Next Article in Journal
Functional Analysis of Membrane-Associated Scaffolding Tight Junction (TJ) Proteins in Tumorigenic Characteristics of B16-F10 Mouse Melanoma Cells
Next Article in Special Issue
Does Telotristat Have a Role in Preventing Carcinoid Heart Disease?
Previous Article in Journal
Modulation of Tau Pathology in Alzheimer’s Disease by Dietary Bioactive Compounds
Previous Article in Special Issue
Complement C3-Deficiency-Induced Constipation in FVB/N-C3em1Hlee/Korl Knockout Mice Was Significantly Relieved by Uridine and Liriope platyphylla L. Extracts
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
IJMS
Volume 25
Issue 2
10.3390/ijms25020832
ijms-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Faster Gastrointestinal Transit, Reduced Small Intestinal Smooth Muscle Tone and Dysmotility in the Nlgn3R451C Mouse Model of Autism

by
Suzanne Hosie
1,
Tanya Abo-Shaban
1,
Kevin Mou
1,
Gayathri K. Balasuriya
1,2,
Mitra Mohsenipour
1,
Mohammed U. Alamoudi
1,3,
Rhiannon T. Filippone
4,
Gabrielle T. Belz
5,
Ashley E. Franks
6,
Joel C. Bornstein
7,
Kulmira Nurgali
4,8,9 and
Elisa L. Hill-Yardin
1,7,*
1
School of Health and Biomedical Sciences, STEM College, RMIT University, Melbourne, VIC 3083, Australia
2
Graduate School of Medicine, Kobe University, Kobe 657-8501, Japan
3
Medical Laboratory Technology Department, Faculty of Applied Medical Sciences, Jazan University, Jazan 45142, Saudi Arabia
4
Institute for Health and Sport, Victoria University, Melbourne, VIC 3021, Australia
5
Frazer Institute, The University of Queensland, Brisbane, QLD 4072, Australia
6
Department of Microbiology, Anatomy, Physiology and Pharmacology, School of Life Sciences, La Trobe University, Melbourne, VIC 3083, Australia
7
Department of Anatomy and Physiology, University of Melbourne, Melbourne, VIC 3010, Australia
8
Department of Medicine Western Health, University of Melbourne, Melbourne, VIC 3010, Australia
9
Regenerative Medicine and Stem Cells Program, Australian Institute for Musculoskeletal Science (AIMSS), Melbourne, VIC 3021, Australia
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2024, 25(2), 832; https://doi.org/10.3390/ijms25020832
Submission received: 2 October 2023 / Revised: 18 November 2023 / Accepted: 12 December 2023 / Published: 9 January 2024
(This article belongs to the Special Issue Molecular Research of Gastrointestinal Disease)
Browse Figures
Versions Notes

Abstract

:
Individuals with autism often experience gastrointestinal issues but the cause is unknown. Many gene mutations that modify neuronal synapse function are associated with autism and therefore may impact the enteric nervous system that regulates gastrointestinal function. A missense mutation in the Nlgn3 gene encoding the cell adhesion protein Neuroligin-3 was identified in two brothers with autism who both experienced severe gastrointestinal dysfunction. Mice expressing this mutation (Nlgn3R451C mice) are a well-studied preclinical model of autism and show autism-relevant characteristics, including impaired social interaction and communication, as well as repetitive behaviour. We previously showed colonic dysmotility in response to GABAergic inhibition and increased myenteric neuronal numbers in the small intestine in Nlgn3R451C mice bred on a mixed genetic background. Here, we show that gut dysfunction is a persistent phenotype of the Nlgn3 R451C mutation in mice backcrossed onto a C57BL/6 background. We report that Nlgn3R451C mice show a 30.9% faster gastrointestinal transit (p = 0.0004) in vivo and have 6% longer small intestines (p = 0.04) compared to wild-types due to a reduction in smooth muscle tone. In Nlgn3R451C mice, we observed a decrease in resting jejunal diameter (proximal jejunum: 10.6% decrease, p = 0.02; mid: 9.8%, p = 0.04; distal: 11.5%, p = 0.009) and neurally regulated dysmotility as well as shorter durations of contractile complexes (mid: 25.6% reduction in duration, p = 0.009; distal: 30.5%, p = 0.004) in the ileum. In Nlgn3R451C mouse colons, short contractions were inhibited to a greater extent (57.2% by the GABAA antagonist, gabazine, compared to 40.6% in wild-type mice (p = 0.007). The inhibition of nitric oxide synthesis decreased the frequency of contractile complexes in the jejunum (WT p = 0.0006, Nlgn3R451C p = 0.002), but not the ileum, in both wild-type and Nlgn3R451C mice. These findings demonstrate that changes in enteric nervous system function contribute to gastrointestinal dysmotility in mice expressing the autism-associated R451C missense mutation in the Neuroligin-3 protein.

1. Introduction

Autism spectrum disorder (ASD; autism) is a neurodevelopmental disorder diagnosed based on repetitive or restricted activities and deficits in communication and social behaviour. Together with core diagnostic criteria, individuals with autism often experience a range of comorbidities such as increased anxiety [1], irritability [2], and gastrointestinal issues [3,4,5,6,7,8,9,10].
More than 1000 gene mutations contribute to ASD [11], and many of them affect neuronal synapse function. Mouse models of autism with gene mutations impacting neuronal synapse function show abnormal brain activity [12,13,14,15,16,17,18,19,20,21,22,23]. Several preclinical models of ASD also show disturbances of enteric neural numbers and caecal size, shifts in the microbiome and gut dysfunction [24,25,26,27,28,29,30,31,32,33]. We propose that mice with mutations impacting the neural circuitry of the brain also show changes in the enteric nervous system within the gastrointestinal tract. However, targeted studies that assess the outputs of neural activity in multiple gut regions are needed to understand the role of these autism-associated mutations in the gut.
It is well established that the Neuroligin-3 cell adhesion protein is located at neuronal synapses in the brain [34,35,36]. In the enteric nervous system, its mRNA is expressed in both neurons and glia [37,38]. The R451C missense mutation in the Nlgn3 gene encoding was first identified in two brothers diagnosed with ASD [39]. This mutation is well characterized and causes the substitution of an arginine residue to cysteine at position 451 in the Neuroligin-3 protein [40,41]. Mice expressing this mutation show a range of autism-relevant traits, including impaired social communication and repetitive behaviours [14,16,18,42,43].
We initially identified a robust aggression phenotype in Nlgn3R451C mice bred on a mixed genetic background [42]. To verify if this trait was due to the R451C autism-associated mutation as opposed to confounding environmental factors, we backcrossed mice for more than 10 generations onto C57BL/6 mice and assessed them for the persistence of heightened aggression alongside disruptions in the brain’s synaptic activity in the amygdala [14]. We previously reported gastrointestinal dysfunction in both patients and mice (hybrid Sv129/C57BL/6 background) with the R451C missense mutation in the Nlgn3 gene [24]. Interestingly, we also established that the R451C missense mutation confers a reduction in caecal weight in mice bred on different genetic backgrounds and housed in different environmental conditions [29]. Our recent reports also demonstrate that this mutation causes dysmotility in the caecum [27] and modifies microbial populations in the ileum [44]. These findings suggest that the R451C mutation influences gut function across different environments. However, given that a comprehensive characterization of gut motility in Nlgn3R451C mice bred on a C57BL/6 genetic background has not yet been conducted, there has been a limited capacity for the comparison of these findings with a substantial proportion of the existing literature describing C57BL/6 intestinal physiology.
Here, we assess the gastrointestinal motility patterns of wild-type (WT) and Nlgn3R451C mice. We demonstrate changes in intestinal transit in vivo as well as altered gastrointestinal motility patterns in isolated regions of both the small intestine and colon of C57BL/6 Nlgn3R451C mutant mice.

2. Results

2.1. Faster Gastrointestinal Transit in Nlgn3R451C Mice

Gastrointestinal function was assessed in wild-type and Nlgn3R451C mice using in vivo X-ray imaging. Transit times were compared between Nlgn3R451C (n = 8) and wild-type (WT) mice (n = 7) by examining the time taken for BaSO4 to travel from the stomach to the anus (whole transit time; WTT), the stomach to the caecum (small intestinal transit time; SITT), and the proximal colon to the anus (colonic transit time; CTT) (Figure 1A,B).
The transit of BaSO4 throughout the full length of the gastrointestinal tract was faster in Nlgn3R451C mice compared to wild-types (WT: 152.9 ± 10.4 min, Nlgn3R451C: 105.6 ± 4.58 min, p = 0.0004; Figure 1C). Regional-specific comparisons indicated that transit times were decreased in both the small and large intestine in Nlgn3R451C compared to wild-type mice (SITT WT: 108.6 ± 7.05 min, Nlgn3R451C: 76.88 ± 3.65 min; p = 0.0011; Figure 1D) (CTT WT: 22.86 ± 3.60 min, Nlgn3R451C: 13.75 ± 1.83 min; p = 0.0354, Figure 1E).

2.2. A Reduced Small Intestinal Smooth Muscle Tone in Nlgn3R451C Mice

The small intestinal lengths were compared prior to and after incubation in the smooth muscle relaxant and calcium channel blocker, nicardipine, in 21 wild-type and 24 Nlgn3R451C mice. Initially, compared to wild-types, Nlgn3R451C mice had longer small intestines (WT: 33.2 ± 0.7 cm; Nlgn3R451C: 35.2 ± 0.5 cm p = 0.044; two-way ANOVA test (factors: genotype and nicardipine treatment), Sidak correction) (Figure 2A). However, following incubation in nicardipine, although the average length of the small intestine increased for both wild-type and Nlgn3R451C samples, there was no difference in the gut length between genotypes (WT: 36.9 ± 0.5 cm, Nlgn3R451C: 37.5 ± 0.6 cm; p = 0.78; two-way ANOVA test, Sidak correction). These findings suggest that Nlgn3R451C mice have a reduced small intestinal smooth muscle tone compared to wild-types.
Colon lengths were measured from 21 wild-type and 28 Nlgn3R451C mice. Similarly to the observations in the small intestine, Nlgn3R451C mice had longer colons compared to wild-types (WT: 69.5 ± 2.4 mm, Nlgn3R451C: 79.3 ± 2.3 mm; p = 0.014; Student’s t-test) (Figure 2B).

2.3. A Reduced Small Intestinal Resting Diameter and Increased Intra-PCC Frequency in Nlgn3R451C Mice

Although it is well established that the R451C mutation in Neuroligin-3 alters neuronal signalling in the brain, little is known about how this mutation impacts the nervous system of the gastrointestinal tract. To examine the impacts on the enteric nervous system (ENS), ENS-regulated intestinal motility patterns were compared in mutant and wild-type mice. Given that different motility patterns, corresponding with known regional-specific physiological roles, occur along the length of the gut, regions of the mouse small intestine (i.e., the ileum and the jejunum) in addition to the colon were assessed to determine region-specific changes and allow for a topographic assessment of the impact of the mutation along the gut.
Historically, much gastrointestinal motility research has focused on the colon, partly due to the difficulty involved in recording the more complex and seemingly irregular motility patterns in the small intestine. The measurement of motility patterns in the small intestine was pioneered in the guinea pig (reviewed in Costa et al., 2021 [45]) using video-imaging techniques [46]. These methods have been translated for utilization in mouse tissue preparations, allowing consistent motility patterns to be recorded and compared in the jejunum of BALB/c and C57BL/6 mice [47]. Alternative methods, such as the utilization of pressure transducers to measure gut contractility, have also been used in the small intestine of mice and have enabled the comparison of motility patterns in the ileum, jejunum and along the entire gastrointestinal tract [48,49,50].
In this study, we have built on previous video imaging of the gut motility experiments to record from small intestinal regions of the mouse gastrointestinal tract. Specifically, we identified that increasing luminal pressure above our previously reported colonic recording settings [24,51] enabled consistent recordings of propagating contractile complexes (PCCs) in the mouse jejunum and ileum. In our experimental set up for small intestinal samples, a luminal pressure of 6–6.5 cm H2O provided increased consistency in the recorded small intestinal contractile patterns compared to a pressure of approximately 2–3 cm of H2O, which is routinely used for colon preparations [51,52,53]. We identified that the level of applied intraluminal pressure is a critical element for the successful recordings of small intestinal motility patterns. This approach, combined with the development of enhanced edge detection software for analysis of the rodent gut contractions in ex vivo preparations [54], enabled a more accurate comparison of motility parameters across experimental groups.
Here, we used the ex vivo organ bath video-imaging technique [53] to assess motility (i.e., PCCs) in the mouse jejunum and ileum (Figure 3). From the spatiotemporal maps generated, the frequency, quiescence, and velocity of PCCs along the gut segments were compared between wild-type and Nlgn3R451C mice. These comparisons revealed no differences in PCC frequency or velocity between the wild-type and Nlgn3R451C jejunum or the ileum. PCC duration was measured at proximal, mid and distal jejunal locations and revealed no differences between genotypes (Figure 4A,B). In the ileum, however, the PCC duration was shorter and a corresponding increase in quiescence was also identified in Nlgn3 R451C mice (Figure 4E,F, Table 1).
To characterise motility patterns in small intestines from wild-type and Nlgn3R451C mice, we used the enhanced edge detection interface in MATLAB (GutMap, available on request Abo-Shaban et al., 2023 [54]). Specifically, we selected three anatomical locations (proximal, mid and distal) in each small intestinal preparation and measured changes in the gut width over a 15 min recording duration. In Nlgn3R451C mice, the jejunal resting diameter was consistently smaller than in wild-type mice (Table 2, Figure 4C). In contrast, when the jejunal constricted diameter was compared between wild-type and Nlgn3R451C mice, no difference was observed (Table 2). In the ileum, cross-sectional analysis revealed no genotype difference in either the resting or constricted diameter (Figure 4G, Table 2).
A power spectrum analysis of the contraction diameter over time enabled the calculation of intra PCC frequency (i.e., the frequency of contractions within a PCC). In the jejunum, intra PCC frequencies measured at the proximal, mid and distal jejunal cross sections were higher in Nlgn3R451C mice compared to wild-types (Table 2, Figure 4D). We observed similar intra PCC frequencies in the ileum in Nlgn3R451C and wild-type mice (Table 2, Figure 4H).
Several neurophysiological studies in mice expressing the R451C mutation have focused on GABA neurotransmission, given its major role as an inhibitory neurotransmitter in the brain. A common finding of these studies is that Nlgn3R451C mice have altered GABAergic neurotransmission in various brain regions [12,18,20]. Therefore, we previously assessed for potential changes in the GABAergic system in the ENS and identified an increased sensitivity of colonic activity to gabazine (a GABAA receptor inhibitor) in Nlgn3R451C compared to wild-type mice [24]. Within the mouse gastrointestinal tract, the colon expresses significant levels of GABA receptors [55,56]; therefore, this experimental approach seemed appropriate for the colon. In the mouse small intestine, however, the contribution of GABAergic activity to gut function is relatively minor, the expression of GABA receptors is minimal and GABA acts as an excitatory neurotransmitter on enteric neurons [55]. In contrast with the CNS, inhibitory signalling in the intestine occurs at neuromuscular junctions, and is predominantly exerted via nitric oxide in the ENS. In this study, we therefore elected to modulate nitric oxide production and measure small intestinal activity using the video-imaging organ bath assay approach. To inhibit nitric oxide production, we incubated jejunal and ileal segments of the small intestine in the nitric oxide synthase inhibitor, N-nitro-L-arginine (NOLA) and performed video imaging of motility patterns.
In the jejunum, PCC motility patterns were modified in the presence of NOLA (Figure 5A). Specifically, an increase in contractile activity resulted in PCCs being no longer distinguishable in 11 out of 17 of the wild-type and 9 out of 16 of the Nlgn3R451C gut segments. On average, NOLA reduced the number of defined PCCs per 15 min in the jejunum in both WT and Nlgn3R451C (WT (control): 6.3 ± 0.4, WT (NOLA): 2.7 ± 0.8; p = 0.0006; Nlgn3R451C (control): 6.3 ± 0.4, Nlgn3R451C (NOLA): 3.0 ± 0.7 PCCs; mean ± SEM, p = 0.002 (two-way ANOVA (factors: genotype and NOLA effect), Sidak correction); Figure 5A,C,E). In contrast, NOLA had no significant effect on ileal PCC frequency per 15 min (WT (control): 7.2 ± 0.3, WT (NOLA): 7.5 ± 0.7; p = 0.94, Nlgn3R451C (control): 7.2 ± 0.3, Nlgn3R451C (NOLA): 7.2 ± 1 PCCs; mean ± SEM, p > 0.99). In addition, NOLA did not alter ileal PCC velocity (WT (control): 0.4 ± 0.1, Nlgn3R451C: (control): 0.4 ± 0.06; p = 0.9, WT (NOLA): −0.1 ± 0.05, Nlgn3R451C (NOLA): −0.13 ± 0.1 mm/s mean ± SEM, p = 0.9) or duration. There were no changes in PCC duration in the proximal ileum under baseline conditions (WT (control): 74.1 ± 5.7, Nlgn3R451C (control): 58.5 ± 4 s p = 0.09, mean ± SEM).
However, upon NOLA application in the same group of mice, in Nlgn3R451C mice, the PCC clusters were distinguishable and retained the form seen in baseline heatmaps, whereas WT PCCs were disrupted. During NOLA application, in Nlgn3R451C mice, the PCC duration in the proximal ileum increased (WT (NOLA): 3.4 ± 0.1, Nlgn3R451C (NOLA): 24.8 ± 5 s p < 0.0001, mean ± SEM). In contrast, in the mid and distal regions of the ileum, the PCC duration decreased (mid ileal region: WT (control): 85.2 ± 6, Nlgn3R451C (control): 63.4 ± 4 s p = 0.009; distal ileum region WT (control): 88.3 ± 6, Nlgn3R451C (control): 61.4 ± 6.5 s p = 0.004, mean ± SEM). However, following the super-fusion of NOLA, the PCC duration increased in the mid region only (mid ileum region: WT (NOLA): 3.2 ± 0.09, Nlgn3R451C (NOLA): 28.0 ± 4 s p < 0.0001). There was no genotype difference in the PCC duration in the distal ileum region during NOLA application (WT (NOLA): 3.5 ± 3, Nlgn3R451C (NOLA): 10.8 ± 6 s p = 0.3, mean ± SEM) (Figure 5B,D,F).

2.4. The Increased Short Colonic Contractions in Nlgn3R451C Mice

Colonic motility was compared using the ex vivo organ bath video-imaging technique in 17 wild-type and 14 Nlgn3R451C mice. Previous findings examining colonic motility in Nlgn3R451C mice bred on a mixed-background strain showed a decrease in the frequency of colonic migrating motor complexes (CMMCs) in the presence of the GABAA receptor antagonists, gabazine and bicuculline [24]. Our previous study [24] showed that the decrease in CMMC frequency was more pronounced in response to gabazine. Therefore, to tease out potential differences in motility patterns in WT and Nlgn3R451C C57BL/6 colons, we similarly applied gabazine to the organ bath. For these experiments examining colonic motility, gabazine was utilised as opposed to NOLA to determine if findings in the brain were replicated to some extent in the ENS. In addition, as outlined previously, the mouse colon is a more suitable region to test GABAA receptor responses compared to the small intestine due to the greater expression of GABA receptors in the mouse colon compared to the small intestine [57].
The properties of CMMCs in WT and Nlgn3R451C were compared in control conditions and in the presence of the GABAA receptor antagonist, gabazine (Figure 6A,B). Although the mean CMMC frequency per 15 min was higher in Nlgn3R451C under control conditions, this did not reach statistical significance (WT control: 9.4 ± 0.4, Nlgn3R451C control: 10.7 ± 0.4, mean ± SEM, p = 0.07). Gabazine reduced CMMC frequency in both WT and Nlgn3R451C colons; however, this was statistically significant in Nlgn3R451C, but not WT colons (WT control: 9.4 ± 0.4, gabazine: 8.6 ± 0.5, mean ± SEM, p = 0.51; Nlgn3R451C control: 10.7 ± 0.4, gabazine: 8.8 ± 0.3, mean ± SEM, p = 0.03; Figure 6C). There were no differences in resting colon diameter (Figure 6D) or CMMC length (Figure 6E) in control conditions or in the presence of gabazine.
We also measured short anal contractions which are defined as contractions that extend less than 50% of the full length of the colon segment and appear in the distal region of the colon. Under control conditions, WT and Nlgn3R451C colons displayed similar short anal contraction frequencies (control WT: 13.6 ± 0.9, Nlgn3R451C: 11.7 ± 1.2, mean ± SEM, p ≥ 0.99). In the presence of gabazine, the short contraction frequency was reduced in both WT and Nlgn3R451C colons. Although Nlgn3R451C mice had fewer short anal contractions compared to WT, this was not statistically different (gabazine WT: 8.1 ± 0.9, gabazine Nlgn3R451C: 5.0 ± 1.0, mean ± SEM, p = 0.64; Figure 6F). When analysing the number of short contractions as a percentage of total colonic contractions, Nlgn3R451C mice had a lower percentage of short anal contractions compared to WT (gabazine WT: 48.2% ± 3.9, gabazine Nlgn3R451C: 32.1% ± 5.2, mean ± SEM, p = 0.016).

3. Discussion

Here, we confirm that C57BL/6 mice with the R451C mutation share a similar phenotype consisting of faster gastrointestinal transit and increased sensitivity to the GABAA receptor antagonist, gabazine, as previously reported in Nlgn3R451C mixed-background mice. In this study, we additionally examined whole gut transit, smooth muscle tone and intestinal motility patterns in the ileum, jejunum and colon of wild-type and Nlgn3R451C mice.
We observed faster full-length gastrointestinal transit in Nlgn3R451C mice. Transit times were also reduced in the small intestine and colon, suggesting that the impact of the R451C mutation on gastrointestinal transit is not restricted to a specific gut region. Notably, children with ASD are seven times more likely to have diarrhoea than neurotypical children [58]; therefore a reduction in transit time in this mouse model may provide a clinically relevant tool for future mechanistic analyses. Our previous findings in Nlgn3R451C mice examined animals bred on a mixed genetic background and showed faster transit in the small intestine alongside elevated numbers of nNOS neurons in the jejunum [24]. Interestingly, these findings are in contrast with another report in mice with a faster gastrointestinal transit at day 3 post-treatment with an anti-cancer agent, 5-fluorouracil (5-FU), associated with a reduction in myenteric nNOS neurons but slower gastrointestinal transit at day 14 post-5-FU treatment [59]. A slower gastrointestinal transit time associated with an increased proportion of myenteric nNOS neurons was observed following 14 days of treatment with another chemotherapeutic drug, oxaliplatin [60]. The differential effects on gastrointestinal transit and enteric nNOS neurons might be due to the differences in the mechanisms of action of various compounds, with 5-FU causing intestinal inflammation and oxaliplatin causing direct toxicity. Moreover, morphological and functional changes in other types of enteric neurons could affect gastrointestinal transit, as was observed in irinotecan-treated mice, which had increased intestinal transit and acute secretory diarrhoea at day 3 post-treatment associated with an increased number of cholinergic neurons and fibres [61]. Chronic intestinal inflammation causes an indiscriminate loss of enteric neurons and an increased colonic transit time [62,63,64]. Alterations of intestinal transit might result from the modulation of both extrinsic (sympathetic and parasympathetic) and intrinsic innervation of the gastrointestinal tract, changes in intestinal smooth muscle tone, morphological and functional changes in interstitial cells of Cajal and neuromuscular transmission [65,66]. Previous examples of inflammatory dysfunction that may impact gut motility in preclinical models of ASD include our previous report in which we identified changes in Iba-1 macrophage density and morphology in gut-associated lymphoid tissue in the caecum of Nlgn3R451C mice under control conditions [29]. Further exploration is needed to determine the mechanism underlying the increased transit in Nlgn3R451C mice but given that individuals with ASD often experience alternating constipation and diarrhea, the presence of this clinically relevant phenotype provides a strong rationale for the use of this model to investigate the causes of gastrointestinal symptoms experienced in ASD.
Surprisingly, we found that Nlgn3R451C mice have longer small intestines and colons but that this was abolished in small intestinal preparations following incubation in the muscle relaxant, nicardipine. The identification of longer colons in Nlgn3R451C mice bred on a mixed genetic background under control conditions suggests that muscle tone is similarly reduced across different gut regions and genetic backgrounds. We speculate that Nlgn3R451C mice have a decreased small intestinal longitudinal and circular smooth muscle tone that may contribute to the increased colon length we observed in the mutants. Although the biological mechanism underlying this increased gut length is unknown, the R451C mutation might potentiate the inhibitory role of NO to reduce smooth muscle activity under baseline conditions. It is well established that Neuroligin-3 interacts with the key enzyme for NO production (neuronal nitric oxide synthase; NOS) [67,68,69]. Furthermore, we previously showed an increase in the number of nNOS neurons in the jejunal myenteric plexus of Nlgn3R451C mice [26] which could boost the production of neuronal NO in these mice. To determine if this is the case, further analyses of wild-type and Nlgn3R451C gastrointestinal tissue at the gene and protein expression level are required.
Nlgn3R451C mice have altered small intestinal motility as assessed via ex vivo organ bath assays. We observed that the diameter of the Nlgn3R451C jejunum was more constricted under resting conditions. Given that we observed an increase in small intestinal length in these mice, this elongation (presumably involving longitudinal smooth muscle relaxation) may occur simultaneously with an elevated contraction of the circular smooth muscle [70]. Nlgn3R451C mice also showed an increase in intra PCC frequency in the jejunum. This high frequency component of the spatiotemporal map has previously been identified to oscillate at a similar frequency to slow waves in the jejunum [47,50]. Slow waves are a rhythmical depolarisation of the smooth muscle and are driven by the pacemaker activity of the interstitial cells of Cajal (ICC) [71,72]. The pacemaker ICC are associated with the myenteric plexus and are electrically coupled to each other and to the smooth muscle [73]. In the small intestine, the amplitude of slow waves is not sufficient to trigger smooth muscle action potentials and muscle contraction, therefore an additional neurogenic component is required for typical motility patterning. In Nlgn3R451C mice, the observed increase in intra PCC frequency may be a result of altered synaptic activity in the enteric neuronal pathway that influences slow wave generation, perhaps via the intramuscular population of ICC, which are innervated.
In the Nlgn3R451C mouse ileum, the motility phenotype differed from the jejunum. We found that the quiescent period between ileal PCCs was increased, along with corresponding shorter PCC durations in the proximal, mid and distal regions of the ileum. Potentially, the reduction in the overall PCC/churning time may cause the general flow of gut content to be less inhibited and, therefore, have a reduced/faster transit time. In turn, less PCC/churning time could also subtly influence the rate of the absorption of nutrients and water from the gastrointestinal content in these mice. This aligns with our data showing faster intestinal transit using X-ray imaging. How the R451C mutation influences the duration of PCCs is unclear, although this could involve an imbalance of neurogenic excitation and inhibition in this region of the gastrointestinal tract.
In this study, we compared regional gastrointestinal motility patterns in the small intestine using an enhanced software interface in MATLAB, including a novel edge detection algorithm for the video imaging of gut contractile activity in fresh tissue preparations [54]. Although the development of the software interface and optimization of experimental conditions (including the level of applied pressure to the lumen of the gastrointestinal tissue sample) improved our ability to record and analyse motility patterns in the mouse jejunum and ileum, the interpretation of these complex small intestinal motility patterns continues to be developed. Further investigations are needed to understand how in vivo gastrointestinal transit data correlates with in vitro motility patterns. For example, some of our ex vivo findings (i.e., an increase in intra PCC frequency in the jejunum and a higher speed of PCCs in the ileum) appear to correlate with the faster transit seen in vivo in Nlgn3R451C mice via X-ray imaging, but potential correlations across the preparations for other parameters, such as the observed increase in baseline jejunal constriction in Nlgn3R451C mice, are less straightforward in terms of our understanding of how they contribute to physiological profiles in intact animals.
We found reduced numbers of short contractions occurring in the distal colon of Nlgn3R451C mice in response to the GABAA receptor antagonist, gabazine, suggesting an increased sensitivity or potentially fewer functional GABAA receptors in the Nlgn3R451C mouse colon. Currently, the precise function of distal short contractions in the mouse colon is unknown. Future studies may assist in gaining further insights into their physiological role/s; however, until then they provide a useful comparison tool for colonic motility patterning across mouse models of a range of clinically relevant disorders [74]. The results of the current study support our previous findings in the Nlgn3R451C mouse model bred on a mixed-background strain [24] and provide further evidence for GABAA-mediated colonic dysmotility in mice expressing the R451C mutation in Neuroligin-3. Overall, these findings suggest that GABAA receptors may be involved in mediating the initiation of colonic short contractions.
In all, these findings suggest that the autism-associated R451C missense mutation in the Nlgn3 gene impacts the structure and function of the mouse gastrointestinal tract. The presence of the Neuroligin-3 cell adhesion protein in the brain is well established [12,16,20,23,35,38], and Nlgn3 is also expressed in the mouse gastrointestinal tract [24,44,52]. In fact, we have recently detected Nlgn3 mRNA in most enteric neuronal and glial populations in the mouse ileum [37]. It is possible that the regional differences in motility we observed are caused by different expression levels of Nlgn3 in the jejunum, ileum and colon; however, this remains to be determined.

4. Materials and Methods

4.1. Mice

Nlgn3R451C mixed background (Sv129/ImJ/C57BL/6) mice were initially obtained from The Jackson Laboratory (Bar Harbour, ME, USA), and subsequently backcrossed with C57BL/6 mice for more than 10 generations and maintained on the C57BL/6 genetic background.
Mice used for X-ray imaging experiments were 14 weeks old and imported from the Florey Institute (Parkville, VIC, Australia) to the RMIT Animal Facility (RAF; Bundoora, VIC, Australia). Mice used for measurements of gut length or intestinal motility experiments were aged between 8–14 weeks and euthanized by cervical dislocation. All experimental procedures undertaken on the mice were approved by the RMIT University Animal Ethics Committee (AEC 1727).

4.2. Whole Body X-ray Imaging

The X-ray imaging technique was undertaken as detailed by McQuade et al., 2016 [59]. In brief, prior to X-ray imaging, mice underwent an acclimatization period of 1 week where they were conditioned to oral gavage by having a plastic gavage tip (Instech Laboratories Inc., Plymouth Meeting, PA, USA; 20 ga × 30 mm) inserted at least three times for each animal, with at least 24 h between each conditioning session. Mice were also conditioned for restraint by placing a transparent plastic restraint tube (Terumo Corporation, Tokyo, Japan; 50 mL) into the mouse cages at least 24 h prior to the X-ray experiment.
For the X-ray procedure, 0.2 mL of barium sulphate (BaSO4; X-OPAQUE-HD, 2.5 g/mL) was administered to mice via oral gavage. Mice were then immobilized in the prone position inside a restraint tube and were X-ray imaged using Fujifilm cassettes (24 × 30 cm) and a HiRay Plus Porta610HF X-ray apparatus (JOC Corp, Kanagawa, Japan; 50 kV, 0.3 milliampere-second, 60 ms exposure time). X-rays were captured immediately after administration of BaSO4, every 5 min for the first hour, every 10 min for the second hour, then every 20 min afterwards, until the first faecal pellet containing BaSO4 was expelled. Animals were free to move between X-rays and were closely monitored during and after all procedures. Images were developed via a Fujifilm FCR Capsula XLII and analysed using eFilm 4.0.2 software.
The rate of gastrointestinal transit was measured by inferring the time (in minutes) it took for BaSO4 to reach different regions of the gut. The transit times of interest were from the stomach to the caecum (small intestinal time; SITT), proximal colon to the anus (colonic transit time; CTT), and the stomach to the anus (whole transit time; WTT). Only mice that produced faecal pellets containing BaSO4 as visualised in the X-ray images were included in the study (out of 16 mice, 1 Nlgn3R451C mouse was excluded for not producing pellets in the time frame).

4.3. Gut Length Measurement

The entire gastrointestinal tract was carefully separated from the mesentery and removed from culled adult male WT and Nlgn3R451C mice. Using dissecting scissors, the small intestine from the pylorus to the ileocaecal junction was detached from the stomach and caecum, laid onto a flat surface and measured using a tape measure. A digital image of the tissue was then acquired. To assess the maximal length of the tissue, a proportion of the small intestinal gut preparations were then placed in a glass beaker containing the L-type calcium channel blocker, nicardipine (Sigma-Aldrich, Castle Hill, NSW, Australia) (3 mM) for 20 min. The small intestinal preparations were then removed from the nicardipine solution, re-measured and re-imaged for comparison.
Colons (proximal colon to rectum) from WT and Nlgn3R451C mice were dissected, and the surrounding mesentery was removed. Colon preparations were attached to an organ bath using a small insect pin (Australia Entomology supplies, AUS). Tissue preparations were positioned adjacent to a printed ruler located in the base of the organ bath and a digital image was acquired. Colon lengths were measured using ImageJ Fiji software v2.9.0 and were calibrated according to the ruler measurements.

4.4. Video Imaging Intestinal Motility

Adult male WT and Nlgn3R451C mice (aged 8–14 weeks) were culled by cervical dislocation and the gastrointestinal tract, from the stomach to the rectum, was removed. Jejunal segments measuring approximately 6 cm in length were taken from a position located 5 cm from the stomach. Ileal tissue measuring approximately 5 cm in length was removed from the location of the ileo-caecal junction.
All intestinal motility experiments were carried out using our previously described video-imaging technique approach for recording colonic motility in mice [53]. As previously reported [53], we applied intraluminal pressure to gastrointestinal tissue preparations in the organ bath as measured via the height of the fluid meniscus on the organ bath apparatus. Meniscus height was determined by subtracting the height of the organ bath from the fluid meniscus height of the front pressure outlet tube and the fluid meniscus height of the back pressure outlet tube.
For the duration of the video-imaging experiment, tissue was continuously super-fused with 1x Krebs solution (composition, mM: 118 NaCl, 4.76 KCl, 0.99 NaH2PO4.2H2O, 1.20 MgSO4.7H2O, 2.5 CaCl2.2H2O, 11.1 D-glucose, 25 NaHCO3). Krebs solution was bubbled with carbogen (95% O2 and 5% CO2) (BOC Limited, North Ryde, NSW, Australia), and the temperature of the organ bath was maintained between 33 and 35 °C.
Experimental protocols consisted of an initial equilibration period (2 × 15 min) followed by control recordings (4 × 15 min), during which time the tissue preparations were incubated in Krebs physiological solution. Subsequently, either 100 µM N-nitro-L-arginine (NOLA) (Sigma-Aldrich, Castle Hill, NSW, Australia) or 10 µM gabazine (Sigma-Aldrich, Castle Hill, NSW, Australia) (dissolved in 1× Krebs solution) was infused into the tissue bath and recordings were made for 1 h (4 × 15 min). Finally, a washout period was conducted and recordings were captured (4 × 15 min) during which the super-fusion was replaced with 1x Krebs solution. Reagent details for organ bath perfusion: NaCl (Chem-Supply, SA046-5KG, Gillman SA, Australia); KCl (Ajax Finechem, AJA383-500G, Wollongong, NSW, Australia); NaH2PO4.2H2O (Chem-Supply, SA328-500G); MgSO4.H2O (Chem-Supply, MA048-500G); CaCl2.2H2O (Ajax Finechem, 127-500G); NaHCO3 (Chem-Supply, SA001-5KG); D-Glucose anhydrous (Chem-Supply, GA018-500G).
Gut contractile activity was recorded at a frame rate of 30 Hz using a Logitech camera (Quickcam Pro 9000)mounted above the organ bath. Spatiotemporal heatmaps in the colon and small intestine, respectively, were generated using in-house software (Scribble v2.10 [53]) or the GutMap MATLAB software interface [54]. A subset of these datasets were analyzed using both Scribble v2.10 and GutMap and yielded identical results. The software performed edge detection, converting an image of the gut tissue into a silhouette from which the number of vertical pixels for each horizontal pixel was counted. A spatiotemporal heatmap was generated by plotting the diameter of the small intestine segment as a function of space and time.

4.5. The Measurement of PCC Parameters: Frequency, Duration, Length and Velocity

Small intestinal heatmaps were analysed in MATLAB R2021b using in-house software GutMap. The frequency of propagating contractile clusters (PCCs) was determined by manually counting contractile clusters that propagated in a consistent direction for more than 50% of the gut length segment (Figure 7A). For each PCC, the duration was determined by measuring the time at the start and end of the PCC and subtracting the difference. To ascertain the maximum length of the PCC, measurements were taken from the most proximal and distal regions of the PCC and the difference was calculated (Figure 7B). The PCC velocity was calculated using GutMap software. To measure the rest period between the PCCs (i.e., quiescence), the time duration was measured between the end of the PCC contraction and the start of the next PCC contraction (Figure 7C). Gut width was plotted against time for each of the selected regions and the average resting diameter and constricted diameter were compared for WT and Nlgn3R451C mice (Figure 7D–G).

4.6. Regional PCC Parameters

Within a single PCC, the duration of individual contractions varied along the length of the tissue; therefore, a single PCC was divided into three types of contractions for analysis (i.e., proximal short, full-length and distal short contractions). Proximal short contractions were defined as short contractions which contracted between the proximal and middle region of the small intestinal preparation. Full-length contractions were defined as contractions which propagated the full length of the gut tissue and, lastly, distal short contractions were defined as contractions occurring between the mid region and distal end of the small intestinal preparation. Contraction velocity for each sample was measured using the in-house-created GutMap software v.1.0 as an average value calculated from the velocity of 6 randomly selected contractions.

4.7. Maximum and Minimum Gut Diameter and Slow Wave Frequency

To measure the maximum and minimum diameter of the gut tissue, measurements of gut width were plotted from the spatiotemporal map against time at selected proximal, middle and distal locations (Figure 3A). The same gut measurements were analysed using the Fast Fourier Transform algorithm resulting in a histogram whereby the peak described the most common frequency between contractions. The frequency of the peaks per intra PCC cluster was measured to provide the slow wave frequency (intra PCC frequency) for each of the selected gut regions. The average intra PCC frequency was calculated across tissue replicates.

4.8. Statistical Analyses

Transit times from X-ray imaging experiments were compared using a Student’s unpaired t-test (Mean ± SEM). Small intestinal length measurements were compared using a two-way ANOVA test with Sidak correction (Mean ± SEM), given that there were four groups including WT and Nlgn3R451C samples treated with Nicardipine. Colon lengths and mouse body weights were compared using a Student’s unpaired t-test (Mean ± SEM). PCC frequency, length, velocity, duration, resting diameter and inter PCC frequency were compared using a two-way ANOVA test with Sidak correction. The intra PCC cluster frequency was compared using a Mann–Whitney U test with Holm–Sidak correction. Two-way ANOVA tests were used for datasets comparing genotype and drug effects (i.e., nicardipine and NOLA). CMMC frequency, colon diameter and colon length, as well as short anal contractions were compared using a one-way ANOVA Holm–Sidak multiple comparisons test. All datasets were screened for normality (Shapiro–Wilk test, except for colonic transit data which was tested using the D’Agostino and Pearson test, given that several of these values were identical and Shapiro–Wilk test is inaccurate for multiple identical data points) and analysed accordingly (either ANOVA or t-tests for normal distributions and Mann–Whitney U test for datasets that did not satisfy normality testing) using Prism v9.5.1 software.

5. Conclusions

Our findings indicate that mice expressing an autism-associated mutation in the gene encoding the Neuroligin-3 protein display gut dysfunction. We showed that gastrointestinal transit along the full length of the gut was faster in Nlgn3R451C mice compared to wild-types. Additionally, when the transit times were assessed for multiple gastrointestinal segments in these mice, we consistently found that the transit in each gastrointestinal region was faster in mutant mice. Nlgn3R451C mice have longer small intestines and colons compared to wild-type mice which could indicate an increased relaxation of smooth muscle, potentially resulting from enteric neural dysfunction. In Nlgn3R451C mice, the jejunal resting diameter was more constricted than in wild-types. Nlgn3R451C mice had altered intestinal motility with faster intra PCC frequency in the proximal, mid and distal sections of the jejunum when compared to wild-type mice. In the ileum, PCC durations were shorter and there was a longer quiescence period between PCCs. Additionally, colons from Nlgn3R451C mice showed an increased sensitivity to the GABAA receptor antagonist gabazine.
Characterising the expression profile of Nlgn3 within the enteric nervous system, including within the specific functional subtypes of enteric neurons is crucial to understanding the impact of the R451C mutation on gut function and is an ongoing area of investigation. These findings have potential implications for enhancing our understanding of the underlying causes of GI disorders associated with autism and for identifying therapeutic targets.

Author Contributions

Conceptualization, K.N., J.C.B., A.E.F. and E.L.H.-Y.; methodology, K.M., T.A.-S., R.T.F., J.C.B., E.L.H.-Y., G.K.B. and M.M.; software, T.A.-S. and E.L.H.-Y.; formal analysis, S.H., T.A.-S., K.M. and M.U.A.; investigation, K.M., T.A.-S., M.M. and M.U.A.; resources, E.L.H.-Y. and K.N.; writing S.H., T.A.-S., K.N., J.C.B., G.T.B., A.E.F. and E.L.H.-Y.; supervision, E.L.H.-Y., R.T.F., G.K.B., G.T.B. and S.H.; project administration, E.L.H.-Y.; funding acquisition, E.L.H.-Y. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by Australian Research Council Future Fellowship FT160100126 to E.L.H.-Y. R.T.F. is supported by the Australian National Health and Medical Research Council Project grant GNT1158952 to J.C.B. and K.N.

Institutional Review Board Statement

The animal study protocol was approved by the Ethics Committee of RMIT (AEC 1727).

Data Availability Statement

Data and the MATLAB analysis software interface are available on request.

Conflicts of Interest

E.L.H.-Y. and A.E.F are scientific advisors for Vernx (now Adepa; no part of this study was funded by Vernx/Adepa).

References

  1. White, S.W.; Oswald, D.; Ollendick, T.; Scahill, L. Anxiety in children and adolescents with autism spectrum disorders. Clin. Psychol. Review. 2009, 29, 216–229. [Google Scholar] [CrossRef] [PubMed]
  2. Fitzpatrick, S.E.; Srivorakiat, L.; Wink, L.K.; Pedapati, E.V.; Erickson, C.A. Aggression in autism spectrum disorder: Presentation and treatment options. Neuropsychiatr. Dis. Treat. 2016, 2016, 1525–1538. [Google Scholar] [CrossRef]
  3. McElhanon, B.O.; McCracken, C.; Karpen, S.; Sharp, W.G. Gastrointestinal symptoms in autism spectrum disorder: A meta-analysis. Pediatrics 2014, 133, 872–883. [Google Scholar] [CrossRef] [PubMed]
  4. Margolis, K.G.; Buie, T.M.; Turner, J.B.; Silberman, A.E.; Feldman, J.F.; Murray, K.F.; McSwiggan-Hardin, M.; Levy, J.; Bauman, M.L.; Veenstra-VanderWeele, J.; et al. Development of a brief parent-report screen for common gastrointestinal disorders in autism spectrum disorder. J. Autism Dev. Disord. 2019, 49, 349–362. [Google Scholar] [CrossRef]
  5. Buie, T.; Campbell, D.B.; Fuchs, I.I.I.G.J.; Furuta, G.T.; Levy, J.; VandeWater, J.; Whitaker, A.H.; Atkins, D.; Bauman, M.L.; Beaudet, A.L.; et al. Evaluation, diagnosis, and treatment of gastrointestinal disorders in individuals with ASDs: A consensus report. Pediatrics 2010, 125 (Supp. 1), S1–S8. [Google Scholar] [CrossRef]
  6. Coury, D.L.; Ashwood, P.; Fasano, A.; Fuchs, G.; Geraghty, M.; Kaul, A.; Mawe, G.; Patterson, P.; Jones, N.E. Gastrointestinal conditions in children with autism spectrum disorder: Developing a research agenda. Pediatrics 2012, 130 (Supp. 2), S160–S168. [Google Scholar] [CrossRef]
  7. Kohane, I.S.; McMurry, A.; Weber, G.; MacFadden, D.; Rappaport, L.; Kunkel, L.; Bickel, J.; Wattanasin, N.; Spence, S.; Murphy, S.; et al. The co-morbidity burden of children and young adults with autism spectrum disorders. PLoS ONE 2012, 7, e33224. [Google Scholar] [CrossRef]
  8. De Magistris, L.; Familiari, V.; Pascotto, A.; Sapone, A.; Frolli, A.; Iardino, P.; Carteni, M.; De Rosa, M.; Francavilla, R.; Riegler, G.; et al. Alterations of the intestinal barrier in patients with autism spectrum disorders and in their first-degree relatives. J. Pediatr. Gastroenterol. Nutr. 2010, 51, 418–424. [Google Scholar] [CrossRef]
  9. Needham, B.D.; Adame, M.D.; Serena, G.; Rose, D.R.; Preston, G.M.; Conrad, M.C.; Campbell, A.S.; Donabedian, D.H.; Fasano, A.; Ashwood, P.; et al. Plasma and fecal metabolite profiles in autism spectrum disorder. Biol. Psychiatry 2021, 89, 451–462. [Google Scholar] [CrossRef]
  10. Sharon, G.; Cruz, N.J.; Kang, D.W.; Gandal, M.J.; Wang, B.; Kim, Y.M.; Zink, E.M.; Casey, C.P.; Taylor, B.C.; Lane, C.J.; et al. Human gut microbiota from autism spectrum disorder promote behavioral symptoms in mice. Cell 2019, 177, 1600–1618. [Google Scholar] [CrossRef]
  11. Arpi, M.N.T.; Simpson, T.I. SFARI genes and where to find them; modelling Autism Spectrum Disorder specific gene expression dysregulation with RNA-seq data. Sci. Rep. 2022, 12, 10158. [Google Scholar] [CrossRef] [PubMed]
  12. Etherton, M.; Földy, C.; Sharma, M.; Tabuchi, K.; Liu, X.; Shamloo, M.; Malenka, R.C.; Südhof, T.C. Autism-linked neuroligin-3 R451C mutation differentially alters hippocampal and cortical synaptic function. Proc. Natl. Acad. Sci. USA 2011, 108, 13764–13769. [Google Scholar] [CrossRef] [PubMed]
  13. Guo, B.; Chen, J.; Chen, Q.; Ren, K.; Feng, D.; Mao, H.; Yao, H.; Yang, J.; Liu, H.; Liu, Y. Anterior cingulate cortex dysfunction underlies social deficits in Shank3 mutant mice. Nat. Neurosci. 2019, 22, 1223–1234. [Google Scholar] [CrossRef] [PubMed]
  14. Hosie, S.; Malone, D.T.; Liu, S.; Glass, M.; Adlard, P.A.; Hannan, A.J.; Hill-Yardin, E.L. Altered Amygdala Excitation and CB1 Receptor Modulation of Aggressive Behavior in the Neuroligin-3(R451C) Mouse Model of Autism. Front. Cell Neurosci. 2018, 12, 234. [Google Scholar] [CrossRef]
  15. Peça, J.; Feliciano, C.; Ting, J.T.; Wang, W.; Wells, M.F.; Venkatraman, T.N.; Lascola, C.D.; Fu, Z.; Feng, G. Shank3 mutant mice display autistic-like behaviours and striatal dysfunction. Nature 2011, 472, 437–442. [Google Scholar] [CrossRef]
  16. Rothwell, P.E.; Fuccillo, M.V.; Maxeiner, S.; Hayton, S.J.; Gokce, O.; Lim, B.K.; Fowler, S.C.; Malenka, R.C.; Südhof, T.C. Autism-associated neuroligin-3 mutations commonly impair striatal circuits to boost repetitive behaviors. Cell 2014, 158, 198–212. [Google Scholar] [CrossRef]
  17. Schmeisser, M.J.; Ey, E.; Wegener, S.; Bockmann, J.; Stempel, A.V.; Kuebler, A.; Janssen, A.-L.; Udvardi, P.T.; Shiban, E.; Spilker, C.; et al. Autistic-like behaviours and hyperactivity in mice lacking ProSAP1/Shank2. Nature 2012, 486, 256–260. [Google Scholar] [CrossRef]
  18. Tabuchi, K.; Blundell, J.; Etherton, M.R.; Hammer, R.E.; Liu, X.; Powell, C.M.; Südhof, T.C. A neuroligin-3 mutation implicated in autism increases inhibitory synaptic transmission in mice. Science 2007, 318, 71–76. [Google Scholar] [CrossRef]
  19. Chai, A.P.; Chen, X.F.; Xu, X.S.; Zhang, N.; Li, M.; Li, J.N.; Zhang, L.; Zhang, D.; Zhang, X.; Mao, R.R.; et al. A temporal activity of CA1 neurons underlying short-term memory for social recognition altered in PTEN mouse models of autism spectrum disorder. Front. Cell. Neurosci. 2021, 15, 699315. [Google Scholar] [CrossRef]
  20. Földy, C.; Malenka, R.C.; Südhof, T.C. Autism-associated neuroligin-3 mutations commonly disrupt tonic endocannabinoid signaling. Neuron 2013, 78, 498–509. [Google Scholar] [CrossRef]
  21. Takumi, T.; Tamada, K.; Hatanaka, F.; Nakai, N.; Bolton, P.F. Behavioral neuroscience of autism. Neurosci. Biobehav. Rev. 2020, 110, 60–76. [Google Scholar] [CrossRef] [PubMed]
  22. Jurgensen, S.; Castillo, P.E. Selective dysregulation of hippocampal inhibition in the mouse lacking autism candidate gene CNTNAP2. J. Neurosci. 2015, 35, 14681–14687. [Google Scholar] [CrossRef] [PubMed]
  23. Guang, S.; Pang, N.; Deng, X.; Yang, L.; He, F.; Wu, L.; Chen, C.; Yin, F.; Peng, J. Synaptopathology involved in autism spectrum disorder. Front. Cell. Neurosci. 2018, 12, 470. [Google Scholar] [CrossRef] [PubMed]
  24. Hosie, S.; Ellis, M.; Swaminathan, M.; Ramalhosa, F.; Seger, G.O.; Balasuriya, G.K.; Gillberg, C.; Rastam, M.; Churilov, L.; McKeown, S.J.; et al. Gastrointestinal dysfunction in patients and mice expressing the autism-associated R451C mutation in neuroligin-3. Autism Res. 2019, 12, 1043–1056. [Google Scholar] [CrossRef]
  25. James, D.M.; Davidson, E.A.; Yanes, J.; Moshiree, B.; Dallman, J.E. The Gut-Brain-Microbiome Axis and Its Link to Autism: Emerging Insights and the Potential of Zebrafish Models. Front. Cell Dev. Biol. 2021, 9, 662916. [Google Scholar] [CrossRef]
  26. Lee, C.Y.Q.; Franks, A.E.; Hill-Yardin, E.L. Autism-associated synaptic mutations impact the gut-brain axis in mice. Brain Behav. Immun. 2020, 88, 275–282. [Google Scholar] [CrossRef]
  27. Lee, C.Y.Q.; Balasuriya, G.K.; Herath, M.; Franks, A.E.; Hill-Yardin, E.L. Impaired cecal motility and secretion alongside expansion of gut-associated lymphoid tissue in the Nlgn3(R451C) mouse model of autism. Sci. Rep. 2023, 13, 12687. [Google Scholar] [CrossRef]
  28. Sauer, A.K.; Bockmann, J.; Steinestel, K.; Boeckers, T.M.; Grabrucker, A.M. Altered Intestinal Morphology and Microbiota Composition in the Autism Spectrum Disorders Associated SHANK3 Mouse Model. Int. J. Mol. Sci. 2019, 20, 2134. [Google Scholar] [CrossRef]
  29. Sharna, S.S.; Balasuriya, G.K.; Hosie, S.; Nithianantharajah, J.; Franks, A.E.; Hill-Yardin, E.L. Altered Caecal Neuroimmune Interactions in the Neuroligin-3(R451C) Mouse Model of Autism. Front. Cell Neurosci. 2020, 14, 85. [Google Scholar] [CrossRef]
  30. De Theije, C.G.; Wopereis, H.; Ramadan, M.; van Eijndthoven, T.; Lambert, J.; Knol, J.; Garssen, J.; Kraneveld, A.D.; Oozeer, R. Altered gut microbiota and activity in a murine model of autism spectrum disorders. Brain Behav. Immun. 2014, 37, 197–206. [Google Scholar] [CrossRef]
  31. Margolis, K.G.; Li, Z.; Stevanovic, K.; Saurman, V.; Israelyan, N.; Anderson, G.M.; Snyder, I.; Veenstra-VanderWeele, J.; Blakely, R.D.; Gershon, M.D. Serotonin transporter variant drives preventable gastrointestinal abnormalities in development and function. J. Clin. Investig. 2016, 126, 2221–2235. [Google Scholar] [CrossRef] [PubMed]
  32. Sgritta, M.; Dooling, S.W.; Buffington, S.A.; Momin, E.N.; Francis, M.B.; Britton, R.A.; Costa-Mattioli, M. Mechanisms underlying microbial-mediated changes in social behavior in mouse models of autism spectrum disorder. Neuron 2019, 101, 246–259. [Google Scholar] [CrossRef] [PubMed]
  33. Bernier, R.; Golzio, C.; Xiong, B.; Stessman, H.A.; Coe, B.P.; Penn, O.; Witherspoon, K.; Gerdts, J.; Baker, C.; Vulto-van Silfhout, A.T.; et al. Disruptive CHD8 mutations define a subtype of autism early in development. Cell 2014, 158, 263–276. [Google Scholar] [CrossRef] [PubMed]
  34. Baudouin, S.J.; Gaudias, J.; Gerharz, S.; Hatstatt, L.; Zhou, K.; Punnakkal, P.; Tanaka, K.F.; Spooren, W.; Hen, R.; De Zeeuw, C.I.; et al. Shared synaptic pathophysiology in syndromic and nonsyndromic rodent models of autism. Science 2012, 338, 128–132. [Google Scholar] [CrossRef]
  35. Budreck, E.C.; Scheiffele, P. Neuroligin-3 is a neuronal adhesion protein at GABAergic and glutamatergic synapses. Eur. J. Neurosci. 2007, 26, 1738–1748. [Google Scholar] [CrossRef]
  36. Uchigashima, M.; Leung, M.; Watanabe, T.; Cheung, A.; Le, T.; Pallat, S.; Dinis, A.L.M.; Watanabe, M.; Kawasawa, Y.I.; Futai, K. Neuroligin3 splice isoforms shape inhibitory synaptic function in the mouse hippocampus. J. Biol. Chem. 2020, 295, 8589–8595. [Google Scholar] [CrossRef]
  37. Herath, M.; Cho, E.; Marklund, U.; Franks, A.E.; Bornstein, J.C.; Hill-Yardin, E.L. Quantitative Spatial Analysis of Neuroligin-3 mRNA Expression in the Enteric Nervous System Reveals a Potential Role in Neuronal-Glial Synapses and Reduced Expression in Nlgn3(R451C) Mice. Biomolecules 2023, 13, 1063. [Google Scholar] [CrossRef]
  38. Gilbert, M.; Smith, J.; Roskams, A.J.; Auld, V.J. Neuroligin 3 is a vertebrate gliotactin expressed in the olfactory ensheathing glia, a growth-promoting class of macroglia. Glia 2001, 34, 151–164. [Google Scholar] [CrossRef]
  39. Jamain, S.; Quach, H.; Betancur, C.; Råstam, M.; Colineaux, C.; Gillberg, I.C.; Soderstrom, H.; Giros, B.; Leboyer, M.; Gillberg, C. Mutations of the X-linked genes encoding neuroligins NLGN3 and NLGN4 are associated with autism. Nat. Genet. 2003, 34, 27–29. [Google Scholar] [CrossRef]
  40. Chubykin, A.A.; Liu, X.; Comoletti, D.; Tsigelny, I.; Taylor, P.; Südhof, T.C. Dissection of synapse induction by neuroligins: Effect of a neuroligin mutation associated with autism. J. Biol. Chem. 2005, 280, 22365–22374. [Google Scholar] [CrossRef]
  41. Comoletti, D.; De Jaco, A.; Jennings, L.L.; Flynn, R.E.; Gaietta, G.; Tsigelny, I.; Ellisman, M.H.; Taylor, P. The Arg451Cys-neuroligin-3 mutation associated with autism reveals a defect in protein processing. J. Neurosci. 2004, 24, 4889–4893. [Google Scholar] [CrossRef] [PubMed]
  42. Burrows, E.L.; Laskaris, L.; Koyama, L.; Churilov, L.; Bornstein, J.C.; Hill-Yardin, E.L.; Hannan, A.J. A neuroligin-3 mutation implicated in autism causes abnormal aggression and increases repetitive behavior in mice. Mol. Autism 2015, 6, 62. [Google Scholar] [CrossRef] [PubMed]
  43. Chadman, K.K.; Gong, S.; Scattoni, M.L.; Boltuck, S.E.; Gandhy, S.U.; Heintz, N.; Crawley, J.N. Minimal aberrant behavioral phenotypes of neuroligin-3 R451C knockin mice. Autism Res. 2008, 1, 147–158. [Google Scholar] [CrossRef] [PubMed]
  44. Herath, M.; Bornstein, J.C.; Hill-Yardin, E.L.; Franks, A.E. The autism-associated Neuroligin-3 R451C mutation alters mucus density and the spatial distribution of bacteria in the mouse gastrointestinal tract. bioRxiv 2022. bioRxiv:06.27.497808. [Google Scholar] [CrossRef]
  45. Costa, M.; Spencer, N.J.; Brookes, S.J. The role of enteric inhibitory neurons in intestinal motility. Auton. Neurosci. 2021, 235, 102854. [Google Scholar] [CrossRef]
  46. Hennig, G.W.; Costa, M.; Chen, B.N.; Brookes, S.J. Quantitative analysis of peristalsis in the guinea-pig small intestine using spatio-temporal maps. J. Physiol. 1999, 517 (Pt. 2), 575–590. [Google Scholar] [CrossRef]
  47. Neal, K.B.; Parry, L.J.; Bornstein, J.C. Strain-specific genetics, anatomy and function of enteric neural serotonergic pathways in inbred mice. J. Physiol. 2009, 587, 567–586. [Google Scholar] [CrossRef]
  48. Abdu, F.; Hicks, G.A.; Hennig, G.; Allen, J.P.; Grundy, D. Somatostatin sst(2) receptors inhibit peristalsis in the rat and mouse jejunum. Am. J. Physiol. Gastrointest. Liver Physiol. 2002, 282, G624–G633. [Google Scholar] [CrossRef]
  49. Costa, M.; Hibberd, T.J.; Keightley, L.J.; Wiklendt, L.; Arkwright, J.W.; Dinning, P.G.; Brookes, S.J.H.; Spencer, N.J. Neural motor complexes propagate continuously along the full length of mouse small intestine and colon. Am. J. Physiol. Gastrointest. Liver Physiol. 2020, 318, G99–G108. [Google Scholar] [CrossRef]
  50. Seerden, T.C.; Lammers, W.J.; De Winter, B.Y.; De Man, J.G.; Pelckmans, P.A. Spatiotemporal electrical and motility mapping of distension-induced propagating oscillations in the murine small intestine. Am. J. Physiol. Gastrointest. Liver Physiol. 2005, 289, G1043–G1051. [Google Scholar] [CrossRef]
  51. Balasuriya, G.K.; Nugapitiya, S.S.; Hill-Yardin, E.L.; Bornstein, J.C. Nitric Oxide Regulates Estrus Cycle Dependent Colonic Motility in Mice. Front. Neurosci. 2021, 15, 647555. [Google Scholar] [CrossRef] [PubMed]
  52. Leembruggen, A.J.; Balasuriya, G.K.; Zhang, J.; Schokman, S.; Swiderski, K.; Bornstein, J.C.; Nithianantharajah, J.; Hill-Yardin, E.L. Colonic dilation and altered ex vivo gastrointestinal motility in the Neuroligin-3 knockout mouse. Autism Res. 2020, 13, 691–701. [Google Scholar] [CrossRef] [PubMed]
  53. Swaminathan, M.; Hill-Yardin, E.; Ellis, M.; Zygorodimos, M.; Johnston, L.A.; Gwynne, R.M.; Bornstein, J.C. Video Imaging and Spatiotemporal Maps to Analyze Gastrointestinal Motility in Mice. J. Vis. Exp. 2016, 108, 53828. [Google Scholar] [CrossRef]
  54. Abo-Shaban, T.; Lee, C.Y.Q.; Hosie, S.; Balasuriya, G.K.; Mohsenipour, M.; Johnston, L.A.; Hill-Yardin, E.L. GutMap: A New Interface for Analysing Regional Motility Patterns in ex vivo Mouse Gastrointestinal Preparations. Bio Protoc. 2023, 13, e4831. [Google Scholar] [CrossRef]
  55. Seifi, M.; Brown, J.F.; Mills, J.; Bhandari, P.; Belelli, D.; Lambert, J.J.; Rudolph, U.; Swinny, J.D. Molecular and functional diversity of GABA-A receptors in the enteric nervous system of the mouse colon. J. Neurosci. 2014, 34, 10361–10378. [Google Scholar] [CrossRef]
  56. Koussoulas, K.; Swaminathan, M.; Fung, C.; Bornstein, J.C.; Foong, J.P.P. Neurally Released GABA Acts via GABA(C) Receptors to Modulate Ca(2+) Transients Evoked by Trains of Synaptic Inputs, but Not Responses Evoked by Single Stimuli, in Myenteric Neurons of Mouse Ileum. Front. Physiol. 2018, 9, 97. [Google Scholar] [CrossRef]
  57. Sang, Q.; Young, H.M. Chemical coding of neurons in the myenteric plexus and external muscle of the small and large intestine of the mouse. Cell Tissue Res. 1996, 284, 39–53. [Google Scholar] [CrossRef]
  58. Schieve, L.A.; Rice, C.; Yeargin-Allsopp, M.; Boyle, C.A.; Kogan, M.D.; Drews, C.; Devine, O. Parent-reported prevalence of autism spectrum disorders in US-born children: An assessment of changes within birth cohorts from the 2003 to the 2007 National Survey of Children’s Health. Matern. Child Health J. 2012, 16 (Suppl. S1), S151–S157. [Google Scholar] [CrossRef]
  59. McQuade, R.M.; Stojanovska, V.; Donald, E.; Abalo, R.; Bornstein, J.C.; Nurgali, K. Gastrointestinal dysfunction and enteric neurotoxicity following treatment with anticancer chemotherapeutic agent 5-fluorouracil. Neurogastroenterol. Motil. 2016, 28, 1861–1875. [Google Scholar] [CrossRef]
  60. McQuade, R.M.; Stojanovska, V.; Stavely, R.; Timpani, C.; Petersen, A.C.; Abalo, R.; Bornstein, J.C.; Rybalka, E.; Nurgali, K. Oxaliplatin-induced enteric neuronal loss and intestinal dysfunction is prevented by co-treatment with BGP-15. Br. J. Pharmacol. 2018, 175, 656–677. [Google Scholar] [CrossRef]
  61. McQuade, R.M.; Stojanovska, V.; Donald, E.L.; Rahman, A.A.; Campelj, D.G.; Abalo, R.; Rybalka, E.; Bornstein, J.C.; Nurgali, K. Irinotecan-Induced Gastrointestinal Dysfunction Is Associated with Enteric Neuropathy, but Increased Numbers of Cholinergic Myenteric Neurons. Front. Physiol. 2017, 8, 391. [Google Scholar] [CrossRef] [PubMed]
  62. Robinson, A.M.; Rahman, A.A.; Carbone, S.E.; Randall-Demllo, S.; Filippone, R.; Bornstein, J.C.; Eri, R.; Nurgali, K. Alterations of colonic function in the Winnie mouse model of spontaneous chronic colitis. Am. J. Physiol. Gastrointest. Liver Physiol. 2017, 312, G85–G102. [Google Scholar] [CrossRef] [PubMed]
  63. Sahakian, L.; Filippone, R.T.; Stavely, R.; Robinson, A.M.; Yan, X.S.; Abalo, R.; Eri, R.; Bornstein, J.C.; Kelley, M.R.; Nurgali, K. Inhibition of APE1/Ref-1 Redox Signaling Alleviates Intestinal Dysfunction and Damage to Myenteric Neurons in a Mouse Model of Spontaneous Chronic Colitis. Inflamm. Bowel Dis. 2021, 27, 388–406. [Google Scholar] [CrossRef] [PubMed]
  64. Venkataramana, S.; Lourenssen, S.; Miller, K.G.; Blennerhassett, M.G. Early inflammatory damage to intestinal neurons occurs via inducible nitric oxide synthase. Neurobiol. Dis. 2015, 75, 40–52. [Google Scholar] [CrossRef] [PubMed]
  65. Huizinga, J.D.; Chen, J.H.; Fang Zhu, Y.; Pawelka, A.; McGinn, R.J.; Bardakjian, B.L.; Parsons, S.P.; Kunze, W.A.; Wu, R.Y.; Bercik, P.; et al. The origin of segmentation motor activity in the intestine. Nat. Commun. 2014, 5, 3326. [Google Scholar] [CrossRef]
  66. Spencer, N.J.; Hu, H. Enteric nervous system: Sensory transduction, neural circuits and gastrointestinal motility. Nat. Rev. Gastroenterol. Hepatol. 2020, 17, 338–351. [Google Scholar] [CrossRef]
  67. Brenman, J.E.; Chao, D.S.; Gee, S.H.; McGee, A.W.; Craven, S.E.; Santillano, D.R.; Wu, Z.; Huang, F.; Xia, H.; Peters, M.F.; et al. Interaction of nitric oxide synthase with the postsynaptic density protein PSD-95 and alpha1-syntrophin mediated by PDZ domains. Cell 1996, 84, 757–767. [Google Scholar] [CrossRef]
  68. Coley, A.A.; Gao, W.J. PSD95: A synaptic protein implicated in schizophrenia or autism? Prog. Neuropsychopharmacol. Biol. Psychiatry 2018, 82, 187–194. [Google Scholar] [CrossRef]
  69. Irie, M.; Hata, Y.; Takeuchi, M.; Ichtchenko, K.; Toyoda, A.; Hirao, K.; Takai, Y.; Rosahl, T.W.; Südhof, T.C. Binding of neuroligins to PSD-95. Science 1997, 277, 1511–1515. [Google Scholar] [CrossRef]
  70. Costa, M.; Wiklendt, L.; Arkwright, J.; Spencer, N.; Omari, T.; Brookes, S.J.; Dinning, P. An experimental method to identify neurogenic and myogenic active mechanical states of intestinal motility. Front. Syst. Neurosci. 2013, 11, 7. [Google Scholar] [CrossRef]
  71. Huizinga, J.D.; Chen, J.-H. Interstitial cells of Cajal: Update on basic and clinical science. Curr. Gastroenterol. Rep. 2014, 16, 363. [Google Scholar] [CrossRef] [PubMed]
  72. Huizinga, J.D.; Lammers, W.J.E.P. Gut peristalsis is governed by a multitude of cooperating mechanisms. Am. J. Physiol. Gastrointest. Liver Physiol. 2009, 296, G1–G8. [Google Scholar] [CrossRef] [PubMed]
  73. Sanders, K.M.; Koh, S.D.; Ward, S.M. Interstitial cells of Cajal as pacemakers in the gastrointestinal tract. Annu. Rev. Physiol. 2006, 68, 307–343. [Google Scholar] [CrossRef] [PubMed]
  74. Swiderski, K.; Bindon, R.; Trieu, J.; Naim, T.; Schokman, S.; Swaminathan, M.; Leembruggen, A.J.L.; Hill-Yardin, E.L.; Koopman, R.; Bornstein, J.C.; et al. Spatiotemporal Mapping Reveals Regional Gastrointestinal Dysfunction in mdx Dystrophic Mice Ameliorated by Oral L-arginine Supplementation. J. Neurogastroenterol. Motil. 2020, 26, 133–146. [Google Scholar] [CrossRef]
Ijms 25 00832 g001
Figure 1. Faster in vivo gastrointestinal transit in Nlgn3R451C mice. (A) Representative X-ray images showing transit of barium sulphate in gastrointestinal tract and faecal pellets (arrows). (B) Diagram of mouse gastrointestinal tract indicating regions measured for small intestinal (beginning of duodenum after the pyloric sphincter to the ileum (before ileo-caecal valve)) (green) and colonic (blue) transit. Whole transit time (WT: W = 0.9, p = 0.2, Nlgn3R451C: W = 0.9, p = 0.4, Shapiro–Wilk test) (C), small intestinal transit time (WT: W = 0.96, p = 0.9, Nlgn3R451C: W = 0.8, p = 0.07, Shapiro–Wilk test) (D) and colonic transit time (WT: W = 0.9, p = 0.2 D’Agostino and Pearson test, Nlgn3R451C: K2 = 4.9, p = 0.08 (Shapiro–Wilk test is inaccurate for several identical data points) (E) were compared between WT (n = 7) and Nlgn3R451C (n = 8) mice. Data represented as scatterplots of mean ± SEM and individual data points. Student’s t-test * p < 0.05, ** p < 0.01, *** p < 0.001. All data passed normality testing.
Figure 1. Faster in vivo gastrointestinal transit in Nlgn3R451C mice. (A) Representative X-ray images showing transit of barium sulphate in gastrointestinal tract and faecal pellets (arrows). (B) Diagram of mouse gastrointestinal tract indicating regions measured for small intestinal (beginning of duodenum after the pyloric sphincter to the ileum (before ileo-caecal valve)) (green) and colonic (blue) transit. Whole transit time (WT: W = 0.9, p = 0.2, Nlgn3R451C: W = 0.9, p = 0.4, Shapiro–Wilk test) (C), small intestinal transit time (WT: W = 0.96, p = 0.9, Nlgn3R451C: W = 0.8, p = 0.07, Shapiro–Wilk test) (D) and colonic transit time (WT: W = 0.9, p = 0.2 D’Agostino and Pearson test, Nlgn3R451C: K2 = 4.9, p = 0.08 (Shapiro–Wilk test is inaccurate for several identical data points) (E) were compared between WT (n = 7) and Nlgn3R451C (n = 8) mice. Data represented as scatterplots of mean ± SEM and individual data points. Student’s t-test * p < 0.05, ** p < 0.01, *** p < 0.001. All data passed normality testing.
Ijms 25 00832 g001
Ijms 25 00832 g002
Figure 2. Longer small intestinal and colon length in Nlgn3R451C mice. (A) Wild-type (WT; n = 21) and Nlgn3R451C (n = 24) small intestinal (SI) gut length in the active state (control) and after incubation in 100 µM of the muscle relaxant nicardipine (* p > 0.05 two-way ANOVA test (variables tested: genotype and nicardipine treatment), Sidak correction). Normality assumptions passed (Shapiro–Wilk normality of residuals test: w = 0.98, p = 0.3). (B) Increased colon length in Nlgn3R451C mice (n = 28) compared to wild-type mice (n = 13) (Student’s t-test. * p > 0.05). Normality assumptions passed (Shapiro–Wilk normality test WT: w = 0.95, p = 0.7; Nlgn3R451C: w = 0.9, p = 0.1). (C) No differences were observed between the body weights in a sample of WT (n = 21) and Nlgn3R451C mice (n = 24) (Student’s t-test. * p = 0.17). Normality assumptions passed (Shapiro–Wilk normality test WT: w = 0.97, p = 0.6; Nlgn3R451C: w = 0.98, p = 0.9). ns: not statistically significant.
Figure 2. Longer small intestinal and colon length in Nlgn3R451C mice. (A) Wild-type (WT; n = 21) and Nlgn3R451C (n = 24) small intestinal (SI) gut length in the active state (control) and after incubation in 100 µM of the muscle relaxant nicardipine (* p > 0.05 two-way ANOVA test (variables tested: genotype and nicardipine treatment), Sidak correction). Normality assumptions passed (Shapiro–Wilk normality of residuals test: w = 0.98, p = 0.3). (B) Increased colon length in Nlgn3R451C mice (n = 28) compared to wild-type mice (n = 13) (Student’s t-test. * p > 0.05). Normality assumptions passed (Shapiro–Wilk normality test WT: w = 0.95, p = 0.7; Nlgn3R451C: w = 0.9, p = 0.1). (C) No differences were observed between the body weights in a sample of WT (n = 21) and Nlgn3R451C mice (n = 24) (Student’s t-test. * p = 0.17). Normality assumptions passed (Shapiro–Wilk normality test WT: w = 0.97, p = 0.6; Nlgn3R451C: w = 0.98, p = 0.9). ns: not statistically significant.
Ijms 25 00832 g002
Ijms 25 00832 g003
Figure 3. Comparison of small intestinal motility patterns in WT and Nlgn3R451C mice. Spatiotemporal maps (15 min duration) from (A,C) jejunum and (B,D) ileum of WT and Nlgn3R451C mice. Calibration bar: 10 mm, 200 s.
Figure 3. Comparison of small intestinal motility patterns in WT and Nlgn3R451C mice. Spatiotemporal maps (15 min duration) from (A,C) jejunum and (B,D) ileum of WT and Nlgn3R451C mice. Calibration bar: 10 mm, 200 s.
Ijms 25 00832 g003
Ijms 25 00832 g004
Figure 4. Small intestinal dysmotility in Nlgn3R451C mice. In the jejunum of Nlgn3R451C mice, no difference was identified in (A) PCC quiescence or (B) PCC duration (Shapiro–Wilk normality of residuals assumption passed w = 0.98, p = 0.2), however, the (C) resting diameter was reduced and the (D) intra PCC frequency was faster in all measured regions. In the ileum of the Nlgn3R451C mice, an increase in (E) PCC quiescence and a reduction in (F) PCC duration in the mid and distal regions was identified. (G) No difference in ileal resting diameter or (H) intra PCC frequency was detected between wild-type and Nlgn3R451C mice. (Student’s t-test. * p > 0.05, ** p < 0.01.)
Figure 4. Small intestinal dysmotility in Nlgn3R451C mice. In the jejunum of Nlgn3R451C mice, no difference was identified in (A) PCC quiescence or (B) PCC duration (Shapiro–Wilk normality of residuals assumption passed w = 0.98, p = 0.2), however, the (C) resting diameter was reduced and the (D) intra PCC frequency was faster in all measured regions. In the ileum of the Nlgn3R451C mice, an increase in (E) PCC quiescence and a reduction in (F) PCC duration in the mid and distal regions was identified. (G) No difference in ileal resting diameter or (H) intra PCC frequency was detected between wild-type and Nlgn3R451C mice. (Student’s t-test. * p > 0.05, ** p < 0.01.)
Ijms 25 00832 g004
Ijms 25 00832 g005
Figure 5. Effect of NOLA on small intestinal motility patterns in wild-type and Nlgn3R451C mice. Spatiotemporal maps (15 min duration) in WT and Nlgn3R451C mouse (A) jejunum and (B) ileum following incubation with NOLA. Average number of PCCs per 15 min before and after incubation with NOLA in (C) jejunum and (D) ileum in WT and Nlgn3R451C mice. (E) The number of PCCs is reduced following NOLA incubation in the jejunum, However, in the ileum (F), PCC numbers persist despite NOLA incubation. Calibration bar: 10 mm, 200 s. Two-way ANOVA test (factors: genotype and NOLA drug), Sidak correction ** p < 0.01, *** p < 0.001.
Figure 5. Effect of NOLA on small intestinal motility patterns in wild-type and Nlgn3R451C mice. Spatiotemporal maps (15 min duration) in WT and Nlgn3R451C mouse (A) jejunum and (B) ileum following incubation with NOLA. Average number of PCCs per 15 min before and after incubation with NOLA in (C) jejunum and (D) ileum in WT and Nlgn3R451C mice. (E) The number of PCCs is reduced following NOLA incubation in the jejunum, However, in the ileum (F), PCC numbers persist despite NOLA incubation. Calibration bar: 10 mm, 200 s. Two-way ANOVA test (factors: genotype and NOLA drug), Sidak correction ** p < 0.01, *** p < 0.001.
Ijms 25 00832 g005
Ijms 25 00832 g006
Figure 6. Gabazine reduces the proportion of short colonic contractions in Nlgn3R451C mice. Representative spatiotemporal maps of WT and Nlgn3R451C colonic activity in (A) control conditions and (B) after administration of 10 µM gabazine to the organ bath. (C) Effect of gabazine on CMMC frequency in WT and Nlgn3R451C mice. No changes were observed for (D) resting colon diameter or (E) CMMC length. (F) The short contraction frequency was reduced in both WT and Nlgn3R451C colons; WT n = 18; Nlgn3R451C n = 14. Calibration bar: 10 mm, 200 s. One-way ANOVA Holm–Sidak multiple comparisons test. * p < 0.05, *** p < 0.001.
Figure 6. Gabazine reduces the proportion of short colonic contractions in Nlgn3R451C mice. Representative spatiotemporal maps of WT and Nlgn3R451C colonic activity in (A) control conditions and (B) after administration of 10 µM gabazine to the organ bath. (C) Effect of gabazine on CMMC frequency in WT and Nlgn3R451C mice. No changes were observed for (D) resting colon diameter or (E) CMMC length. (F) The short contraction frequency was reduced in both WT and Nlgn3R451C colons; WT n = 18; Nlgn3R451C n = 14. Calibration bar: 10 mm, 200 s. One-way ANOVA Holm–Sidak multiple comparisons test. * p < 0.05, *** p < 0.001.
Ijms 25 00832 g006
Ijms 25 00832 g007
Figure 7. PCC analysis method. (A) Frequency was calculated by counting each PCC (arrows) that occurred during each 15 min recording. PCC duration was measured at the proximal, mid and distal location shown by arrows on map (B). (C) Quiescence was measured as the time interval between PCCs (as indicated by the arrow on the map). (D) Representative spatiotemporal map from a wild-type mouse indicating location of proximal (black), mid (red) and distal (green) gut width measurements. (E–G) Gut width measurements against time for the anatomical locations indicated in A; inserts represent enlarged single PCCs (dashed boxes).
Figure 7. PCC analysis method. (A) Frequency was calculated by counting each PCC (arrows) that occurred during each 15 min recording. PCC duration was measured at the proximal, mid and distal location shown by arrows on map (B). (C) Quiescence was measured as the time interval between PCCs (as indicated by the arrow on the map). (D) Representative spatiotemporal map from a wild-type mouse indicating location of proximal (black), mid (red) and distal (green) gut width measurements. (E–G) Gut width measurements against time for the anatomical locations indicated in A; inserts represent enlarged single PCCs (dashed boxes).
Ijms 25 00832 g007
Table 1. Small intestinal motility parameters from the jejunum and ileum in wild-type and Nlgn3R451C mice.
Table 1. Small intestinal motility parameters from the jejunum and ileum in wild-type and Nlgn3R451C mice.
Small Intestinal Motility ParameterJejunum Ileum
WT
n = 17		Nlgn3R451C
n = 16		Normality Passed?WT
n = 16		Nlgn3R451C
n = 16		Normality Passed?
Full length PCC Frequency
(No. of PCCs/15 min)		6.3 ± 0.46.3 ± 0.4Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.9, p = 0.051		7.2 ± 0.37.2 ± 0.3Yes. WT: w = 0.99, p > 0.99.
Nlgn3R451C: w = 0.97, p = 0.8
Full length PCC Quiescence (s)39.4 ± 5.337.6 ± 5.8Yes. WT: w = 0.9, p = 0.2.
Nlgn3R451C: w = 0.9, p = 0.3 		35.8 ± 2.754.3 ± 6.8 *Yes. WT: w = 0.96, p = 0.6.
Nlgn3R451C: w = 0.9, p = 0.06
Full length PCC Velocity (mm/s)0.5 ± 0.020.6 ± 0.06Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.9, p = 0.4		−0.3 ± 0.1−0.4 ± 0.2Yes. WT: w = 0.9, p = 0.4.
Nlgn3R451C: w = 0.98, p = 0.9
Proximal region PCC duration (s)30.9 ± 430.8 ± 4.5Yes. WT: w = 0.9, p = 0.1.
Nlgn3R451C: w = 0.96, p = 0.7		74.1 ± 5.758.5 ± 4Yes. WT: w = 0.9, p = 0.2.
Nlgn3R451C: w = 0.96, p = 0.7
Mid region PCC duration (s)41.6 ± 4.339.4 ± 5.6Yes. WT: w = 0.9, p = 0.1.
Nlgn3R451C: w = 0.9, p = 0.4		85.2 ± 5.663.4 ± 3.7 †Yes. WT: w = 0.98, p = 0.98.
Nlgn3R451C: w = 0.96, p = 0.7
Distal region PCC duration (s)34.5 ± 2.834.4 ± 7.8Yes. WT: w = 0.97, p = 0.7.
Nlgn3R451C: w = 0.9, p = 0.4		88.3 ± 6.1 61.4 ± 6.5 †Yes. WT: w = 0.99, p = 0.99.
Nlgn3R451C: w = 0.9, p = 0.2
Mean ± SEM, genotype comparisons; * p < 0.05 † p < 0.01. Shapiro–Wilk normality test performed.
Table 2. Regional small intestinal motility parameters from jejunum and ileum in wild-type and Nlgn3 R451C mice.
Table 2. Regional small intestinal motility parameters from jejunum and ileum in wild-type and Nlgn3 R451C mice.
Small Intestinal Motility ParametersJejunum Ileum
WT
n = 17		Nlgn3R451C
n = 16		Normality Passed?WT
n = 16		Nlgn3R451C
n = 16		Normality Passed?
Resting diameter (mm)Prox 4.7 ± 0.14.2 ± 0.1 *Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.9, p = 0.1		3.4 ± 0.13.6 ± 0.1Yes. WT: w = 0.98, p = 0.96.
Nlgn3R451C: w = 0.9, p = 0.07
Mid 4.7 ± 0.14.2 ± 0.1 *Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.96, p = 0.6		3.3 ± 0.13.4 ± 0.1Yes. WT: w = 0.98, p = 0.9.
Nlgn3R451C: w = 0.9, p = 0.07
Distal 4.9 ± 0.14.3 ± 0.1 †Yes. WT: w = 0.9, p = 0.4.
Nlgn3R451C: w = 0.95, p = 0.5		3.2 ± 0.13.3 ± 0.1Yes. WT: w = 0.9, p = 0.2.
Nlgn3R451C: w = 0.9, p = 0.1
Constricted diameter (mm)Prox 3.9 ± 0.13.5 ± 0.1Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.9, p = 0.1		2.7 ± 0.12.9 ± 0.1Yes. WT: w = 0.95, p = 0.6.
Nlgn3R451C: w = 0.9, p = 0.06
Mid 3.7 ± 0.13.5 ± 0.1Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.95, p = 0.5		2.5 ± 0.12.7 ± 0.1Yes. WT: w = 0.98, p = 0.9.
Nlgn3R451C: w = 0.9, p = 0.2
Distal 4.0 ± 0.13.6 ± 0.1 *Yes. WT: w = 0.98, p = 0.95. Nlgn3R451C: w = 0.9, p = 0.42.5 ± 0.12.7 ± 0.1Yes. WT: w = 0.9, p = 0.3.
Nlgn3R451C: w = 0.9, p = 0.1
Intra PCC frequency (sec−1)Prox CI: 0.5–0.7CI: 0.6–0.7 *No. w = 0.95, p = 0.0002CI: 0.3–0.6CI: 0.4–0.5No. w = 0.91, p < 0.0001
Mid CI:0.5–0.7CI: 0.6–0.7 *CI: 0.3–0.6CI: 0.4–0.6
Distal CI: 0.5–0.7CI: 0.5–0.6 *CI: 0.4–0.6CI: 0.4–0.5
Mean ± SEM, genotype comparisons; confidence intervals (CI) * p < 0.05 † p < 0.01. Shapiro–Wilk normality test performed.
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Hosie, S.; Abo-Shaban, T.; Mou, K.; Balasuriya, G.K.; Mohsenipour, M.; Alamoudi, M.U.; Filippone, R.T.; Belz, G.T.; Franks, A.E.; Bornstein, J.C.; et al. Faster Gastrointestinal Transit, Reduced Small Intestinal Smooth Muscle Tone and Dysmotility in the Nlgn3R451C Mouse Model of Autism. Int. J. Mol. Sci. 2024, 25, 832. https://doi.org/10.3390/ijms25020832

AMA Style

Hosie S, Abo-Shaban T, Mou K, Balasuriya GK, Mohsenipour M, Alamoudi MU, Filippone RT, Belz GT, Franks AE, Bornstein JC, et al. Faster Gastrointestinal Transit, Reduced Small Intestinal Smooth Muscle Tone and Dysmotility in the Nlgn3R451C Mouse Model of Autism. International Journal of Molecular Sciences. 2024; 25(2):832. https://doi.org/10.3390/ijms25020832

Chicago/Turabian Style

Hosie, Suzanne, Tanya Abo-Shaban, Kevin Mou, Gayathri K. Balasuriya, Mitra Mohsenipour, Mohammed U. Alamoudi, Rhiannon T. Filippone, Gabrielle T. Belz, Ashley E. Franks, Joel C. Bornstein, and et al. 2024. "Faster Gastrointestinal Transit, Reduced Small Intestinal Smooth Muscle Tone and Dysmotility in the Nlgn3R451C Mouse Model of Autism" International Journal of Molecular Sciences 25, no. 2: 832. https://doi.org/10.3390/ijms25020832

APA Style

Hosie, S., Abo-Shaban, T., Mou, K., Balasuriya, G. K., Mohsenipour, M., Alamoudi, M. U., Filippone, R. T., Belz, G. T., Franks, A. E., Bornstein, J. C., Nurgali, K., & Hill-Yardin, E. L. (2024). Faster Gastrointestinal Transit, Reduced Small Intestinal Smooth Muscle Tone and Dysmotility in the Nlgn3R451C Mouse Model of Autism. International Journal of Molecular Sciences, 25(2), 832. https://doi.org/10.3390/ijms25020832

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop