose.

Fig. 1
figure 1

In silico genome-scale metabolic model analysis for the growth of Saccharomyces cerevisiae during l-fucose metabolism. A Fucose metabolism for cellular growth and detailed stoichiometry of each reaction. B In silico calculation of fucose uptake and growth rates, C Relationship between oxygen supply and growth on d-glucose or l-fucose

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Because the concentrations of oxygen vary in each part of the intestine, the amount of oxygen required to aerobically metabolize a carbon source is an important factor [40]. To infer how efficiently the yeast metabolizes l-fucose in the intestine, the oxygen requirements for the growth of l-fucose metabolizing yeast were compared to those for d-glucose metabolizing yeast (Fig. 1C). When 1 mmol of each carbon source was metabolized, yeast metabolizing d-glucose required less than 0.1 mmol oxygen for growth, whereas yeast metabolizing l-fucose required at least 0.507 mmol oxygen (Fig. 1C). These results show that the growth of yeast that can metabolize l-fucose is more oxygen-dependent than that of yeast metabolizing d-glucose. Under anaerobic conditions, S. boulardii consumes glucose and efficiently synthesizes energy and building blocks via pentose phosphate (PP) pathway and amino acid synthesis without gluconeogenesis. On the other hand, the two intermediates produced by fucose metabolism are DHAP and pyruvate, the initial and final molecules of lower glycolysis, so S. boulardii that metabolizes l-fucose need to building blocks via gluconeogenesis [39]. Under aerobic conditions, pyruvate is used for energy production through TCA cycle and DHAP is used for the synthesis of building blocks, so carbon fluxes of fucose metabolism can be more efficient than. Under anaerobic conditions where TCA cycle is unavailable and more DHAP is introduced into the glycolytic flux to synthesize energy resulting in reduced metabolic flux to synthesize building blocks. In addition, activation of the (S)-lactaldehyde-(S)-lactate-pyruvate pathway is difficult due to the lack of an oxidizing agent (Fig. 1A). In summary, fucose metabolism is highly oxygen dependent due to inefficient carbon fluxes and cofactor imbalance.

Construction of a S. cerevisiae strain that can metabolize l-fucose

The GEM model showed that the expression of undesignated fucose transporter, fucose mutarotase (fucU), fucose isomerase (fucI), fuculose kinase (fucK), and fuculose-1-phosphate aldolase (fucA) in S. cerevisiae was sufficient to allow the cells to metabolize l-fucose for growth (Fig. 1). In a previous study, Yu et al. reported that S. cerevisiae can transport small amounts of l-fucose [41]. In addition, the fucose permease (fucP) from the prokaryotic E. coli is less likely to be expressed in the eukaryotic S. cerevisiae. Therefore, except the fucose transporter, fucU, fucI, fucK, and fucA from E. coli K12 MG1655 were overexpressed in S. cerevisiae CEN. PK strain (S. cerevisiae FC; Table 1). However, neither wild-type S. cerevisiae (S. cerevisiae WT) nor S. cerevisiae FC was able to metabolize l-fucose in the yeast nitrogen base (YNB) medium (Fig. 2A, B). This could be because the yeast cells could not import enough l-fucose. To identify an appropriate transporter, we compared the l-fucose transport efficiency of an HXT-null S. cerevisiae expressing each hexose transporter (Table 1) [42]. We found that HXT2, HXT4, HXT6, or HXT7 expressing strains were able to transport l-fucose, and that the HXT4 strain had the highest fucose transport ability (Fig. 2C); therefore, we constructed a S. cerevisiae FCT strain that overexpressed fucose catabolic genes and HXT4 (Table 1). Under aerobic conditions, S. cerevisiae FCT metabolized l-fucose (0.27 ± 0.018 mmol fucose/g DCW/h) in the YNB medium. This strain was also able to grow on l-fucose (specific growth rates: 0.034 ± 0.001/h) and produced 1,2-PDO (0.045 ± 0.004 mmol 1,2-PDO/g DCW/h) (Fig. 2D). According to the GEM results, S. cerevisiae showed optimal growth when LAD was converted to lactate rather than 1,2-PDO (Fig. 1A); therefore, 1,2-PDO oxidoreductase was not overexpressed in S. cerevisiae FCT. The production of 1,2-PDO without the overexpression of 1,2-PDO oxidoreductase indicates that S. cerevisiae has an unidentified or promiscuous 1,2-PDO oxidoreductase that is expressed during fucose metabolism.

Table 1 Strains, plasmids, and primers used in this study
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Fig. 2
figure 2

Growth profiles of Saccharomyces cerevisiae while metabolizing l-fucose and comparisons of fucose transport efficiency. A Growth profile of wild-type S. cerevisiae, B Growth profile of S. cerevisiae FC, C Intracellular l-fucose concentrations in the HXT-Null strain and HXT1-7 overexpressed strains. D Growth profile of S. cerevisiae FCT. Three biological replicates were used

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Fermentation profiles of S. boulardii metabolizing l-fucose under different oxygen concentrations

To construct an engineered S. boulardii strain that can metabolize l-fucose, the genes necessary for fucose catabolism and HXT4 were overexpressed in S. boulardii (S. boulardii FCT; Table 1). Under aerobic conditions, wild-type S. boulardii (S. boulardii WT) was not able to metabolize l-fucose in YNB medium, whereas S. boulardii FCT was able to metabolize l-fucose (0.209 ± 0.004 mmol fucose/g DCW/h) and produce biomass (growth rate: 0.047 ± 0.001/h) and 1,2-PDO (0.018 ± 0.003 mmol 1,2-PDO/g DCW/h). During the first 72 h, S. boulardii FCT metabolized 14.69 ± 0.98 mmol fucose and produced 1.19 ± 0.16 mmol 1,2-PDO. S. boulardii FCT consumed the same amount of fucose as S. cerevisiae FCT and produced less 1,2-PDO and more biomass. Although the genomes of S. cerevisiae and S. boulardii are almost identical, it is known that the metabolism is slightly different due to mutations of various genes. For example, due to a point mutation in PGM2, S. boulardii metabolizes galactose very slowly [36] unlike S. cerevisiae which can metabolizes galactose rapidly. The overall metabolic changes induced by unknown mutations in those yeast strains might have led to different biomass and 1,2-PDO synthesis between S. cerevisiae FCT and S. boulardii FCT.

To examine the fucose metabolism of S. boulardii FCT in the intestinal environment, where the supply of oxygen is limited, we investigated its growth profiles under microaerobic and anaerobic conditions. Under microaerobic conditions, S. boulardii metabolized l-fucose (0.081 ± 0.001 mmol fucose/g DCW/h) and produced biomass (growth rate: 0.002 ± 0.0002/h) and 1,2-PDO (0.050 ± 0.004 mmol/g DCW/h). During the first 216 h, S. boulardii FCT metabolized 7.70 ± 0.88 mmol fucose and produced 2.89 ± 0.20 mmol 1,2-PDO. Under strict anaerobic conditions, S. boulardii metabolized l-fucose (0.045 ± 0.014 mmol fucose/g DCW/h) and produced 1,2-PDO (0.033 ± 0.003 mmol/g DCW/h) without growth. During the first 72 h, S. boulardii FCT metabolized 3.43 ± 0.27 mmol fucose and produced 1.83 ± 0.07 mmol 1,2-PDO. Because the oxygen supply was limited, yeast synthesized 1,2-PDO instead of biomass.

The high oxygen dependence of the (S)-lactaldehyde-(S)-lactate-pyruvate pathway inhibits the growth of S. boulardii FCT when it metabolizes l-fucose under anaerobic conditions. The GEM results revealed that the key steps for fucose-dependent yeast growth were the conversion of LAD to (S)-lactate and then to pyruvate using two oxidizing agents (Fig. 1A). In addition, we found that yeast growth based on fucose metabolism is highly oxygen-dependent because the (S)-lactaldehyde-(S)-lactate-pyruvate pathway requires many oxidizing agents (Fig. 1C). In the growth profile of S. boulardii FCT, which can metabolize l-fucose, the growth slowed markedly under microaerobic conditions and completely stopped under strict anaerobic conditions (Fig. 3C, D). Interestingly, S. boulardii FCT was able to metabolize l-fucose, even in an oxygen-limited environment, and showed a tendency to synthesize 1,2-PDO rather than biomass. These results suggest that under the conditions of limited oxygen supply, S. boulardii FCT metabolizes l-fucose through a specific metabolic pathway distinct from that predicted by the GEM.

Fig. 3
figure 3

Growth profiles of Saccharomyces boulardii while metabolizing l-fucose under different aerobic conditions. A Growth profiles of wild-type S. boulardii, B Growth profiles of S. boulardii FCT under aerobic conditions, C Growth profiles of S. boulardii FCT under microaerobic conditions, D Growth profiles of S. boulardii FCT under strict anaerobic conditions. Three biological replicates were used

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Prediction of yeast fucose metabolism under aerobic and anaerobic conditions using EFMA

The GEM results predicted the growth profile of S. boulardii FCT under aerobic conditions to be similar to that of the fermentation profile but did not predict the synthesis of 1,2-PDO (Fig. 3B). In addition, when the supply of oxygen was limited, S. boulardii FCT still metabolized l-fucose but produced 1,2-PDO instead of biomass (Fig. 3C, D). These results suggest that the fucose metabolism pathways predicted by the GEM and the cellular fucose metabolism pathways are different, especially in an oxygen-limited environment. We used EFMA to investigate the fucose metabolic pathways that allow the yeast to grow and produce energy along with small amounts of 1,2-PDO under aerobic conditions and to produce energy and large amounts of 1,2-PDO under anaerobic conditions (Fig. 4). DHAP and LAD are key intermediates in fucose metabolism. DHAP is also an intermediate in glycolysis and can be directly used for the synthesis of energy and building blocks (Fig. 4A). On the other hand, LAD can be used for the synthesis of building blocks only after it is converted to pyruvate by the (S)-lactaldehyde-(S)-lactate-pyruvate pathway [LAD to (S)-lactate pathway] or the (S)-lactaldehyde-pyruvaldehyde®lactate-pyruvate pathway (LAD to pyruvaldehyde pathway; Fig. 1A). The pathways that convert LAD to pyruvate require oxidative power (Fig. 1A). Alternatively, reductive power can be used to directly convert LAD to 1,2-PDO (Fig. 1A).

Fig. 4
figure 4

Elementary flux mode analysis for elucidating fucose metabolism under aerobic and anaerobic conditions. A Schematic diagram for putative fucose metabolism under aerobic conditions (B) and under anaerobic conditions. C Amount of 1,2-PDO and biomass produced by metabolizing fucose under aerobic conditions, D Stoichiometry for the maximum production of 1,2-PDO, biomass or energy in each condition

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A set of elementary flux modes to produce biomass and 1,2-PDO using each pathway under aerobic conditions was investigated (Fig. 4A). The LAD to (S)-lactate pathway had 39 models, and the LAD to pyruvaldehyde pathway had 51 models (Fig. 4C). In the LAD to (S)-lactate pathway, 1 M l-fucose was metabolized to synthesize up to 110.35 g/L biomass or up to 1 M 1,2-PDO and 47.46 g/L biomass (Fig. 4C, D). In the LAD to pyruvaldehyde pathway, 1 M l-fucose was metabolized to produce up to 0.73 M 1,2-PDO and 65.57 g/L biomass or up to 1 M 1,2-PDO and 47.46 g/L biomass (Fig. 4C, D). In the LAD to (S)-lactate pathway model, all fucose was converted into biomass, which was consistent with the production of 1,2-PDO and biomass in the fermentation experiment (Fig. 4C). The EFMA results also showed that neither the LAD to (S)-lactate pathway nor the LAD to the pyruvaldehyde pathway could be maintained under anaerobic conditions because NAD+ could not be regenerated quickly enough (Fig. 4B). Instead, the yeast synthesized 1 M of ATP by converting 1 M of l-fucose into 1 M of 1,2-PDO and 1 M of pyruvate (Fig. 4B, D). This is consistent with the result that the yeast synthesized more 1,2-PDO than biomass when oxygen was limited (Fig. 3C, D).

Saccharomyces boulardii FCT, which can metabolize l-fucose, synthesizes small amounts of 1,2-PDO and large amounts of biomass through the (S)-lactaldehyde-(S)-lactate-pyruvate pathway under aerobic conditions; however, under anaerobic conditions, it synthesizes large amounts of 1,2-PDO to generate energy but does not produce much biomass. During fermentation under aerobic conditions, S. boulardii FCT used most of the l-fucose to synthesize biomass. This result was consistent with the predictions of multiple EFMA models for the LAD to (S)-lactate pathway when only l-fucose was available for biomass synthesis (Fig. 4C). In addition, other EFMA models for the (S)-lactate pathway used l-fucose for the simultaneous synthesis of relatively small amounts of biomass and large amounts of 1,2-PDO (Fig. 4C). On the other hand, the EFMA models for the pyruvaldehyde pathway predicted synthesis of at least 0.72 M of 1,2-PDO while metabolizing 1 M of l-fucose, which was markedly different from the fermentation data (Fig. 4C). These results indicate that S. boulardii, which metabolizes l-fucose under aerobic conditions, mostly synthesizes biomass along with a small amount of 1,2-PDO using the LAD to (S)-lactate pathway. Under microaerobic and strict anaerobic conditions, S. boulardii FCT metabolized l-fucose, and synthesized more 1,2-PDO, along with little or no biomass (Fig. 3C, D). The EFMA model showed that S. boulardii FCT metabolizes l-fucose under anaerobic conditions and produces 1,2-PDO, pyruvate, and ATP. When oxygen is limited, S. boulardii FCT may decrease biomass synthesis but increase 1,2-PDO synthesis by shifting the metabolic flux away from the LAD to (S)-lactate pathway and towards the production of 1,2-PDO and energy. Although pyruvate has not been quantified in anaerobic fermentation profiles, this could be because pyruvate is used in many different metabolic fluxes, as the molecule is a major metabolite in various metabolic processes, including glycolysis, gluconeogenesis, and pyruvic acid metabolism.

As S. boulardii FCT can consume l-fucose and synthesize energy and biological building blocks, it may have better metabolic activity than wild-type S. boulardii in the intestine. Although S. boulardii FCT showed a decrease in biomass synthesis under low-oxygen conditions, it still grew under microaerobic conditions (Fig. 3C). S. boulardii FCT also generated energy while synthesizing 1,2-PDO under strict anaerobic conditions (Figs. 3D and 4D). Because the oxygen concentration in the human intestine is very different depending on the location (apical mucosa closest to the lumen: 0.1–1%; intestinal wall: ~ 6%; colonic muscle wall: 7–10%) [40], S. boulardii FCT might be able to synthesize energy and biological building blocks from l-fucose under aerobic, microaerobic, and anaerobic conditions. Wild type S. boulardii can stay for 3 days in the intestine of a normal mouse, and can colonize the intestine of a gnotobiotic mouse [8]. The amount of l-fucose in the intestine is about 0.1 mmol, which can be continuously supplied by the host [31]. Assuming microaerobic conditions (Fig. 3C), 1 g DCW of S. boulardii FCT consumes 5.832 mmol of l-fucose, producing 0.144 g of biomass and 3.6 mmol of 1,2 PDO over 3 days. The growth rate of S. boulardii FCT on l-fucose may be insufficient to colonize the intestine before excretion. However, l-fucose still can be used for cell growth or survival by supplying energy and building blocks in the absence of other nutrient and as a supplementary energy source when S. boulardii FCT consumes other nutrients in the intestine. Animal studies would demonstrate the enhanced metabolic activity of S. bouarldii FCT in vivo. To do so, the integration of l-fucose metabolizing genes into the genome will be necessary to stably produce the heterologous enzymes in the intestine.

Conclusion

Saccharomyces boulardii is a probiotic yeast that is widely used as a therapeutic agent for the treatment of intestinal diseases. In this study, we constructed S. cerevisiae and S. boulardii strains that metabolize l-fucose by selecting genes required for fucose metabolism based on GEM data and overexpressing fucose catabolic genes from E. coli and the transporter gene HXT4 from S. cerevisiae. We also proposed mechanisms by which yeast strains metabolize l-fucose and generate biomass, 1,2-PDO, and energy under aerobic and anaerobic conditions. S. boulardii that can metabolize l-fucose in the intestine can continuously receive a carbon source from the host and could exert improved probiotic effects as a result. To our knowledge, this is the first study in which S. cerevisiae and S. boulardii strains capable of metabolizing l-fucose have been constructed. This strategy could also be used to enhance the metabolic activity of other probiotic microorganisms in the gut.

Materials and methods

Strains, plasmid construction, and culture conditions

The fucU, fucA, fucK, and fucI genes from E. coli K12 MG1655 and HXT4 gene from S. cerevisiae CEN. PK2-1D were inserted into the plasmids pRS423GPD, pRS424GPD, and pRS426GPD [43]. E. coli DH5α was used for the construction and amplification of the plasmids. S. cerevisiae CEN. PK2-1D [44] and S. boulardii ATCC MYA-796 [36] were used. The plasmids were transformed into S. cerevisiae or S. boulardii using the lithium acetate/single-stranded carrier DNA/polyethylene glycol method [45]. E. coli strains were cultured in Luria–Bertani (LB) medium containing 100 µg/mL ampicillin at 37 °C and 200 rpm for amplification of plasmids. The S. cerevisiae or S. boulardii strains harboring the plasmids were cultured in yeast synthetic complete (YSC) medium containing 6.7 g/L yeast nitrogen base without amino acids, 20 g/L l-fucose (Biosynth Carbosynth, U.K.), and 0.70 g/L CSM-HIS-TRP-URA (MP Biomedicals). For tests under aerobic conditions, S. cerevisiae or S. boulardii were cultured in 100 mL fucose media in 250 mL flasks with shaking at 200 rpm. For tests under microaerobic conditions, S. boulardii was cultured in 100 mL fucose media in 160 mL serum bottles in a jar containing Anaero Pack-MicroAero (Mitsubishi Gas Chemical, Japan; O2 concentration of 6–12%, CO2 concentration of 5–8%) without shaking. After each sampling, the Anaero Pack was replaced. For tests under strict anaerobic conditions, S. boulardii was cultured in 100 mL fucose media in 160 mL serum bottles in an anaerobic chamber (Vinyl anaerobic chamber Type B; Coy Laboratory Products) without shaking. The atmosphere in the anaerobic chamber consisted of 90% nitrogen (v/v), 5% carbon dioxide (v/v), and 5% hydrogen (v/v).

Analyses of extracellular metabolites

For the identification and quantification of extracellular metabolites, including d-glucose (Sigma-Aldrich), l-fucose (Sigma-Aldrich), and 1,2-PDO (Sigma-Aldrich), a high-performance liquid chromatography (HPLC) system equipped with a refractive index detector, Agilent 1100 (Agilent Technologies), and an Aminex HPX-87 H organic acid column (Bio-Rad) was used. We used a constant flow rate of 0.5 mL/min at 65 °C and 0.01 NH2SO4 as the mobile phase. The retention times of each metabolite were 17.373 min for d-glucose, 12.828 min for l-fucose, and 20.132 min for 1,2-PDO, respectively.

Comparison of fucose transport efficiency among innate hexose transporters in S. cerevisiae

To investigate the fucose transport efficiency of each hexose transporter, the HXT-Null strain and the strains overexpressing HXT 1–7 were cultured in 5 mL of yeast extract and peptone (YP) media. The HXT-Null strain was cultured in YP containing ethanol (20 g/L) and the rest of the strains were cultured in YP containing glucose (20 g/L), and cells entering the intermediate exponential phase were harvested (OD 13/mL). The harvested cells were washed three times with distilled water (DW) and then cultured in 1 mL of YP with l-fucose (2 g/L) medium at 30 °C and 250 rpm for 4 h, and then 1 mL of cells was collected. The harvested cells were reconstituted in 500 µL of DW containing glass beads and vortexed for 1 h. The samples were centrifuged at 13,000 rpm for 30 min and 400 µL of the supernatant was collected and dried. The dried samples were reconstituted in 120 µL of DW, and the fucose concentration of each sample was analyzed by HPLC.

GEM analysis to simulate the growth of S. cerevisiae that can metabolize l-fucose

The GEM for S. cerevisiae (yeast-GEM; version 8.5.0) [37] was used to simulate the growth of S. cerevisiae with the ability to metabolize l-fucose. To enable the simulation of fucose metabolism, β-l-fucose exchange, β-l-fucose transport, α-l-fucose exchange, α-l-fucose transport, fucose isomerase, fuculose kinase, fuculose-1-phosphate aldolase, 1,2-PDO oxidoreductase, and 1,2-PDO transport reactions were included in the model (Additional file 1). Extracellular β-l-fucose, cytoplasmic β-l-fucose, extracellular α-l-fucose, cytoplasmic α-l-fucose, cytoplasmic fuculose, cytoplasmic fuculose-1-phosphate, cytoplasmic 1,2-PDO, and extracellular 1,2-PDO were added to the model as the metabolites. MATLAB (version R2016b), Gurobi (version 8.0.1), and Cobra Toolbox (version 2.26) [46, 47] were used for GEM analysis. The MATLAB data file was uploaded to BioModels (MODEL2209060001).

EFMA to elucidate the metabolic pathway of l-fucose under aerobic and anaerobic conditions

To elucidate the pathways of fucose metabolism in more detail, we modified the previously reported EFMA of S. cerevisiae [38]. Because this model contains many central carbon metabolic pathways, such as glycolysis, gluconeogenesis, the pentose phosphate pathway, and the TCA cycle, we introduced enzymes such as fucose isomerase, fuculose kinase, fuculose-1-phosphate aldolase, 1,2-PDO oxidoreductase, (S)-lactaldehyde dehydrogenase, (S)-lactic acid dehydrogenase, methylglyoxal reductase, and (D)-lactate dehydrogenase into the model. In addition, to obtain the absolute amount of the synthesized dried cell weight, we summed up the number moles of the building blocks (acetyl-CoA 0.269 M, α-ketoglutarate 0.11 M, erythrose-4-phosphate 0.003 M, 3-phosphoglyceric acid 0.006 M, glyceraldehyde-3-phosphate 0.001 M, phosphoenolpyruvate 0.006 M, pyruvate 0.018 M, ribulose-5-phosphate 0.003 M, glucose-6-phosphate 0.025 M, and oxaloacetate 0.01 M) required for cell growth and regarded it as the cell dry weight (15.74 g/L). The OD was converted to yeast dry cell weight based on a previously reported value [48].

Availability of data and materials

The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.

References

  1. Edwards-Ingram L, Gitsham P, Burton N, Warhurst G, Clarke I, Hoyle D, et al. Genotypic and physiological characterization of Saccharomyces boulardii, the probiotic strain of Saccharomyces cerevisiae. Appl Environ Microbiol. 2007;73:2458–67.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  2. Everard A, Matamoros S, Geurts L, Delzenne NM, Cani PD. Saccharomyces boulardii administration changes gut microbiota and reduces hepatic steatosis, low-grade inflammation, and fat mass in obese and type 2 diabetic db/db mice. mBio. 2014;5:e01011-4.

    Article  Google Scholar 

  3. Castagliuolo I, LaMont JT, Nikulasson ST, Pothoulakis C. Saccharomyces boulardii protease inhibits Clostridium difficile toxin A effects in the rat ileum. Infect Immun. 1996;64:5225–32.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  4. Castagliuolo I, Riegler MF, Valenick L, LaMont JT, Pothoulakis C. Saccharomyces boulardii protease inhibits the effects of Clostridium difficile toxins A and B in human colonic mucosa. Infect Immun. 1999;67:302–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  5. McFarland LV. Systematic review and meta-analysis of Saccharomyces boulardii in adult patients. World J Gastroenterol. 2010;16:2202–22.

    Article  PubMed  PubMed Central  Google Scholar 

  6. Pais P, Almeida V, Yılmaz M, Teixeira MC. Saccharomyces boulardii: what makes it tick as successful probiotic? J Fungi. 2020;6:78.

    Article  CAS  Google Scholar 

  7. Klein SM, Elmer GW, McFarland LV, Surawicz CM, Levy RH. Recovery and elimination of the biotherapeutic agent, Saccharomyces boulardii, in healthy human volunteers. Pharm Res. 1993;10:1615–9.

    Article  CAS  PubMed  Google Scholar 

  8. Durmusoglu D, Al’Abri I, Collins SP, Beisel C, Crook N. Establishing probiotic Saccharomyces boulardii as a model organism for synthesis and delivery of biomolecules. bioRxiv. 2020. https://www.biorxiv.org/content/https://doi.org/10.1101/2020.01.22.915389v1.

  9. Fietto JLR, Araújo RS, Valadão FN, Fietto LG, Brandão RL, Neves MJ, et al. Molecular and physiological comparisons between Saccharomyces cerevisiae and Saccharomyces boulardii. Can J Microbiol. 2004;50:615–21.

    Article  CAS  PubMed  Google Scholar 

  10. Dalmasso G, Loubat A, Dahan S, Calle G, Rampal P, Czerucka D. Saccharomyces boulardii prevents TNF-α-induced apoptosis in EHEC-infected T84 cells. Res Microbiol. 2006;157:456–65.

    Article  CAS  PubMed  Google Scholar 

  11. Czerucka D, Dahan S, Mograbi B, Rossi B, Rampal P. Saccharomyces boulardii preserves the barrier function and modulates the signal transduction pathway induced in enteropathogenic Escherichia coli-infected T84 cells. Infect Immun. 2000;68:5998–6004.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  12. Pontier-Bres R, Munro P, Boyer L, Anty R, Imbert V, Terciolo C, et al. Saccharomyces boulardii modifies Salmonella Typhimurium traffic and host immune responses along the intestinal tract. PLoS ONE. 2014;9:e103069.

    Article  PubMed  PubMed Central  Google Scholar 

  13. Guyard-Nicodème M, Keita A, Quesne S, Amelot M, Poezevara T, Le Berre B, et al. Efficacy of feed additives against Campylobacter in live broilers during the entire rearing period. Poult Sci. 2016;95:298–305.

    Article  PubMed  Google Scholar 

  14. Line J, Bailey J, Cox N, Stern N. Yeast treatment to reduce Salmonella and Campylobacter populations associated with broiler chickens subjected to transport stress. Poult Sci. 1997;76:1227–31.

    Article  CAS  PubMed  Google Scholar 

  15. Czerucka D, Piche T, Rampal P. Review article: yeast as probiotics—Saccharomyces boulardii. Aliment Pharmacol Ther. 2007;26:767–78.

    Article  CAS  PubMed  Google Scholar 

  16. McCullough MJ, Clemons KV, McCusker JH, Stevens DA. Species identification and virulence attributes of Saccharomyces boulardii (nom. inval.). J Clin Microbiol. 1998;36:2613–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  17. Cui B, Lin L, Wang B, Liu W, Sun C. Therapeutic potential of Saccharomyces boulardii in liver diseases: from passive bystander to protective performer? Pharm Res. 2022;175:106022.

    Article  CAS  Google Scholar 

  18. McFarland LV. Chapter 18—Common organisms and probiotics: Saccharomyces boulardii. In: Floch MH, Ringel Y, Allan Walker W, editors. The microbiota in gastrointestinal pathophysiology. Boston: Academic Press; 2017. p. 145–64.

    Chapter  Google Scholar 

  19. Kelesidis T, Pothoulakis C. Efficacy and safety of the probiotic Saccharomyces boulardii for the prevention and therapy of gastrointestinal disorders. Th Adv Gastroenterol. 2012;5:111–25.

    Article  Google Scholar 

  20. Canani RB, Cirillo P, Terrin G, Cesarano L, Spagnuolo MI, Vincenzo AD, et al. Probiotics for treatment of acute diarrhoea in children: randomised clinical trial of five different preparations. BMJ. 2007;335:340.

    Article  PubMed  PubMed Central  Google Scholar 

  21. Lewis SJ, Potts LF, Barry RE. The lack of therapeutic effect of Saccharomyces boulardii in the prevention of antibiotic-related diarrhoea in elderly patients. J Infect. 1998;36:171–4.

    Article  CAS  PubMed  Google Scholar 

  22. Surawicz CM, McFarland LV, Greenberg RN, Rubin M, Fekety R, Mulligan ME, et al. The search for a better treatment for recurrent Clostridium difficile disease: use of high-dose vancomycin combined with Saccharomyces boulardii. Clin Infect Dis. 2000;31:1012–7.

    Article  CAS  PubMed  Google Scholar 

  23. Blehaut H, Massot J, Elmer GW, Levy RH. Disposition kinetics of Saccharomyces boulardii in man and rat. Biopharm Drug Dispos. 1989;10:353–64.

    Article  CAS  PubMed  Google Scholar 

  24. Barc M-C, Charrin-Sarnel C, Rochet V, Bourlioux F, Sandré C, Boureau H, et al. Molecular analysis of the digestive microbiota in a gnotobiotic mouse model during antibiotic treatment: influence of Saccharomyces boulardii. Anaerobe. 2008;14:229–33.

    Article  CAS  PubMed  Google Scholar 

  25. Samonis G, Falagas ME, Lionakis S, Ntaoukakis M, Kofteridis DP, Ntalas I, et al. Saccharomyces boulardii and Candida albicans experimental colonization of the murine gut. Med Mycol. 2011;49:395–9.

    Article  CAS  PubMed  Google Scholar 

  26. Rodrigues AC, Nardi RM, Bambirra EA, Vieira EC, Nicoli JR. Effect of Saccharomyces boulardii against experimental oral infection with Salmonella Typhimurium and Shigella flexneri in conventional and gnotobiotic mice. J Appl Bacteriol. 1996;81:251–6.

    Article  CAS  PubMed  Google Scholar 

  27. Sommer F, Bäckhed F. The gut microbiota—masters of host development and physiology. Nat Rev Microbiol. 2013;11:227–38.

    Article  CAS  PubMed  Google Scholar 

  28. Pereira FC, Berry D. Microbial nutrient niches in the gut. Environ Microbiol. 2017;19:1366–78.

    Article  PubMed  PubMed Central  Google Scholar 

  29. Louis P, Hold GL, Flint HJ. The gut microbiota, bacterial metabolites and colorectal cancer. Nat Rev Microbiol. 2014;12:661–72.

    Article  CAS  PubMed  Google Scholar 

  30. Sicard J-F, Le Bihan G, Vogeleer P, Jacques M, Harel J. Interactions of intestinal bacteria with components of the intestinal mucus. Front Cell Infect Microbiol. 2017;7:387.

    Article  PubMed  PubMed Central  Google Scholar 

  31. Pacheco AR, Curtis MM, Ritchie JM, Munera D, Waldor MK, Moreira CG, et al. Fucose sensing regulates bacterial intestinal colonization. Nature. 2012;492:113–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  32. Stahl M, Friis LM, Nothaft H, Liu X, Li J, Szymanski CM, et al. l-fucose utilization provides Campylobacter jejuni with a competitive advantage. Proc Natl Acad Sci USA. 2011;108:7194–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  33. Goto Y, Uematsu S, Kiyono H. Epithelial glycosylation in gut homeostasis and inflammation. Nat Immunol. 2016;17:1244–51.

    Article  CAS  PubMed  Google Scholar 

  34. Katayama T, Sakuma A, Kimura T, Makimura Y, Hiratake J, Sakata K, et al. Molecular cloning and characterization of Bifidobacterium bifidum 1,2-α-l-fucosidase (AfcA), a novel inverting glycosidase (glycoside hydrolase family 95). J Bacteriol. 2004;186:4885–93.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  35. Hooper LV, Xu J, Falk PG, Midtvedt T, Gordon JI. A molecular sensor that allows a gut commensal to control its nutrient foundation in a competitive ecosystem. Proc Natl Acad Sci USA. 1999;96:9833–8.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  36. Liu J-J, Kong II, Zhang G-C, Jayakody LN, Kim H, Xia P-F, et al. Metabolic engineering of probiotic Saccharomyces boulardii. Appl Environ Microbiol. 2016;82:2280–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  37. Lu H, Li F, Sánchez BJ, Zhu Z, Li G, Domenzain I, et al. A consensus S. cerevisiae metabolic model Yeast8 and its ecosystem for comprehensively probing cellular metabolism. Nat Commun. 2019;10:3586.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  38. Matsuda F, Furusawa C, Kondo T, Ishii J, Shimizu H, Kondo A. Engineering strategy of yeast metabolism for higher alcohol production. Microb Cell Fact. 2011;10:70.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Kim J, Cheong YE, Jung I, Kim KH. Metabolomic and transcriptomic analyses of Escherichia coli for efficient fermentation of l-fucose. Mar Drugs. 2019;17:82.

    Article  CAS  PubMed Central  Google Scholar 

  40. Schwerdtfeger LA, Nealon NJ, Ryan EP, Tobet SA. Human colon function ex vivo: dependence on oxygen and sensitivity to antibiotic. PLoS ONE. 2019;14:e0217170.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Yu S, Liu J-J, Yun EJ, Kwak S, Kim KH, Jin Y-S. Production of a human milk oligosaccharide 2′-fucosyllactose by metabolically engineered Saccharomyces cerevisiae. Microb Cell Fact. 2018;17:101.

    Article  PubMed  PubMed Central  Google Scholar 

  42. Xu H. Engineering Saccharomyces cerevisiae for cellulosic ethanol production. Master’s thesis, University of Illinois at Urbana-Champaign. 2015. https://www.ideals.illinois.edu/items/91351.

  43. Christianson TW, Sikorski RS, Dante M, Shero JH, Hieter P. Multifunctional yeast high-copy-number shuttle vectors. Gene. 1992;110:119–22.

    Article  CAS  PubMed  Google Scholar 

  44. Entian K-D, Kötter P. 23 Yeast mutant and plasmid collections. In: Brown AJP, Tuite M, editors. Methods in microbiology. Boston: Academic Press; 1998. p. 431–49.

    Google Scholar 

  45. Gietz RD, Schiestl RH. High-efficiency yeast transformation using the LiAc/SS carrier DNA/PEG method. Nat Protoc. 2007;2:31–4.

    Article  CAS  PubMed  Google Scholar 

  46. Heirendt L, Arreckx S, Pfau T, Mendoza SN, Richelle A, Heinken A, et al. Creation and analysis of biochemical constraint-based models using the COBRA Toolbox v.3.0. Nat Protoc. 2019;14:639–702.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Vlassis N, Pacheco MP, Sauter T. Fast reconstruction of compact context-specific metabolic network models. PLoS Comput Biol. 2014;10:e1003424.

    Article  PubMed  PubMed Central  Google Scholar 

  48. Sohn SB, Kim TY, Lee JH, Lee SY. Genome-scale metabolic model of the fission yeast Schizosaccharomyces pombe and the reconciliation of in silico/in vivo mutant growth. BMC Syst Biol. 2012;6:49.

    Article  PubMed  PubMed Central  Google Scholar 

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Acknowledgements

This work was supported by the Korea University Food Safety Hall for the Institute of Biomedical Science and Food Safety and by a Korea University Grant.

Funding

This work was financially supported by the Ministry of Trade, Industry & Energy (20018132) and the Korea Institute of Planning and Evaluation for Technology in Food, Agriculture, Forestry, and Fisheries funded by the Ministry of Agriculture, Food and Rural Affairs (321036051SB010).

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Authors and Affiliations

  1. Carl R. Woese Institute for Genomic Biology, University of Illinois at Urbana-Champaign, Urbana, IL, 61801, USA

    Jungyeon Kim & Yong-Su Jin

  2. Department of Biotechnology, Graduate School, Korea University, Seoul, 02841, Republic of Korea

    Jungyeon Kim, Yu Eun Cheong, Sora Yu & Kyoung Heon Kim

  3. Department of Food Science and Human Nutrition, University of Illinois at Urbana-Champaign, Urbana, IL, 61801, USA

    Yong-Su Jin

  4. Department of Food Bioscience and Technology, College of Life Sciences and Biotechnology, Korea University, Seoul, 02841, Republic of Korea

    Kyoung Heon Kim

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Contributions

JK, YSJ, and KHK conceived and designed the experiments. JK, YEC, and SY performed the experiments. JK analyzed the data. JK wrote this manuscript. YSJ and KHK reviewed and revised the manuscript. All authors read and approved the final manuscript.

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Supplementary Information

Additional file 1.

Genome-scale metabolic model of Saccharomyces cerevisiae that metabolizes fucose. Table S1. Sequences of the plasmids constructed in this study.

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Kim, J., Cheong, Y.E., Yu, S. et al. Strain engineering and metabolic flux analysis of a probiotic yeast Saccharomyces boulardii for metabolizing l-fucose, a mammalian mucin component. Microb Cell Fact 21, 204 (2022). https://doi.org/10.1186/s12934-022-01926-x

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Keywords

Microbial Cell Factories

ISSN: 1475-2859

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