Search tips
Search criteria 


Logo of ncommsLink to Publisher's site
Nat Commun. 2016; 7: 11905.
Published online 2016 June 15. doi:  10.1038/ncomms11905
PMCID: PMC4912612

Genetically and functionally defined NTS to PBN brain circuits mediating anorexia


The central nervous system controls food consumption to maintain metabolic homoeostasis. In response to a meal, visceral signals from the gut activate neurons in the nucleus of the solitary tract (NTS) via the vagus nerve. These NTS neurons then excite brain regions known to mediate feeding behaviour, such as the lateral parabrachial nucleus (PBN). We previously described a neural circuit for appetite suppression involving calcitonin gene-related protein (CGRP)-expressing PBN (CGRPPBN) neurons; however, the molecular identity of the inputs to these neurons was not established. Here we identify cholecystokinin (CCK) and noradrenergic, dopamine β-hydroxylase (DBH)-expressing NTS neurons as two separate populations that directly excite CGRPPBN neurons. When these NTS neurons are activated using optogenetic or chemogenetic methods, food intake decreases and with chronic stimulation mice lose body weight. Our optogenetic results reveal that CCK and DBH neurons in the NTS directly engage CGRPPBN neurons to promote anorexia.

Metabolic homoeostasis requires coordination of central circuits that balance energy input with its output. Coordination is achieved via long-term signals responding to energy status as well as short-term signals, such as those that drive the initiation or termination of a meal. Following ingestion, gut distention and satiety hormones released from the intestine and pancreas are detected by vagal afferents that relay this information to the area postrema and nucleus of the solitary tract (NTS) neurons in the brainstem1. The relevant, satiety-related neurons in the NTS receiving this information relay it to other nuclei involved in suppressing feeding behaviour. One of the major targets receiving viscerosensory information from the NTS is the lateral parabrachial nucleus (PBN)2,3,4,5,6.

Our lab recently described a neural circuit mediating appetite suppression that involves a distinct population of neurons in the lateral PBN expressing the neuropeptide CGRP (CGRPPBN neurons)7. Activation of CGRPPBN neurons or their projections in the central nucleus of the amygdala (CeA) decreases feeding by hungry mice. Consistently, inhibition of CGRPPBN neurons attenuates anorexic responses to satiety hormones, and other anorexigenic agents such as lithium chloride and lipopolysaccharide7. Furthermore, this population of neurons and their excitatory inputs from the NTS are necessary for the starvation phenotype that occurs in mice following ablation of hypothalamic agouti-related peptide (AgRP)-expressing neurons6,7. Either inhibition of CGRPPBN neurons or inactivation of glutamatergic signalling from the NTS to the PBN can rescue these mice from starvation after AgRP neuron ablation6,7. The excitatory input driving CGRP neurons is, therefore, an important component of the functionally identified CGRPPBN-to-CeA anorexic neural circuit. In this study, we aimed to identify NTS neurons with direct excitatory connections to CGRPPBN neurons and explore their role in feeding behaviour.

The NTS is a heterogeneous brain region with many neuronal types expressing a variety of neuropeptides and neuromodulators8,9,10. We applied contemporary neuron-manipulation techniques to two distinct populations of NTS neurons (cholecystokinin (CCK)- and dopamine β-hydroxylase (DBH)-expressing neurons) that have been implicated in feeding behaviour. CCK- and DBH-expressing neurons are located in the caudal portion of the NTS, which is widely accepted as the ‘visceral' portion of the NTS, receiving input from the gut via the vagus nerve, in contrast to the rostral portion, which receives and relays taste information in the rodent11,12. CCK is well-known for its ability to decrease feeding. CCK is a satiety hormone produced and released by cells in the gastrointestinal tract in response to food intake and acts on a number of systems to signal the presence of food and ultimately contribute to meal termination13. However, CCK is also a neuropeptide and it can suppress feeding when it is administered centrally14,15. There is relatively little information regarding the function of CCK-expressing neurons within the caudal NTS; however, anatomical studies demonstrated that these neurons project to the lateral PBN3, the area where anorexigenic CGRPPBN neurons reside. While norepinephrine has been shown to both increase and decrease feeding, depending on the site and type of receptors activated (for review see ref. 16), many studies implicate the A2 population of DBH-expressing cells in the NTS in satiety. For example, A2 neurons are activated by the satiety hormone CCK17 as well as by large meals in rats18. Furthermore, anorexia induced by either CCK or lithium chloride is significantly attenuated in rats in which A2 noradrenergic neurons in the NTS are ablated using a saporin toxin-conjugated DBH antibody19,20. In addition, anatomical studies establish a dense projection from DBH neurons in the caudal NTS to the lateral PBN4,21.

Therefore, we hypothesized that CCKNTS and DBHNTS neuronal projections to CGRPPBN neurons might mediate anorexia. First, we provide evidence that these two separate populations of NTS neurons become activated during feeding and not during a fast. We demonstrate that artificial activation of either CCKNTS or DBHNTS neurons, or their axonal projections within the PBN, is sufficient to attenuate food intake by hungry mice. We then use channelrhodopsin-assisted analysis to demonstrate that both CCKNTS and DBHNTS neurons engage CGRPPBN neurons via direct glutamatergic inputs.


Food intake activates genetically distinct NTS neurons

To substantiate a role for both CCKNTS and DBHNTS neurons in food intake, we compared activation of these cells in animals that had been fasted to those that had fasted and then fed. To visualize CCKNTS neurons, a Cre recombinase-dependent adeno-associated virus (AAV) virus (AAV1-DIO-YFP) that allows expression of yellow fluorescent protein (YFP) was injected into the NTS of CckCre/+ mice. To label DBHNTS neurons, we used an antibody to tyrosine hydroxylase, an essential enzyme for norepinephrine biosynthesis. Mice were fasted overnight after which one group of mice (refed group) was allowed unrestricted access to normal chow for 2 h. The total number of CCK and DBH neurons per slice was the same between groups; however, the refed group showed significantly greater amount of Fos immunoreactivity in both the YFP- and tyrosine hydroxylase-positive neurons compared with the fasted group (Fig. 1a,b). Approximately 40 and 60% of the CCK- and DBH-expressing neurons expressed Fos, respectively. These data corroborate previous reports showing that DBHNTS neurons are activated by a large meal18, and demonstrate that CCKNTS neurons are also activated by food intake.

Figure 1
CCKNTS and DBHNTS neurons are activated by food intake.

Analysis of CCKNTS and DBHNTS neurons within the same coronal brain sections across several levels of the mid-caudal NTS clearly revealed that they are two distinct populations of neurons. Brain slices (average of 3 each) from 17 individual CckCre/+ mice injected into the NTS with AAV1-DIO-YFP were labelled using a tyrosine hydroxylase antibody. No overlap between CCK-expressing cells and tyrosine hydroxylase-positive cells was observed at any level of the NTS, except for a single neuron in one animal at the level of the area postrema. This separation agrees with studies in the rat showing that A2, noradrenergic neurons do not co-express CCK, in contrast to more rostral C2, adrenergic neurons22,23. CCKNTS and DBHNTS populations were observed at similar expression levels across the NTS and were intermixed throughout, although CCK neurons appeared at slightly more lateral portions within the NTS than DBH neurons (Supplementary Fig. 1).

DREADD activation increases firing rate of NTS neurons

Selective activation and visualization of CCKNTS and DBHNTS neurons was achieved by NTS injection of AAV encoding a Cre-dependent Gαq-coupled designer receptor exclusively activated by designer drugs (DREADD) fused to the fluorescent protein mCherry (AAV1-DIO-hM3Dq:mCherry). Intraperitoneal (i.p.) injection of the otherwise inert ligand, clozapine-N-oxide (CNO), activates the hM3Dq receptor in vivo. This technique has been shown to increase activity in several different neuronal types24,25. To determine whether CNO could directly activate CCKNTS and DBHNTS neurons expressing the hM3Dq receptor, electrophysiological analysis was performed on NTS brain slices taken from CckCre/+ and DbhCre/+ mice that had been injected at least 3 weeks before with either AAV1-DIO-hM3Dq:mCherry (hM3Dq) or, as a control, AAV1-DIO-mCherry (Fig. 2a). Spiking was recorded using cell-attached patches. In the presence of CNO, both CCKNTS and DBHNTS neurons reliably (4/4 in both cases) increased the frequency of action potentials several fold compared with the vehicle (Fig. 2b,c). In contrast, CNO had no effect on cells expressing mCherry alone (Fig. 2c). The increase was observed in the presence of glutamate and GABA receptor inhibitors, suggesting a direct effect of CNO on these cells.

Figure 2
Activation of NTS neurons via a Gq-coupled receptor increases firing rate in vitro.

Activation of CCKNTS or DBHNTS neurons decreases feeding

To investigate the effect of CCKNTS neuronal activation on food intake, we bilaterally transduced neurons in the NTS of CckCre/+mice with either the excitatory hM3Dq receptor or, as a control, mCherry. Saline was injected i.p. twice daily for 3 days to establish baseline food intake. During baseline measurements, no differences in cumulative amount of food intake were observed between the two groups of mice at 2, 4 or 24 h after lights out (data not shown). Subsequently, CNO was injected (0.8 mg per kg body weight i.p.) twice daily over the course of 4 days. Treatment with CNO decreased feeding in hM3Dq-expressing animals by >50% compared with baseline when measured at 2 and 4 h after lights out (Fig. 3a,b); however, 24-h food intake was not significantly influenced (Fig. 3c). The same experimental paradigm was carried out using DbhCre/+ mice. We observed significantly decreased food intake at both the 2- and 4-h time points after lights out (Fig. 3e,f), whereas 24-h food intake was only affected on the first day after CNO injection (Fig. 3g). Meal analysis revealed that the decrease in food intake was due to both a decrease in meal size and meal number for both genotypes (Supplementary Fig. 2).

Figure 3
Activation of CCKNTS or DBHNTS neurons suppresses food intake.

Compared with CNO-treated controls, both CckCre/+ and DbhCre/+mice transduced with the virus expressing hM3Dq decreased their body weight over the course of the experiment (Fig. 3d,h). Although moderate, the significant drop in body weight without consistent changes in 24-h food intake suggests that activation of CCKNTS or DBHNTS neurons also increases energy expenditure.

In addition to reducing food intake during the normal feeding cycle, we also observed that activation of CCKNTS or DBHNTS neurons with hM3Dq and CNO is sufficient to suppress food intake by hungry mice. For this experiment, mice were food restricted and kept at 85–90% of their pre-restriction body weight. CNO or saline was injected during the light cycle, 45 min later food was provided and the amount consumed in 1 h was measured. Activation of CCKNTS neurons with CNO decreased 1-h food intake by 42%, while activation of DBHNTS neurons decreased food intake by 57% when compared with intake after saline injection (Fig. 3i). No differences were observed between saline and CNO treatment in animals expressing mCherry only.

Activation does not induce anxiety-like behaviour

Because behavioural state can influence feeding, we examined whether the inhibition of food intake was due to anxiety. Mice from the previous experiments were placed in an open-field arena 45 min after injection of CNO. No differences were observed between mCherry- and hM3Dq-expressing mice in the time spent in the centre of the open field providing evidence that activation of CCKNTS or DBHNTS neurons does not cause overt anxiety (Supplementary Fig. 3a). Although there was a significant decrease in total distance travelled after CNO injection in mice expressing hM3Dq in DBHNTS neurons and a trend towards a decrease in the CCK group (Supplementary Fig. 3b), this result is likely due to the satiation effect of activating these neurons because mice that are not hungry forage less in a novel environment.

Activation of CCKNTS or DBHNTS neurons induces Fos

One week after mice underwent food intake and behavioural experiments, CNO was injected and brain tissue was evaluated 3 h later for Fos immunoreactivity as an indirect marker of neuronal activity. Animals expressing hM3Dq showed abundant Fos immunoreactivity in the NTS and the lateral PBN (Fig. 4a–c). In contrast, minimal Fos labelling was observed in these regions in mice expressing mCherry alone. Importantly, the amount of Fos labelling observed in both the NTS and PBN was associated with the degree of CNO-induced suppression of feeding in both CckCre/+ and DbhCre/+mice expressing hM3Dq. For this analysis, each genotype was split into a high- and a low-Fos-expressing group based on the median. Average food intake for the first 4 h after CNO injection was then compared for each group. In both the NTS and the PBN, the high-Fos group had significantly greater suppression of food intake when compared with the low-Fos group (Fig. 4d). For simplicity of presentation, the CCKNTS and DBHNTS groups were combined; however, the results are also significant when analysed separately.

Figure 4
CCKNTS or DBHNTS neuronal activation induces Fos in the NTS and in the PBN.

Within the PBN, a substantial portion of Fos labelling following CNO activation of either CCKNTS or DBHNTS neurons co-localized with CGRP immunoreactive neurons (Supplementary Fig. 4). The distribution of co-labelled cells was similar anatomically to that observed after refeeding after a fast26. In both studies, a subset of CGRPPBN neurons that were Fos-negative was detected in the most ventral lateral aspect of the external lateral PBN within an area of the PBN with a dense clustering of CGRP-immunopositive fibres.

Mice expressing the hM3Dq receptor displayed CNO-induced activation in a number of discrete brain regions, which may reflect direct or indirect projections from CCKNTS or DBHNTS neurons. In addition to the NTS and the PBN, increased Fos immunoreactivity was encountered in several forebrain regions including the bed nucleus of the stria terminalis (BNST), amygdala and paraventricular nucleus of the hypothalamus (Supplementary Fig. 5a–c). Within the BNST, the vast majority of expression was restricted to the oval nucleus (BNSTov). Within the amygdala, dense expression occurred almost exclusively within the CeA. Sparse Fos expression was also observed in the periaqueductal grey (Supplementary Fig. 5d). Minimal Fos labelling was observed in these regions in control mice expressing mCherry alone.

Injection of CNO activated CCKNTS neurons that were virally transduced to express hM3Dq. However, when we analysed Fos in the NTS following CNO injection, the majority of Fos-positive NTS cells did not express hM3Dq:mCherry, suggesting that non-CCK neurons were also activated following CNO. We found ~20% of the noradrenergic cells in the NTS co-expressed Fos (Supplementary Fig. 6). In addition, a dense network of local mCherry-expressing fibres was observed in the NTS of CckCre/+ animals expressing hM3Dq:mCherry or mCherry. This finding suggests that activation of CCKNTS neurons stimulates DBHNTS neurons and other unidentified neurons in the NTS. Activation of DBHNTS neurons also appeared to induce Fos in non-DBH neurons; however, this effect was almost entirely restricted to more rostral portions of the NTS. In the caudal NTS, DBHNTS neuronal fibres appeared more restricted, unlike the extensive web-like network of CCKNTS neuron fibres in the same area.

CCKNTS and DBHNTS neurons directly activate CGRPPBN neurons

Because CNO-mediated activation of CCKNTS or DBHNTS neurons induced Fos expression in a sub-population of CGRPPBN neurons, we examined whether there are direct synaptic connections between the genetically defined NTS populations and CGRPPBN neurons. For these experiments, double knock-in CckCre/+::CalcaCre:GFP/+ or DbhCre/+::CalcaCre:GFP/+ mice were generated to allow visualization of the nuclear-localized Cre:GFP from the Calca locus that encodes CGRP. These mice were injected into the NTS with AAV1-DIO-synaptophysin:mCherry virus. This allowed us to visualize the close proximity of mCherry-labelled CCKNTS or DBHNTS axons with GFP-expressing, CGRP neurons in the lateral PBN (Fig. 5a). The mCherry-labelled axons of CCKNTS or DBHNTS neurons in the PBN were predominantly lateral to the CGRPPBN cell bodies where there is an extensive dendritic field27,28,29.

Figure 5
CCKNTS and DBHNTS neurons send direct, excitatory input to CGRPPBN neurons.

For electrophysiological recordings, PBN slices were obtained from double knock-in mice previously injected into the NTS with Cre-dependent AAV1-DIO-ChR2:mCherry that expresses channelrhodopsin:mCherrry fusion protein. This preparation allowed excitation within the lateral PBN of genetically identified, mCherry-labelled fibres from CCKNTS or DBHNTS neurons while recording responses from GFP-labelled CGRP neurons (Fig. 5b). Because of the dense population of CGRP neurons that reside in the hypoglossal nucleus near the NTS, we first performed control experiments and verified that injections into the NTS and hypoglossal nucleus of a CalcaCre:GFP/+ mouse did not label any projections to the PBN. Recording the activity of GFP-labelled CGRPPBN neurons in slices from these mice revealed that they are intrinsically active with a low firing frequency (2.4±0.45 Hz, n=23), resting membrane potential of −71.3±1.1 mV and a high input resistance (1.12±0.11 GΩ, n=23). Photoactivation of nearby ChR2:mCherry fibres from CCKNTS or DBHNTS neurons induced action potentials (Fig. 5c,d) demonstrating that both inputs can efficiently activate CGRPPBN neurons. Indeed, 2- to 5-ms pulses of blue light elicited excitatory currents in CGRPPBN neurons from both inputs with millisecond latency (range 4–6 ms) and sub-millisecond jitter (0.23±0.036 and 0.22±0.028 ms for CCK, and DBH inputs, respectively; Fig. 5e–g), both indicative of monosynaptic connections30,31. Synaptic currents (amplitude 53±10.1 and 21.6±4.5 pA for CCK, and DBH inputs, respectively, MP=−80 mV) from both inputs were completely abolished by inhibitors of AMPA and NMDA receptors (Fig. 5h–j); thus, revealing glutamate as a principle transmitter at these synapses. These results support previous observations that ~80% of DBHNTS neurons are glutamatergic and that the majority of NTS to PBN transmission is via excitatory, glutamatergic neurons5,32. Of 52 patch-clamped CGRP neurons from 17 CckCre/+::CalcaCre:GFP/+ mice and 14 DbhCre/+::CalcaCre:GFP/+ mice, 12 responded to photoactivation of either input, suggesting that only a subset of CGRPPBN neurons receive innervations from CCKNTS or DBHNTS neurons. Altogether, these data demonstrate that appetite-suppressing CGRPPBN neurons7 are directly activated by glutamatergic CCKNTS and DBHNTS neurons.

NTS to PBN axon stimulation decreases food intake

Because CCKNTS and DBHNTS neurons send axonal projections to several brain regions, it was important to determine whether the projection to the PBN could be responsible for the suppression of food intake. CckCre/+ or DbhCre/+ mice were injected with AAV1-DIO-ChR2:mCherry or the control AAV-DIO-mCherry virus and fibre optic ferrules were placed above the lateral PBN (Fig. 6a). At least 3 weeks after viral injection, the mice were connected to a blue laser and either exposed to no stimulation (light off) or PBN terminals were photoactivated (30 Hz, 10 ms pulses, 1 s stimulation every 5 s) for 2.5 h starting 30 min before lights out. In previous studies, 30 Hz stimulation of CGRPPBN neurons expressing ChR2 was sufficient to produce significant effects on feeding7,33 and induce expression of Fos7. In both CckCre/+ and DbhCre/+ mice, a significant decrease in food consumption was observed by both groups of ChR2-expressing mice during fibre stimulation within the PBN, when compared with their non-stimulated baseline intake or when compared with controls expressing only mCherry (Fig. 6b,c).

Figure 6
Activation of CCKNTS and DBHNTS axon terminals in the PBN suppresses food intake.

Photostimulation of ChR2-expressing terminals within the lateral PBN inhibited feeding; however, we cannot rule out the occurrence of antidromic action potentials activating cell bodies of the NTS neurons, which may then activate axon collaterals projecting to other brain regions. Indirect evidence suggests this is unlikely since low levels of Fos immunoreactivity were observed in NTS sections following 2 h of PBN stimulation in either CckCre/+ or DbhCre/+ mice expressing ChR2 (average per slice: 9.9±1.8 and 16.9±4.4 for CckCre/+ and DbhCre/+ mice, respectively, n=3 sections each from three animals per group); see Fig. 4 for background levels of Fos expression and the effects of direct activation of these NTS neurons.


Our study extends the neural network for anorexia by providing new insights into specific neuronal circuitry between the NTS and the PBN that suppresses appetite. Using electrophysiology coupled with optogenetics, we demonstrate direct excitatory connections from both CCKNTS and DBHNTS neurons onto CGRPPBN neurons that have been shown to promote anorexia7. In vitro, these connections were capable of inducing action potentials in downstream CGRPPBN neurons. Using chemogenetic (DREADD) and optogenetic (ChR2) approaches to selectively activate either CCKNTS or DBHNTS neurons or their terminals within the PBN in vivo, we establish that activation of either NTS population can decrease food intake. Because both populations of NTS neurons are activated by consumption of a large meal, our combined results suggest that they relay satiation signals from the gut to forebrain via CGRPPBN neurons.

Activation of either CCKNTS or DBHNTS neurons with hM3Dq and CNO decreased feeding and induced Fos expression in CGRPPBN neurons as well as neurons in the CeA and BNST that are known to be downstream targets of CGRPPBN neurons7. Inactivation of CGRPPBN neurons with tetanus toxin mitigates the anorexigenic responses to i.p. injections of CCK, the glucagon-like peptide-1 (GLP-1) agonist exendin 4, or leptin26. Altogether, these observations provide compelling evidence that the CCKNTS- and DBHNTS-to-CGRPPBN pathways are among those that relay viscerosensory signals and promote satiation. There may be cross talk between NTS neuron populations that are activated by visceral input because hM3Dq-mediated activation of CCKNTS neurons induces Fos not only in CCK neurons but also in neighbouring neurons, including DBHNTS neurons.

The robust inhibition of food intake we observed in hM3Dq-expressing animals lasted 4–6 h when giving CNO injections twice daily with little difference in 24-h food intake. A single injection of CNO has variable duration peaking between 5 and 50 min and lasting between 1 and 9 h (refs 34, 35). The mice apparently compensated for the decreased food intake that occurred during the first few hours after CNO injection by ingesting greater amounts of food once the effect of CNO subsided. Although 24-h food intake was not affected, activation of either CCKNTS or DBHNTS neurons induced a modest, but significant, decrease in body weight. In addition to processing viscerosensory signals from the gut and relaying them to forebrain nuclei to inhibit feeding, these NTS neurons presumably influence energy expenditure. Therefore, activating CCKNTS or DBHNTS neurons in response to a large meal signals energy availability and promotes energy expenditure possibly via connections to the sympathetic nervous system36,37.

We demonstrate an important role for two genetically distinct NTS neurons in appetite suppression and provide evidence for a direct and functional connection with the lateral PBN. However, there are additional neuronal populations in the NTS that send projections to the PBN4. Therefore, the CCKNTS and DBHNTS projections to the CGRPPBN neurons likely represent a subset of functionally relevant NTS projections to the PBN that mediate food intake. The NTS is a highly heterogeneous region containing multiple cell types. Just as in our refeeding study, many of the NTS neurons activated by gut distention, satiety hormones or anorexigenic agents are molecularly undefined38,39,40,41. A few other NTS cell types have been shown to affect feeding behaviour. For example, acute activation of pro-opiomelanocortin (POMC)-expressing neurons in the NTS using CNO and hM3Dq expression inhibits baseline feeding42. Increasing meal size or doses of the satiety hormone CCK activates increasing numbers of Fos-positive GLP-1- and prolactin-releasing peptide (PrRP)-expressing neurons in the NTS, suggesting that they may also relay satiation signals17,18. The presence of ghrelin and leptin receptors on multiple neuron populations in the NTS also suggests a role for NTS signalling in control of food intake8,43,44. There is notable overlap of neuropeptide expression within the NTS. For example, some NTS neurons expressing GLP-1 also express CCK and vice versa8. The majority of DBHNTS neurons also co-express PrRP18,45. GLP-1 neurons also co-express somatostatin and met-enkephalin, but they appear to be distinct from A2, DBHNTS neurons19,46,47.

The rodent PBN relays a wide variety of sensory signals (including taste, temperature, pain and visceral malaise) to forebrain nuclei2,3,6,7. The CGRPPBN neurons appear to mediate conditions that threaten homoeostasis, ranging from mild satiation in response to a large meal, to visceral malaise due to nausea or inflammation, to pain produced by heat or foot shock7,33,48,49. Only a quarter of CGRP neurons tested responded to photostimulation of either CCKNTS or DBHNTS inputs. While this is consistent with a functionally specialized sub-population of these neurons, their relatively small fraction can also be explained by either insufficient expression of ChR2 in terminals, variability of light intensity in the slice or reduction of dendrites and axons during slice preparation. These experimental constraints imply that the actual number of CGRP neurons receiving CCK and DBH inputs is likely to be higher. Robust photoactivation of all CGRPPBN neurons promotes freezing behaviour49. Our optogenetic and chemogenetic stimulation paradigms involving only CCKNTS- and DBHNTS-targeted CGRPPBN neurons did not induce freezing behaviour; likewise, chemogenetic activation did not produce anxiety as measured by the open-field test, suggesting that the NTS to PBN circuit examined here does not relay aversive signals.

NTS neurons communicate viscerosensory information to the PBN as one important pathway in appetite suppression; however, they also project axons to other brain regions that have been implicated in modulating food intake9,50,51,52. CCKNTS and DBHNTS neurons are known to project to brain regions where we observed Fos induction; consequently, signalling in those brain regions may also modulate feeding. Our data add to the growing recognition of multiple genetically identified neural circuits that influence feeding behaviour. An understanding of these circuits and their interactions will undoubtedly open up new avenues for therapeutic intervention for a number of metabolic and feeding disorders. While we cannot determine whether disruptions in CCKNTS or DBHNTS neurons specifically contribute to pathology in humans, it is abundantly clear that disruption of normal signalling of either CCK or noradrenergic systems as a whole can promote feeding-related disorders. For example, polymorphisms in either CCK, or its receptor (CCK-1R) or β2-adrenoceptor genes have been linked to obesity and type 2 diabetes in humans53,54,55,56,57,58. We speculate that mutations in genes expressed in the neural circuit that we describe here may contribute to maladaptive eating patterns.



All animals were heterozygous male mice group housed before stereotaxic surgery and maintained on a 12-h light/dark cycle with ad libitum access to rodent diet (Picolab, #5053) unless otherwise stated. For behavioural testing, 3- to 5-month-old animals were individually housed 1 week before habituation in Biodaq cages. Mouse lines used were DbhIRES-Cre/+, with IRES-Cre targeted to a site just downstream of the termination codon in the last exon (provided by Dr. Steven Thomas at University of Pennsylvania), CckIRES-Cre/+ (Jackson laboratory, CckTM1.1(cre)Zjh/J)59; and CalcaCre:GFP mice (generated by Dr. Richard Palmiter at the University of Washington)7; all mouse lines were backcrossed to C57BL/6 mice for >6 generations. For electrophysiology studies, either DbhCre/Cre or CckCre/Cre homozygous mice were bred with CalcaCre:GFP/Cre:GFPhomozygous mice (Jackson laboratory Calcatm1.1(cre/EGFP)Rpa)7. This breeding paradigm yielded double knock-in mice that were heterozygous for each allele. All animal experiments were approved by the University of Washington Institutional Animal Care and Use Committee (IACUC).

Virus production

Cre-dependent pAAV-Ef1α-DIO-YFP, pAAV-Ef1α-DIO-mCherry and pAAV-Ef1α-DIO-ChR2:mCherry plasmids were provided by K. Deisseroth and Cre-dependent pAAV-hSyn-DIO-hM3Dq:mCherry DNA plasmid was provided by B. Roth. pAAV1-Ef1α-DIO-synaptophysin:mCherry plasmid was generated from pAAV-Ef1α-DIO-synaptophysin:GFP7 by replacing the GFP fragment with mCherry. Viruses were prepared in our laboratory using serotype 1 helper plasmid by transfecting HEK293 cells, purifying lysates through a series of sucrose and CsCl ultracentifugation steps and dialysis. Final pellets were suspended in 0.1 M phosphate-buffered saline (PBS) at a titre of approximately 2 × 109 particles per μl.

Stereotaxic surgery

Mice were anaesthetised with isoflurane vapour and secured in a stereotaxic frame (David Kopf Instruments). The head of the animal was tilted nose up by 10 degrees. After incision, the skull was exposed and two drill holes were created at the following coordinates from bregma (anteroposterior −6.38 mm, medial lateral: ±0.4 mm). A 5 μl Hamilton syringe with a 32-gauge needle was then inserted into each drill hole and lowered down −7.1 mm from bregma. Virus (300 nl) was injected at a rate of 150 nl min-1. After 5 min, the needle was retracted and the incision was closed with sterile suture. In mice used for in vivo optogenetic experiments two fibre optic cannulae (Doric Lenses) were implanted above the lateral PBN (anteroposterior:−5.1 mm, medial lateral: ±1.7 mm, dorsal ventral: 3.0 mm) and affixed to the skull using Metabond (Parkell) and dental cement.

Slice optogenetics and electrophysiology

After allowing at least 2 weeks after surgery for viral expression, 8- to 20-week-old male mice were used for in vitro slice electrophysiology recordings 3–4 h after the start of the light cycle. Because stress-released hormones can modify neuronal networks and thus affect our observations, we handled mice with special precautions by deeply anaesthetizing them with isoflurane in their housing room before decapitation. Brains were quickly removed into ice-cold sucrose cutting solution (in mM: 11 D-glucose, 234 sucrose, 2.5 KCl, 1.25 NaH2PO4, 5 MgCl2, 0.2 CaCl2, 26 NaHCO3) continuously aerated with carbogen gas mixture (5% CO2, 95% O2). Coronal 200–250-μm thick slices were cut from NTS and PBN regions by a Leica TV1000S vibratome in ice-cold cutting solution and transferred for recovery to recording artificial cerebrospinal fluid (ACSF, in mM: NaCl 115, KCl 3, CaCl2 2, MgCl2 1, NaH2PO4 1, NaHCO3 25 and D-glucose 11; osm 295, pH 7.4 when aerated with carbogen) for 30 min at 33 °C. They were kept in the same carbogen-aerated solution at room temperature for at least 1 h before recordings. The recording chamber was perfused with carbogenated 33 °C ACSF at a rate of 1.5–2 ml min−1. CCKNTS or DBHNTS neurons and axons were identified by mCherry expression and CGRP neurons were identified by nuclear GFP expression using a Nikon ECLIPSE FN1 microscope, NIR Apo 40 × /0.8N.A. objective, Photometrics CoolSNAP ES2 camera. Because GFP and ChR2 have overlapping excitation spectra, GFP imaging can also result in unwanted ChR2 activation and transmitter release. To avoid this, we imaged GFP under conditions of globally inhibited synaptic transmission in ACSF with a high Mg2+/Ca2+ ratio and low Ca2+ (5 mM Mg2+and 0.1 mM Ca2+). Visually-guided patching was performed with the oblique LED illumination technique60,61 and IR-LED emitting 850-nm light positioned at 23–25o near the meniscus. Patch pipettes were of 4–5 MΩ resistance when filled with intracellular solution (in mM: 100 Cs-methanosulfonate, 25 CsCl, 2 MgCl2, 10 HEPES, 0.4 EGTA, 4 ATP, 0.4 GTP, 10 phosphocreatine, mosm 295, pH 7.3). Resting membrane potential was measured immediately after forming whole-cell patch corresponding to a holding potential of 0 and corrected for liquid junction potential. Cell-input resistance was calculated based on steady-state holding current required for hyperpolarizing 5 mV/200 ms step from the resting membrane potential and recordings were rejected if the access resistance exceeded 20 MΩ. Synaptic currents were evoked by optical activation of ChR2 with 2- to 5-ms pulses of blue light (up to 3 mW optic power) either from a 473 nm laser (LaserGLOW), or an optic fibre positioned over the slice or from a high power 460 nm LED (UHP-LED, Prizmatix) and microscope objective. The same energy light pulses did not elicit any activity in CGRP neurons from mice not expressing ChR2, thus excluding a possibility of non-specific, heat-evoked responses under our conditions. Synaptic latency was measured as the time between onset of blue-light pulse and the onset of synaptic current. Synaptic jitter was calculated as a standard deviation in variation of synaptic latency over multiple trials (25–50) in a particular neuron. Currents were elicited at 10-s intervals between successive trials, recorded in 2–5 kHz bandwidth (A-M System patch-clamp amplifier), digitized at 20 kHz (Digidata 1440A, Molecular Devices) and acquired by pCLAMP10 software (Molecular Devices).

To test the effect of CNO on hM3Dq and mCherry-expressing cells, CNO was applied via superfusion in the presence of 20 μM CNQX, 100 μM D-AP5 and 100 μM picrotoxin. A glass tube (400 μm diameter) filled with extracellular ACSF plus inhibitors and 3 μM CNO was positioned over a slice just before superfusion and CNO was delivered to the slice by gravity for ~30–40 s. Spiking was recorded in cell-attached configuration to be minimally invasive and preserve G-protein signal-transduction. The recording patch-pipette was filled with extracellular ACSF and spikes were loose-patch recorded at 0 holding current. The effect of CNO was measured for 30 s as the fold change in spiking rate was relative to the basal frequency before CNO. When indicated, AMPA and NMDA glutamate receptors were inhibited by a cocktail of CNQX (20 μM, Tocris) and D-AP5 (100 μM, Tocris) added to ACSF, and GABAA receptors were inhibited by picrotoxin (100 μM, Tocris).

Food intake measurements

For non-food-restricted intake measurements, animals were individually housed in BioDAQ cages (Research Diets, Inc.) to continuously measure food intake. After 1 week habituation to the cages and food (Research Diets, Inc. D12450B), animals were injected with saline for 3 days before being injected with CNO (0.8 mg per kg body weight, i.p., Tocris) twice daily for 4 days. The two injections were given 30 min before lights out and 4 h after the onset of the light cycle. Daily body weight was measured for all animals 30 min before lights out.

For the food-restriction assay, animals were weighed daily and the amount of food was adjusted to bring animals to 85–90% of their pre-restriction body weight. Once animals were at 85–90% body weight, they were also given 0.3 g of the test diet (Bio-Serve dustless pellets, F0071) for 3 days to prevent neophobia during testing. This diet was chosen over normal chow as it allows for more accurate measurements. One day before testing, animals were injected with saline and placed into a new clean cage for 1 h. On test day 1 during the light cycle, animals were randomly given either saline or CNO (0.8 mg kg−1, i.p.) and placed into a clean cage 45 min before given access to 2 g of the test diet for 1 h after which food intake was measured and animals were returned to their home cages. On test day 2, the same procedure was repeated except that animals previously tested with CNO were given saline and vice versa.

For the fasting refeeding experiments, mice were fasted for 18 h. Mice in the refed group were given normal chow for 2 h (controls had no food). Animals were perfused at the end of the 2-h feeding period and food intake was measured.

In vivo optogenetics

All animals were injected with both ChR2 and hM3Dq viruses. Animals were pre-screened for the ability of CNO to decrease baseline food intake greater than 40% at 2 and 4 h after lights out. Prescreening was performed to insure correct viral targeting to the NTS before optogenetic experiments were performed; approximately 60% of mice passed this screen. Animals were next acclimated to the fibre optic cables and feeding paradigm on the night before testing. On subsequent nights, animals were attached to fibre optic cables and all food was removed from the cage 2 h before lights out. At lights out, food was returned and measured again 2 h later. For baseline feeding (2 days) no stimulation occurred. 2-h non-stimulated baseline intake was not different between groups (Control group: 0.7±0.08 g; ChR2 group: 0.8±0.06 g). On the third day, blue light (473 nm) was delivered in 10-ms pulses at 30 Hz for 1 s every 5 s starting at 30 min before lights out and ending when food consumption was measured 2.5 h later.

Open-field testing

Open-field testing was performed after mice had at least 5 days of ad libitum access to normal chow. One day before testing, animals were given an injection of saline equal to the volume of CNO to be given (0.8 mg kg−1 i.p.). The following day all mice were given CNO (0.8 mg kg−1 i.p.) 45 min before being placed in the outer circumference of a circular open-field arena and allowed to move freely for 10 min. The open field is a circular polypropylene container 42-cm in diameter with 36-cm high walls. The sessions were captured digitally and the amount of time animals spent in the centre of the field (denoted as a virtual circle 14.5 cm in diameter in the centre of the field) as well as velocity and distance travelled were measured using Ethovision software (Noldus).


Three hours after CNO injections (0.8 mg kg−1) mice were anaesthetised with pentobarbital and perfused transcardially with PBS followed by 4% paraformaldehyde in PBS. Brains were extracted, post-fixed overnight and protected in 30% sucrose dissolved in PBS for cryosectioning (30-μm sections). Sections were collected in cold PBS.

Brain sections were permeabilized with 0.2% Triton X-100 (PBST) for 30 min and treated with a blocking solution containing PBST and 3% normal donkey serum (Jackson Immunoresearch) for 1 h at room temperature. Sections were incubated overnight at 4 °C in block solution containing goat polyclonal Fos antibody (1:500; Santa Cruz Biotech, sc-52) and either rabbit polyclonal DsRed antibody (1:1,000; Clontech, #632496) rabbit polyclonal tyrosine hydroxylase antibody (1:1,000; Millipore, AB152) or mouse monoclonal CGRP antibody (1:5,000; Abcam, ab81887). For fasting refeeding experiments, Chicken GFP antibody (1:10,000 Abcam, ab13970) was also used in the same sections. To visualize nuclei of CGRP neurons in the PBN of CalcaCRE:GFP/+ mice, a rabbit polyclonal green fluorescent protein antibody (1:1,000; Life Technologies, A11122) was used. After primary antibody incubation and washes in PBS, sections were incubated in Cy5-cojugated, donkey anti-goat IgG, Alexa Fluor 594 donkey anti-rabbit IgG, and/or either Alexa Fluor 488 donkey anti-rabbit IgG or Alexa Fluor 488 donkey anti-chicken IgG (1:500; Jackson Immunoresearch) in block solution for 2 h at room temperature. Finally, sections were washed in PBS, mounted onto glass slides, and coverslipped with DAPI Fluromount-G (Southern Biotech, 0100-290) before image acquisition.

Quantification of Fos was performed bilaterally on every 6th section in the following areas: in the NTS from bregma −6.96 to −7.9 mm; PBN from bregma −4.9 to −5.45 mm (four sections from each area per mouse); amygdala from bregma −1.2 to −1.75 mm (approximately three sections per mouse) and on every third section in the BNST from bregma −0.2 to +0.1 mm (three sections per mouse). Images were collected on either a Nikon upright epifluorescent microscope with a QImaging Camera or a laser-scanning Olympus FV1200 confocal microscope. For co-localization, z-series images were taken and counts were performed from collapsed images generated in FV−10 Ver. 4.0a viewer.


Data were analysed using Prism 5.0 (GraphPad Software). Two animals were excluded from data analysis because post hoc histological analysis revealed no viral transduction as indicated by mCherry fluorescence. One animal was excluded from data analysis because post hoc histological analysis revealed fibre optic cannulae placement was anterior to the PBN. Figures were prepared using Photoshop and Illustrator CS5 (Adobe Systems).

Data availability

Detailed statistics and data that support the findings of this study are available from the corresponding author on request.

Additional information

How to cite this article: Roman, C. W. et al. Genetically and functionally defined NTS to PBN brain circuits mediating anorexia. Nat. Commun. 7:11905 doi: 10.1038/ncomms11905 (2016).

Supplementary Material

Supplementary Information:

Supplementary Figures 1-6


We thank Dr Steven Thomas for providing the DbhCre/+ mouse line, Drs B. Roth and K. Deisseroth for plasmids, M. Chiang for mouse husbandry, Drs M. Carter, S. Han, and M. Patterson for suggestions and technical advice as well as colleagues from the Palmiter laboratory for feedback and advice. This work was supported by the National Institutes of Health grants T32DK007247 (CWR) and R01-DA24908 (RDP).


Author contributions R.D.P. and C.W.R. conceived and designed the study with an input from V.A.D. C.W.R. performed and analysed all behavioural and immunohistological experiments. V.A.D. obtained and analysed electrophysiology data. C.W.R., R.D.P. and V.A.D. wrote the manuscript.


  • Ritter R. C. Gastrointestinal mechanisms of satiation for food. Physiol. Behav. 81, 249–273 (2004). [PubMed]
  • Becskei C., Grabler V., Edwards G. L., Riediger T. & Lutz T. A. Lesion of the lateral parabrachial nucleus attenuates the anorectic effect of peripheral amylin and CCK. Brain Res. 1162, 76–84 (2007). [PubMed]
  • de Araujo I. E. Gustatory and homeostatic functions of the rodent parabrachial nucleus. Ann. NY Acad. Sci. 1170, 383–391 (2009). [PubMed]
  • Herbert H. & Saper C. B. Cholecystokinin-, galanin-, and corticotropin-releasing factor-like immunoreactive projections from the nucleus of the solitary tract to the parabrachial nucleus in the rat. J. Comp. Neurol. 293, 581–598 (1990). [PubMed]
  • Jhamandas J. H. & Harris K. H. Excitatory amino acids may mediate nucleus tractus solitarius input to rat parabrachial neurons. Am. J. Physiol. 263, R324–R330 (1992). [PubMed]
  • Wu Q., Clark M. S. & Palmiter R. D. Deciphering a neuronal circuit that mediates appetite. Nature 483, 594–597 (2012). [PMC free article] [PubMed]
  • Carter M. E., Soden M. E., Zweifel L. S. & Palmiter R. D. Genetic identification of a neural circuit that suppresses appetite. Nature 503, 111–114 (2013). [PMC free article] [PubMed]
  • Garfield A. S. et al. Neurochemical characterization of body weight-regulating leptin receptor neurons in the nucleus of the solitary tract. Endocrinology 153, 4600–4607 (2012). [PMC free article] [PubMed]
  • Rinaman L. Ascending projections from the caudal visceral nucleus of the solitary tract to brain regions involved in food intake and energy expenditure. Brain Res. 1350, 18–34 (2010). [PMC free article] [PubMed]
  • Hisadome K., Reimann F., Gribble F. M. & Trapp S. CCK stimulation of GLP-1 neurons involves alpha1-adrenoceptor-mediated increase in glutamatergic synaptic inputs. Diabetes 60, 2701–2709 (2011). [PMC free article] [PubMed]
  • Altschuler S. M., Bao X. M., Bieger D., Hopkins D. A. & Miselis R. R. Viscerotopic representation of the upper alimentary tract in the rat: sensory ganglia and nuclei of the solitary and spinal trigeminal tracts. J. Comp. Neurol. 283, 248–268 (1989). [PubMed]
  • Shapiro R. E. & Miselis R. R. The central organization of the vagus nerve innervating the stomach of the rat. J. Comp. Neurol. 238, 473–488 (1985). [PubMed]
  • Moran T. H. & Schwartz G. J. Neurobiology of cholecystokinin. Crit. Rev. Neurobiol. 9, 1–28 (1994). [PubMed]
  • Della Fera M. A. & Baile C. A. CCK-octapeptide injected in CSF causes satiety in sheep. Ann. Rech. Vet. 10, 234–236 (1979). [PubMed]
  • Schick R. R., Harty G. J., Yaksh T. L. & Go V. L. Sites in the brain at which cholecystokinin octapeptide (CCK-8) acts to suppress feeding in rats: a mapping study. Neuropharmacology 29, 109–118 (1990). [PubMed]
  • Wellman P. J. Norepinephrine and the control of food intake. Nutrition 16, 837–842 (2000). [PubMed]
  • Maniscalco J. W. & Rinaman L. Overnight food deprivation markedly attenuates hindbrain noradrenergic, glucagon-like peptide-1, and hypothalamic neural responses to exogenous cholecystokinin in male rats. Physiol. Behav. 121, 35–42 (2013). [PMC free article] [PubMed]
  • Kreisler A. D., Davis E. A. & Rinaman L. Differential activation of chemically identified neurons in the caudal nucleus of the solitary tract in non-entrained rats after intake of satiating vs. non-satiating meals. Physiol. Behav. 136, 47–54 (2014). [PMC free article] [PubMed]
  • Rinaman L. Hindbrain noradrenergic lesions attenuate anorexia and alter central cFos expression in rats after gastric viscerosensory stimulation. J. Neurosci. 23, 10084–10092 (2003). [PubMed]
  • Rinaman L. & Dzmura V. Experimental dissociation of neural circuits underlying conditioned avoidance and hypophagic responses to lithium chloride. Am. J. Physiol. Regul. Integr. Comp. Physiol. 293, R1495–R1503 (2007). [PubMed]
  • Kawai Y., Takagi H., Yanai K. & Tohyama M. Adrenergic projection from the caudal part of the nucleus of the tractus solitarius to the parabrachial nucleus in the rat: immunocytochemical study combined with a retrograde tracing method. Brain Res. 459, 369–372 (1988). [PubMed]
  • Kawai Y., Takagi H. & Tohyama M. Co-localization of neurotensin- and cholecystokinin-like immunoreactivities in catecholamine neurons in the rat dorsomedial medulla. Neuroscience 24, 227–236 (1988). [PubMed]
  • Rinaman L. Hindbrain noradrenergic A2 neurons: diverse roles in autonomic, endocrine, cognitive, and behavioral functions. Am. J. Physiol. Regul. Integr. Comp. Physiol. 300, R222–R235 (2011). [PubMed]
  • Armbruster B. N., Li X., Pausch M. H., Herlitze S. & Roth B. L. Evolving the lock to fit the key to create a family of G protein-coupled receptors potently activated by an inert ligand. Proc. Natl Acad. Sci. USA 104, 5163–5168 (2007). [PubMed]
  • Urban D. J. & Roth B. L. DREADDs (designer receptors exclusively activated by designer drugs): chemogenetic tools with therapeutic utility. Annu. Rev. Pharmacol. Toxicol. 55, 399–417 (2015). [PubMed]
  • Campos C. A., Bowen A. J., Schwartz M. W. & Palmiter R. D. Parabrachial CGRP neuronscontrol meal termination. Cell Metab. 23, 811–820 (2016). [PMC free article] [PubMed]
  • Herbert H. & Bellintani-Guardia B. Morphology and dendritic domains of neurons in the lateral parabrachial nucleus of the rat. J. Comp. Neurol. 354, 377–394 (1995). [PubMed]
  • Milner T. A. & Pickel V. M. Ultrastructural localization and afferent sources of substance P in the rat parabrachial region. Neuroscience 17, 687–707 (1986). [PubMed]
  • Takeuchi Y., McLean J. H. & Hopkins D. A. Reciprocal connections between the amygdala and parabrachial nuclei: ultrastructural demonstration by degeneration and axonal transport of horseradish peroxidase in the cat. Brain Res. 239, 583–588 (1982). [PubMed]
  • Appleyard S. M. et al. Visceral afferents directly activate catecholamine neurons in the solitary tract nucleus. J. Neurosci. 27, 13292–13302 (2007). [PubMed]
  • Doyle M. W. & Andresen M. C. Reliability of monosynaptic sensory transmission in brain stem neurons in vitro. J. Neurophysiol. 85, 2213–2223 (2001). [PubMed]
  • Stornetta R. L., Sevigny C. P. & Guyenet P. G. Vesicular glutamate transporter DNPI/VGLUT2 mRNA is present in C1 and several other groups of brainstem catecholaminergic neurons. J. Comp. Neurol. 444, 191–206 (2002). [PubMed]
  • Carter M. E., Han S. & Palmiter R. D. Parabrachial calcitonin gene-related peptide neurons mediate conditioned taste aversion. J. Neurosci. 35, 4582–4586 (2015). [PMC free article] [PubMed]
  • Agulhon C. et al. Modulation of the autonomic nervous system and behaviour by acute glial cell Gq protein-coupled receptor activation in vivo. J. Physiol. 591, 5599–5609 (2013). [PubMed]
  • Alexander G. M. et al. Remote control of neuronal activity in transgenic mice expressing evolved G protein-coupled receptors. Neuron 63, 27–39 (2009). [PMC free article] [PubMed]
  • Bamshad M., Song C. K. & Bartness T. J. CNS origins of the sympathetic nervous system outflow to brown adipose tissue. Am. J. Physiol. 276, R1569–R1578 (1999). [PubMed]
  • Llewellyn-Smith I. J. et al. Spinally projecting preproglucagon axons preferentially innervate sympathetic preganglionic neurons. Neuroscience 284, 872–887 (2015). [PMC free article] [PubMed]
  • Lam D. D. et al. Distribution and neurochemical characterization of neurons within the nucleus of the solitary tract responsive to serotonin agonist-induced hypophagia. Behav. Brain Res. 196, 139–143 (2009). [PMC free article] [PubMed]
  • Li A. J., Wang Q., Davis H., Wang R. & Ritter S. Orexin-A enhances feeding in male rats by activating hindbrain catecholamine neurons. Am. J. Physiol. Regul. Integr. Comp. Physiol. 309, R358–R367 (2015). [PubMed]
  • Williams D. L., Schwartz M. W., Bastian L. S., Blevins J. E. & Baskin D. G. Immunocytochemistry and laser capture microdissection for real-time quantitative PCR identify hindbrain neurons activated by interaction between leptin and cholecystokinin. J. Histochem. Cytochem. 56, 285–293 (2008). [PMC free article] [PubMed]
  • Zhang X. & Fogel R. Involvement of glutamate in gastrointestinal vago-vagal reflexes initiated by gastrointestinal distention in the rat. Auton. Neurosci. 103, 19–37 (2003). [PubMed]
  • Zhan C. et al. Acute and long-term suppression of feeding behaviour by POMC neurons in the brainstem and hypothalamus, respectively. J. Neurosci. 33, 3624–3632 (2013). [PubMed]
  • Lin Y. et al. Ghrelin acts at the nucleus of the solitary tract to decrease arterial pressure in rats. Hypertension 43, 977–982 (2004). [PubMed]
  • Zigman J. M., Jones J. E., Lee C. E., Saper C. B. & Elmquist J. K. Expression of ghrelin receptor mRNA in the rat and the mouse brain. J. Comp. Neurol. 494, 528–548 (2006). [PMC free article] [PubMed]
  • Chen C., Dun S. L., Dun N. J. & Chang J. K. Prolactin-releasing peptide-immunoreactivity in A1 and A2 noradrenergic neurons of the rat medulla. Brain Res. 822, 276–279 (1999). [PubMed]
  • Sawchenko P. E., Arias C. & Bittencourt J. C. Inhibin beta, somatostatin, and enkephalin immunoreactivities coexist in caudal medullary neurons that project to the paraventricular nucleus of the hypothalamus. J. Comp. Neurol. 291, 269–280 (1990). [PubMed]
  • Larsen P. J., Tang-Christensen M., Holst J. J. & Orskov C. Distribution of glucagon-like peptide-1 and other preproglucagon-derived peptides in the rat hypothalamus and brainstem. Neuroscience 77, 257–270 (1997). [PubMed]
  • Hunt S. P. & Mantyh P. W. The molecular dynamics of pain control. Nat. Rev. Neurosci. 2, 83–91 (2001). [PubMed]
  • Han S., Soleiman M. T., Soden M. E., Zweifel L. S. & Palmiter R. D. Elucidating an affective pain circuit that creates a threat memory. Cell 162, 363–374 (2015). [PMC free article] [PubMed]
  • Katsurada K. et al. Endogenous GLP-1 acts on paraventricular nucleus to suppress feeding: projection from nucleus tractus solitarius and activation of corticotropin-releasing hormone, nesfatin-1 and oxytocin neurons. Biochem. Biophys. Res. Commun. 451, 276–281 (2014). [PubMed]
  • Romano A. et al. Hindbrain noradrenergic input to the hypothalamic PVN mediates the activation of oxytocinergic neurons induced by the satiety factor oleoylethanolamide. Am. J. Physiol. Endocrinol. Metab. 305, E1266–E1273 (2013). [PubMed]
  • D'Agostino G. et al. Appetite controlled by a cholecystokinin nucleus of the solitary tract to hypothalamus neurocircuit. Elife 5, e12225 (2016). [PMC free article] [PubMed]
  • Arya R. et al. Evidence of a novel quantitative-trait locus for obesity on chromosome 4p in Mexican Americans. Am. J. Hum. Genet. 74, 272–282 (2004). [PubMed]
  • de Krom M. et al. Common genetic variations in CCK, leptin, and leptin receptor genes are associated with specific human eating patterns. Diabetes 56, 276–280 (2007). [PubMed]
  • Marchal-Victorion S. et al. Genetic, pharmacological and functional analysis of cholecystokinin-1 and cholecystokinin-2 receptor polymorphism in type 2 diabetes and obese patients. Pharmacogenetics 12, 23–30 (2002). [PubMed]
  • Miller L. J., Holicky E. L., Ulrich C. D. & Wieben E. D. Abnormal processing of the human cholecystokinin receptor gene in association with gallstones and obesity. Gastroenterology 109, 1375–1380 (1995). [PubMed]
  • Kawaguchi H. et al. beta2- and beta3-Adrenoceptor polymorphisms relate to subsequent weight gain and blood pressure elevation in obese normotensive individuals. Hypertens. Res. 29, 951–959 (2006). [PubMed]
  • Masuo K. et al. Beta2-adrenoceptor polymorphisms relate to obesity through blunted leptin-mediated sympathetic activation. Am. J. Hypertens. 19, 1084–1091 (2006). [PubMed]
  • Taniguchi H. et al. A resource of Cre driver lines for genetic targeting of GABAergic neurons in cerebral cortex. Neuron 71, 995–1013 (2011). [PMC free article] [PubMed]
  • Safronov B. V., Pinto V. & Derkach V. A. High-resolution single-cell imaging for functional studies in the whole brain and spinal cord and thick tissue blocks using light-emitting diode illumination. J. Neurosci. Methods 164, 292–298 (2007). [PMC free article] [PubMed]
  • Santos S. F. et al. Transmission efficacy and plasticity in glutamatergic synapses formed by excitatory interneurons of the substantia gelatinosa in the rat spinal cord. PLoS ONE 4, e8047 (2009). [PMC free article] [PubMed]

Articles from Nature Communications are provided here courtesy of Nature Publishing Group