Journal of Neurogastroenterology and Motility 2019; 25(3): 413-422  https://doi.org/10.5056/jnm19036
Effects of Intraduodenal Infusion of the Bitter Tastant, Quinine, on Antropyloroduodenal Motility, Plasma Cholecystokinin, and Energy Intake in Healthy Men
Vida Bitarafan,1 Penelope C E Fitzgerald,1 Tanya J Little,1 Wolfgang Meyerhof,2 Tongzhi Wu,1,3 Michael Horowitz,1,3 and Christine Feinle-Bisset1*
1Adelaide Medical School and National Health and Medical Research Council of Australia (NHMRC) Centre of Research Excellence in Translating Nutritional Science to Good Health, University of Adelaide, Adelaide, Australia; 2Center for Integrative Physiology and Molecular Medicine, Saarland University, Homburg, Germany; and 3Endocrine and Metabolic Unit, Royal Adelaide Hospital, Adelaide, Australia
Correspondence to: Christine Feinle-Bisset, PhD
Adelaide Medical School, Faculty of Health and Medical Sciences, University of Adelaide, Adelaide SA 5005, Australia
Tel: +61-8-8313-6053, Fax: +61-8-8313-7794, E-mail: christine.feinle@adelaide.edu.au
Received: February 14, 2019; Revised: March 22, 2019; Accepted: April 7, 2019; Published online: July 1, 2019.
© The Korean Society of Neurogastroenterology and Motility. All rights reserved.

cc This is an Open Access article distributed under the terms of the Creative Commons Attribution Non-Commercial License (http://creativecommons.org/licenses/by-nc/4.0) which permits unrestricted non-commercial use, distribution, and reproduction in any medium, provided the original work is properly cited.
Abstract

Background/Aims

Nutrient-induced gut hormone release (eg, cholecystokinin [CCK]) and the modulation of gut motility (particularly pyloric stimulation) contribute to the regulation of acute energy intake. Non-caloric bitter compounds, including quinine, have recently been shown in cell-line and animal studies to stimulate the release of gastrointestinal hormones by activating bitter taste receptors expressed throughout the gastrointestinal tract, and thus, may potentially suppress energy intake without providing additional calories. This study aims to evaluate the effects of intraduodenally administered quinine on antropyloroduodenal pressures, plasma CCK and energy intake.

Methods

Fourteen healthy, lean men (25 ± 5 years; BMI: 22.5 ± 2.0 kg/m2) received on 4 separate occasions, in randomized, double-blind fashion, 60-minute intraduodenal infusions of quinine hydrochloride at doses totaling 37.5 mg (“Q37.5”), 75 mg (“Q75”) or 225 mg (“Q225”), or control (all 300 mOsmol). Antropyloroduodenal pressures (high-resolution manometry), plasma CCK (radioimmunoassay), and appetite perceptions/gastrointestinal symptoms (visual analog questionnaires) were measured. Ad libitum energy intake (buffet-meal) was quantified immediately post-infusion. Oral quinine taste-thresholds were assessed on a separate occasion using 3-alternative forced-choice procedure.

Results

All participants detected quinine orally (detection-threshold: 0.19 ± 0.07 mmol/L). Intraduodenal quinine did not affect antral, pyloric or duodenal pressures, plasma CCK (pmol/L [peak]; control: 3.6 ± 0.4, Q37.5: 3.6 ± 0.4, Q75: 3.7 ± 0.3, Q225: 3.9 ± 0.4), appetite perceptions, gastrointestinal symptoms or energy intake (kcal; control: 1088 ± 90, Q37.5: 1057 ± 69, Q75: 1029 ±70, Q225: 1077 ± 88).

Conclusion

Quinine, administered intraduodenally over 60 minutes, even at moderately high doses, but low infusion rates, does not modulate appetite-related gastrointestinal functions or energy intake.

Keywords: Cholecystokinin; Energy intake; Gastrointestinal hormones; Pylorus; Quinine
Introduction

Dietary nutrients are known to potently modulate gastrointestinal (GI) functions, including gut hormones and motor functions that underlie the slowing of gastric emptying, resulting in reductions in energy intake and blood glucose.13 There is increasing interest in the effects of bitter compounds to stimulate these GI functions by activating subtypes of the taste 2 receptor (TAS2R) family of G protein-coupled receptors expressed on enteroendocrine cells throughout the human GI tract,47 particularly given the potential to suppress energy intake without providing additional calories.

The outcomes of studies in both cell lines and experimental animals suggest potent effects of bitter agonists to modulate gut hormone release.810 For example, denatonium benzoate (DB) and phenylthiocarbamide (PTC) have been reported to stimulate cholecystokinin (CCK) secretion from mouse STC-1 cells8 and DB to stimulate glucagon-like peptide-1 (GLP-1) and peptide YY (PYY) secretion from both human NCI-H716 cells and isolated duodenal tissue from mice.10 Moreover, intragastric DB and PTC, but not quinine hydrochloride (Q-HCl), stimulate the release of ghrelin in mice.9 Interestingly, in the latter study, PTC, but not DB or Q-HCl, slowed gastric emptying, which was unaffected by administration of either the CCK-A receptor antagonist, devazepide, or the GLP-1 antagonist, exendin-(9–39).9 Finally, in mice a mixture of bitter tastants, including Q-HCl, DB, and PTC, increased food intake in the first 30 minutes post-administration, while during the subsequent 4 hours there was a marked suppression of food intake.9 It is, however, important to note that some bitter agonists used in these studies (eg, PTC8), at the doses administered, have, in other studies, induced strong Ca2+ responses in control cells devoid of bitter receptors,11 thus, some of the reported effects may not be specific to bitter receptor activation.

In humans, studies relating to the effects of bitter agonists on gut hormone secretion, GI motility and/or energy intake have yielded inconsistent results and, if any, modest effects.5,6,12,13 Intragastric administration of 18 mg Q-HCl in an acid-resistant capsule, had no effect on absolute plasma CCK concentrations, while the change in plasma CCK relative to baseline was slightly greater 30 minutes after consumption of a standardized meal following quinine compared with control,12 and intraduodenal infusion of a higher dose (75 mg) did not affect plasma CCK, GLP-1, or PYY.5 Intragastric administration of 10 μmol/kg Q-HCl (~250 mg in a 65 kg person) reduced plasma motilin and ghrelin moderately,6 while DB,14 or intraduodenal Q-HCl,12 had no effect on ghrelin. Intragastric administration of DB impaired fundic relaxation4 and decreased antral, but not duodenal, motility,14 while Q-HCl reduced ‘fluctuations in antral motility.’6 Finally, intragastric Q-HCl (18 mg) modestly reduced energy intake12 and, at the much higher dose of ~250 mg, the amount consumed of a palatable chocolate milk shake in healthy women,13 while intraduodenal Q-HCl at an intermediate dose (75 mg) had no effect.5

While these studies provide evidence that some bitter compounds modulate GI functions and energy intake, there are important issues which have not been addressed, including the effects of quinine across a wide range of doses, the relevance of the location of delivery (ie, stomach vs small intestine), and also whether any effects on energy intake are related to those on GI hormone and/or motor functions. The aim of this study was, therefore, to investigate the effects of intraduodenal infusion of a wide range of doses of quinine, given as Q-HCl, on upper GI motor function, gut hormones, appetite perceptions, and energy intake. We chose intraduodenal infusion because it allows delivery in a standardized fashion, without potential confounding influences from the rate of gastric emptying.

Materials and Methods

Participants

Fourteen healthy, lean, young men (mean age: 25 ± 5 years; body mass index [BMI]: 22.5 ± 2.0 kg/m2) participated in the study. Participants were recruited through flyers placed around the Royal Adelaide Hospital and local universities, and classified advertisements placed in local newspapers. Exclusion criteria were smoking, consumption of > 20 g alcohol/day, any medical condition, surgery, or the use of medications known to affect energy intake, appetite, or GI function. All participants were required to be weight-stable (< 5% change in body weight) for at least 3 months before participation, and unrestrained eaters with a score of 12 on the eating-restraint component of the Three-Factor Eating Questionnaire.15 The Central Adelaide Local Health Network Human Research Ethics Committee approved the study protocol (Protocol No. HREC/16/RAH/410), and the study was performed in accordance with the Declaration of Helsinki. Each participant provided informed, written consent before their inclusion. Once a participant was enrolled into the study, they were assigned to a randomized treatment order generated by a research officer who was not involved in the data analysis, using an online tool.16 The study was registered as a clinical trial with the Australian New Zealand Clinical Trial Registry (Trial No. 12617000719336).17

Study Outline

The study evaluated the dose-related effects of 60-minute intraduodenal infusions of Q-HCl delivering either (1) 37.5 mg (“Q37.5”, 0.625 mg/min), (2) 75 mg (“Q75”, 1.25 mg/min) or (3) 225 mg (“Q225”, 3.75 mg/min), or (4) 0.9% saline (“control”), on antropyloroduodenal pressures, plasma CCK, appetite perceptions, GI symptoms and energy intake in healthy men (Fig. 1).

Test Solutions

Q-HCl solutions were prepared by dissolving 0.047 g, 0.094 g or 0.281 g Q-HCl (Sinkona Indonesia Lestari, West Java, Indonesia) and 1.44 g, 1.44 g, or 1.36 g NaCl, respectively, in 150 mL distilled water to achieve the required loads. The control solution contained 1.45 g NaCl in 150 mL distilled water. All solutions were isotonic (300 mOsmol) and administered intraduodenally at a rate of 2 mL/min for 60 minutes. The 2 lower doses of Q-HCl (37.5 mg and 75 mg) were selected based on studies in healthy subjects in which 18–75 mg Q-HCl reportedly stimulated CCK secretion,12 and reduced,12 or had no effect on energy intake.5 The dose of 225 mg was chosen based on recent reports that Q-HCl at ~250 mg reduced the release of both motilin and ghrelin as well as hedonic eating moderately.6,13

Study Protocol

Each participant was studied on 4 occasions, separated by 3–10 days, in a randomized, double-blind fashion. Participants were instructed to refrain from vigorous exercise and alcohol consumption for 24 hours before each study and were provided with a standardized meal (Beef Lasagne; McCain Food, Wendouree, Victoria, Australia; energy content: 602 kcal) to be consumed by 7:00 PM on the night before each visit.

On each study day, the participant arrived at the Clinical Research Facility at the Adelaide Medical School, University of Adelaide, at 8:00 AM after an overnight fast (from food and fluids except water after 7:00 PM, and from water after 6:30 AM). On arrival, an intravenous cannula was placed in a right forearm vein for blood sampling, and the participant was intubated with a small-diameter (external diameter: 3.5 mm), 17-channel manometric catheter (Dentsleeve International, Mui Scientific, Mississauga, Ontario, Canada), which was inserted into the stomach through an anaesthetized nostril and allowed to pass into the duodenum by peristalsis.18 The manometric catheter consisted of 16 side-holes spaced at 1.5 cm intervals, measuring pressures in the antrum, pylorus, and duodenum.19,20 An additional channel was positioned ~14.5 cm distal to the pylorus and used for intraduodenal infusion of Q-HCl or control solutions. The correct positioning of the catheter was maintained by continuous measurement of the transmucosal potential difference between the most distal antral, and the most proximal duodenal, channels.21 Once the catheter was positioned correctly (within 59 ± 4 minutes across study days and participants) and immediately after the occurrence of a phase III of the interdigestive migrating motor complex (time from catheter insertion to the occurrence of phase III (minutes); control: 67 ± 7, Q37.5: 72 ± 11, Q75: 84 ± 16, Q225: 76 ± 14, NS), during phase I (a period of motor quiescence), a baseline blood sample was collected, and the participant completed a visual analogue scale (VAS) questionnaire to assess appetite-related perceptions (hunger, fullness, desire to eat, prospective food consumption), and GI symptoms (nausea, bloating),22 and fasting motility was monitored continuously for 10 minutes (t = −10–0 minutes). At t = 0 minutes, intraduodenal infusion of either Q-HCl or control commenced for 60 minutes. During the infusion, antropyloroduodenal pressures were recorded continuously, while blood samples for measurement of gut hormones and blood glucose were collected, and VAS questionnaires completed every 15 minutes. At t = 60 minutes, the intraduodenal infusion was terminated and the participant extubated. The participant was then presented with a standardized, cold, buffet-style meal and instructed to consume as much, or as little, food as they wished until they felt comfortably full, for up to 30 minutes (t = 60–90 minutes).23 The meal comprised 4 slices (~120 g) of whole-meal bread, 4 slices (~120 g) of white bread, 100 g sliced ham, 100 g sliced chicken, 85 g sliced cheddar cheese, 100 g lettuce, 100 g sliced tomato, 100 g sliced cucumber, 22 g mayonnaise, 20 g margarine, 1 apple (~170 g), 1 banana (~190 g), 175 g strawberry yogurt, 100 g chocolate custard, 120 g fruit salad, 375 mL iced coffee, 300 mL orange juice, and 600 mL water. The buffet meal had a total energy content of ~2300 kcal (~27% fat, ~52% carbohydrate, and ~21% protein) and weight of ~2924.23 At t = 90 minutes, after completion of the meal, a final blood sample was taken, and the VAS completed, and the participant was then allowed to leave the laboratory.

On a separate day, oral taste detection thresholds for Q-HCl were quantified.24

Measurements

Oral quinine taste-thresholds

Detection thresholds for Q-HCl were determined using the ascending series 3-Alternate Forced Choice technique.24 Participants were asked to abstain from food, beverages and oral care products for at least 2 hours prior to the test, and to prevent confounding from non-taste sensory inputs, all tests were conducted while wearing nose clips. Taste samples were prepared by adding Q-HCl at varying concentrations (0.00125, 0.0025, 0.0125, 0.025, 0.075, 0.25, 0.75, 1.5, 3, 7.5, 15, 30, and 75 mmol/L) to distilled water.25 Control samples consisted of distilled water. Samples were prepared fresh on the day of testing. Participants were presented with 3 samples per set, 2 controls and 1 containing Q-HCl, in ascending order from the lowest to the highest concentration. Participants rinsed their mouth with distilled water before beginning the task and between each sample set. In each set, participants were asked to identify the “odd” sample. If incorrect, they were presented with 3 samples at the next higher concentration and, if correct, with 3 more samples at the same concentration. This procedure continued until the participant identified the odd sample at a given concentration 3 consecutive times, and that concentration was defined as their detection threshold for Q-HCl.

Appetite perceptions, gastrointestinal symptoms, and energy intake

Appetite perceptions (including hunger, fullness, desire to eat, and prospective food consumption) were quantified with validated 100-mm VAS questionnaires.22 Nausea and bloating were also assessed. Energy intake (kcal) was calculated from the amount of food and liquids (g) consumed at the buffet meal, measured by weighing each food item before presentation and at the end of the meal, using commercial software (FoodWorks 8.0; Xyris Software, Highgate Hill, Queensland, Australia).23

Antropyloroduodenal motility

Antropyloroduodenal pressures were digitized and recorded using a computer-based system running commercially available software (Solar GI, MMS Data base software, version 8.17; Medical Measurement Systems BV, Enschede, The Netherlands), and stored for subsequent analysis. The number and amplitude of antral, isolated pyloric, and duodenal pressure waves, as well as basal pyloric pressure, using custom-written software modified to our requirements (kindly provided by Professor Emeritus A Smout, University Medical Centre, Amsterdam, The Netherlands), as described previously.26

Plasma cholecystokinin and blood glucose concentrations

Blood samples were collected into ice-chilled ethylenediamine-tetraacetic acid-coated tubes. Plasma was separated by centrifugation at ~1830 g for 15 minutes at 4°C within 15 minutes of collection and stored at −70°C until assayed.

Plasma CCK-8 concentrations (pmol/L) were measured by radioimmunoassay after ethanol extraction using an adaptation of the method of Santangelo et al.27 Intra- and inter-assay coefficients of variation were ~9.2% and 13.7%, respectively. The detection limit was 1 pmol/L.

Blood glucose was determined with a portable glucometer (Medisense Precision QLD; Abbott Laboratories, North Ryde, New South Wales, Australia), and was quantified because of the potential of quinine to cause hypoglycaemia.

Statistical Methods

The number of participants was determined by power calculations based on our previous work.28 We calculated that with 14 participants, we would be able to detect a 15% decrease in energy intake at α = 0.05, with a power of 80%.

Baseline values for all data were calculated as means of values obtained between t = −10 and t = 0 minutes. For antral, isolated pyloric, and duodenal pressure waves, total numbers, and mean amplitudes were calculated over the 60-minute infusion period. Number and amplitude of antral and duodenal pressure waves were used to calculate motility indices (MI) using the following equation: MI (mmHg·number) = natural logarithm {[sum of amplitudes × number of contractions (pressure waves)] + 1}.29 Basal pyloric pressures were averaged over the 60-minute infusion period. Plasma CCK and blood glucose concentrations were measured in duplicate and expressed as means at each time point.

Statistical analyses were performed with SPSS software (version 24.0; IBM Corp, Somers, NY, USA). VAS scores, plasma CCK and blood glucose concentrations were analyzed using repeated-measures 2-way ANOVA, with treatment (Q37.5, Q75, Q225, and control) and time (0–60 minutes) as factors. Sphericity of the time effect for all models was evaluated by Mauchly’s test and, when violated, the adjusted Greenhouse-Geisser P-value was reported. Motility data, energy intake and amount of food and liquids consumed from the test meal were analyzed using one-way ANOVA. Post-hoc comparisons, adjusted for multiple comparisons by Bonferroni’s correction, were performed where ANOVAs revealed significant effects. Comparisons of post-meal (t = 90 minutes) vs pre-meal (t = 60 minutes) CCK and glucose concentrations were done using Student’s paired t test. All data are reported as means ± SEMs. All tests were 2-tailed, and differences were considered statistically significant at P < 0.05.

Results

All subjects completed all 4 study visits and tolerated the experimental procedures well, and detected Q-HCl orally (detection-threshold: 0.19 ± 0.07 mmol/L).

Energy Intake

There was no effect of treatment on energy intake (kcal) or the amount consumed (g) from the buffet meal (Table 1).

Appetite Perceptions and Gastrointestinal Symptoms

There were no differences in baseline ratings, or any effect of treatment or time, on ratings of hunger, desire to eat, prospective food consumption, fullness, nausea, or bloating (Fig. 2A–F).

Antropyloroduodenal Pressures

Baseline values for antral, pyloric or duodenal pressures did not differ between study days, and there was no effect of treatment on the total number, mean amplitude, or MI, of antral or duodenal pressures, basal pyloric pressure or the number or amplitude of isolated pyloric pressure waves (Table 2).

Plasma Cholecystokinin Concentrations

There were no differences in baseline plasma CCK concentrations between study days, and no effect of treatment on plasma CCK. Plasma CCK increased substantially in response to the buffet meal with all treatments (time effect: P < 0.05), with no difference between treatments (Fig. 3A).

Blood Glucose Concentrations

There were no differences in baseline values for blood glucose between study days, and no effect of treatment on blood glucose. In response to the buffet meal, blood glucose increased with all treatments (time effect: P < 0.05), with no difference between treatments (Fig. 3B).

Discussion

Our study indicates that slow intraduodenal administration of quinine over 60 minutes, at the loads used, does not affect the acute antropyloroduodenal motility, plasma CCK or energy intake responses to quinine, and, therefore, at least under these conditions, does not appear to be a potent stimulus for small-intestinal bitter taste receptors to modulate appetite-related GI functions and energy intake.

There has been much interest in characterising the effects of bitter compounds on gut hormone release,810,12 since (1) bitter taste receptors are expressed on enteroendocrine cells in the GI lumen, (2) gut hormones, including CCK, GLP-1, and PYY, mediate the effects of nutrients on GI motor function and gastric emptying, and (3) gut hormones play a critical role in the regulation of appetite and energy intake.3,30 Results from studies in humans have, however, been inconsistent, and effects, if any, appear to be modest.5,6,1214 We were particularly interested in the effect of quinine on CCK, given the findings in preclinical studies of potent CCK release by other bitter substances8 and our previous work in humans demonstrating potent release of CCK by dietary nutrients, associated with marked suppression of energy intake.19,28 In line with the previous studies in humans on the effects of quinine on plasma CCK levels,5,12 we found no effect of even the highest dose of intraduodenal quinine on plasma CCK concentrations. Thus, our data suggest that Q-HCl, administered at a slow rate, is not a potent stimulus for enteroendocrine cells that release CCK.

Previous studies on the effects of bitter compounds on GI motor functions have yielded diverse, and inconsistent, outcomes. For example, in mouse gastric tissue, DB and chloroquine stimulated, while PTC inhibited, antral contractility.4 Moreover, in mice, intragastric gavage of PTC, but not DB or Q-HCl, slowed gastric emptying.9 In humans, intragastric administration of DB has been reported to impair nutrient-induced fundic relaxation4 and decrease antral, but not duodenal, motility, but to have no effect on gastric emptying of a solid meal.14 Intragastric administration of ~250 mg reduced ‘fluctuations in antral motility.’6 We found that intraduodenal infusion of Q-HCl, using a wide range of doses that spanned those used in previous studies of the effects of quinine on gut hormone release, motility, and energy intake,5,6,12 had no effect on antral, pyloric or duodenal pressures, suggesting that quinine, when administered intraduodenally at a slow rate, at the loads used, does not modulate antropyloroduodenal motility in humans. Since CCK potently modulates upper GI motor function,3133 the absence of CCK release in the current study likely explains the lack of effect of Q-HCl on antropyloroduodenal pressures.

In line with the lack of effect of Q-HCl to modulate upper GI motility, particularly pyloric pressures, or stimulate CCK, both of which we have identified as key determinants of the subsequent suppression of energy intake in response to duodenal nutrients,1,34 we found no effect of Q-HCl to reduce appetite or energy intake. In a recent study, DB reduced hunger ratings in the fasting state, and decreased hunger and increased satiety after a meal, but did not significantly reduce caloric intake from a standardized meal, with substantial variability between individuals.14 Moreover, while intragastric administration of 18 mg Q-HCl reduced energy intake in one study12 and, at a much higher dose (~250 mg), modestly reduced the amount consumed of a palatable milk shake in healthy females,13 intraduodenal infusion of 75 mg Q-HCl was ineffective.5 Thus, overall findings are mixed, and more studies are warranted to determine the conditions under which bitter substances, including Q-HCl, stimulate GI functions that underlie the regulation of energy intake, and suppress energy intake.

A key issue with the existing research on the effects of bitter compounds on GI function and energy intake is the substantial variation in outcomes between studies, which is potentially attributable to a number of factors. These include variations in the bitter compounds used and the doses applied, administration of the compounds to cell models vs into the stomach or small intestine of humans or animals, and using either bolus administration or slower infusions over time.46,8,10,1214 There are currently 25 known subtypes of TAS2Rs in humans,35 and different bitter agonists activate different combinations of receptor subtypes, for example, quinine activates 9 subtypes of TAS2Rs, including TAS2R4, 7, 10, 14, 39, 40, 43, 44, and 46, and DB activates 8 subtypes, including TAS2R4, 8, 10, 13, 39, 43, 46, and 47.35 The difference in the subtypes of TAS2Rs that are activated by each bitter compound,35 as well as species differences in TAS2Rs,11 are likely to explain some of the differences in observed effects. Stimulation of the release of gut hormones by bitter compounds depends on the presence of specific bitter receptor subtypes on enteroendocrine cells; evidence of the identity, and functions, of some subtypes on enteroendocrine cells is emerging. For example, a recent study in humans reported that TAS2R38s are expressed on human colonic enteroendocrine cells and are colocalized with immunoreactivity for CCK, GLP-1 or PYY.36 Interestingly, neither quinine nor DB activate the TAS2R38 subtype.35 The regional distribution of bitter receptor subtypes across the stomach, small and large intestines may also vary.37 Thus, much more research is required to better understand the roles and functions of the various bitter receptor subtypes in humans, as well as their specific activation by particular bitter compounds. Inter-individual variations in bitter taste perception that have been documented for oral taste38 may also exist in the gut and, thus, influence the responses to intraluminal bitter compounds. Finally, the GI responses to bitter substances may be influenced by the habitual diet, in analogy to fat,39 with evidence of an inverse relationship between intake of bitter vegetables and the ability to taste the bitter substance, 6-n-propylthiouracil in children;40 furthermore, the ability to taste bitter may also be modified by dietary energy and fat consumption.41,42

Some potential limitations of our study should be recognized. We only studied males, as they have been shown to be more sensitive to dietary manipulations,43 while, in contrast, it has been reported recently14 that females appear to be more sensitive to bitter taste, however, all our volunteers readily detected Q-HCl. Our study evaluated the effects of intraduodenal, rather than intragastric or oral, Q-HCl administration, thus, studies are warranted to elucidate the relative contributions of gastric and oral perception of bitter taste to the regulation of GI functions and appetite. We only analyzed the effects on plasma CCK concentrations, and not other gut hormones, including GLP-1, PYY, or ghrelin, but given that we found no effects on GI motility or energy intake, we believe that any effects on other hormones would be unlikely.

In conclusion, our study establishes that intraduodenal administration of Q-HCl, over a wide range of doses, when infused over a 60-minute period, does not affect antropyloroduodenal pressures, plasma CCK or energy intake. Further studies are warranted that evaluate conditions under which quinine may stimulate bitter receptors to modulate appetite-related GI functions and energy intake, including the effects of varying concentrations of quinine, and the relative effects of oral, intragastric and intraduodenal administration.

Acknowledgements
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We thank Kylie Lange, National Health and Medical Research Council of Australia (NHMRC) Centre of Research Excellence in Translating Nutritional Science to Good Health, The University of Adelaide, a professional biostatistician, for statistical support, and Mr Scott Standfield for performing the biochemical assay for cholecystokinin.

Figures
Fig. 1. Schematic representation of the study design. At t = −10 minutes, immediately after the occurrence of a phase III, ie, during phase I, with the multi-lumen manometric catheter positioned across the pylorus, a baseline blood sample was collected, and the participant completed a visual analogue scale (VAS) questionnaire for the assessment of appetite-related perceptions. The recording of pressures in the antropyloroduodenal region was also commenced. At t = 0 minutes, intraduodenal infusion of quinine hydrochloride at 37.5 mg (Q37.5), 75 mg (Q75), 225 mg (Q225), or control commenced for 60 minutes. During the infusion, antropyloroduodenal pressures were recorded continuously, and blood samples and VAS ratings were collected at 15-minute intervals. At t = 60 minutes, the intraduodenal infusion was terminated, and the catheter removed. The participant was then presented with a buffet-style meal and instructed to eat until he was comfortably full. At t = 90 minutes, another blood sample was collected, and a VAS questionnaire administered, after which the participant was free to leave the laboratory.

Fig. 2. Scores for hunger (A), desire to eat (B), prospective food consumption (C), fullness (D), bloating (E), and nausea (F) during 60-minute intraduodenal infusions (t = 0–60 minutes) of quinine hydrochloride at 37.5 mg (Q37.5), 75 mg (Q75), 225 mg (Q225), or control, and after the buffet meal, at t = 90 minutes. Two-way ANOVAs, with treatment and time as factors, were used to assess differences between treatments. Post-hoc comparisons, adjusted for multiple comparisons by Bonferroni’s correction, were used to determine significant differences between either dose or control. Comparisons of post (t = 90 minutes) vs pre-meal (t = 60 minutes) data were done with Student’s paired t test. Data are expressed as means ± SEMs; n = 14. ID, intraduodenal.

Fig. 3. Plasma cholecystokinin (A) and blood glucose (B) concentrations during 60-minute intraduodenal infusions (t = 0–60 minutes) of quinine hydrochloride at 37.5 mg (Q37.5), 75 mg (Q75), 225 mg (Q225), or control, and after the buffet meal, at t = 90 minutes. Data were analyzed using 2-way ANOVA, with treatment and time as factors. Comparison of post (t = 90 minutes) vs pre-meal (t = 60 minutes) concentrations were done with Student’s paired t test. Data are expressed as means ± SEMs; n = 14. ID, intraduodenal.

Tables

Energy Content and Amount of Food and Liquids Consumed at the Buffet Meal Immediately After 60-minute Intraduodenal Infusions of Quinine Hydrochloride or Control

ParameterCQ37.5Q75Q225P-value
Energy intake (kcal)1088 ± 901057 ± 691029 ± 701077 ± 88NS
Amount consumed (g)1157 ± 901161 ± 841113 ± 761144 ± 98NS

C, saline control; Q37.5, quinine hydrochloride load of 37.5 mg; Q75, quinine hydrochloride load of 75 mg; Q225, quinine hydrochloride load of 225 mg; NS, non-significant.

Data are means ± SEMs (n = 14).

P-values for main treatment effects were determined by one-way ANOVA.


Number, Amplitude, and Motility Index of Antral and Duodenal Pressure Waves, Basal Pyloric Pressure, and Number and Amplitude of Isolated Pyloric Pressure Waves During 60-minute Intraduodenal Infusions of Quinine Hydrochloride or Control

ParameterCQ37.5Q75Q225P-value
Antral pressure waves
 Number39 ± 1327 ± 1137 ± 1229 ± 13NS
 Amplitude (mmHg)29 ± 621 ± 730 ± 543 ± 11NS
 Motility index (mmHg·min)8 ± 16 ± 19 ± 17 ± 1NS
Basal pyloric pressure (mmHg)1 ± 1−2 ± 10 ± 0−1 ± 1NS
Isolated pyloric pressure waves
 Number21 ± 515 ± 322 ± 616 ± 4NS
 Amplitude (mmHg)76 ± 973 ± 1659 ± 851 ± 10NS
Duodenal pressure waves
 Number253 ± 31266 ± 52248 ± 32235 ± 46NS
 Amplitude (mmHg)26 ± 128 ± 224 ± 225 ± 1NS
 Motility index (mmHg·min)14 ± 014 ± 014 ± 014 ± 0NS

C, saline control; Q37.5, quinine hydrochloride load of 37.5 mg; Q75, quinine hydrochloride load of 75 mg; Q225, quinine hydrochloride load of 225 mg; NS, non-significant.

Data are means ± SEMs (n = 14).

P-values for main treatment effects were determined by one-way ANOVA.


Footnotes

Financial support: The authors acknowledge the following sources of funding: International Postgraduate Scholarship provided by the University of Adelaide (2017–20; to Vida Bitarafan), NHMRC Senior Research Fellowship (Grant No. 1103020, 2016–21; to Christine Feinle-Bisset), NHMRC Career Development Award (Grant No. 1022706, 2012–19; to Tanya J Little), Florey Fellowship from the Royal Adelaide Hospital Research Foundation (ID: 9757, 2018–20; to Tongzhi Wu), and NHMRC Project Grant, which funded this research (Grant No. 1078471, 2015–19; to Christine Feinle-Bisset).

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

Author contributions: Christine Feinle-Bisset and Tanya J Little contributed to study concept and design; Vida Bitarafan and Penelope C E Fitzgerald conducted experiments; Vida Bitarafan analyzed data; Vida Bitarafan, Tanya J Little, Wolfgang Meyerhof, Tongzhi Wu, Michael Horowitz, and Christine Feinle-Bisset interpreted results of experiments; Vida Bitarafan and Christine Feinle-Bisset drafted manuscript; Vida Bitarafan, Penelope C E Fitzgerald, Tanya J Little, Wolfgang Meyerhof, Tongzhi Wu, Michael Horowitz, and Christine Feinle-Bisset edited and revised manuscript; Vida Bitarafan, Penelope C E Fitzgerald, Tanya J Little Wolfgang Meyerhof, Tongzhi Wu, Michael Horowitz, and Christine Feinle-Bisset approved final version of manuscript; and Christine Feinle-Bisset acquired funding and had overall responsibility for the project.

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