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Article

Oral Temperature and pH Influence Dietary Nitrate Metabolism in Healthy Adults

by
Stuart P. Cocksedge
1,
Adam J. Causer
2,
Paul G. Winyard
3,
Andrew M. Jones
2 and
Stephen J. Bailey
1,*
1
School of Sport, Exercise and Health Sciences, Loughborough University, Loughborough LE11 3TU, UK
2
Sport and Health Sciences, University of Exeter, Exeter EX1 2LU, UK
3
Exeter Medical School, University of Exeter, Exeter EX1 2LU, UK
*
Author to whom correspondence should be addressed.
Nutrients 2023, 15(3), 784; https://doi.org/10.3390/nu15030784
Submission received: 24 December 2022 / Revised: 23 January 2023 / Accepted: 28 January 2023 / Published: 3 February 2023
(This article belongs to the Section Nutrition and Public Health)
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Abstract

:
This study tested the hypothesis that the increases in salivary and plasma [NO2−] after dietary NO3− supplementation would be greater when oral temperature and pH were independently elevated, and increased further when oral temperature and pH were elevated concurrently. Seven healthy males (mean ± SD, age 23 ± 4 years) ingested 70 mL of beetroot juice concentrate (BR, which provided ~6.2 mmol NO3−) during six separate laboratory visits. In a randomised crossover experimental design, salivary and plasma [NO3−] and [NO2−] were assessed at a neutral oral pH with a low (TLo-pHNorm), intermediate (TMid-pHNorm), and high (THi-pHNorm) oral temperature, and when the oral pH was increased at a low (TLo-pHHi), intermediate (TMid-pHHi), and high (THi-pHHi) oral temperature. Compared with the TMid-pHNorm condition (976 ± 388 µM), the mean salivary [NO2−] 1–3 h post BR ingestion was higher in the TMid-pHHi (1855 ± 423 µM), THi-pHNorm (1371 ± 653 µM), THi-pHHi (1792 ± 741 µM), TLo-pHNorm (1495 ± 502 µM), and TLo-pHHi (2013 ± 662 µM) conditions, with salivary [NO2−] also higher at a given oral temperature when the oral pH was increased (p < 0.05). Plasma [NO2−] was higher 3 h post BR ingestion in the TMid-pHHi, THi-pHHi, and TLo-pHHi conditions, but not the TLo-pHNorm and THi-pHNorm conditions, compared with TMid-pHNorm (p < 0.05). Therefore, despite ingesting the same NO3− dose, the increases in salivary [NO2−] varied depending on the temperature and pH of the oral cavity, while the plasma [NO2−] increased independently of oral temperature, but to a greater extent at a higher oral pH.

1. Introduction

The inorganic anions, nitrate (NO3−) and nitrite (NO2−), have historically been considered as adverse carcinogenic agents or to be inert derivatives of nitric oxide (NO) oxidation [1]. However, more recent data indicate that NO3− and NO2− can be recycled back to the multifaceted physiological signalling molecule, NO, and that dietary NO3− supplementation can enhance aspects of health and exercise performance [2,3]. While ~60% of ingested NO3− is excreted in the urine [4], ~25% is extracted from the circulation by the salivary glands [5], via the NO3−/H+ cotransporter, sialin [6]. NO3− is concentrated within, and subsequently excreted by, the salivary glands [7] for subsequent reduction to NO2− by certain taxa of the oral microflora [8,9,10]. NO2−-rich saliva is then swallowed and subsequently reduced to NO and various reactive nitrogen intermediates within the stomach [2,11], but it is also clear that circulating plasma [NO2−] is increased post NO3− supplementation [7,12]. This circulating plasma NO2− can undergo a one-electron reduction to NO, in a reaction catalysed by numerous NO2− reductases [13,14], with improvements in cardiovascular health markers and exercise responses positively associated with oral NO3− reduction and the increase in plasma [NO2−] after NO3− supplementation [13,15,16,17]. Therefore, enhancing dietary NO3− metabolism has the potential to augment NO synthesis and to improve various aspects of human health and function.
There is evidence that mammalian tissues have the capacity to directly reduce NO3− to NO2− via xanthine oxidoreductase [18,19], in addition to NO3− reduction catalysed by the oral microbiome [8,9,10]. However, it has been suggested that humans have a greater proportional dependence on NO3− reduction via the oral microbiome than by xanthine oxidoreductase compared with some other mammals [18]. As such, oral NO3− reduction is integral to NO3− metabolism and its accompanying physiological effects [20]. Indeed, the administration of chlorohexidine-containing mouthwash, which transiently eradicates oral bacteria, essentially abolishes the increases in salivary and plasma [NO2−] and the alterations in vascular function and exercise capacity that ensue after NO3− ingestion [21,22,23,24,25]. There is also evidence that oral NO3− reduction to NO2− is independently influenced by oral pH and environmental temperature. Specifically, oral NO3− reduction is enhanced with increasing the pH, with peak oral NO3− reduction suggested to occur at pH 8 [26,27,28], and by an increase in oral temperature, as inferred by the greater oral NO3− reduction in summer months, compared with autumn or winter months [26,28]. However, oral temperature and pH were not directly determined in these previous studies, and it is unclear whether combining elevated oral temperature and pH elicits an additive effect on oral NO3− reduction. In addition, the extent to which potential changes in oral NO3− reduction with altered oral temperature and pH influences plasma [NO2−] after dietary NO3− supplementation has yet to be investigated. This is important in order to improve our understanding of the factors that can influence dietary NO3− metabolism in healthy humans, with potential implications for the physiological and performance effects afforded by dietary NO3− supplementation.
The purpose of the present study was to assess the independent and combined effects of altering oral temperature and pH on the salivary and plasma [NO2−] after ingesting a fixed NO3− bolus in healthy adults. It was hypothesised that increasing the oral temperature and pH would independently and additively increase the salivary and plasma [NO2−] after dietary NO3− supplementation.

2. Materials and Methods

2.1. Participant Characteristics

Seven males (mean ± SD, age 23 ± 4 years, height 1.79 ± 0.06 m, and body mass 76 ± 11 kg) were recruited from the university student community to participate in this study. All procedures employed in this study were approved by the Institutional Research Ethics Committee. Participants gave their written informed consent to participate prior to the commencement of the study, after the experimental procedures, associated risks, and potential benefits of participation had been explained. Participants were instructed to arrive at each laboratory testing session in a rested state after an overnight fast. As the reduction of NO3− to NO2− in the oral cavity is thwarted by antibacterial mouthwash [23], participants were required to refrain from mouthwash use for the duration of the study. Similarly, as cigarette smokers exhibit impaired salivary NO3− uptake and NO3− metabolism after dietary NO3− supplementation compared with non-smokers, non-smoking participants were recruited to participate in the current study [29]. Each participant was also asked to avoid the consumption of NO3−-rich, iodide-rich [30], and glucosinolate/thiocyante-rich [31] foods for 48 h, and from caffeine and alcohol ingestion 12 and 24 h before each test, respectively. All participants were instructed to maintain their habitual physical activity pattern for the duration of the study, and to avoid strenuous exercise in the 24 h preceding the testing sessions. All tests were performed at the same time of day (±1 h) in an air-conditioned laboratory at 20 °C.

2.2. Experimental Design

Participants were required to report to the laboratory on seven occasions over a 4–7-week period to complete the experimental testing. On the first visit to the laboratory, participants were familiarized with all procedures used in the study, including venous cannulation, saliva sampling, oral temperature assessment, and mouth rinse administration (see below). For the remaining six visits, participants ingested a 70 mL beetroot juice concentrate (BR), which contained ~6.2 mmol NO3−, and the temperature and pH of the oral cavity were manipulated to assess the effect of these variables on dietary NO3− metabolism. Specifically, salivary and plasma [NO3−] and [NO2−] were assessed pre and post BR ingestion in the following experimental conditions: low oral temperature, neutral oral pH (TLo-pHNorm); low oral temperature, high oral pH (TLo-pHHi); intermediate oral temperature, neutral pH (TMid-pHNorm); intermediate oral temperature, high oral pH (TMid-pHHi); high oral temperature, neutral oral pH (THi-pHNorm); and high oral temperature and pH (THi-pHHi). These experimental conditions were administered in a randomized crossover experimental design.

2.3. Data Collection Procedures

Participants arrived at the laboratory in the morning and were provided with a standardized breakfast of 54 g of porridge oats (Oats So Simple, Quaker Oats) prepared with 180 mL of tap water and one 20 g sachet of golden syrup (Lyle’s golden syrup). A cannula (Insyte-W TM Becton-Dickinson, Madrid, Spain) was subsequently inserted into a forearm vein and a baseline blood sample was drawn into a 6 mL lithium-heparin vacutainer (Sarstedt, Leicester, UK). Blood samples were centrifuged at 3500× g and 4 °C for 10 min, within 1 min of collection. The plasma was subsequently extracted and immediately frozen at −80 °C for later analysis of [NO3−] and [NO2−]. The cannula was kept patent through the infusion of 0.9% saline at a rate of 10 mL·h−1 for the duration of the protocol. An unstimulated saliva sample (~1.2 mL) was then obtained and immediately analysed for salivary pH using a SI series pH meter (Sentron, Leek, The Netherlands), which was calibrated prior to each test according to the manufacturer’s instructions. Saliva was subsequently frozen at −80 °C for later analysis of [NO3−] and [NO2−]. Baseline oral cavity temperature was measured for 10 min by placing a temperature probe (Carefusion, IL, USA) under the tongue with a closed mouth and with participants breathing through their nose. Data were captured at 0.33 Hz via a Squirrel SQ2020 Series Data Logger (Grant, Cambridgeshire, UK). Participants then consumed a 70 mL BR bolus, and blood and saliva were sampled hourly for 3 h post BR ingestion and processed as described above.
After BR ingestion, the temperature of the oral cavity was measured for a further 5 min with a closed mouth and nasal breathing in the TempMid-pHNorm and TempMid-pHHi conditions, or with an open mouth with the participants breathing only through the mouth in the TempLo-pHNorm and TempLo-pHHi conditions. In the TempHi-pHNorm and TempHi-pHHi conditions, participants breathed through their nose with a closed mouth and two fleeced, neck hot water bottles containing boiling water were applied anti-parallel. Specifically, the apex of the inferior hot water bottle was in contact with the posterior surface of the neck, with the apex of the superior hot water bottle in contact with the anterior surface of the neck. The superior surface of the upper hot water bottle rested on the submandibular space. In addition, a heated gel pack (Reliance Medical, Cheshire, UK), which was heated for 45 s in a microwave oven, was applied to the left cheek and held in place with an elastic Velcro strap. Participants adopted these respective breathing patterns and mouth positions for 2.5 h. In all tests, participants employed nasal breathing with a closed mouth for the remaining 30 min of the condition. Hot water bottles and gel packs were replaced every 30 min up to 2.5 h to maintain the elevated oral cavity temperature based on the data obtained from pilot testing in the TempHi-pHNorm and TempHi-pHHi conditions. The temperature of the oral cavity was measured for 10 min at 30 min intervals throughout the protocol.
Following oral temperature assessment, participants mouth rinsed with a 30 mL solution for 2 min. Participants were instructed to swallow any saliva in their mouth prior to the mouth rinse, to avoid swallowing the mouth rinse, and to spit the mouth rinse into a beaker when instructed after 2 min had elapsed. In the TempMid-pHNorm, TempHi-pHNorm, and TempLo-pHNorm conditions, participants rinsed with 30 mL tap water (pH 7.3 ± 0.1) while participants rinsed with a 30 mL 4.2 M NaHO3 solution (pH 8.1 ± 0.1) in the TempMid-pHHi, TempHi-pHHi, and TempLo-pHHi conditions. In the TempMid-pHNorm and TempMid-pHHi conditions, mouth rinses were heated to 35.0 ± 1.2 °C in an attempt to maintain oral temperature, whereas mouth rinses were administered at room temperature (20.7 ± 0.1 °C) in the TempLo-pHNorm and TempLo-pHHi conditions in an attempt to lower oral temperature, and heated to 40.4 ± 0.7 °C in an attempt to increase oral temperature in the TempHi-pHNorm and TempHi-pHHi conditions. Mouth rinses were administered every 7.5 min based on pilot testing, which revealed that this provided a mean salivary pH of ~8 over this timeframe in the pHHI conditions. Mouth rinsing ceased 2.5 h post BR ingestion.
Oral temperature at each time point was taken as the mean temperature over the final 5 min of collection, with the overall oral temperature for each experimental condition taken as the mean oral temperature over the first 2.5 h of the protocol. Overall salivary pH was taken as the mean salivary pH at the start of the protocol and 1 and 2 h post BR consumption.

2.4. [NO2−] and [NO3−] Analysis

Salivary and plasma [NO2−] and [NO3−] were analysed as described previously [29,30,31]. Prior to [NO2−] and [NO3−] analysis, all glassware, utensils, and surfaces were rinsed with deionized water to remove residual NO intermediates. Plasma samples were deproteinized using zinc sulfate (ZnSO4)/sodium hydroxide (NaOH) precipitation prior to the determination of [NO3−]. Firstly, 500 μL of 0.18 N NaOH was added to 100 µL of sample followed by 5 min incubation at room temperature. Subsequently, samples were treated with 300 μL aqueous ZnSO4 (5% w/v) and vortexed for 30 s before undergoing an additional 10 min incubation period at room temperature. The samples were then centrifuged at 3500× g for 5 min, and the supernatant was removed for subsequent analysis. The [NO3−] of the deproteinized plasma sample was determined by its reduction to NO in the presence of 0.8 % (w/v) vanadium chloride in 1 M hydrochloric acid within an air-tight purging vessel. Plasma samples were introduced to the vessel via 50 uL injections into the septum at the top of the vessel. The spectral emission of electronically excited nitrogen dioxide, derived from the reaction of NO with ozone, was detected by a thermoelectrically cooled, red-sensitive photomultiplier tube housed in a Sievers gas-phase chemiluminescence nitric oxide analyser (Sievers NOA 280i. Analytix Ltd., Durham, UK). The [NO3−] was determined by plotting the signal (mV) area against a calibration plot of sodium nitrate standards. The [NO2−] of the undiluted (non-deproteinized) plasma was determined by its reduction to NO in the presence of glacial acetic acid and aqueous sodium iodide (4% w/v), with the calibration performed using sodium nitrite standards. Then, 100 uL injections were used for the plasma [NO2−] determination. After thawing at room temperature, the saliva samples were centrifuged for 10 min at 17,000× g and the supernatant was removed for subsequent analysis. The supernatant was diluted 100-fold with deionized water and [NO3−] and [NO2−] were determined from 50 uL injections using the same reagents describe above for the plasma analyses.

2.5. Statistics

A two-way (condition × time) repeated measures ANOVA was employed to determine the independent and combined effects of manipulating oral temperature and pH on salivary and plasma [NO3−] and [NO2−]. A one-way repeated measures ANOVA was employed to determine the effects of oral temperature and pH manipulation on the mean salivary and plasma [NO3−] and [NO2−], oral temperature, and salivary pH across the experimental conditions. Where the analysis revealed a significant main or interaction effect, Fishers Least Significant Difference tests were employed to determine the origin of such effects. All data are presented as mean ± SD, unless otherwise indicated. Statistical significance was accepted when p < 0.05.

3. Results

3.1. Oral Temperature

The oral temperature over the first 2.5 h of the protocol is presented in Figure 1. There was a main effect for the condition on oral temperature (p < 0.01). Oral temperature was higher in the TMid-pHNorm and TMid-pHHi conditions compared with the TLo-pHNorm and TLo-pHHi conditions, and higher in the THi-pHNorm and THi-pHHi conditions compared with the TMid-pHNorm, TMid-pHHi, TLo-pHNorm, and TLo-pHHi conditions (p < 0.01 for all comparisons). The mean oral temperature in the high, intermediate, and low temperature conditions was 36.2 ± 0.3 °C, 34.9 ± 1.2 °C, and 33.6 ± 1.7 °C, respectively.

3.2. Salivary pH

The salivary pH over the first 2 h of the protocol is presented in Figure 1. There was a main effect for condition on salivary pH (p < 0.01). Salivary pH was higher in the TMid-pHHi, THi-pHHi, and TLo-pHHi conditions compared with the TMid-pHNorm, THi-pHNorm, and TLo-pHNorm conditions (p < 0.01 for all comparisons). The mean salivary pH in the high and normal conditions was 7.8 ± 0.2 and 6.7 ± 0.2, respectively.

3.3. Salivary [NO3−]

The salivary [NO3−] at baseline and 1, 2, and 3 h post BR ingestion and the mean salivary [NO3−] 1–3 h post BR ingestion are presented in Figure 2. There was a main effect for time (p < 0.001), with salivary [NO3−] increasing above baseline in all experimental conditions. Salivary [NO3−] was lower in the TMid-pHHi condition compared with the THi-pHNorm, THi-pHHi, and TLo-pHNorm conditions 1 h following BR ingestion (p < 0.05). The mean salivary [NO3−] 1–3 h post BR ingestion was also lower in the TMid-pHHi condition compared with the THi-pHNorm, THi-pHHi, and TLo-pHNorm conditions (p < 0.05).

3.4. Salivary [NO2−]

The salivary [NO2−] at baseline and 1, 2, and 3 h post BR ingestion and the mean salivary [NO2−] 1–3 h post BR ingestion are presented in Figure 3. There were main effects for time (p < 0.001) and condition (p < 0.01), as well as a condition × time interaction effect (p < 0.05), for salivary [NO2−]. Salivary [NO2−] was higher 1 and 2 h post BR ingestion in the TMid-pHHi, THi-pHHi, TLo-pHNorm, and TLo-pHHi conditions compared with the TMid-pHNorm condition (p < 0.05), and higher than the TMid-pHNorm condition in all of the other experimental conditions 3 h post BR ingestion (p < 0.05). There was a main effect for condition on the mean salivary [NO2−] 1–3 h post BR consumption (p < 0.01) with the mean salivary [NO2−] being higher than the TMid-pHNorm (976 ± 388 µM) condition in TMid-pHHi (1855 ± 423 µM) and all other experimental conditions (p < 0.05), higher than the THi-pHNorm (1371 ± 653 µM) condition in the THi-pHHi (1792 ± 741 µM) and TLo-pHHi (2013 ± 662 µM) conditions (p < 0.05), and higher than the TLo-pHNorm (1495 ± 502 µM) condition in the TLo-pHHi condition (p < 0.05).

3.5. Plasma [NO3−]

The plasma [NO3−] at baseline and 1, 2, and 3 h post BR ingestion and the mean plasma [NO3−] 1–3 h post BR ingestion are presented in Figure 4. There was a main effect for time (p < 0.001) with plasma [NO3−] increasing above baseline in all experimental conditions. There were no between-condition differences in the plasma [NO3−] at 1, 2, and 3 h post BR ingestion or the mean plasma [NO3−] 1–3 h post BR ingestion (p > 0.05).

3.6. Plasma [NO2−]

The plasma [NO2−] at baseline and 1, 2, and 3 h post BR ingestion and the mean plasma [NO2−] 1–3 h post BR ingestion are presented in Figure 5. There were main effects for time (p < 0.001) and condition (p < 0.05). The plasma [NO2−] 3 h post BR ingestion was higher than the TMid-pHNorm (179 ± 65 nM) condition in the TMid-pHHi (227 ± 93 nM), THi-pHHi (245 ± 99 nM), and TLo-pHHi (268 ± 110 nM) conditions (p < 0.05), but not the THi-pHNorm (227 ± 73 nM) and TLo-pHNorm (210 ± 87 nM) conditions (p > 0.05). There was a main effect for condition on the mean plasma [NO2−] 1–3 h post BR consumption (p < 0.01) with the mean plasma [NO2−] higher than the TMid-pHNorm (160 ± 34 nM) condition in the THi-pHHi (246 ± 75 nM) condition (p < 0.05), but not the TMid-pHHi (192 ± 89 nM), THi-pHNorm (211 ± 45 nM), TLo-pHNorm (163 ± 51 nM), or TLo-pHHi (220 ± 71 nM) conditions (p > 0.05).

4. Discussion

In the present study, modulating oral cavity temperature and pH influenced oral NO3− reduction, as reflected by the altered salivary [NO2−] after NO3−-rich BR ingestion. Specifically, compared with the standard conditions of oral temperature and pH, elevating or lowering oral temperature and increasing oral pH independently augmented mean salivary [NO2−] after ingesting the same oral NO3− dose. However, the effects of oral temperature and pH were not additive, as the mean salivary [NO2−] after BR ingestion was increased at a given temperature with a higher pH, with no differences between the high pH conditions. Plasma [NO2−] 3 h post NO3− ingestion was not significantly impacted by oral temperature, but was elevated at a given oral temperature when pH was increased, with no difference between the high pH conditions. Therefore, while the observation that mean salivary [NO2−] increased to a greater extent after NO3− ingestion when oral temperature and pH were independently increased is consistent with our first experimental hypothesis, the lack of an additive effect of the increasing oral temperature and pH on salivary and plasma [NO2−] after NO3− ingestion does not support our second experimental hypothesis. These original observations improve our understanding of the factors that can influence dietary NO3− metabolism in humans, and suggest that oral pH appears to have a greater overall influence than oral temperature.
Consistent with numerous previous reports [7,8,15,22,23,24,25,29,30,31], acute NO3− ingestion increased salivary and plasma [NO3−] and [NO2−]. There were no between-condition differences in plasma [NO3−] in the present study. The mean salivary [NO3−] 1–3 h post BR ingestion was lower in the TMid-pHHi condition compared to the THi-pHNorm, THi-pHHi and TLo-pHNorm conditions. The mechanisms for this effect may be linked to the influence of temperature and pH, and the interaction between these variables, on the salivary flow rate [32,33]. In addition, a physiological increase in temperature could have increased the NO3− reductase activity of the oral microbiome, leading to a lower salivary [NO3−] in the THi-pHNorm and THi-pHHi conditions compared with the TMid-pHHi condition. Moreover, the uptake of NO3− into the salivary glands is linked to the content and activity of the NO3−/H+ cotransporter, sialin [6]. The activity of sialin is pH-dependent and increases as extracellular pH declines [6], which could account for the lower salivary [NO3−] in the TMid-pHHi condition compared with the THi-pHNorm and TLo-pHNorm conditions. It is likely that some combination of these factors contributed to the lower salivary [NO3−] post BR ingestion in the TMid-pHHi condition compared with the THi-pHNorm, THi-pHHi, and TLo-pHNorm conditions.
Compared with the TMid-pHNorm condition, the mean salivary [NO2−] 1–3 h post BR ingestion was higher in all of the remaining experimental conditions (TMid-pHHi, THi-pHNorm, THi-pHHi, TLo-pHNorm, and TLo-pHHi). The greater increase in salivary [NO2−] after BR ingestion in the current study in TempHi-pHNorm compared with TempMid-pHNorm is consistent with previous reports of enhanced oral NO3− reduction in the summer compared with the autumn or winter [26,28]. Our findings extend these earlier observations as oral temperature was not directly determined, and other factors that could influence oral NO3− reduction and could have changed between seasons were not assessed in these studies. The increase in salivary [NO2−] after BR when oral temperature is increased is likely to be mediated by an increased rate of oral NO3− reduction by the commensal bacteria at a higher temperature. However, the increase in salivary [NO2−] after BR ingestion in the current study was also greater in TLo-pHNorm compared with TMid-pHNorm. This effect may be linked to an enhanced salivary flow rate and altered salivary composition at a lower temperature [34]. These effects might have enabled greater delivery of the NO3− substrate to the oral NO3− reducing bacteria, as well as other potential molecules transported in the saliva that could aid NO3− reduction to NO2−.
Salivary [NO2−] after BR ingestion was higher in TMid-pHHi compared with TMid-pHNorm. This observation is consistent with previous reports that a more alkaline pH can aid NO3− reduction to NO2− [26,27,28,35]. The mean salivary pH in the TMid-pHHi, THi-pHHi, and TLo-pHHi conditions in the present study was 7.8 ± 0.2 and close to the purported optimal of pH 8 for oral NO3− reduction [26,27,28]. It is now clear that certain genera of the oral microflora, including Actinomyces, Granulicatella, Haemophilus, Neisseria, Prevotella, Rothia, and Veillonella catalyse the reduction of NO3− to NO2− [8,9,10]. There is evidence that acute [36,37] and short-term [10] NO3− supplementation modulates the abundance of some bacterial species, with increases in Neisseria and Rothia and declines in Prevotella and Veillonella having been reported. Moreover, it has been reported that the abundance and/or NO3− reductase activity of some of these bacteria, such as Prevotella, Rothia, and Veillonella is enhanced with a more alkaline pH [35,38], which may account for the higher salivary [NO2−] after BR ingestion when oral pH was elevated in the current study. In addition, it is clear that in more acidic conditions, there is increased protonation of NO2− to nitrous acid, which is subsequently decomposed to NO and other reactive nitrogen intermediates [20]. Indeed, it has been reported that exposing NO3− reducing bacteria to a more acidic pH leads to greater NO2− reduction compared with a more alkaline pH [35]. Therefore, the greater salivary [NO2−] after BR ingestion when oral pH was increased in the current study may be linked to greater oral NO3− reduction, via the increased abundance or NO3− reductase activity of NO3− reducing bacteria, and to a lower decomposition of the synthesised NO2− in the oral cavity. While the increasing oral temperature and pH independently increased the mean salivary [NO2−] after BR ingestion, these effects were not additive or synergistic.
Following acute ingestion of BR, plasma [NO2−] typically peaks after 2.5–3 h, concomitant with peak reductions in blood pressure [12,39]. As such, our discussion of the plasma [NO2−] data is focused on the 3 h time point, which has greater potential physiological relevance compared with the mean plasma [NO2−] 1–3 h post BR ingestion. Although the increasing core temperature via hot water immersion can increase the plasma [NO2−] [40], local heating does not appear to have the same effect [41]. Consistent with this latter observation, local heating (or cooling) of the oral cavity did not impact plasma [NO2−] in the current study after BR ingestion. Conversely, compared with TMid-pHNorm, plasma [NO2−] 3 h post BR ingestion was higher in TMid-pHHi, THi-pHHi, and TLo-pHHi. Therefore, while increasing the oral temperature and pH can independently increase salivary [NO2−] post BR ingestion, the plasma [NO2−] post BR ingestion was not impacted by altering oral temperature but was elevated when increasing the oral pH. Collectively, these data suggest that manipulating the oral pH has a greater overall impact on dietary NO3− metabolism than oral temperature.
The original observations presented in this study improve our understanding of some of the factors that impact dietary NO3− metabolism in healthy adults. As improvements in cardiovascular health markers and exercise responses are positively associated with oral NO3− reduction and the increase in plasma [NO2−] after NO3− supplementation [12,15,16,17], our findings might have implications for the potential for BR supplementation to enhance vascular function and exercise performance. Our findings also have implications for the standardisation of practices in future studies assessing the effects of NO3− supplementation on salivary and plasma [NO2−], as the former can be altered by oral temperature and pH, and the latter can be altered by oral pH. However, it is acknowledged that a major limitation of the current study is the small sample size, such that the preliminary findings presented in this pilot study require more comprehensive investigation in future studies. While participants were instructed to avoid NO3−-rich foods for 48 h prior to the testing sessions, the lack of dietary assessment to evaluate NO3− intake prior to and during the experimental testing is a limitation of the current study. In addition, other aspects of oral physiology, such as salivary flow rate and the composition of the oral microbiome, were not measured and would have provided greater insight into the mechanisms responsible for our observations. Indeed, it is possible that altering the oral pH influenced the salivary flow rate and that nasal breathing with a closed mouth in the higher oral temperature conditions altered the oral cavity oxygen tension, which could have impacted the activity of the oral anaerobic NO3− reducing bacteria. While breathing with an open mouth and only breathing through the mouth successfully lowered oral temperature, this also likely impacted mouth dryness, which could have influenced other aspects of oral physiology, such as the salivary flow rate. Moreover, although the temperature manipulations were effective at eliciting the desired directional modulation of oral temperature within participants, there was pronounced between-participant variability in the changes in oral temperature induced by the oral temperature manipulations in the current study. Therefore, further research is required to evaluate the effect of oral temperature and its interaction with oral pH on dietary NO3− metabolism and its physiological effects. It should also be recognised that while increasing oral pH via mouth rinses may increase salivary and plasma [NO2−] after NO3− supplementation, the consumption of beverages with a high pH has the potential to compromise some of the beneficial responses observed following NO3− supplementation by increasing the gastric pH and altering the formation of reactive nitrogen intermediates in the stomach and their appearance in the plasma. Indeed, it has been reported that while increasing gastric pH had no influence on the plasma [NO2−], this attenuated plasma [S-nitrosothiols] and the lowering of blood pressure after NO3− supplementation [42].

5. Conclusions

The present study indicates that independently increasing or lowering oral temperature or increasing oral pH significantly increased mean salivary [NO2−] after NO3− supplementation. However, the increase in plasma [NO2−] 3 h after NO3− supplementation was not impacted by altering the oral temperature, but was increased when the oral pH was elevated, irrespective of oral temperature. These observations contribute to understanding the factors that can influence dietary NO3− metabolism in healthy humans and highlight the need to standardise oral temperature and pH when assessing salivary [NO2−], and oral pH when assessing plasma [NO2−] in NO3− supplementation studies.

Author Contributions

Conceptualization, all authors; methodology, S.P.C., A.J.C. and S.J.B.; formal analysis, S.P.C. and S.J.B.; data curation, S.P.C. and S.J.B.; writing—original draft preparation, S.P.C. and S.J.B.; writing—review and editing, all authors; visualization, all authors; supervision, A.M.J. and S.J.B. All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

All experimental procedures were approved by the Sport and Health Sciences Ethics Committee at the University of Exeter (151021/B/06).

Informed Consent Statement

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

Data Availability Statement

Data are available from the corresponding author upon reasonable request.

Conflicts of Interest

The authors declare no conflict of interest.

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Figure 1. Oral temperature (upper panel) and salivary pH (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHHi) conditions. The oral temperature data are expressed as the mean responses over the first 2.5 h of the protocol, while the salivary pH data are expressed as the mean responses over the first 2 h of the protocol. The filled bars represent the group mean ± SEM responses. * indicates higher than TLo-pHNorm and TLo-pHHi (p < 0.05). # indicates higher than TMid-pHNorm, TMid-pHHi, TLo-pHNorm and TLo-pHHi (p < 0.05). ¥ indicates higher than TMid-pHNorm, THi-pHNorm, and TLo-pHNorm (p < 0.05).
Figure 1. Oral temperature (upper panel) and salivary pH (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHHi) conditions. The oral temperature data are expressed as the mean responses over the first 2.5 h of the protocol, while the salivary pH data are expressed as the mean responses over the first 2 h of the protocol. The filled bars represent the group mean ± SEM responses. * indicates higher than TLo-pHNorm and TLo-pHHi (p < 0.05). # indicates higher than TMid-pHNorm, TMid-pHHi, TLo-pHNorm and TLo-pHHi (p < 0.05). ¥ indicates higher than TMid-pHNorm, THi-pHNorm, and TLo-pHNorm (p < 0.05).
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Figure 2. Salivary nitrate concentration ([NO3−]) time-course (upper panel) and the mean salivary [NO3−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHLo) conditions. Salivary [NO3−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean salivary [NO3−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHHi lower than THi-pHNorm, THi-pHHi, and TLo-pHNorm (p < 0.05).
Figure 2. Salivary nitrate concentration ([NO3−]) time-course (upper panel) and the mean salivary [NO3−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHLo) conditions. Salivary [NO3−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean salivary [NO3−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHHi lower than THi-pHNorm, THi-pHHi, and TLo-pHNorm (p < 0.05).
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Figure 3. Salivary nitrite concentration ([NO2−]) time-course (upper panel) and the mean salivary [NO2−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHLo) conditions. Salivary [NO2−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean salivary [NO2−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHNorm lower than TMid-pHHi, THi-pHHi, TLo-pHNorm, and TLo-pHHi (p < 0.05). # indicates TMid-pHNorm lower than TMid-pHHi, THi-pHNorm, THi-pHHi, TLo-pHNorm, and TLo-pHHi (p < 0.05). Φ indicates lower than THi-pHHi and TLo-pHHi (p < 0.05). ¥ indicates lower than TLo-pHHi (p < 0.05).
Figure 3. Salivary nitrite concentration ([NO2−]) time-course (upper panel) and the mean salivary [NO2−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature−high pH (TLo-pHLo) conditions. Salivary [NO2−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean salivary [NO2−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHNorm lower than TMid-pHHi, THi-pHHi, TLo-pHNorm, and TLo-pHHi (p < 0.05). # indicates TMid-pHNorm lower than TMid-pHHi, THi-pHNorm, THi-pHHi, TLo-pHNorm, and TLo-pHHi (p < 0.05). Φ indicates lower than THi-pHHi and TLo-pHHi (p < 0.05). ¥ indicates lower than TLo-pHHi (p < 0.05).
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Figure 4. Plasma nitrate concentration ([NO3−]) time-course (upper panel) and the mean plasma [NO3−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−..high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature and pH (TLo-pHLo) conditions. Plasma [NO3−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean plasma [NO3−] at 1–3 h of the protocol (lower panel).
Figure 4. Plasma nitrate concentration ([NO3−]) time-course (upper panel) and the mean plasma [NO3−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−..high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature and pH (TLo-pHLo) conditions. Plasma [NO3−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean plasma [NO3−] at 1–3 h of the protocol (lower panel).
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Figure 5. Plasma nitrite concentration ([NO2−]) time-course (upper panel) and the mean plasma [NO2−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature and pH (TLo-pHLo) conditions. Plasma [NO2−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean plasma [NO2−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHNorm lower than TMid-pHHi, THi-pHHi, and TLo-pHHi (p < 0.05). # indicates lower than THi-pHHi (p < 0.05).
Figure 5. Plasma nitrite concentration ([NO2−]) time-course (upper panel) and the mean plasma [NO2−] at 1–3 h of the protocol (lower panel) after acute nitrate-rich beetroot juice ingestion in intermediate temperature−neutral pH (TMid-pHNorm), intermediate temperature−high pH (TMid-pHHi), high temperature−neutral pH (THi-pHNorm), high temperature and pH (THi-pHHi), low temperature−neutral pH (TLo-pHNorm), and low temperature and pH (TLo-pHLo) conditions. Plasma [NO2−] values across the protocol (upper panel) are expressed as group mean values with error bars omitted for clarity. The filled bars represent the group mean ± SEM responses in each experimental condition for mean plasma [NO2−] at 1–3 h of the protocol (lower panel). * indicates TMid-pHNorm lower than TMid-pHHi, THi-pHHi, and TLo-pHHi (p < 0.05). # indicates lower than THi-pHHi (p < 0.05).
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Cocksedge, S.P.; Causer, A.J.; Winyard, P.G.; Jones, A.M.; Bailey, S.J. Oral Temperature and pH Influence Dietary Nitrate Metabolism in Healthy Adults. Nutrients 2023, 15, 784. https://doi.org/10.3390/nu15030784

AMA Style

Cocksedge SP, Causer AJ, Winyard PG, Jones AM, Bailey SJ. Oral Temperature and pH Influence Dietary Nitrate Metabolism in Healthy Adults. Nutrients. 2023; 15(3):784. https://doi.org/10.3390/nu15030784

Chicago/Turabian Style

Cocksedge, Stuart P., Adam J. Causer, Paul G. Winyard, Andrew M. Jones, and Stephen J. Bailey. 2023. "Oral Temperature and pH Influence Dietary Nitrate Metabolism in Healthy Adults" Nutrients 15, no. 3: 784. https://doi.org/10.3390/nu15030784

APA Style

Cocksedge, S. P., Causer, A. J., Winyard, P. G., Jones, A. M., & Bailey, S. J. (2023). Oral Temperature and pH Influence Dietary Nitrate Metabolism in Healthy Adults. Nutrients, 15(3), 784. https://doi.org/10.3390/nu15030784

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