Intestinal microbiota as a tetrahydrobiopterin exogenous source in hph-1 mice

Tetrahydrobiopterin (BH4) is a cofactor of a number of regulatory enzymes. Although there are no known BH4 exogenous sources, the tissue content of this biopterin increases with age in GTP cyclohydrolase 1-deficient hyperphenylalaninemia-1 (hph-1) mice. Since certain bacteria are known to generate BH4, we hypothesize that generation of this biopterin by the intestinal microbiota contributes to its tissue increase in hph-1 adult mice. The goal of this study was to comparatively evaluate hph-1 mice and wild-type C57Bl/6 controls for the presence of intestinal BH4-producing bacteria. Newborn and adult mice fecal material was screened for 6-pyruvoyltetrahydropterin synthase (PTPS-2) an enzyme only present in BH4-generating bacteria. Adult, but not newborn, wild-type control and hph-1 mouse fecal material contained PTPS-2 mRNA indicative of the presence of BH4-generating bacteria. Utilizing chemostat-cultured human fecal bacteria, we identified the PTPS-2-producing bacteria as belonging to the Actinobacteria phylum. We further confirmed that at least two PTPS-2-producing species, Aldercreutzia equolifaciens and Microbacterium schleiferi, generate BH4 and are present in hph-1 fecal material. In conclusion, intestinal Actinobacteria generate BH4. This finding has important translational significance, since manipulation of the intestinal flora in individuals with congenital biopterin deficiency may allow for an increase in total body BH4 content.

It is, therefore, possible that hph-1 mice are able to obtain BH4 in adult life via exogenous sources, yet this biopterin is not present in food.
The intestinal microbiota has been recently gaining a lot of attention as an enteral source of metabolites that contribute to the endogenous pool [10][11][12] . Cyanobacteria such as Synechococcus elongatus (S. elongatus), depend on pterins for pigment color generation and contain 6-pyruvoyltetrahydropterin synthase (EC 4.2.3.12; PTPS) an enzyme only present in BH4-generating bacteria 13 and regulated by the PTPS-2 gene. We hypothesized that the intestinal microbiota also contains bacteria capable of generating BH4, and that PTPS-2 expression could be used as a biomarker for this activity. We therefore screened fecal material from wild type and hph-1 mice for the presence of BH4-generating bacteria. We then went on to screen representative human microbial communities for PTPS-2 expression. We present data demonstrating that adult mice and human intestinal microbiota contain bacteria capable of BH4 generation.

Results
Tissue BH4 content. We first conducted a comparative analysis of adult hph-1 and wild type control mice BH4 tissue content. As shown in Fig. 1, when compared with wild type animals, the hph-1 mouse large intestine (bowel), lung, brain and aorta BH4 tissue content was significantly reduced (P < 0.01), although this biopterin was present in all measured tissues.
Fecal material PTPS-2 mRNA expression. We proceeded to screen colonic material from newborn and adult mice for the presence of PTPS-2. PTPS-2 mRNA expression was detectable in wild type and hph-1 adult mice, but absent in the newborn animals ( Fig. 2A). No significant difference in PTPS-2 mRNA expression was observed between the mouse strains.
Identification of the PTPS-2 containing intestinal bacteria. We used diverse, defined pools of bacterial isolates from human feces that were cultured as communities in chemostat bioreactors 14,15 to evaluate the presence of PTPS-2 expressing bacteria. As shown in Fig. 2B, PTPS-2 mRNA expression was detected in the two distinct chemostat fecal microbiota cultures, MET-1 and MET-2.
To identify the PTPS-2 expressing bacteria species in the chemostat-cultured fecal material, we first divided the communities up by phyla and evaluated each of these groups individually. The strains expressing PTPS-2 are illustrated in the Table 1.
We next proceeded to screen colonic material from the newborn and adult mice for the presence of Actinobacteria-specific 16S rRNA, and confirmed that this bacterial phylum can be detected in adult mice (Fig. 3).
Actinobacteria generate BH4. We first screened adult hph-1 mouse colonic fecal material for the presence of BH4 and determined the content of this biopterin to be 1.2 ± 0.1 ng/g of fecal material (N = 3). Using human Figure 1. Adult wild type and hph-1 bowel, lung, brain and aorta BH4 tissue content. N = 4 for all strain/ organ groups. **P < 0.01 when compared with wild type group by Student unpaired t-test.
The potential for generation of BH4 by intestinal Actinobacteria is prevalent. Using a library of human feces-derived Actinobacteria spp., we went on to screen for the presence of PTPS-2 in these strains in order to assess how widespread BH4 generation ability is among this phylum. We axenically cultured 31 additional Actinobacteria isolates and assessed them for the presence of PTSPS-2 by real-time-qPCR. We found several isolates which expressed PTPS-2 (Table 1), including representatives of several species of Bifidobacterium that have been previously noted to be of importance to neonatal health 16,17 .

Discussion
In this study, we documented the presence of BH4-generating bacteria in the mouse gut microbiota. The microbes responsible for BH4 production in the intestinal microbiota were found to belong to the Actinobacteria phylum, and we went on to show that strains of several Actinobacteria spp. derived from the human gut are able to express the PTPS-2 gene, accounting for BH4 generation in defined, chemostat-cultured, human fecal material.
hph-1 mice show a 90% decrease in GTPCH1 expression when compared with wild-type controls [18][19][20][21] . This deficiency results in low to absent tissue BH4 levels at birth. The hph-1 mouse tissue BH4 increases with age 1,22 and the adult hph-1 mouse ileal tissue BH4 content is similar to that of wild-type control animals 23 .
The partial and age-dependent GTPCH1 expression/activity in the hph-1 mice contributes to the higher tissue BH4 content in adult hph-1 mice, when compared with early in life. Yet other factors likely play a role in the age-related organ BH4 content changes. In the present study, we hypothesize, and provide supporting evidence, that the rodent and human intestinal microbiota are capable of generating this biopterin.
Over the last two decades, both green sulfur bacteria and cyanobacteria have been postulated as BH4 producers based on the discovery of PTPS-2 orthologs in their genomes 13,24,25 . Pteridines are involved in pigmentation and thus the biopterin generating ability of these bacteria may relate to photosynthetic requirements. However, while bacterial BH4 production ability is established, phototrophic bacteria do not colonize the intestine, and thus the extent to which the intestinal microbiota is capable of BH4 generation, and its contribution to the endogenous pool of this biopterin, to the best of our knowledge has not been adequately investigated.
Bacteria are known to generate nutritional factors that can be absorbed by the gastrointestinal tract and play important functional roles in mammals. Examples of this process include orally derived nitrate 26,27 and folic acid [28][29][30] . A stable oral form of BH4 is currently in use clinically (Kuvan©) attesting to the gastrointestinal route as an efficient transporter of this biopterin 31 . It is likely, therefore, that the generation of BH4 by the intestinal microbiota contributes to its presence in adult hph-1 tissues.
It is known that the gut microbiota modulates the development of the enteric nervous system in mice 10 . We show in the present study that Bifidobacterium spp., a major group of Actinobacteria within the mammalian gut microbiota, and the predominant intestinal genus in breast-fed infants 32 , express PTPS-2. In addition, we have shown that human breast milk has a high BH4 content 33 and may thus be an important contributor to the endogenous BH4 pool early in life. In fact, idiopathic hypertrophic pyloric stenosis is rarely present in breast-fed infants 34 . These data together with the present finding that PTPS-2 expressing bacteria were not detected in newborn mice suggest that major contributors to the BH4 endogenous pool are breast milk early in life followed by the intestinal microbiota as it becomes established into adulthood. We anticipate this may be of particular importance in subjects with inborn errors of biopterin metabolism in which BH4 synthesis has been compromised.
Although our screening for the presence of human-derived Actinobacteria spp. with PTPS-2 expression ability was limited, it is important to note that this activity does not seem to be species specific. In three cases, we noted that PTPS-2 expression could be detected for one but not another strain of the same species (Bifidobacterium infantis, Eggerthella lenta and Gordonibacter urolithinfaciens). This suggests that either there are differences in PTPS-2 gene presence among strains of the same species, or that gene expression is limited by environmental conditions. Further work is necessary to definitively delineate the presence of PTPS-2 genes across the Actinobacteria phylum, and to assess whether these genes are active in the mammalian intestine and responsible for BH4 production that can be utilized by the host for metabolic purposes. This study has some limitations. Our primary goal was to identify specific bacteria capable of BH4 generation. Although we began our studies by assessing BH4 production in a mouse model, we went on to screen defined chemostat-cultured human fecal material for the presence of PTPS-2 expressing bacteria since we considered this translationally relevant to human disease. Indeed, our chemostat bioreactor model is set up to mimic conditions of the human intestine and not easily adaptable for inoculation by mouse fecal pellets. Thus, we have not assessed mouse-derived Actinobacteria in this study beyond our initial screening.
In conclusion, the intestinal microbiota contains BH4 generating bacteria and these likely contribute to the age-dependent rise in tissue levels of this biopterin in hph-1 mice, a BH4 deficient strain. The human gut microbiota additionally contains PTPS-2-expressing bacterial species within the Actinobacteria phylum. Our findings have important translational significance, since manipulation of the intestinal flora may significantly influence the total body BH4 content, and this may be therapeutically useful in cases of BH4 insufficiency.   each pterin analytical standard and stable isotope were prepared as 1 mmol/L in water containing 0.2% dithiothreitol (DTT) and aliquots were stored at − 80 °C. All other chemicals and reagents were obtained from Sigma Aldrich (Oakville, ON, Canada).

Animals. All procedures were conducted in agreement with the Canadian Animals for Research Act (1990)
Canadian Council on Animal Care (CCAC) regulations, and the study protocol was approved by the Hospital for Sick Children's Animal Care Committee. Adult hph-1 mice were bred in-house and genotyped to confirm homozygous, dominantly-inherited GTPCH1 gene deficiency (data not shown). C57Bl/6 mice (Charles River, ON, Canada) were utilized as wild type controls, since this is the background of the hph-1 mice utilized in this study.
All animals were fed regular rodent pellets (Ren's Feed & Supply Ltd. Aberfoyle, ON, Canada) and housed under standard lighting and temperature conditions. Newborn (< 8 days of age) and adult (> 60 days old) wild-type and hph-1 mice of both sexes were studied. The animals were killed through cervical dislocation (newborn), or pentobarbital sodium (60 mg/kg ip -adult) and tissue from several organs was quickly excised, snap-frozen in liquid nitrogen and stored for later processing. The large bowel was isolated for fecal material collection and subsequently snap frozen for further processing.
Actinobacteria culture. For assessment of PTPS-2 gene presence among Actinobacteria, selected Actinobacteria strains (all originally isolated from human sources) were cultured at 37 °C on Fastidious Anaerobe Agar (FAA, Acumedia, Lansing, MI) supplemented with 5% (v/v) defibrinated sheep's blood (Hemostat Laboratories, Dixon, CA). All incubations were carried out anaerobically, except for NEC1 FAA aer, 22-5-S 1 D5 FAA aer, 32-6-I 1 BHI aer and NEC1 5 TSA aer, which were cultured in air. For each strain, isolated colonies were selected, resuspended in Tris-EDTA, and subjected to DNA extraction. Briefly, cells were broken open by first incubating each sample with 0.2 mg proteinase K and 0.5 mg lysozyme (Sigma Aldrich) for 1 hr at 37 °C, bead-beating with glass beads at 3000 rpm for 4 minutes, and then heating to 90 °C for 10 minutes. Broken cells were then subjected to DNA extraction using the Promega Maxwell 16 instrument according to manufacturer's instructions. Extracted, purified gDNA was subjected to real-time q-PCR analysis as described below.
Tissue and bacteria pellet BH4 analysis. Determination of BH4 in tissue and bacterial pellets was performed by LC-MS/MS as previously described 35 with modifications to sample preparation. Briefly, analysis was performed on an AB Sciex 5500QTRAP mass spectrometer (Foster City, CA, USA) coupled with a Shimadzu Nexera ultrahigh pressure liquid chromatograph system (Kyoto, Japan). Pterins were separated by a binary gradient using reversed-phase HPLC on an EZfaast 250 × 2 mm 4 μ m AAA-MS column, with a 4 × 2 mm Security Guard column. A calibration curve was prepared in water containing 0.2% dithiothreitol (DTT) (Sigma Aldrich, Oakville, ON) over the range of 25-1600 nmol/L for BH4. A deproteinization solution containing internal standards for 15 N-BH4 was prepared in 0.1 M perchloric acid (Sigma Aldrich) containing 0.2% DTT at a final concentration of 1000 nmol/L each.
Tissue sample preparation involved deproteinizing at a 1:5 or 1:10 dilution with deproteinization solution and homogenizing with pestle using an overhead stirrer. Following deproteinization the tissue sample was centrifuged at 14800 rpm at 4 °C for 10 minutes. 30 μ l of supernatant was combined with 120 μ l of water containing 0.2% DTT. Processed supernatants were transferred to a microtiter plate and 10 μ L was injected for analysis.
Prepared cell pellets were separately resuspended in 100 μ L of 10 mM Tris-HCl, pH 8.0, 1 mM EDTA. After sonication (1 minute), each homogenate was separately mixed with an equal volume of acidic iodine solution (2% KI, 1% I 2 (w/v) in 1 N HCl). After vortexing, the mixture was left in the dark for 1 hour at room temperature and then centrifuged at 20,000 g for 15 minutes at 4 °C. The supernatants were mixed with one-tenth volume of 5% (w/v) ascorbic acid to reduce excess iodine and assayed.
For quantification, expression of the target gene was normalized to the expressed bacterial 16S rRNA, that was amplified using the following primers: 16S rRNA-Forward, AGAGTTTGATCCTGGCTCAG, and 16S rRNA-Reverse 36 . Colonic content wet-dry weight ratios were obtained for further normalization 37 .

Identification of intestinal microbiota capable of generating BH4. Fecal microbiota species
expressing PTPS-2 were identified by utilizing two defined microbial ecosystems. These defined ecosystems, MET-1 and MET-2, were each simplified consortia of approximately 30 microbial strains each, isolated from healthy human stool samples (1 ecosystem per individual), and were cultured in single-stage chemostats set to mimic the conditions of the distal colon 38 ; briefly, a temperature of 37 °C, pH 7, and retention time of 24 hrs, using a growth medium rich in insoluble fibre and mucin 39 . The bacterial species that comprise MET-1 are described by Petrof et al. 15 , and those that comprise MET-2 are described by Yen et al. 14 . The presence of PTPS-2 in each community was determined, and those ecosystems positive for PTPS-2 expression were further examined by qPCR of their individual components to identify the specific bacterial strains.
For the determination of biopterin generation by specific Actinobacteria spp. strains, each strain was separately grown on FAA with 5% (v/v) defibrinated sheep's blood as above for 3 days to obtain biomass to inoculate broth cultures for expansion of biomass for experiments. M. schleiferi 22-5-I 1_FAA_NB_aer was grown in trypticase soy broth (EMD Biosciences, Etobicoke, ON) supplemented with hemin and menadione, whereas A. equolifaciens 22-5-I 11_TSAB was grown in Wilkins-Chalgren broth supplemented with 0.3 g/L Cysteine HCl. Both strains were cultured for 3 days at 37 °C under anaerobic conditions (N 2 :CO 2 :H 2 , 90:5:5) in a Concept 400 anaerobe chamber (Ruskinn, UK), and the resulting culture was briefly centrifuged to pellet the bacterial cells.
The bacterial pellets were separately resuspended in RNAlater ® Stabilization Solution (ThermoFisher Scientific, Burlington, ON, Canada) and stored at − 80 °C until further processing.
Prepared cell pellets were separately resuspended in 100 μ L of 10 mM Tris-HCl, pH 8.0, 1 mM EDTA. After sonication (1 minute), each homogenate was separately mixed with an equal volume of acidic iodine solution (2% KI, 1% I 2 (w/v) in 1 N HCl). After vortexing, the mixture was left in the dark for 1 hour at room temperature and then centrifuged at 20,000 g for 15 minutes at 4 °C. The supernatants were mixed with one-tenth volume of 5% (w/v) ascorbic acid to reduce excess iodine, and assayed by HPLC using an Ultimate 3000 Dionex system (ThermoFisher Scientific, Oakville, ON, Canada) equipped with a Kinetex ™ 5 μ m C18 100 Å, LC Column 150 × 4.6 mm (Phenomenex) and a fluorescence detector (Dionex RF 200 Fluorescence Detector). Biopterin was eluted with 10 mM potassium phosphate buffer (pH 6.0) at a flow rate of 0.7 mL/minute and monitored at excitation and emission wavelengths of 350 and 450 nm, respectively utilizing a commercially available standard (L-biopterin; Cedarlane, Burlington, ON, Canada). The HPLC data was acquired and processed using Chromeleon version 6.80 software (ThermoFisher Scientific, Burlington, ON, Canada).
Statistical methods. Data were first evaluated to determine Gaussian distribution by Skewness, Kurtosis and Omnibus testing to confirm normal distribution. Data were analyzed by unpaired Student's t-test. Statistical significance was determined at P < 0.05. All statistical analyses were performed with the Number Cruncher Statistical System software (NCSS, Kaysville, Utah, USA). Data are presented as means ± SEM.