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The Journal of Neuroscience logoLink to The Journal of Neuroscience
. 2013 Jan 9;33(2):840–851. doi: 10.1523/JNEUROSCI.3215-12.2013

Neonatal Leptin Exposure Specifies Innervation of Presympathetic Hypothalamic Neurons and Improves the Metabolic Status of Leptin-Deficient Mice

Karine Bouyer 1, Richard B Simerly 1,✉
PMCID: PMC3610601  NIHMSID: NIHMS431495  PMID: 23303959

Abstract

The paraventricular nucleus of the hypothalamus (PVH) consists of distinct functional compartments regulating neuroendocrine, behavioral, and autonomic activities that are involved in the homeostatic control of energy balance. These compartments receive synaptic inputs from neurons of the arcuate nucleus of the hypothalamus (ARH) that contains orexigenic agouti-related peptide (AgRP) and anorexigenic pro-opiomelanocortin (POMC) neuropeptides. The axon outgrowth from the ARH to PVH occurs during a critical postnatal period and is influenced by the adipocyte-derived hormone leptin, which promotes its development. However, little is known about leptin's role in specifying patterns of cellular connectivity in the different compartments of the PVH. To address this question, we used retrograde and immunohistochemical labeling to evaluate neuronal inputs onto sympathetic preautonomic and neuroendocrine neurons in PVH of leptin-deficient mice (Lepob/Lepob) exposed to a postnatal leptin treatment. In adult Lepob/Lepob mice, densities of AgRP- and α-melanocortin stimulating hormone (αMSH)-immunoreactive fibers were significantly reduced in neuroendocrine compartments of the PVH, but only AgRP were reduced in all regions containing preautonomic neurons. Moreover, postnatal leptin treatment significantly increased the density of AgRP-containing fibers and peptidergic inputs onto identified preautonomic, but not onto neuroendocrine cells. Neonatal leptin treatment neither rescued αMSH inputs onto neuroendocrine neurons, nor altered cellular ratios of inhibitory and excitatory inputs. These effects were associated with attenuated body weight gain, food intake and improved physiological response to sympathetic stimuli. Together, these results provide evidence that leptin directs cell type-specific patterns of ARH peptidergic inputs onto preautonomic neurons in the PVH, which contribute to normal energy balance regulation.

Introduction

The hypothalamus is distinct in its ability to integrate humoral signals with sensory information from the environment and translate it into metabolic output through the control of neuroendocrine secretions or autonomic responses. The paraventricular nucleus of the hypothalamus (PVH) has long been recognized as a key site for such integration because of its highly organized structure consisting of functionally relevant subcompartments (Biag et al., 2012). Whereas its magnocellular and medial parvocellular parts are involved in the control of hormone secretion from the anterior pituitary, the lateral parvocellular part innervates regions of the brainstem and spinal cord that regulate the activity of autonomic neurons and provides inputs to several midbrain regions involved in coordination of a variety of goal-oriented behaviors (Swanson, 2000). In this way, information about current metabolic state is integrated, such that counter-regulatory, endocrine, autonomic, and behavioral responses are coordinated to maintain energy balance.

The arcuate nucleus of the hypothalamus (ARH) innervates a number of regions involved in regulating energy balance, and two populations of peptidergic neurons provide convergent inputs to neuroendocrine and preautonomic PVH neurons (Elias et al., 1998; Fekete et al., 2000). Orexigenic neuropeptide-Y (NPY) neurons, which coexpress agouti-related peptide (AgRP), and anorexigenic POMC neurons, which produce melanocortin peptides including α-melanocortin stimulating hormone (αMSH), play important roles in regulating food intake and glucose metabolism (Coppari et al., 2005). The adipocyte-derived hormone leptin represents a key peripheral signal that is required to maintain normal body weight. Moreover, it acts directly on NPY and POMC neurons with opposing effects on neuronal activity and gene expression to regulate energy balance (Schwartz et al., 2000; Cowley et al., 2001; van den Top et al., 2004).

In addition to its regulatory role in mature animals, leptin functions as a developmental signal during formation of ARH connectivity (Simerly, 2008). ARH projections to the PVH develop primarily between the fourth and 14th postnatal day, and leptin is required for normal development of this pathway. Projections of both ARH NPY and POMC neurons to the PVH are disrupted in Lepob/Lepob mice, and exogenous leptin treatment of neonatal, but not adult, Lepob/Lepob mice rescues these peptidergic projections (Bouret et al., 2004b). While leptin plays a central role in promoting the outgrowth of hypothalamic feeding pathways, whether it also specifies patterns of innervation to functionally distinct subcompartments of the PVH is unknown. To address this question, we labeled neuroendocrine or sympathetic preautonomic neurons in the PVH and measured the density of ARH-derived peptidergic inputs onto these identified neurons in adult mice exposed to different postnatal leptin environments. We also assessed the long-term physiological impact of postnatal leptin by evaluating different components of energy balance in these mice. The results indicate that postnatal leptin impacts peptidergic innervation of neuroendocrine and sympathetic preautonomic neurons with both cell type and target-neuron specificity, as well as effects sustained improvements in metabolic function.

Materials and Methods

Animals and treatments.

Newborn leptin-deficient mice (Lepob/Lepob) and their wild-type (WT) littermates were bred by pairing heterozygous male and female mice (The Jackson Laboratory). Litter size was adjusted to 7 pups per litter on the first postnatal day (P1) to ensure adequate and standardized nutrition until weaning. Groups of Lepob/Lepob and WT male littermates were treated daily (between 10:00 A.M. and 12:00 P.M.) with intraperitoneal injections of leptin (10 μg/g; Peprotech Inc.; Lepob/Lepob Leptin group), or vehicle alone (WT Vehicle and Lepob/Lepob Vehicle groups), starting at P4, for a total of 11 d (P4–P14). Mice from all experimental groups were weaned on P22 and maintained in mixed genotype groups until either assessment of metabolic parameters or injection of the tracer for brain neuroanatomical study.

Studies were performed in accordance with the guidelines of the National Institutes of Health and approved by the Saban Research Institute, Children's Hospital Los Angeles' Institutional Committee for the Care and Use of Animals in Research and Education.

Physiological measures.

Body weight was monitored daily from P4 to P22 (weaning) and weekly from P23 through P119 (n > 25 per group).

Food intake measurements were performed at 11 weeks of age (n ≥ 8 per group). Mice were housed individually in cages, and food consumption was measured every 12 h for 3 d from preweighted portions of food.

Glucose tolerance was performed at 6–7 weeks of age (n ≥ 9 per group). After an overnight fasting, glucose (1.5 mg/g body weight, i.p.) was injected, and blood glucose levels were measured 0, 15, 30, 45, 60, 90, 120, and 150 min following the glucose challenge. To determine insulin tolerance, 7- to 8-week-old mice (n ≥ 8 per group) were fasted for 6 h before testing. A bolus of insulin (0.75 U/kg body weight) (HumilinR, Lilly) was administered intraperitoneally, and blood glucose levels were measured 0, 15, 30, 45, 60, 90 and 120 min following the insulin challenge.

Cold challenge was performed at 9–10 weeks of age (n ≥ 8 per group). Mice were placed at 4°C in individual cages with food and water ad libitum. Core body temperature was recorded at time 0 (at the onset of cold exposure) and then every 30 min of cold exposure using a rodent rectal probe (Physitemp).

Twelve-week-old mice were injected intraperitoneally at 9:00 A.M. and 6:30 P.M. with vehicle (5 mm sodium citrate buffer, pH 4.0) or leptin (2 mg/kg; n ≥ 7 per group) according to the following scheme: vehicle injections for 3 d, followed by leptin injections for 3 d. Food intake was monitored twice daily during injection periods.

Analytical procedures.

Blood glucose levels were determined using a Glucometer (FreeStyle Lite, Abbott), and nonesterified free fatty acids (NEFA) using a colorimetric assay (Wako) (n ≥ 4 per group).

Histomorphological assessment of white adipose tissue.

Intrascapular brown adipose tissue (BAT) and epididymal white adipose tissue (WAT) fat depots were collected at 20 weeks of age (n = 4 per group), fixed in 4% paraformaldehyde solution, embedded in paraffin, cut into 8-μm-thick sections, and respectively immunostained with a perilipinA/B antibody (Sigma) or stained with hematoxylin and eosin. Representative WAT images were taken with a Zeiss LSM 710 confocal microscope with a 20× objective. Adipocyte size was determined for WAT with ImageJ software (National Institutes of Health, Bethesda, MD), measuring a minimum of 160 cells per sample.

Retrograde labeling and immunohistochemistry of brain tissue.

Retrograde labeling of the fluorescent tracer Fluorogold (FG) (2% FG; Fluorochrome) was performed under two experimental conditions as previously described (Biag et al., 2012): (1) injection in the spinal cord and (2) injection in the bloodstream intraperitoneally.

To visualize preautonomic neurons that send descending projections to innervate preganglionic sympathetic neurons in the spinal cord, injections of the retrograde tracer were centered in the intermediolateral column between thoracic vertebrae T1-T2. Alternatively, to label PVH neuroendocrine neurons, we used the permeability of the blood brain barrier at the level of the median eminence and neurohypophysis, where the neuroendocrine PVH neurons send their axon terminals. The blood brain barrier is indeed impaired in these regions, thereby allowing the uptake, retrograde transport and accumulation in cell bodies of the tracer when injected in the blood (Swanson and Kuypers, 1980). For both conditions, mice were killed at P120, and 5–8 mice were analyzed per treatment group.

At (1) 7 d or (2) 24 h following tracer injection, mice were deeply anesthetized with tribromoethanol (Sigma-Aldrich), and perfused transcardially with normal saline, followed by a 4% paraformaldehyde solution (Electron Microscopy Sciences) in 0.1 m borate buffer at pH 9.5 for 20 min. Brains were carefully dissected, postfixed for 4 h in 4% paraformaldehyde solution containing 20% sucrose, and then placed overnight in 0.02 m potassium phosphate buffer solution (KPBS) containing 20% sucrose for cryoprotection. Series of consecutive 20-μm-thick frozen sections were collected through the PVH of each brain and subsequently processed for multiple immunofluorescence detection.

Sections were blocked overnight in a solution containing 0.3% Triton X-100 in KPBS and 2% normal donkey serum or normal goat serum followed by 72 h incubation with primary antibody at 4°C with constant agitation. Sections were incubated with the appropriate secondary antibodies conjugated to Alexa Fluor (488, 568, and 647; Invitrogen Life Technologies) for 1 h at room temperature to localize the primary antibodies. To visualize peptidergic inputs onto retrogradely labeled PVH neurons, primary antibodies used were rabbit anti-AgRP (Phoenix Pharmaceuticals), sheep anti-αMSH (Millipore) and the mouse anti-HuC/D, marker of neuronal cells (Invitrogen Life Technologies). Colocalization of AgRP- and αMSH-immunoreactive inputs with the presynaptic markers synaptophysin and synapsin was performed using mouse anti-synaptophysin (Synaptic Systems) or rabbit anti-synapsin 1/2 (Synaptic Systems) antisera. Glutamatergic and GABAergic inputs onto identified soma in the PVH were visualized by using rabbit anti-vGlut2 (Synaptic Systems) and guinea-pig anti-VGAT (Synaptic Systems) antisera. The specificities of the antibodies were established by staining with heterologous primary and secondary antibodies and it was determined that there was no cross-reaction between them. All sections were mounted on gelatin-coated slides, and coverslipped using Prolong Gold Antifade mounting medium (Invitrogen Life Technologies).

Image analysis of retrogradely labeled brain sections.

Immunostained sections through the PVH were examined on a laser scanning confocal microscope (Zeiss LSM 710) equipped with a 63× (numerical aperture 1.4) oil-corrected objective and an automated optical configuration optimized for sequential visualization of each fluorescence channel. Morphological landmarks and cytoarchitectonic features (Dong, 2008; Biag et al., 2012) were used to define matched anatomical subregions of the PVH. For each tissue volume sampled, adjacent image planes through the z-axis were collected at a frequency of ∼0.4 μm through the entire thickness of the PVH. To minimize optical distortions, images were deconvolved through an iterative restoration procedure (Volocity restoration software, Improvision; PerkinElmer). Three-dimensional (3D) reconstructions of the image volumes were then prepared for each multichannel set of images using Volocity visualization software. To measure overall densities of labeled fibers in distinct regions of the PVH, images were binarized, skeletonized and the total fiber length contained in the image volume was measured using Volocity quantitation software. To resolve (1) presynaptic markers for GABA (vesicular GABA transporter) and glutamatergic terminals (vesicular glutamate transporter 2) and (2) terminals labeled for AgRP and αMSH that are apposed to soma of FG-labeled neuronal cell bodies, confocal images through the PVH were post-processed by using Volocity 3D visualization software. The density of neuronal inputs to identified PVH neurons was quantified using Volocity image analysis software. Each putative neuronal input was defined as a 3-dimensional object in direct contact (voxel to voxel apposition) with the postsynaptic target neuron labeled with Hu/CD (Movie 1). Retrogradely transported FG mainly accumulates in the lysosomal compartment (Persson and Havton, 2009). Therefore, to define the somatic borders of preautonomic or neuroendocrine neurons in the quantitation process the somatic marker HuC/D was preferred to the native FG fluorescence to avoid inaccurate delineation of the somatic compartment. Using a subtractive approach, we performed the quantification of terminals apposed to identified PVH neurons, as defined by HuC/D immunostaining, which contain the retrograde tracer FG (Movie 1). The number of peptidergic or presynaptic inputs was normalized to a set volume of somal marker (1000 μm3) and expressed as a density. This image processing routine was optimized for unambiguous identification of closely apposed nerve terminals onto PVH neurons. The accuracy of this quantitative procedure was verified by comparing it with results obtained by manual counting in a limited set of experimental material. All modules of Volocity software were run on a Mac Pro computer (Apple) supported by a dedicated high performance cluster computing system (Dell Computer) and the Imaging Computing Server utility software (Improvision).

Movie 1.
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DOI: 10.1523/JNEUROSCI.3215-12.2013.video.1
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Video of three-dimensional visualization of neuronal inputs onto identified PVH neurons. Rotating rendering of a 4-channel image stack illustrating the visualization and quantification protocol used to measure the density of neuronal inputs onto identified PVH neurons. By using Volocity image analysis software, each putative presynaptic excitatory (vGlut2, red channel) or inhibitory (VGAT, green channel) input was defined as a three-dimensional object in direct contact with the postsynaptic target neuron (magenta and cyan, respectively). The limits of the postsynaptic neuron were defined with HuC/D immunostaining (blue channel) and preautonomic neurons represent a subset of these cells that contained the retrograde tracer Fluorogold (orange channel). IML, Intermediolateral column.

Terminology.

The use of the terms “apposition,” “close contact,” or “terminal” in this article refers to histochemically labeled axonal structures that are in direct contact with a cell body that has been labeled with a specific neuronal marker (HuC/D). Labeled boutons (typically 1–3 μm in diameter) were visualized by using histochemical markers (αMSH, AgRP, VGAT, and vGlut2) and resolved as “touching objects” that are immediately adjacent to cell bodies (with no unlabeled voxel between the terminal and the cell body) in 3D reconstructions of tissue volumes, according to parameters specified in Volocity software. Although determination that a particular point of contact between an axon terminal and a target cell qualifies as a morphologically defined synapse requires ultrastructural analysis, the densities of such contacts likely reflects the overall density of neurochemically defined inputs to populations of identified neurons in the PVH. Because AgRP is colocalized with NPY in the ARH and its expression is increased in Lepob/Lepob mice, changes in AgRP immunostained terminals likely reflect changes in axon density. Changes in αMSH staining may reflect combined changes in axon density and gene expression, as discussed previously (Bouret et al., 2004b).

Statistics.

Significance was tested using Prism software (GraphPad Software Inc.). One-way ANOVA followed by a pairwise post hoc test was used to test for significant differences between experimental groups; a p value of 0.05 or less was defined as significant. The statistical significance of differences in body weight, GTT, ITT, and core temperature (cold exposure) was determined using two-way ANOVA followed by a post hoc test.

Results

Leptin specifies the peptidergic innervation of preautonomic neurons in the PVH

To determine whether feeding-related neuropeptidergic terminal fields projecting to preautonomic (PA) neuronal components of the PVH are dependent on leptin, we examined the density of AgRP- and αMSH-containing fibers in regions of the PVH that contain high densities of preautonomic neurons in adult Lepob/Lepob mice. To visualize these neurons in the PVH we injected a retrograde tracer FG into the upper thoracic level of the spinal cord (see injection site, Fig. 1A,B), which contains preganglionic sympathetic motor neurons of the intermediolateral column (Luiten et al., 1985). As previously described (Biag et al., 2012), dense clusters of FG-labeled neurons were located in the lateral hypothalamic area and in discrete components of the PVH. The highest concentrations of FG-labeled PA neurons were in the caudal two-thirds of the PVH including the dorsolateral region of the medial parvicellular compartment (PVHmpv) at the level of the PVH, posterior magnocellular part, medial zone, as well as in the caudal most part of the PVHmpv. FG-labeled PA neurons were also clustered in the dorsal parvicellular compartment of the PVH (PVHdp) (Fig. 2A). Finally, at more caudal levels, the lateral parvicellular compartment of the PVH (PVHlp), just rostral to the dorsomedial nucleus of the hypothalamus (DMH) also contained a high density of FG-labeled cells (Fig. 2A, last panel). The majority of these FG-labeled neurons were located ipsilateral to the injection site, but a few cells were also detected on the contralateral PVH.

Figure 1.

Figure 1.

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Fluorogold injection site in the thoracic spinal cord. A, Schematic overview of the thoracic level of the spinal cord. B, Illustration of a representative injection site of Fluorogold (green channel) in the intermediolateral column of the thoracic spinal cord visualized using DAPI nuclear staining (red channel).

Figure 2.

Figure 2.

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Leptin impacts the peptidergic innervation of preautonomic divisions in adult mouse PVH. A, Representative confocal images through the level of the PVH (delineated using antisera against HuC/D, red channel), illustrating the pattern of retrograde labeling following injection of Fluorogold (green channel) in the spinal cord of WT mice at the upper thoracic level (T1–T2). Preautonomic neurons were observed in the rostral and caudal aspects of the ventral medial parvicellular (rmpv and cmpv), dorsal parvicellular (dp) and lateral parvicellular (lp) parts. Outlined regions identify volumes of quantification. V3, Third ventricle. Scale bar, 100 μm. B, Quantitative comparison of the density of AgRP- and αMSH-immunoreactive fibers innervating the mpv, dp, and lp autonomic parts of the PVH in WT (n = 6), Lepob/Lepob vehicle-treated (n = 5), and Lepob/Lepob leptin-treated mice (n = 6). The values represent mean ± SEM of fiber length per set of volume sampled. Significance between groups was determined using one-way ANOVA followed by pairwise post hoc tests; ***p < 0.001, **p < 0.01, and *p < 0.05 between vehicle- or leptin-treated Lepob/Lepob mice and their WT littermates. mpv, Ventral zone of the medial parvicellular part; dp, dorsal parvicellular; lp, lateral parvicellular parts of the PVH.

AgRP-immunoreactive (AgRP-IR) fibers were not uniformly distributed in all parts of the PVH that contain PA neurons. (Fig. 2B). The highest densities of AgRP-IR fibers were in the ventral part of the PVHmpv, and in the PVHdp. Densities of AgRP-IR fibers were considerably lower in the PVHlp. In sharp contrast, the density of αMSH-IR fibers appeared to be distributed homogeneously in all autonomic regions analyzed. The density of AgRP-IR fibers was severely reduced in all regions of the PVH that contain PA neurons in adult Lepob/Lepob mice that received vehicle treatment postnatally, compared with that observed in WT littermates (Fig. 2B). In contrast to AgRP, the density of αMSH-IR fibers was only reduced in the PVHlp of Lepob/Lepob mice (Fig. 2B; densities of αMSH-IR fibers in other PA compartments sampled (mpv and dp) did not appear to be affected by leptin deficiency.

To determine whether postnatal leptin exposure could reverse the decreased densities of AgRP-IR and αMSH-IR fibers observed in Lepob/Lepob mice, neonatal Lepob/Lepob mice were treated intraperitoneally with recombinant leptin daily from P4 through P14. These exogenous postnatal leptin treatments were sufficient to significantly increase the density of AgRP-IR fibers in all PA compartments of the PVH to levels similar to those of their WT littermates (Fig. 2B). In contrast, postnatal leptin treatment did not appear to influence the densities of αMSH-IR in the regions analyzed (Fig. 2B). Thus, in keeping with earlier observations, leptin deficiency impairs the development of AgRP-containing projections from the ARH to regions of the PVH that contain PA neurons, and daily treatment with leptin during a discrete postnatal period is sufficient to rescue the density of AgRP-IR fibers in these parts of the PVH.

Although the regional analysis of changes in peptidergic fibers in regions that contain PA neurons suggest that innervation of these neurons is similarly affected, we used confocal microscopy combined with computer-assisted 3D rendering and image analysis to measure the number of AgRP- and αMSH-containing terminals that are in close apposition to FG-labeled PVH neurons. We first confirmed that such putative peptidergic inputs to PVH neurons were also immunoreactive for either synaptophysin (AgRP immunostaining) or synapsin 1/2 (αMSH immunostaining), suggesting that these points of contact do indeed represent synapses (Fig. 3A,B). The results of the analysis confirmed that the density of AgRP neuronal inputs onto identified PA neurons was decreased significantly in Lepob/Lepob mice compared with that of WT Vehicle littermates (Fig. 3C). However, the density of αMSH neuronal inputs appeared to be similar regardless of leptin levels (Fig. 3D). Furthermore, daily intraperitoneal injections of leptin to Lepob/Lepob neonates significantly increased the average number of AgRP-IR neuronal inputs onto PA neurons to levels comparable to that of WT littermates in nearly all of the PA divisions of the PVH analyzed (Fig. 3C). These changes in terminal density are not due to leptin-induced changes in cell size because the average volumes containing HuC/D- and FG-labeled (preautonomic) neurons in the PVH volumes sampled were not altered significantly by leptin deficiency (data not shown).

Figure 3.

Figure 3.

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Leptin impacts the axonal terminal densities of preautonomic divisions in adult mouse PVH. A, B, Single confocal image: plane of HuC/D, AgRP, synaptophysin (A) and HuC/D, αMSH, synapsin 1/2 (B) triple-labeled immunofluorescence at the level of the PVH of WT mouse. Arrows indicate examples of dual-labeled AgRP and synaptophysin (A), or αMSH- and synapsin 1/2-immunopositive (B) terminals in close contact with PVH soma (identified using antisera against HuC/D). Scale bar, 10 μm. C, D, Quantitative comparison of the number of AgRP (C) and αMSH-IR (D) varicosities in close apposition to spinal cord projecting neurons of the PVH in WT (n = 6), Lepob/Lepob vehicle-treated (n = 5), and Lepob/Lepob leptin-treated mice (n = 6). The values represent mean ± SEM of density of inputs. Significance between groups was determined using one-way ANOVA followed by pairwise post hoc tests; ***p < 0.001, **p < 0.01, and *p < 0.05 between vehicle- or leptin-treated Lepob/Lepob mice and their WT littermates.

Together, these observations suggest that the density of AgRP-containing inputs onto PA neurons in the PVH is dependent on leptin and that administration of leptin during the early postnatal period is sufficient to restore normal patterns of cellular innervation in Lepob/Lepob mice. Conversely, inputs to PA neurons containing melanocortin peptides appear to be leptin-independent, suggesting a cell type-specific modulation of peptidergic innervation of PA neurons by leptin during postnatal development.

Postnatal leptin exposure does not rescue peptidergic innervation of neuroendocrine neurons in the PVH

To assess whether leptin is required for normal innervation patterns to neuroendocrine (NE) neurons in the PVH, we labeled neurons with projections to regions that lack a blood–brain barrier. In the PVH, NE neurons project to the median eminence or to the posterior lobe of the pituitary and can be labeled by infusions of retrograde tracers into the blood. Injections of FG into the bloodstream of WT and Lepob/Lepob mice resulted in clusters of intensely labeled neurons in both the arcuate and supraoptic hypothalamic nuclei, as well as in several components of the PVH, as described previously (Biag et al., 2012). In these mice, FG-labeled neurons were located in the magnocellular and parvicellular components of the PVH, regions known to contain neuroendocrine neurons that project to the median eminence.

To determine whether feeding-related neuropeptidergic terminal fields projecting to neurosecretory components of the PVH are dependent on leptin, we examined the density of AgRP- and αMSH-containing fibers in two regions of the PVH that contain high densities of neurosecretory neurons: the dorsal region of the medial parvicellular dorsal (mpd) and, at more caudal levels, a region, designated here as PVHpml, composed primarily of magnocellular neurons (Fig. 4A). Although AgRP- and αMSH-immunoreactive (IR) fibers were codistributed in parts of the PVH that contain NE neurons, clear differences were apparent in their regional densities. In the PVH of both vehicle-injected WT and Lepob/Lepob mice, there were four to five times fewer αMSH-IR fibers compared with AgRP-IR fibers (Fig. 4B). In adult Lepob/Lepob mice, the density of AgRP- and αMSH-IR fibers were reduced in both the PVHmpd and PVHpml, compared with their WT littermates (Fig. 4B). Quantitative analysis of peptidergic fiber densities in regions of the PVH that contain NE neurons revealed that leptin treatment did not restore the density of AgRP- or αMSH-IR fibers in Lepob/Lepob mice levels observed in their WT littermates (Fig. 4B).

Figure 4.

Figure 4.

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Postnatal leptin exposure does not rescue peptidergic innervation of neurosecretory divisions in adult mouse PVH. A, Representative confocal images through the level of the PVH (delineated using antisera against HuC/D, red channel) illustrate the pattern of retrograde labeling following injection of Fluorogold in the blood compartment (green channel). Fluorogold labeling is observed in the medial parvicellular part, dorsal zone (mpd) and the posterior magnocellular part, lateral zone (pml) of the PVH. Outlined regions identify volumes of quantification. V3, Third ventricle. Scale bar, 100 μm. B, Quantitative comparison of the density of AgRP- and αMSH-immunoreactive fibers innervating the mpd and pml neuroendocrine parts of the PVH in WT (n = 6), Lepob/Lepob vehicle-treated (n = 5), and Lepob/Lepob leptin-treated mice (n = 6). The values represent mean ± SEM of fiber length per set of volume sampled. Significance between groups was determined using one-way ANOVA followed by pairwise post hoc tests; ***p < 0.001, **p < 0.01 and *p < 0.05 between vehicle- or leptin-treated Lepob/Lepob mice and their WT littermates.

Similar to the analysis of peptidergic innervation of PA neurons in the PVH, the dependence of cellular patterns of innervation onto neurosecretory PVH neurons was assessed by measuring densities of AgRP- and αMSH-containing nerve terminals in close apposition to NE neurons in the PVH (Fig. 5A). Consistent with the regional analysis, the density of AgRP and αMSH neuronal inputs onto NE neurons was significantly decreased in Lepob/Lepob mice compared with that of WT littermates, in both the PVHmpd and PVHpml (Fig. 5B). Moreover, neonatal leptin treatment failed to significantly increase the number of AgRP- or αMSH-IR neuronal inputs onto neurosecretory neurons in both compartments analyzed (Fig. 5B). Together, these data suggest that leptin exposure is required to maintain normal patterns of peptidergic innervation of NE neurons in the PVH. However, an early postnatal treatment with leptin is not sufficient to rescue the innervation deficit caused by leptin insufficiency.

Figure 5.

Figure 5.

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Leptin modulates neuropeptidergic terminal densities to neurosecretory neurons in the adult PVH. A, High magnification confocal images of AgRP, αMSH, FG and HuC/D immunofluorescence in the neurosecretory division of the PVH. Three-dimensional rendering view of the image volume depicting the quantification of terminal densities (AgRP, blue objects and αMSH, pink objects) in close contact with neuronal cells (HuC/D) filled with FG retrograde tracer (orange objects, right). Post-processing, reconstruction, and quantitative analyses of confocal images were performed using Improvision Volocity software. Scale bar, 20 μm. B, Quantitative comparison of AgRP- and αMSH-IR varicosities in close apposition to neurosecretory neurons of the PVH in WT (n = 6), Lepob/Lepob vehicle-treated (n = 5), and Lepob/Lepob leptin-treated mice (n = 6). The values represent mean ± SEM of number of inputs per volume analyzed. Significance between groups was determined using one-way ANOVA followed by pairwise post hoc tests; ***p < 0.001 and *p < 0.05 between vehicle- or leptin-treated Lepob/Lepob mice and their WT littermates. mpd, Medial parvicellular part, dorsal zone; pml, posterior magnocellular part, lateral zone of the PVH.

GABAergic and glutamatergic innervation of functionally identified PVH neuronal compartments is not impacted by leptin exposure

To determine whether leptin is required to maintain normal patterns of GABAergic or glutamatergic connectivity in the PVH, we compared the density of nerve terminals containing presynaptic markers for GABAergic or glutamatergic neurons within functionally distinct compartments of the PVH (e.g., neuroendocrine vs autonomic) (Fig. 6A). In contrast to the results obtained for neuropeptide-containing neurons, densities of VGAT- and vGlut2-IR terminals onto neurosecretory and preautonomic neurons displayed only minor decreases in Lepob/Lepob mice. In addition, the overall ratio of excitatory to inhibitory inputs onto neurosecretory or preautonomic neurons in the PVH was not influenced by leptin exposure during the developmental period. Furthermore, daily intraperitoneal injections of exogenous leptin to Lepob/Lepob mice from P4 to P14 only slightly decreased densities of VGAT and vGlut2 terminals onto neuroendocrine and preautonomic compartments of the PVH (Fig. 6B,C). Together, these data show that alterations of leptin availability in early development are not translated into significant changes in cellular ratios of inhibitory and excitatory synapses onto functional subpopulations of PVH neurons. It could indicate that the action of leptin occurs through a cell type-specific mechanism.

Figure 6.

Figure 6.

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GABAergic and glutamatergic innervation of functionally identified adult PVH neuronal compartments. A, Confocal images illustrating GABAergic (VGAT) and Glutamatergic (vGlut2) immunoreactive appositions on preautonomic neurons visualized by the fluorescent dye Fluorogold following spinal cord injection. Scale bar, 5 μm. B, C, Quantitative comparison of the density or ratio of vGlut2-IR over VGAT-IR terminals onto preautonomic (B) or neurosecretory (C) neurons in the PVH in WT (n = 6), Lepob/Lepob vehicle-treated (n = 5), and Lepob/Lepob leptin-treated mice (n = 6). The values represent mean ± SEM of number of inputs per volume sampled. Significance between groups was determined using one-way ANOVA followed by pairwise post hoc tests **p < 0.01, *p < 0.05 between vehicle- or leptin-treated Lepob/Lepob mice and their WT littermates. am, Anterior magnocellular part; dp, dorsal parvicellular part; f, forniceal part; mm, medial magnocellular part; mpv, medial parvicellular part, ventral zone, rostral (rmpv) and caudal aspects (cmpv); mpd, medial parvicellular part, dorsal zone; lp, lateral parvicellular part; pmm, posterior magnocellular part, medial zone; pml, posterior magnocellular part, lateral zone; pv, periventricular part of the PVH; IML, intermediolateral column; PP, posterior pituitary; ME, median eminence. Schematics are adapted from Biag et al. (2012).

Postnatal leptin treatment reduces body weight and food intake of adult Lepob/Lepob mice

To explore the long-term physiological impact of postnatal leptin exposure, leptin-deficient mice and WT littermates were treated during the postnatal period (P4–P14) with exogenous leptin (10 μg/g) (Lepob/Lepob Leptin group) or vehicle alone (WT Vehicle and Lepob/Lepob Vehicle groups) and their growth curves monitored daily from P4 to P22 (weaning) and weekly from P23 to P92. Consistent with previous reports, body weight did not differ between Lepob/Lepob and WT mice throughout the postnatal period (P4–P22). However, treatment of postnatal Lepob/Lepob mice with leptin (P4–P14) exerted a moderate but significant impact on body weight with Lepob/Lepob Leptin mice exhibiting a reduced rate of weight gain from P15 to P19, which normalized by weaning (Fig. 7A).

Figure 7.

Figure 7.

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Postnatal leptin exposure reduces body weight gain and food intake of adult leptin-deficient mice. A, B, Preweaning (A) and postweaning (B) growth curves of WT vehicle-treated (WT Veh), Lepob/Lepob vehicle-treated (Lepob/Lepob Veh), and Lepob/Lepob leptin-treated (Lepob/Lepob Lep), male mice (n > 25 per group). C–E, Food intake measurement normalized to body weight (BW) per 24 h (C) and during the light period (D) and dark period (E) of 11-week-old WT Vehicle (n = 15), Lepob/Lepob Vehicle (n = 8), and Lepob/Lepob Leptin male mice (n = 12). F, Graphical representation of the relative distribution of total food intake during the light and dark periods. #p < 0.05 between vehicle- and leptin-treated Lepob/Lepob mice. Basal glucose levels in ad libitum fed (G) or 14 h fasting (H) male WT (n = 15), Lepob/Lepob vehicle-treated (n = 9), and Lepob/Lepob leptin-treated male mice (n = 12) at 6–8 weeks of age. I, Following a bolus of glucose (intraperitoneal injection), glucose tolerance test (GTT) was analyzed in 6- to 7-week-old mice. J, Insulin tolerance test (ITT) was assessed following an insulin bolus in 7- to 8-week-old WT (n = 15), Lepob/Lepob Vehicle (n = 9), and Lepob/Lepob Leptin male mice (n = 12). All data are mean ± SEM. One-way or two-way ANOVA and pairwise post hoc tests were performed for each dependent variable. *p < 0.05, **p < 0.01, and ***p < 0.001. In A and B, only the significance between vehicle- or leptin-treated Lepob/Lepob mice is represented.

In adulthood (after P23), Lepob/Lepob leptin-treated mice remained markedly obese compared with WT littermates and by 5–6 weeks of age were significantly lighter compared with Lepob/Lepob vehicle-treated littermates (4.32% at P92). These changes in body weight persisted throughout adulthood (up to 13 weeks of age; Fig. 7B). Postnatal leptin also normalized the elevated food consumption that is characteristic of Lepob/Lepob mice (Fig. 7C). In leptin-treated Lepob/Lepob mice there were significant reductions in daily food intake, in both light and dark periods, compared with Lepob/Lepob Vehicle mice (Fig. 7D,E). Moreover, postnatal leptin normalized circadian patterns of eating, which are disrupted in Lepob/Lepob mice (Ho and Chin, 1988). Lepob/Lepob Vehicle mice ate 23.78 ± 1.76% of their food in the light period compared with 17.69 ± 0.83% for WT Vehicle mice (Fig. 7F), whereas leptin-treated mice ate 19.33 ± 1.07% during the light period suggesting that postnatal leptin exposure was able to restore the temporal distribution of meals in adulthood. Lepob/Lepob mice also display perturbations in glucose homeostasis so we performed glucose tolerance tests at P35 and insulin tolerance tests at P45 on Lepob/Lepob mice exposed to postnatal leptin. As expected, leptin-deficient mice displayed increased fasted and fed glucose levels compared with their wild-type littermates (Fig. 7G,H), but neonatal leptin treatment of Lepob/Lepob mice had no discernable effect on fasted or fed glucose levels, nor were improvements detected in either GTT or ITT in leptin-treated Lepob/Lepob mice compared with vehicle-treated controls (Fig. 7I,J).

Postnatal leptin treatment normalizes temperature regulation and adipose tissue metabolism in Lepob/Lepob mice

Because postnatal leptin treatment rescued innervation of preautonomic neurons in the PVH we evaluated whether these neuroanatomical changes were associated with a normalization of peripheral measures of autonomic function. We first assessed the ability of Lepob/Lepob mice to maintain their core body temperature when exposed to a cold environment. Lepob/Lepob mice treated postnatally with leptin displayed significantly improved maintenance of body temperature when placed in a cold environment (4°C), compared with vehicle-treated controls (Fig. 8A). This finding suggests that postnatal leptin exposure permanently improves thermoregulation, perhaps through normalization of autonomic responses to cold challenge. It is more difficult to maintain body temperature in the fasted state due to a reduction in sympathetic activity impacting brown adipose tissue. Whereas postnatally leptin-treated Lepob/Lepob mice exhibit hypothermia in an ad libitum feeding state, they performed better in maintaining their body core temperature when fasted for 14 h (Fig. 8B–D), arguing in favor of an improved sympathetic response of BAT in the leptin-treated group. Leptin-dependent improvements in BAT responses were also consistent with fat pad histology. Histomorphological analysis of epididymal WAT revealed a significant decrease in mean white adipocyte cell size in adult Lepob/Lepob mice that received postnatal leptin treatment, compared with that of Lepob/Lepob mice treated with vehicle alone (Fig. 8E top, F). Similarly, hematoxylin and eosin staining of interscapular BAT in adult Lepob/Lepob mice treated with leptin postnatally appeared smaller than those in the vehicle-treated mice (Fig. 8E, bottom). Finally, plasmatic NEFA concentrations, which represent an index of lipid mobilization, were significantly decreased in Lepob/Lepob mice that received postnatal leptin, compared with the vehicle-treated group (Fig. 8G). Together these data suggest that treatment of Lepob/Lepob mice with leptin during postnatal life enhances responses to sympathetic stimuli in adulthood, and improves sympathetic outflow.

Figure 8.

Figure 8.

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Postnatal leptin treatment improves the thermogenic response of leptin-deficient mice during a cold or a nutritional challenge. A, Core temperature during a 210 min cold challenge at +4°C of 9- to 10-week-old WT Vehicle (n = 15), Lepob/Lepob Vehicle (n = 8), and Lepob/Lepob Leptin male mice (n = 12). B, C, Basal core body temperatures of ad libitum fed (B) or 14 h fasting (C) WT Veh (n = 15), Lepob/Lepob Vehicle (n = 8), and Lepob/Lepob Leptin (n = 12) male mice at 8–10 weeks. D, Basal core temperature difference (delta temperature) between fed and fasted states. E, Representative confocal images of epididymal WAT labeled using an antisera against PerilipinA/B (top) and bright-field images of BAT stained with hematoxylin and eosin on paraffin-embedded sections (bottom) from 20-week-old WT Vehicle (n = 4), Lepob/Lepob Vehicle (n = 4), and Lepob/Lepob Leptin (n = 4) male mice. Scale bars: 50 μm for WAT and 200 μm for BAT. F, Quantification of WAT cell surface area. G, Plasma levels of NEFA at 20 weeks. All data are mean ± SEM. One-way or two-way ANOVA and pairwise post hoc tests were performed for each dependent variable. *p < 0.05, **p < 0.01, and ***p < 0.001. In A, only the significance between vehicle- or leptin-treated Lepob/Lepob mice is represented.

Postnatal leptin treatment improves leptin sensitivity of adult Lepob/Lepob mice

Hypothalamic circuits that relay leptin signals are an important component of leptin's ability to regulate food intake (Buettner et al., 2008). Therefore, if postnatal leptin is required for normal development of these pathways then Lepob/Lepob mice that receive leptin during the postnatal critical period for development of ARH projections to the PVH should be more responsive to leptin. To test this hypothesis, we examined physiological responses to low-dose leptin treatment at 12 weeks of age. Adult mice were injected twice daily with Sodium Citrate (vehicle solution) for 3 d followed by 3 d of recombinant leptin (2 mg/kg) and food intake monitored twice daily during the 2 injection periods. Lepob/Lepob mice treated with leptin during postnatal life (PN-L) appeared to be significantly more responsive to leptin in adulthood. Leptin injections reduced food intake 2.43-fold in PN-L Lepob/Lepob mice, but only 1.76-fold in vehicle-treated controls (Fig. 9A). The inhibitory effect of leptin on food intake during leptin treatment, appeared more pronounced in adult PN-L Lepob/Lepob mice compared with adult PN-V Lepob/Lepob mice, particularly after 48–72 h of leptin treatment (Fig. 9B). The enhanced ability of leptin to reduce food intake in Lepob/Lepob mice does not seem to be due to alterations in numbers of neurons in the ARH that express leptin receptors. We examined the impact of leptin deficiency on the total number of leptin receptor expressing cells in the ARH of adult Lepob/Lepob mice by evaluating numbers of GFP-labeled cells in the ARH of Lepob/Lepob mice crossed with LepR-CreRosa26 reporter mice. In the ARH, the average number of LepR-GFP neurons per hemi-section did not differ between WT-LepR-GFP mice (71.09 ± 10.10, n = 5) and Lepob/Lepob-LepR-GFP mice (84.33 ± 6.818, n = 4) (data not shown), suggesting that the alterations in leptin-sensitive pathways observed in Lepob/Lepob mice are not likely to result from an impaired number of leptin-responsive cells in the ARH.

Figure 9.

Figure 9.

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Postnatal leptin treatment increases in vivo leptin anorectic response in Lepob/Lepob mice. In vivo leptin sensitivity in adult mice exposed to different neonatal leptin environments. Twelve-week-old mice (n = 7–9 mice per group) were injected intraperitoneally twice daily with Sodium Citrate (Vehicle) for 3 d, then with leptin (2 mg/kg) for 3 d. Food intake was measured twice a day during the two injection periods. A, Average 24 h food intake during injection periods. B, Food intake following leptin treatment is represented as a percentage of inhibition versus control treatment. All data are mean ± SEM. Two-way ANOVA and pairwise post hoc test were performed for each dependent variable. *p < 0.05, **p < 0.01, ***p < 0.001.

Discussion

To accomplish the sensory-motor integration necessary for homeostatic regulation, appropriate patterns of hypothalamic connectivity must be established during development linking neurons that respond to environmental signals with neurons that control hormone secretion from the pituitary or autonomic function. ARH neurons relay metabolic signals through projections established during postnatal development. Normal formation of these pathways requires the presence of leptin which promotes outgrowth of axons during a discrete postnatal critical period (Bouret et al., 2004a,b). Here, we found that postnatal leptin also specifies cellular targeting of ARH inputs within specific regional domains of preautonomic components of the PVH and exerts heterogeneous actions on targeting AgRP- and αMSH-containing projections to the PVH. These permanent effects of leptin on patterning of ARH projections to the PVH are associated with attenuated body weight gain, reduced food intake, and improved physiological responses to sympathetic stimuli in adult Lepob/Lepob mice.

Densities of axon terminals and neuronal inputs to both neuroendocrine and preautonomic compartments are permanently reduced in Lepob/Lepob mice, demonstrating that leptin exposure is necessary for normal development of ARH-derived projections to both of these functional domains of the PVH. Surprisingly, we did not observe significant restorative effects of neonatal leptin treatment on peptidergic innervation of NE neurons, suggesting a requirement for sustained leptin action on this circuit. However, it remains to be determined whether AgRP or αMSH innervation of subpopulations of neuroendocrine neurons are uniquely impacted by leptin's developmental actions. For example, leptin may be required to specify normal densities of NPY/AgRP inputs onto TRH neurons, but not onto other cell types. It is equally likely that in addition to neonatal exposure, leptin may be required throughout adulthood to maintain peptidergic inputs onto NE neurons in the PVH in much the same way that sex steroid hormones are required in mature animals to maintain sexually dimorphic patterns of connectivity and physiological responses (Simerly, 2002; McCarthy et al., 2009).

The density of AgRP fibers was particularly high in parts of the PVH containing large numbers of preautonomic neurons, whereas POMC-derived fibers were sparsely distributed. AgRP innervation of PE neurons was dependent on postnatal leptin, similar to findings in NE compartments of the PVH. However, postnatal leptin treatment was sufficient to rescue AgRP fiber innervation densities onto preautonomic neurons to levels typical of WT mice. A surprising finding was that POMC/αMSH innervation onto preautonomic neurons appears to be relatively resistant to the developmental effects of leptin, since we observed neither a decrease in innervation of preautonomic neurons in Lepob/Lepob mice, nor any detectable increase in the density of terminals onto preautonomic neurons in animals treated with exogenous leptin. This finding is consistent with an earlier observation that reactivation of melanocortin-4 receptor (MC4-R) in SIM-1-expressing neurons does not impact energy expenditure (Balthasar et al., 2005), while reactivation of melanocortin signaling in sympathetic motor neurons reduces body weight gain and improves the energy expenditure deficit typical of MC4-R-null mice (Rossi et al., 2011). One possible explanation for the target-specific effects of leptin on POMC innervation in the PVH is that NE and PA neurons may be innervated by different subpopulations of POMC neurons. This notion is in line with several observations that indicate heterogeneity of POMC neurons. The electrophysiological properties of POMC neurons in response to glucose, insulin and leptin are not uniform in the ARH (Ibrahim et al., 2003; Parton et al., 2007; Williams et al., 2010) and diversity in their neurotransmitter phenotype has also been reported (Hentges et al., 2009). In addition, a detailed characterization of NPY and POMC neuronal lineages revealed that a subpopulation of POMC precursors give rise to other mature cell types, including a subpopulation of NPY neurons (Padilla et al., 2010). Thus, both the cell type and target-specific sensitivity to the developmental actions of leptin may reflect differences in neurotrophic responses of each subpopulation of neurons that are directed toward specific neuronal targets in the PVH. Whether target-specific differences in developmental sensitivity to leptin are due to cell type-specific signaling pathways coupled to leptin receptors, as was reported for the neurotrophic actions of leptin on NPY and POMC neurons (Bouret et al., 2012), remains to be determined.

In addition to regulatory effects conveyed by peptidergic projections from ARH to PVH, the activity of hypothalamic neurons is controlled by glutamatergic and GABAergic inputs. PVH neurons receive both glutamatergic and GABAergic innervation from the ARH with the majority of NPY/AgRP neurons containing GABA, while POMC neurons are primarily glutamatergic (Horvath et al., 1997; Collin et al., 2003). However, we did not observe a comparable degree of developmental plasticity in the density of either vGlut2- or VGAT-labeled inputs to NE or PA neurons. Moreover, ratios of these inputs to subpopulations of NE or PA neurons in the PVH appeared to be remarkably stable between WT and Lepob/Lepob mice. It should be noted, however, that we do not know whether compensatory changes in synapse density may occur later in development, as has been observed in other brain regions, impacting circuit architecture and neuronal homeostasis (Cesa and Strata, 2009; Lu et al., 2009; Blankenship and Feller, 2010). Moreover, Pinto et al. (2004) demonstrated that treatment of adult Lepob/Lepob mice with leptin rapidly alters the ratio of glutamatergic and GABAergic synapses onto NPY and POMC neurons in the ARH, suggesting that acute exposure to leptin may modulate the excitatory and inhibitory balance in mature animals. It is equally plausible that a majority of inputs to PVH neurons may arise from non-ARH and non-leptin-sensitive sources, thereby masking leptin's modulatory effect on a subset of excitatory or inhibitory inputs to ARH neurons. Anatomical studies show a dense population of GABAergic interneurons surrounding the PVH, which innervate PVH cells (Roland and Sawchenko, 1993) and could potentially compensate for loss of leptin-dependent excitatory or inhibitory inputs to NE or PA neurons. Alternatively, a recent gene-targeting study revealed that leptin mediates its anorectic action predominantly via a distributed network of presynaptic GABAergic neurons that collectively reduce inhibitory tone to POMC neurons (Vong et al., 2011). Thus, leptin may also act upstream of POMC neurons to specify patterns of connectivity that alter neuronal response properties of these important cells.

Variation in the timing and amplitude of the leptin surge increases susceptibility to obesity later in life (Yura et al., 2005; Delahaye et al., 2008). We observed a slight, but significant, decrease in body weight gain and food intake in adult Lepob/Lepob mice treated postnatally with leptin, despite the magnitude of obesity conferred by the Lepob/Lepob genotype. Furthermore, Lepob/Lepob mice treated postnatally with leptin exhibit enhanced responsiveness to exogenous leptin in adulthood, demonstrating that exposure to leptin during a discrete developmental window is sufficient to impact leptin sensitivity later in life. These observations are consistent with our structural findings that postnatal leptin treatment can rescue patterns of neuronal targeting in the PVH. The ability of postnatal leptin to restore targeting of peptidergic innervation to PA neurons in the PVH corresponds to the improved sympathetic responses observed in Lepob/Lepob mice when challenged in a cold environment, or by fasting. Furthermore, activation of neurons in the PVH inhibits BAT sympathetic nerve activity and BAT thermogenesis (Madden and Morrison, 2009). Therefore the improved innervation of PA neurons in the PVH may contribute to the improved thermogenic response observed in Lepob/Lepob mice that received postnatal leptin. The DMH also represents a major target for leptin-dependent ARH projections (Bouret et al., 2004a) and growing evidence suggests involvement of the DMH in mediating the effects of melanocortins on energy expenditure and regulation of BAT thermogenesis (Enriori et al., 2011; Zhang et al., 2011). Whether a developmental action of postnatal leptin on ARH projections to the DMH is required to maintain normal control of energy expenditure remains to be established.

We currently know little about the molecular guidance cues that control development of hypothalamic circuits. Studies in extrahypothalamic neural systems have identified a variety of molecular mechanisms mediating circuit development, including competitive interactions between neighboring branch arbors, synapse-dependent branch stabilization (Gibson and Ma, 2011), as well as contact-mediated guidance cues (Kolodkin and Tessier-Lavigne, 2010). Indeed, diffusible guidance molecules such as Netrins, Slits, and Semaphorins are highly expressed in the PVH during development, with expression of their cognate receptors on ARH neurons (Bouret, 2010). Interestingly, in mice that are deficient in Contactin, a cell adhesion molecule involved in the formation of axonal projections, innervation of the PVH by AgRP and αMSH axon terminals is significantly impaired (Fetissov et al., 2005). Regardless of the target molecules mediating cell type-specific patterns of innervation in the PVH, the ability of leptin to specify patterns of neuronal connectivity during development may differentially impact distinct components of autonomic regulation, while imposing a requirement for sustained leptin action for accurate control of neuroendocrine responses. Unraveling the mechanisms through which leptin imprints patterns of connectivity in the hypothalamus during critical periods of development will enable a better understanding of how factors that alter postnatal leptin secretion impact the architecture of metabolic circuitry controlling energy homeostasis throughout life.

Footnotes

This work was supported by National Institutes of Health Grants DK065900 and DK057768 to (R.B.S.), and the French Foundation for Medical Research (postdoctoral fellowship to K.B.). We thank Dr. H.-W. Dong (LONI, Department of Neurology, UCLA School of Medicine) for invaluable advice on surgical procedures, anatomical definitions, and for kindly providing us with the PVH schematic used in this manuscript.

The authors declare no competing financial interests.

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