Skip to main content
Download PDF

SerpinA3N is a novel hypothalamic gene upregulated by a high-fat diet and leptin in mice

Genes & Nutrition volume 13, Article number: 28 (2018) Cite this article

Abstract

Background

Energy homeostasis is regulated by the hypothalamus but fails when animals are fed a high-fat diet (HFD), and leptin insensitivity and obesity develops. To elucidate the possible mechanisms underlying these effects, a microarray-based transcriptomics approach was used to identify novel genes regulated by HFD and leptin in the mouse hypothalamus.

Results

Mouse global array data identified serpinA3N as a novel gene highly upregulated by both a HFD and leptin challenge. In situ hybridisation showed serpinA3N expression upregulation by HFD and leptin in all major hypothalamic nuclei in agreement with transcriptomic gene expression data. Immunohistochemistry and studies in the hypothalamic clonal neuronal cell line, mHypoE-N42 (N42), confirmed that alpha 1-antichymotrypsin (α1AC), the protein encoded by serpinA3, is localised to neurons and revealed that it is secreted into the media. SerpinA3N expression in N42 neurons is upregulated by palmitic acid and by leptin, together with IL-6 and TNFα, and all three genes are downregulated by the anti-inflammatory monounsaturated fat, oleic acid. Additionally, palmitate upregulation of serpinA3 in N42 neurons is blocked by the NFκB inhibitor, BAY11, and the upregulation of serpinA3N expression in the hypothalamus by HFD is blunted in IL-1 receptor 1 knockout (IL-1R1−/−) mice.

Conclusions

These data demonstrate that serpinA3 expression is implicated in nutritionally mediated hypothalamic inflammation.

Background

Once considered problematic for only the Western, developed world, the burden of obesity today encompasses most countries [1], with shifts in global eating patterns causing detrimental changes in body weight and composition, associated diseases and decreased quality of life [2, 3]. The development of effective treatments for obesity has not been fruitful, with the continued futility of dieting methodologies for sustained weight loss, and gastric surgery being the only current long-term solution [4,5,6], putting health care systems under an enormous amount of pressure. In order for more effective, preventative measures to be put in place, it is crucial to understand the mechanisms that cause obesity. The overconsumption of energy-dense foods, particularly those high in long-chain saturated fat and sugar, appears to be a primary driving force behind the obesity epidemic [7]. These foods have been shown to have a powerful effect on the hypothalamus in rodent models, resulting in inflammation and astrogliosis that is implicated in diet-induced obesity [8,9,10].

Energy balance, food intake and consequently body weight are effectively regulated by a well-defined and complex hypothalamic system. Briefly, two distinct types of neurons have been identified as important in energy balance regulation: orexigenic neurons expressing neuropeptide Y (NPY) and agouti-related peptide (AgRP) and anorexigenic neurons expressing proopiomelanocortin (POMC) and cocaine- and amphetamine-regulated transcript (CART). Both orexigenic and anorexigenic neurons express leptin receptors, highlighting the importance of this hormones in the system. Leptin acts on multiple levels in hypothalamic neurons, effecting gene transcription, post-translational processing as well as membrane polarisation to inhibit AgRP/NPY neurons while activating POMC/CART neurons, resulting in a stable body weight [11]. In the obese state, the ability of leptin to regulate feeding behaviour as well as peripheral glucose homeostasis is diminished as a result of hypothalamic insensitivity to this hormone [12,13,14,15,16].

When animals are fed a high-fat diet (HFD), they ingest more energy than they expend, resulting in increased adiposity, and eventually obesity, suggesting that a HFD compromises the hypothalamic systems that regulate food intake. This has been confirmed in a number of rodent studies showing that a HFD induces inflammation in the hypothalamus activating microglia, astrocytes and neurons via a Toll-like receptor 4 (TLR4)-dependent mechanism [17,18,19] and the IKKβ/NFκB and JNK inflammatory pathways [20,21,22,23,24] resulting in leptin and insulin insensitivity. Blocking or inhibiting inflammation in the hypothalamus prevents leptin and insulin insensitivity and obesity induced by a HFD [22, 23, 25, 26].

In order to further explore the mechanisms linking HFD to hypothalamic dysfunction and leptin insensitivity, we carried out a microarray-based transcriptomics experiment to determine gene expression changes in response to a HFD as well as leptin challenge. One of the genes that was considerably upregulated by both leptin and HFD was serpinA3N, the gene encoding the anti-protease, alpha-1-antichymotrypsin (α1AC). In the periphery, α1AC is an acute phase protein produced by hepatocytes [27] and has been recently identified as a marker of reactive astrogliosis in the brain [28]. Increased levels of α1AC in the brain are commonly associated with inflammatory conditions such as Alzheimer’s disease [29, 30].

In the present study we identified, using transcriptomics, that the gene, serpinA3n, is highly expressed in the hypothalamus and is upregulated by leptin and HFD, a finding confirmed by semi-quantitative in situ hybridisation. Furthermore, we have shown that nutritional factors, as well as time on experiment, play a role in the hypothalamic nuclei-specific regulation of serpinA3N expression. As the expression of serpinA3N in the periphery has been reported to be dependent on inflammation and IL-1 stimulation [31,32,33,34], we tested the effect of HFD on hypothalamic serpinA3N expression in IL-1 receptor 1 knockout mice (IL-1R1−/−) and in the hypothalamic clonal neuronal cell line, mHypoE-N42 (N42) which we challenged with oleic and palmitic acid, the latter, with and without blocking the NFκB pathway. In IL-1R1−/− mice, HFD challenge failed to upregulate serpinA3N expression in contrast to wild-type mice and in N42 cells oleic acid downregulated serpinA3N while palmitate upregulated expression which was negated by inhibiting the NFκB pathway, confirming that HFD-induced expression is dependent on inflammation. Also, as increased serpinA3N expression in the brain has previously been identified as a marker of astrocyte activation [28], we examined α1AC immunoreactivity in the hypothalamus together with that of glial fibrillary acidic protein (GFAP), an astrocyte marker, ionised calcium binding adaptor molecule 1 (Iba1), a microglial marker, and NPY and AgRP, markers of neurons important in energy balance. Immunoreactive α1AC cells were larger and dissimilar to astrocytes and microglia having a distinctive neuronal shape and close associations with NPY and AgRP beaded fibres, also pointing to neuronal expression of serpinA3N. In addition, using Western blotting, the protein product of serpinA3N, α1AC, was detected in N42 neurons in much lower levels than that found in the media demonstrating that the protein is secreted. The expression of serpinA3N in and the secretion of α1AC from these cells confirmed neuronal expression of serpinA3N.

Results

Transcriptomics

Transcriptomic data revealed the regulation of serpinA3N gene expression in total dissected hypothalamic tissue from mice maintained on a LFD or HFD for 1 or 4 weeks and either challenged with vehicle or leptin. A three-way ANOVA showed significant effects of HFD (P = 0.0007), leptin challenge (P = 2.55 × 10−6), and time on diet (P = 1.34 × 10−6). However, there was no interaction between these factors (Fig. 1). A full list of changed genes can be found at NCBI’s Gene Expression Omnibus and is accessible through GEO Series accession number GSE113943 (https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi).

Fig. 1
figure 1

Data derived from NuGO Affymetrics arrays from the hypothalamus of C57BL/6J mice maintained on a HFD or LFD for 1 and 4 weeks challenged with IP vehicle or leptin. The log of serpinA3N gene expression is represented by box and whisker plots. Three-way ANOVA showed a significant effect of diet, leptin challenge and time on the diet but no interaction between any of these factors (n = 10)

Full size image

Localisation of serpinA3N and α1AC in the hypothalamus

In situ hybridisation using a serpinA3N-specific riboprobe revealed specific labelling throughout the hypothalamus with particularly high levels of expression in the arcuate nuclei (ARC), ventromedial (VMH) and dorsomedial nuclei (DMH). The labelling extended out to the edges of the lateral hypothalamus (LH) (Fig. 2a). Immunoreactive α1AC in the ARC of the hypothalamus revealed a neuronal morphology (Fig. 2b–e). Dual staining using an anti-mouse α1AC antibody (brown) alongside blue anti-GFAP (astrocyte specific) and anti-Iba1 (microglia specific) staining showed smaller and distinctly different cell morphologies with closely associated but not overlapping staining (Fig. 2b, c). Staining with both anti-NPY and anti-AgRP (blue) showed beaded fibres closely associated with anti-α1AC-positive neurons (brown) (Fig. 2d, e).

Fig. 2
figure 2

a Representative in situ autoradiograph of a C57BL/6J mouse brain section after 4 weeks of HFD showing serpinA3N expression in the arcuate nuclei (ARC), the ventromedial nuclei of the hypothalamus (VMH), the dorsomedial nuclei of the hypothalamus (DMH) and the lateral hypothalamus (LH). b–e Representative immunostaining of α1AC (brown) and b GFAP, c Iba1, d AgRP and e NPY (all blue) in the arcuate nuclei after 1 week of HFD. Bar = 20 μm

Full size image

Regulation of serpinA3N and expression by HFD and time

A robust increase in labelling was seen after just 1 week on a HFD. It was possible to distinguish distinct hypothalamic nuclei which expressed high levels of serpinA3N including the ARC, VMH, DMH, and LH (Fig. 3a, b). Quantification of hypothalamic nuclei including the ARC, VMH, DMH (Fig. 3c–e) and LH (not shown) confirmed the increase in serpinA3N gene expression by a HFD seen in transcriptomics studies. Expression in the ARC was significantly increased by around 50% after 4 weeks on the HFD compared to LFD control (Fig. 3c). In comparison, the level of gene expression in the VMH and DMH was increased by approximately 2.5 and 4 times after only 1 week, respectively. After 16 weeks on the HFD, the labelling in these nuclei had increased to approximately eight times of that seen in LFD fed mice at week 1 (Fig. 3d, e). Analysis of the gene expression data by two-way ANOVA confirmed that serpinA3N gene expression increased with time on the diet and there was no interaction between diet and time for the ARC and DMH but there was for the VMH (P < 0.05) indicating that the age of the animals may also lead to increases in serpinA3N gene expression in the ARC, VMH and DMH over the 16 weeks of the experiment (Fig. 3c–e).

Fig. 3
figure 3

Representative in situ autoradiographs of C57BL/6J mouse brain sections showing serpinA3N expression in a LFD-fed mouse and b HFD-fed mouse. Levels of serpinA3N gene expression in LFD- and HFD-fed mice measured by semi-quantitative in situ hybridisation c in the arcuate nuclei (ARC), d the ventromedial nuclei of the hypothalamus (VMH) and e the dorsomedial nuclei of the hypothalamus (DMH). Two-way ANOVA showed a significant effect of diet P < 0.001 for the ARC, VMH and DMH and time P < 0.001 for the VMH and P < 0.05 for the ARC and DMH with an interaction between diet and time P < 0.05 for the VMH only. One-way ANOVA showed differences between HFD and LFD from 4 weeks onwards for the ARC and for all times tested for the VMH and DMH. *P < 0.05, **P < 0.01, ***P < 0.001 (n = 6)

Full size image

Regulation of serpinA3N expression by leptin

To further investigate the regulation of serpinA3N by leptin, in situ hybridisation was carried out on both leptin-deficient mice (ob/ob) and mice lacking functional leptin receptors (db/db) and their lean littermates (Fig. 4a–d). Images from ob/ob, db/db and lean mice show a much lower level of serpinA3N gene expression in ob/ob and db/db mice (Fig. 4a, b). Quantification of labelling showed a difference of the order of seven to ten times lower levels of gene expression in db/db and ob/ob mice compared to their lean littermates (Fig. 4c, d).

Fig. 4
figure 4

Representative in situ autoradiographs of mouse brain sections showing serpinA3N expression in a ob/ob mouse on a C57BL/6J background and b lean C57BL/6J mouse. Levels of serpinA3N gene expression in the arcuate nuclei measured by semi-quantitative in situ hybridisation of c db/db on a C57BL/6J background and lean C57BL/6J mice, d ob/ob and lean mice, e ob/ob mice injected with IP vehicle (veh.) or leptin after either 1 or 4 h (h) and f lean mice injected with IP vehicle (veh.) or leptin after either 1 or 4 h (h). *** P < 0.001 (n = 6)

Full size image

Treatment of ob/ob mice with leptin (10 mg/ml injected IP) resulted in a time-dependent increase in serpinA3N expression with a 10-fold increase within 1 h and a 14-fold increase after 4 h (Fig. 4e). While leptin challenge in lean mice did not increase serpinA3N levels of expression above basal after 1 h, leptin challenge did increase levels of expression significantly after 4 h but only by approximately 70% (Fig. 4f) compared to the 14-fold increase seen in ob/ob mice 4 h after leptin challenge.

Regulation of serpinA3N expression by HFD in the absence of leptin

Transcriptomics data indicated that the effects of leptin and HFD were independent. To confirm this, ob/ob mice, lacking leptin, were fed either a LFD (10% of calories from fat), or a HFD (45% or 60% of calories from fat). The HFD led to a large increase in serpinA3N gene expression compared to the LFD in the nuclei expressing the gene. Quantification of labelling showed an increase of around 20–30 times in both the ARC and the VMH after 8 weeks on a HFD (Fig. 5a, b).

Fig. 5
figure 5

Levels of serpinA3N gene expression measured by semi-quantitative in situ hybridisation in the a arcuate nuclei (ARC) and b ventromedial nuclei of the hypothalamus (VMH) of ob/ob mice fed either a LFD, 10% energy (kCal) from fat, or HFD either 45% or 60% energy (kCal) from fat for 8 weeks. ***P < 0.001 (n = 6)

Full size image

Regulation of serpinA3N expression by fasting and refeeding

In mice fasted for 24 h, serpinA3N expression increased throughout the hypothalamus. Expression increased by around 40% in the ARC and 200% in the VMH. Refeeding the mice for 24 h returned levels of expression to those seen in the fed animals (Fig. 6a, b).

Fig. 6
figure 6

Levels of serpinA3N gene expression measure by semi-quantitative in situ autoradiography in the a arcuate nuclei (ARC) and b ventromedial nuclei of the hypothalamus (VMH) of C57Bl/6J mice either fed, fasted for 24 h or refed for 24 h. *P < 0.05, **P < 0.01 (n = 8)

Full size image

Regulation of serpinA3N by HFD in IL-1R1 −/− mice

Feeding IL-1R1−/− mice, a HFD for 8 weeks appeared to increase serpinA3N by a relatively small amount in the ARC, VMH and DMH compared to the effects seen in wild-type mice. There was substantial variability in the response to the HFD which failed to reach statistical significance (Fig. 7a–c).

Fig. 7
figure 7

Levels of serpinA3N gene expression measured by semi-quantitative in situ autoradiography in the a arcuate nuclei (ARC), b ventromedial nuclei of the hypothalamus (VMH) and c dorsomedial nuclei of the hypothalamus (DMH) in IL-1R1−/− mice on a C57BL/6J background fed either a LFD or HFD for 8 weeks (n = 9 for HFD and n = 5 for LFD)

Full size image

Regulation of SerpinA3N in N42 cultured hypothalamic neurons

Leptin challenge upregulated serpinA3N gene expression by twofold compared to vehicle-treated N42 neurons. IL-6 and TNFα were also upregulated. A similar effect was induced by 200 μM palmitic acid. In comparison, 200 μM oleic acid downregulated the gene expression of all three genes (Fig. 8a–c). The upregulation of serpinA3N, IL-6 and TNFα gene expression by palmitate was significantly reduced in the presence of the NFκB inhibitor, BAY11 (Fig. 8d–f).

Fig. 8
figure 8

a–f In mHypoE-N42 cells, a–c SerpinA3N, IL-6 and TNFα gene expression were all upregulated by leptin and palmitic acid challenge and downregulated by oleic acid. d–f The upregulation of SerpinA3N, IL-6 and TNFα gene expression by palmitic acid was blocked by the NKκB inhibitor BAY11. P < 0.05, ***P < 0.001, **P < 0.01. NS not significant

Full size image

α1AC secretion from N42 cultured neurons

SDS-PAGE gels of media from cultured N42 neurons showed the presence of several protein bands of different molecular weights but not in cell free media (Fig. 9). Using Western blotting, cell free media displayed extremely faint immunoreactive α1AC bands but culture media from N42 neurons showed two immunoreactive bands, the lower at 59 kDa corresponding to the molecular weight of α1AC (positive control). The band above may correspond to a different post-translationally modified form of the protein. The cell lysate in contrast showed only extremely faint immunoreactive bands including one at 59 kDa (Fig. 9).

Fig. 9
figure 9

Representative SDS PAGE gel and immunoblot showing alpha-1-antichymotrypsin (α1AC), secreted into the media from N42 neuronal cells. No bands are visible with media alone. The blot shows two immunoreactive bands in the media from N42 neurons

Full size image

Discussion

Hypothalamic inflammation in response to a HFD in rodents is well-documented after both short- and long-term exposure to HFD [17,18,19, 35, 36]. In the present study transcriptomics data show that, a so far unreported gene, associated with inflammation in the periphery, serpinA3N, is strongly upregulated by HFD and leptin in the hypothalamus. An incidental finding is that serpinA3N is also upregulated by time on experiment which corresponds to the increasing age of the mice. Surprisingly, these effects were largely independent of one another indicating that while hypothalamic serpinA3N expression is regulated by a number of factors these appear to act via independent pathways.

It can be difficult to differentiate between the effects of a HFD and that of diet-induced obesity as the former rapidly leads to the latter. In the present study, the effects of obesity and a HFD are separated in obese ob/ob mice, which, though obese, normally have relatively low levels of hypothalamic serpinA3N gene expression, but when challenged with a HFD, the level of expression is rapidly upregulated demonstrating that the level of serpinA3N expression is regulated by a HFD rather than obesity per se. Also, the possibility that increased caloric intake rather than diet composition is responsible for the upregulation of serpinA3N cannot be ruled out completely in our animal studies. However, ob/ob mice are hyperphagic, but as noted above, they express relatively low levels of hypothalamic serpinA3N when not exposed to a HFD. Additionally, the pro-inflammatory long-chain saturated fat, palmitic acid, upregulates expression of serpinA3N in the clonal neuronal cell line N42, while oleic acid, an anti-inflammatory monounsaturated fatty acid, decreases gene expression indicating that fatty acids have a direct effect on serpinA3N expression in neurons, supporting the contention that serpinA3N expression responds to the increased long-chain saturated fat in the diet rather than to increased caloric intake.

In the periphery, α1AC, the protein encoded by serpinA3N, serves as an acute phase protein produced by the liver, in response to inflammation and binds to proteases, thus limiting inflammation-related damage [37, 38]. In the brain, α1AC has been shown to be associated with inflammation and elevated levels are found in Alzheimer’s disease, closely linked with amyloid plaques [38,39,40]. Other observed functions of peripheral α1AC include inhibition of oxygen uptake and superoxide generation in granulocytes [41], DNA binding independent of its anti-protease activity, regulation of its own gene expression, and inhibition of DNA polymerase and DNA primase activity [42, 43]. However, the target protein for, and the function of, α1AC in the hypothalamus remains to be identified.

In the present study, in situ hybridisation revealed a widespread localisation of serpinA3N expression throughout the hypothalamus in a pattern corresponding to major nuclei indicating that the expression is neuronal. This is further supported by immunohistochemistry where dual immunostaining for α1AC and both the astrocyte marker, GFAP, and the microglial marker Iba1 reveal no overlap in staining and immunopositive α1AC show a characteristic neuronal shape which is both larger and distinctly different from that of GFAP and Iba1 immunopositive cells. Dual staining with NPY and AgRP shows close associations between α1AC immunopositive fibres and NPY and AgRP beaded fibres. Also, in N42 clonal neurons in culture, which have been used previously to investigate hypothalamic control mechanisms [44], the expression of serpinA3N is upregulated by both leptin and palmitate in a manner consistent with that seen in the hypothalamus in response to leptin challenge and a HFD. Taking all of this evidence together, serpinA3N measured in the present study appears largely neuronal in origin. Nonetheless, in a previous genomic study involving two mouse models of brain injury (ischemic stroke and neuroinflammation), serpinA3N was identified as a marker of reactive astrogliosis [28], and as HFD has been shown to induce astrogliosis in mice [17, 45], then potentially, some of the increase in serpinA3N expression may be astrocytic. Thus, we cannot rule out that part of the increased gene expression seen may occur in astrocytes.

In the liver, increased levels of serpinA3N gene expression and subsequently increased levels of α1AC, like all acute phase proteins, are stimulated by inflammation, particularly by raised circulating levels of IL-6 and IL-1 type cytokines working via STAT3 activation and increased NFκB [46]. In N42 neurons, both IL-6 and TNFα were upregulated in parallel with serpinA3N by leptin and palmitic acid, with palmitic acid stimulated gene expression inhibited by BAY11 blocking the NFκB pathway. These results together with the lack of HFD-induced serpinA3N upregulation in IL-1R1−/− mice clearly indicated that hypothalamic serpinA3N is involved in the inflammatory response as in the periphery.

Leptin stimulates the release of IL-1β in the hypothalamus [47] while a HFD does not appear to upregulate IL-1β in this brain area [17] but IL-1β does increase in the periphery in obesity [48] indicating a more complex relationship between HFD, IL-1β and serpinA3N upregulation. Circulating interleukins do not readily cross the blood-brain barrier but influence the brain via intermediate mechanisms [49]. The source of the interleukins and the mechanisms underlying upregulation of serpinA3N expression by a HFD requires further investigation. While there is no significantly different upregulation of serpinA3N gene expression in IL-1R1−/− mice, there is an indication of a variable response to HFD which may be due to increases in circulating leptin levels in response to increasing adiposity and, thus, increasing leptin levels.

While in the absence of leptin, signalling levels of serpinA3N expression in the hypothalamus are low and leptin challenge upregulates serpinA3N expression, the localisation and pattern of leptin-stimulated expression differs from that induced by a HFD. Leptin-induced serpinA3N expression increases mainly in the ARC, VMH and throughout the hypothalamus up to the borders of the LH with no clear demarcation of hypothalamic nuclei other than the ARC and VMH. The role of leptin in the stimulation of serpinA3N expression on a HFD, however, appears to be relatively small as a HFD upregulates serpinA3N gene expression to a much greater degree in ob/ob mice, in the absence of leptin, compared to lean mice in the presence of leptin. The reasons for this are not clear, but counterintuitively, it may be that the presence of leptin is somehow protective against the induction of serpinA3N gene expression by a HFD. Leptin receptors are present on both neurons and astrocytes and leptin may be upregulating serpinA3N in either or both these cell types [50], with the upregulation of serpinA3N in N42 hypothalamic neurons confirming the neuronal regulation of serpinA3N by leptin. Nonetheless, circulating leptin levels do not appear to be a major regulator of serpinA3N gene expression in the fasting and refed states as the regulation or serpinA3N occurs in opposition to circulating leptin levels, with fasting, which causes leptin levels to drop, increasing serpinA3N gene expression, while refeeding, which increases circulating leptin levels [51], results in decreased serpinA3N gene expression. However, this may be explained by the stimulation of serpinA3N gene expression by the increased levels of circulating free fatty acids which occur during fasting [52].

Leptin insensitivity, induced by a HFD, is well documented [22]. While this concept was not specifically tested in the present study, the transcriptomics data which combined leptin challenge on a LFD and HFD indicated that the effect of diet was separate from that of leptin challenge and that there was no interaction between the two indicating that upregulation of serpinA3N gene expression by leptin is unaffected by HFD; however, this remains to be specifically tested.

Increased time on experiment or age of the mice also appears to be a factor in the upregulation of serpinA3N gene expression in the ARC, VMH and DMH of the hypothalamus. Although the effects of extreme ageing were not investigated in the present study, the mice were older at the end of both the transcriptomics and the in situ hybridisation studies on HFD than at the beginning and both showed a clear effect on serpinA3N gene expression with time despite being measured by different approaches. The mice exposed to the HFD for the longest period of time varied in age between 12 weeks at the beginning of the study and 28 weeks at the end on the study. Twelve weeks of age corresponds to a young mature adult, and 28 weeks corresponds to early middle age with mice showing some signs of age-related changes [53]. Ageing has also been reported to induce inflammation in the hypothalamus via the IKKβ/NFκB pathway. Indeed, hypothalamic inflammatory changes have shown to control systemic ageing demonstrating the importance of this phenomenon to the health of the whole organism [54].

Conclusions

We have shown the upregulation of a novel hypothalamic gene, serpinA3N, by HFD and leptin. Increasing age and fasting also resulted in an upregulation although to a lesser extent. The upregulation of serpinA3N expression by leptin and palmitic acid was confirmed in N42 neurones in culture along with the upregulation of IL-6 and TNFα, two classical markers of inflammation. Blocking the NFκB inflammatory pathway by BAY11 not only prevented the upregulation of IL-6 and TNFα, but also that of serpinA3N. The protein product of serpinA3N, α1AC, is found in the media from cultured N42 neurons but is difficult to visualise within the cell lysate indicating that α1AC is a secreted protein in the hypothalamus as it is in the periphery.

These data strongly support the contention that serpinA3N expression is a marker of inflammation in the hypothalamus regulated by nutritional status and leptin and indicate a potential role for α1AC in hypothalamic inflammation and the regulation of energy balance.

Methods

Animal studies

All experiments were carried out according to the institutional and national guidelines of the European Convention of Vertebrate Animals Used for Experimentation, under European Council Directive 86/609/EEC dated November 1986. For the transcriptomics studies, male, 16-week-old, C57BL/6J mice were obtained from Charles River laboratories (Maastricht, The Netherlands) and housed in pairs in the light- and temperature-controlled animal facility of Wageningen University (12:12-h light/dark cycle at 22 °C). Mice were maintained for 1 or 4 weeks on either a HFD (45% kCal from fat) or LFD (10% kCal from fat) (Research Diet Services BV, Wijk bij Duurstede, The Netherlands) modelled on (D12451 and D12450B respectively Research Diets, NJ, USA). (Please see https://researchdiets.com/opensource-diets/dio-series-diets for diet composition details). For this study, palm oil was used in place of lard. They were then challenged with three intraperitoneal (IP) injections of murine leptin (2 mg/kg body weight) (R&D Systems, Abingdon, UK) or carrier at 24, 15 and approximately 3 h prior to killing in the early morning (n = 10). This experiment was part of the NuGO Proof of Principle studies as previously described [55].

To further investigate the regulation of serpinA3N gene expression on a HFD, male C57BL/6J mice (Harlan, Bicester, UK), aged 12 weeks, were singly housed on grid floors and fed either a HFD (60% kCal from fat) or a LFD (10% kCal from fat) (D12452 and D12450B respectively, Research Diets, NJ, USA—see web site above for detailed dietary breakdown), ad libitum for 3 days, 1, 4, 8, 12 or 16 weeks and killed either by exsanguination or by perfusion fixation (1 week) with 4% paraformaldehyde in phosphate buffered saline (PBS) under terminal anaesthesia (n = 6). To further investigate the upregulation of serpinA3N by leptin, male mice on the C57BL/6J background either leptin deficient (ob/ob) or lacking functional leptin receptors (db/db) and their lean littermates (Harlan, Bicester, UK) were killed for in situ hybridisation (n = 6). Leptin-deficient ob/ob mice and lean littermates (n = 6) were also challenged with vehicle or leptin by intraperitoneal (IP) injection (2 mg/kg body weight) and killed either 1 or 4 h later as detailed above. Food intake in response to leptin was not measured at this time because any changes were deemed to be impractical to measure with any accuracy due to the fact that leptin challenge was carried out over such a short period of time during the light period when food intake is already low. To confirm the upregulation of serpinA3N expression by HFD is independent from that of leptin, ob/ob mice were fed either a LFD 10% kCal from fat or a HFD either 45% or 60% kCal from fat in the form of lard (diets detailed above) for 8 weeks prior to killing by exsanguination.

To test the effect of nutritional status on hypothalamic serpinA3N gene expression, C57BL/6J mice were fasted for 24 h or fed ad libitum on standard mouse diet prior to killing. Refed animals were allowed access to food ad libitum for a period of 24 h after fasting (n = 8).

To test the possibility that inflammation plays a role in the effect of HFD on the expression of serpinA3N, mice from IL-1R1−/− breeding pairs, on C57BL/6J background, purchased from Jackson laboratories were bred at University College Dublin (UCD) for 6–10 generations under specific pathogen-free conditions. Male IL-1R1−/− mice were then fed HFD, 45% kCal or LFD, 10% kCal from fat for 12 weeks prior to killing (D12451 and D12450B respectively, Research Diets, NJ, USA). In this study, palm oil was used instead of lard (n = 9 HFD and n = 5 chow).

Transcriptomics

Hypothalami were dissected and snap-frozen in liquid nitrogen and stored at − 80 °C until RNA extraction. Total RNA was extracted using TRIzol reagent (Invitrogen, Carlsbad, CA), and the mRNA purified with RNeasy Mini Kit (Qiagen, Venlo, The Netherlands) with 1% β-mercapto ethanol and treated with DNAse. The mRNA integrity was checked on an Agilent 2100 Bioanalyzer (Agilent Technologies, Amsterdam, The Netherlands) (average RIN 9.2), and individual RNA samples (4 μg per animal) were labelled and hybridised on a Affymetrix NuGO mouse array as described previously [35].

In situ hybridisation

The riboprobe for serpinA3N, accession no. BC013651, was derived using the forward primer 5′CTACGCGGGCAAGAGGA3′ and the reverse primer 5′AAGGGGGCAATTTCAGTTT3′. The size of the amplified insert was 543 bp. Automated sequencing was performed to verify the probe sequence.

Messenger RNA levels were quantified by in situ hybridisation, on 20-μm thick coronal hypothalamic cryo-sections, using techniques described in detail elsewhere [56]. Briefly, slides were fixed in 4% (w/v) paraformaldehyde in 0.1 mol/l PBS for 20 min at room temperature, washed in PBS, incubated in 0.1 mmol/l triethanolamine for 2 min and acetylated in 0.1 mmol/l triethanolamine and 0.25% (v/v) acetic anhydride for 10 min. Sections were dehydrated in ethanol and dried under vacuum before hybridisation with riboprobes at 106 cpm/ml for 18 h at 58 °C. After hybridisation, sections were desalted through a series of washes in standard saline citrate (SSC) to a final stringency of 0.1× SSC at 60 °C for 30 min, treated with RNase A and dehydrated in ethanol. Slides were apposed to Biomax MR (Sigma-Aldrich, UK) together with [14C] micro-scale standards (Amersham International, Amersham, UK) at room temperature for varying lengths of time depending on the probes used to ensure that the optical density of areas to be measured fall within the linear region of the standard curve.

Autoradiographs were scanned on a Umax Power Look II (UMAX Data Systems, Fremont, CA, USA). Integrated optical densities (IOD) of specific nuclei were quantified with reference to a mouse brain atlas [57] using the Image Pro-plus system (Media Cybernetics, Silver Springs, MD, USA). IOD was converted to nCi/g using [14C] microscale standard curves for measures of total gene expression.

Immunohistochemistry

Frozen sections (20 μm) were first incubated with goat anti-mouse serpinA3N (R&D Systems cat. no. AF4709) at a dilution of 1:1000 overnight at 4 °C then incubated for 30 min at room temperature with biotinylated anti-goat IgG (Vector Labs cat. no. PK-6105) according to the manufacturer’s instructions followed by ABC reagent (Vector Labs cat. no. PK-6105) and stained with 3,3′-diaminobenzidine (DAB) substrate solution (brown) (Vector Labs cat. no. SK-4100). Sections were then thoroughly washed and incubated with either chicken anti-GFAP (Millipore, UK cat. no. AB5541), rabbit anti-IbA1 (Wako cat. no. 019-19741), rabbit anti-NPY (ThermoFisher Scientific cat. no. PA5-19568) or rabbit anti-AgRP (Phoenix Pharmaceuticals cat. no. H-003-57) at a dilution of 1:300 overnight at 4 °C and then at room temperature for 30 min with either goat anti-chicken IgG (Vector Labs cat. no. BA-9010) at a dilution of 1:200 followed by Vectastain Elite ABC kit (goat IgG) (Vector Labs cat. no. PK-6105) or directly with the Vectastain Elite ABC kit (goat IgG) and stained with Vector SG (blue) (Vector Labs cat. no. SK-4700). Control sections omitted the primary antibodies.

Neuronal culture and reagents

To investigate the regulation of serpinA3N gene expression specifically in neurons, the embryonic immortalised hypothalamic cell line, N42, was used (Cellution Biosystems Inc., Ontario, Canada. Please see https://www.cedarlanelabs.com/Products/Detail/CLU122 for a comprehensive list of all genes expressed by these cells including the leptin receptor). These cells have been previously shown to provide a good model for hypothalamic neuron gene expression studies [44].

Cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM) (Life Technologies, Paisley, UK) supplemented with 10% fetal bovine serum and 1% penicillin/streptomycin (Life Technologies) maintained at 37 °C under 5% CO2. Neurons were grown in 60-mm plates (n = 6) to 90% confluence then challenged with either 50 nM leptin (R&D Systems, Abingdon, UK), 200 μM palmitic acid or 200 μM oleic acid conjugated to fatty acid-free bovine serum albumin (BSA) (Sigma-Aldrich, UK), or the appropriate vehicle as a control. For leptin, this was a mixture of 12 μM HCl and 6 μM NaOH and for fatty acids 50 μM fatty acid-free BSA. To inhibit the NFkB pathway, N42 neurons were treated with 50 μM BSA or 200 μM palmitate in the presence and absence of 25 μM of the NFkB inhibitor BAY 11-7082 (Cayman Chemical, UK). All solutions were filter sterilised prior to use. For all treatments, medium was removed after 6 h.

Real-time PCR

After the challenge, the medium was removed and cells were lysed using RLT lysis buffer (RNeasy Mini Kit Qiagen, Venlo, The Netherlands). Cell lysates were then collected and RNA extracted using an RNeasy Mini Kit (Qiagen) following the manufacturer’s instructions. RNA integrity was assessed by an Agilent 2100 Bioanalyzer (Agilent Technologies, Amsterdam, The Netherlands). One microgram of total RNA was reverse transcribed to generate cDNA using Superscript II reverse transcriptase (Life Technologies, CA, USA). Real-time PCR was carried out using Taqman Fast Universal PCR master mix (Applied Biosystems, USA) according to manufacturer’s instructions using the following Taqman assays: B2M (Mm00437762_m1), serpinA3N (Mm00776439_m1), IL-6 (Mm00446190_m1) and TNFα (Mm00443258_m1). Each reaction used 1 μL of cDNA template.

Western blotting

N42 neurons were grown as described earlier. The cell culture medium was collected and protein concentrated using an Amicon Ultra-0.5 Centrifugal Filter (10 K device, Millipore, UK). For lysate preparation, cells were scraped into 1 ml of PBS and pelleted by centrifugation; 1 ml of M-PER mammalian protein extraction reagent (Thermo scientific) was added to the cell pellet before sonication using a Sanyo Soniprep 1500 to ensure complete cell lysis. Protein concentrations were determined using the Pierce 660 nm protein assay reagent (Thermo Scientific). Samples were then diluted 3:1 with 4× Laemmli sample buffer (Bio-Rad, UK) with 2-mercaptoethanol (9:1 ratio) and boiled for 10 min, and 2 μg of protein was loaded on the gels. For media in which no cells were cultured, used as a control, an amount equivalent to 5 μL of concentrated media was loaded and as a positive control 12.5 ng of recombinant mouse serpin α1AC protein (R&D Systems). Proteins were separated on 10% mini-PROTEANTGX Precast Gels (Bio-Rad) and transferred to a PVDF Membrane (Bio-Rad) before immuno-detection using goat anti-mouse serpinA3N (R&D Systems) and peroxidase-linked secondary antibody (Donkey polyclonal antibody to goat IgG (HRP), abcam, UK). Chemiluminescent signal on the blots was detected using a Fujifilm LAS-3000 Imager after incubation with Clarity Western ECL substrate kit (Bio-Rad) using the manufacturer’s recommended protocol. Additional gels were run in parallel and stained with Colloidal Coomassie Blue (Safe Stain) (Severn Biotech Ltd) in order to visualise total protein present in cell media and lysates.

Statistical analysis

Data are presented as mean ± SEM and were analysed using GenStat (GenStat, Eighth Edition (2005), VSN International Ltd., Oxford). In the case of experiments testing the influence of a single factor, a one-way ANOVA was performed. Where two or three factors were compared in a single experiment, a two- or three-way ANOVA followed by post hoc Student’s t tests based on the LSD were performed. In this case, the ANOVA results are expressed in the figure legend and the results of the Student t test are represented on the graph. P < 0.05 was considered statistically significant.

Abbreviations

AgRP:

Agouti-related peptide

ANOVA:

Analysis of variance

ARC:

Arcuate nuclei

BSA:

Bovine serum albumin

CART:

Cocaine- and amphetamine-regulated transcript

db/db :

Diabetic obese mice with a spontaneous non-functional mutation in the leptin receptor

DMEM:

Dulbecco’s modified Eagle’s medium

DMH:

Dorsomedial nuclei of the hypothalamus

GFAP:

Glial fibrillary acidic protein

HFD:

High-fat diet

Iba1:

Ionised calcium binding adaptor molecule 1

IKKβ:

Inhibitor of nuclear factor kappa-B kinase subunit β

IL-1:

Interleukin-1

IL-1R1 −/− :

Interleukin-1 receptor knockout mice

IL-6:

Interleukin-6

IOD:

Integrated optical density

IP:

Intraperitoneal

JNK:

c-Jun amino-terminal kinase

kCal:

Kilocalories

LFD:

Low-fat diet

LH:

Lateral hypothalamus

LSD:

Least significant difference

N42:

mHypoE-N42 hypothalamic neuronal cell line

NFκB:

Nuclear factor kappa-light-chain-enhancer of activated B cells

NPY:

Neuropeptide Y

NuGO:

Nutrigenomics Organization

ob/ob :

Obese mice with a spontaneous mutation in the gene which produces leptin

PBS:

Phosphate-buffered saline

POMC:

Proopiomelanocortin

SEM:

Standard error of the mean

SSC:

Standard saline citrate

TLR4:

Toll-like receptor 4

TNFα :

Tumor necrosis factor alpha

UCD:

University College Dublin

VMH:

Ventromedial nuclei of the hypothalamus

α1AC:

Alpha 1-antichymotrypsin

References

  1. World Health Organisation. Obesity and overweight. Fact sheet No311. 2014.

    Google Scholar 

  2. Brown WV, Fujioka K, Wilson PW, Woodworth KA. Obesity: why be concerned? Am J Med. 2009;122:S4–11.

    Article  Google Scholar 

  3. Luchsinger JA, Gustafson DR. Adiposity, type 2 diabetes, and Alzheimer’s disease. J Alzheimers Dis. 2009;16:693–704.

    Article  Google Scholar 

  4. Mann T, Tomiyama AJ, Westling E, Lew AM, Samuels B, Chatman J. Medicare’s search for effective obesity treatments: diets are not the answer. Am Psychol. 2007;62:220–33.

    Article  Google Scholar 

  5. Madsbad S, Dirksen C, Holst JJ. Mechanisms of changes in glucose metabolism and bodyweight after bariatric surgery. Lancet Diabetes Endocrinol. 2014;2:152–64.

    Article  CAS  Google Scholar 

  6. Maclean PS, Bergouignan A, Cornier MA, Jackman MR. Biology’s response to dieting: the impetus for weight regain. Am J Phys. 2011;301:R581–600.

    CAS  Google Scholar 

  7. Jeffery RW, Harnack LJ. Evidence implicating eating as a primary driver for the obesity epidemic. Diabetes. 2007;56:2673–6.

    Article  CAS  Google Scholar 

  8. Berkseth KE, Guyenet SJ, Melhorn SJ, Lee D, Thaler JP, Schur EA, et al. Hypothalamic gliosis associated with high fat diet feeding is reversible in mice: a combined immunohistochemical and magnetic resonance imaging study. Endocrinology. 2014;141:2858–67.

    Article  Google Scholar 

  9. Gao Y, Ottaway N, Schriever SC, Legutko B, Garcia-Caceres C, de lF, et al. Hormones and diet, but not body weight, control hypothalamic microglial activity. Glia. 2014;62:17–25.

    Article  Google Scholar 

  10. Thaler JP, Schwartz MW. Minireview: inflammation and obesity pathogenesis: the hypothalamus heats up. Endocrinology. 2010;151:4109–15.

    Article  CAS  Google Scholar 

  11. Zigman JM, Elmquist JK. Minireview: from anorexia to obesity--the yin and yang of body weight control. Endocrinology. 2003;144:3749–56.

    Article  CAS  Google Scholar 

  12. Halaas JL, Boozer C, Blair-West J, Fidahusein N, Denton DA, Friedman JM. Physiological response to long-term peripheral and central leptin infusion in lean and obese mice. Proc Natl Acad Sci. 1997;94:8878–83.

    Article  CAS  Google Scholar 

  13. Scarpace PJ, Zhang Y. Leptin resistance: a prediposing factor for diet-induced obesity. Am J Phys. 2009;296:R493–500.

    CAS  Google Scholar 

  14. Van Dijk G, De Vries K, Nyakas C, Buwalda B, Adage T, Kuipers F, et al. Reduced anorexigenic efficacy of leptin, but not of the melanocortin receptor agonist melanotan-II, predicts diet-induced obesity in rats. Endocrinology. 2005;146:5247–56.

    Article  CAS  Google Scholar 

  15. Koch C, Augustine RA, Steger J, Ganjam GK, Benzler J, Pracht C, et al. Leptin rapidly improves glucose homeostasis in obese mice by increasing hypothalamic insulin sensitivity. J Neurosci. 2010;30:16180–7.

    Article  CAS  Google Scholar 

  16. Tups A, Benzler J, Sergi D, Ladyman SR, Williams LM. Central regulation of glucose homeostasis. Compr Physiol. 2017;7:741–64.

    Article  Google Scholar 

  17. Thaler JP, Yi CX, Schur EA, Guyenet SJ, Hwang BH, Dietrich MO, et al. Obesity is associated with hypothalamic injury in rodents and humans. J Clin Invest. 2012;122:153–62.

    Article  CAS  Google Scholar 

  18. Milanski M, Degasperi G, Coope A, Morari J, Denis R, Cintra DE, et al. Saturated fatty acids produce an inflammatory response predominantly through the activation of TLR4 signaling in hypothalamus: implications for the pathogenesis of obesity. J Neurosci. 2009;29:359–70.

    Article  CAS  Google Scholar 

  19. Kleinridders A, Schenten D, Konner AC, Belgardt BF, Mauer J, Okamura T, et al. MyD88 signaling in the CNS is required for development of fatty acid-induced leptin resistance and diet-induced obesity. Cell Metab. 2009;10:249–59.

    Article  CAS  Google Scholar 

  20. Zhang X, Zhang G, Zhang H, Karin M, Bai H, Cai D. Hypothalamic IKKbeta/NF-kappaB and ER stress link overnutrition to energy imbalance and obesity. Cell. 2008;135:61–73.

    Article  CAS  Google Scholar 

  21. Cai D, Liu T. Inflammatory cause of metabolic syndrome via brain stress and NF-kappaB. Aging. 2012;4:98–115.

    Article  CAS  Google Scholar 

  22. Koch CE, Lowe C, Pretz D, Steger J, Williams LM, Tups A. High-fat diet induces leptin resistance in leptin-deficient mice. J Neuroendocrinol. 2014;26:58–67.

    Article  CAS  Google Scholar 

  23. Hirosumi J, Tuncman G, Chang L, Gorgun CZ, Uysal KT, Maeda K, et al. A central role for JNK in obesity and insulin resistance. Nature. 2002;420:333–6.

    Article  CAS  Google Scholar 

  24. Tuncman G, Hirosumi J, Solinas G, Chang L, Karin M, Hotamisligil GS. Functional in vivo interactions between JNK1 and JNK2 isoforms in obesity and insulin resistance. Proc Natl Acad Sci. 2006;103:10741–6.

    Article  CAS  Google Scholar 

  25. Vijay-Kumar M, Aitken JD, Carvalho FA, Cullender TC, Mwangi S, Srinivasan S, et al. Metabolic syndrome and altered gut microbiota in mice lacking Toll-like receptor 5. Science. 2010;328:228–31.

    Article  CAS  Google Scholar 

  26. Benzler J, Ganjam GK, Legler K, Stohr S, Kruger M, Steger J, et al. Acute inhibition of central c-Jun N-terminal kinase restores hypothalamic insulin signalling and alleviates glucose intolerance in diabetic mice. J Neuroendocrinol. 2013;25:446–54.

    Article  CAS  Google Scholar 

  27. Baker C, Belbin O, Kalsheker N, Morgan K. SERPINA3 (aka alpha-1-antichymotrypsin). Front Biosci. 2007;12:2821–35.

    Article  CAS  Google Scholar 

  28. Zamanian JL, Xu L, Foo LC, Nouri N, Zhou L, Giffard RG, et al. Genomic analysis of reactive astrogliosis. J Neurosci. 2012;32:6391–410.

    Article  CAS  Google Scholar 

  29. Sardi F, Fassina L, Venturini L, Inguscio M, Guerriero F, Rolfo E, et al. Alzheimer’s disease, autoimmunity and inflammation. The good, the bad and the ugly. Autoimmun Rev. 2011;11:149–53.

    Article  CAS  Google Scholar 

  30. Furby A, Leys D, Delacourte A, Buee L, Soetaert G, Petit H. Are alpha-1-antichymotrypsin and inter-alpha-trypsin inhibitor peripheral markers of Alzheimer’s disease? J Neurol Neurosurg Psychiatry. 1991;54:469.

    Article  CAS  Google Scholar 

  31. Cichy J, Potempa J, Chawla RK, Travis J. Stimulatory effect of inflammatory cytokines on alpha 1-antichymotrypsin expression in human lung-derived epithelial cells. J Clin Invest. 1995;95:2729–33.

    Article  CAS  Google Scholar 

  32. Cichy J, Potempa J, Chawla RK, Travis J. Regulation of alpha 1-antichymotrypsin synthesis in cells of epithelial origin. FEBS Lett. 1995;359:262–6.

    Article  CAS  Google Scholar 

  33. Mrak RE, Griffin WS. Interleukin-1 and the immunogenetics of Alzheimer disease. J Neuropathol Exp Neurol. 2000;59:471–6.

    Article  CAS  Google Scholar 

  34. Machein U, Lieb K, Hull M, Fiebich BL. IL-1 beta and TNF alpha, but not IL-6, induce alpha 1-antichymotrypsin expression in the human astrocytoma cell line U373 MG. Neuroreport. 1995;6:2283–6.

    Article  CAS  Google Scholar 

  35. Cai D. Neuroinflammation in overnutrition-induced diseases. Vitam Horm. 2013;91:195–218.

    Article  CAS  Google Scholar 

  36. Williams LM. Hypothalamic dysfunction in obesity. Proc Nutr Soc. 2012;71:521–33.

    Article  CAS  Google Scholar 

  37. Dickson I, Alper CA. Changes in serum proteinase inhibitor levels following bone surgery. Clin Chim Acta. 1974;54:381–5.

    Article  CAS  Google Scholar 

  38. Zhang S, Janciauskiene S. Multi-functional capability of proteins: alpha1-antichymotrypsin and the correlation with Alzheimer’s disease. J Alzheimers Dis. 2002;4:115–22.

    Article  CAS  Google Scholar 

  39. Licastro F, Mallory M, Hansen LA, Masliah E. Increased levels of alpha-1-antichymotrypsin in brains of patients with Alzheimer’s disease correlate with activated astrocytes and are affected by APOE 4 genotype. J Neuroimmunol. 1998;88:105–10.

    Article  CAS  Google Scholar 

  40. Abraham CR, Selkoe DJ, Potter H. Immunochemical identification of the serine protease inhibitor alpha 1-antichymotrypsin in the brain amyloid deposits of Alzheimer's disease. Cell. 1988;52:487–501.

    Article  CAS  Google Scholar 

  41. Kilpatrick L, Johnson JL, Nickbarg EB, Wang ZM, Clifford TF, Banach M, et al. Inhibition of human neutrophil superoxide generation by alpha 1-antichymotrypsin. J Immunol. 1991;146:2388–93.

    CAS  PubMed  Google Scholar 

  42. Takada S, Tsuda M, Yamamura M, Katsunuma T. Effect of alpha-1-antichymotrypsin on activity of DNA primase isolated from human stomach adenocarcinoma cells. Biochem Int. 1988;16:949–54.

    CAS  PubMed  Google Scholar 

  43. Tsuda M, Masuyama M, Katsunuma T. Inhibition of human DNA polymerase alpha by alpha 1-antichymotrypsin. Cancer Res. 1986;46:6139–42.

    CAS  PubMed  Google Scholar 

  44. Titolo D, Cai F, Belsham DD. Coordinate regulation of neuropeptide Y and agouti-related peptide gene expression by estrogen depends on the ratio of estrogen receptor (ER) α to ERβ in clonal hypothalamic neurons. Mol Endocrinol. 2006;20:2080–92.

    Article  CAS  Google Scholar 

  45. Buckman LB, Thompson MM, Moreno HN, Ellacott KL. Regional astrogliosis in the mouse hypothalamus in response to obesity. J Comp Neurol. 2013;521:1322–33.

    Article  CAS  Google Scholar 

  46. Bode JG, Albrecht U, Haussinger D, Heinrich PC, Schaper F. Hepatic acute phase proteins--regulation by IL-6- and IL-1-type cytokines involving STAT3 and its crosstalk with NF-kappaB-dependent signaling. Eur J Cell Biol. 2012;91:496–505.

    Article  CAS  Google Scholar 

  47. Luheshi GN, Gardner JD, Rushforth DA, Loudon AS, Rothwell NJ. Leptin actions on food intake and body temperature are mediated by IL-1. Proc Natl Acad Sci. 1999;96:7047–52.

    Article  CAS  Google Scholar 

  48. Lyons CL, Kennedy EB, Roche HM. Metabolic inflammation-differential modulation by dietary constituents. Nutrients. 2016;8:247.

    Article  Google Scholar 

  49. Rivest S. How circulating cytokines trigger the neural circuits that control the hypothalamic-pituitary-adrenal axis. Psychoneuroendocrinology. 2001;26:761–88.

    Article  CAS  Google Scholar 

  50. Kim JG, Suyama S, Koch M, Jin S, Argente-Arizon P, Argente J, Liu ZW, Zimmer MR, Jeong JK, Szigeti-Buck K, Gao Y, Garcia-Caceres C, Yi CX, Salmaso N, Vaccarino FM, Chowen J, Diano S, Dietrich MO, Tschöp MH, Horvath TL. Leptin signaling in astrocytes regulates hypothalamic neuronal circuits and feeding. Nat Neurosci. 2014;17:908–10.

    Article  CAS  Google Scholar 

  51. Hardie LJ, Rayner DV, Holmes S, Trayhurn P. Circulating leptin levels are modulated by fasting, cold exposure and insulin administration in lean but not Zucker (fa/fa) rats as measured by ELISA. Biochem Biophys Res Commun. 1996;223:660–5.

    Article  CAS  Google Scholar 

  52. Teusink B, Voshol PJ, Dahlmans VE, Rensen PC, Pijl H, Romijn JA, Havekes LM. Contribution of fatty acids released from lipolysis of plasma triglycerides to total plasma fatty acid flux and tissue-specific fatty acid uptake. Diabetes. 2003;52:614–20.

    Article  CAS  Google Scholar 

  53. Flurkey K, Currer JM, Harrison D. Mouse models in aging research. In: The mouse in biomedical research. 2nd ed. Amsterdam: Elsevier; 2007. p. 637–72.

    Chapter  Google Scholar 

  54. Zhang G, Li J, Purkayastha S, Tang Y, Zhang H, Yin Y, Li B, Liu G, Cai D. Hypothalamic programming of systemic ageing involving IKK-β, NF-κB and GnRH. Nature. 2013;497:211–6.

    CAS  PubMed  Google Scholar 

  55. Baccini M, Bachmaier EM, Biggeri A, Boekschoten MV, Bouwman FG, Brennan L, et al. The NuGO proof of principle study package: a collaborative research effort of the European Nutrigenomics Organisation. Genes Nutr. 2008;3:147–51.

    Article  CAS  Google Scholar 

  56. Mitchell SE, Robinson JJ, King ME, McKelvey WAC, Williams LM. Interleukin-8 in the cervix of non-pregnant ewes pregnancy. Reproduction. 2002;124:409–16.

    Article  CAS  Google Scholar 

  57. Paxinos G, Tork I, Tecott LH, Valentino KL. Atlas of the developing rat brain. San Diego: Academic; 1991.

    Google Scholar 

  58. Edgar R, Domrachev M, Lash AE. Gene Expression Omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res. 2002;30:207–10.

    Article  CAS  Google Scholar 

Download references

Funding

LMW, CG, ACM, EB, AM, BdR, MVB, MM and C-DM were supported by a project grant from NuGO; LMW, AM and FHM were supported by a project support grant from the British Society for Neuroendocrinology; DS was supported by a SULSA studentship; FHM was supported by a EASTBIO DTP BBSRC studentship; LMW, CG, ACM, EB, BdR, C-DM, FMC, PN, JED and NH were funded by the Scottish Government’s Rural and Environment Science and Analytical Services Division (RESAS).

AT and KC were funded by the German Ministry of Research and Education (Ref. No: 0315087).

HMR was supported by the Irish Department of Agriculture, Food and Marine ImmunoMet Programme (14/F/828). FCM and HMR were supported by Science Foundation Ireland Principal Investigator Programme (11/PI/1119).

RN and CD were supported by grants from Ministerio de Economia y Competitividad (CD: BFU2011-29102; RN: BFU2012-35255), Xunta de Galicia (RN: EM 2012/039 and 2012-CP069). Centro de Investigación Biomédica en Red (CIBER) de Fisiopatología de la Obesidad y Nutrición (CIBERobn). CIBERobn is an initiative of the Instituto de Salud Carlos III (ISCIII) of Spain which is supported by FEDER funds. The research leading to these results has also received funding from the European Community’s Seventh Framework Programme under the following grants: no 245009: NeuroFAST to CD and ERC StG-2011-OBESITY53-281408 to RN.

Availability of data and materials

The transcriptomic data discussed in this publication have been deposited in NCBI’s Gene Expression Omnibus [58] and are accessible through GEO Series accession number GSE113943 (https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE113943) (https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi).

Author information

Authors and Affiliations

  1. Rowett Institute, University of Aberdeen, Aberdeen, AB25 2ZD, UK

    Domenico Sergi, Fiona M. Campbell, Christine Grant, Amanda C. Morris, Eva-Maria Bachmair, Fiona H. McLean, Aifric Muller, Nigel Hoggard, Baukje de Roos, Darcy Kahn, Phyllis Nicol, Janice E. Drew & Lynda M. Williams

  2. Department of Animal Physiology, Faculty of Biology, Philipps University Marburg, Karl-von-Frisch Str. 8, 35043, Marburg, Germany

    Christiane Koch, Jonas Benzler & Alexander Tups

  3. Centre for Neuroendocrinology and Brain Health Research Centre, Department of Physiology, School of Medical Sciences, University of Otago, Dunedin, 9054, New Zealand

    Christiane Koch, Jonas Benzler & Alexander Tups

  4. Department of Physiology, University of Santiago de Compostela, 15705, Santiago de Compostela, Spain

    Begona Porteiro, Ruben Nogueiras & Carlos Dieguez

  5. CIBER Fisiopatología de la Obesidad y Nutrición (CIBERobn), Madrid, Spain

    Begona Porteiro, Ruben Nogueiras & Carlos Dieguez

  6. Nutrition, Metabolism and Genomics Group, Division of Human Nutrition, Wageningen University, Wageningen, The Netherlands

    Mark V. Boekschoten

  7. Nutrigenomics Research Group, UCD Conway Institute, University College Dublin, Dublin, Ireland

    Fiona C. McGillicuddy & Helen M. Roche

  8. Biomathematics & Statistics Scotland (BioSS), Rowett Institute, University of Aberdeen, Aberdeen, AB25 2ZD, UK

    Claus-Dieter Mayer

  9. Nutrigenomics and Systems Nutrition Group, Norwich Medical School, University of East Anglia, Norwich, NR4 7UQ, UK

    Michael Muller

Authors
  1. Domenico Sergi
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Fiona M. Campbell
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Christine Grant
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Amanda C. Morris
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Eva-Maria Bachmair
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Christiane Koch
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Fiona H. McLean
    View author publications

    You can also search for this author in PubMed Google Scholar

  8. Aifric Muller
    View author publications

    You can also search for this author in PubMed Google Scholar

  9. Nigel Hoggard
    View author publications

    You can also search for this author in PubMed Google Scholar

  10. Baukje de Roos
    View author publications

    You can also search for this author in PubMed Google Scholar

  11. Begona Porteiro
    View author publications

    You can also search for this author in PubMed Google Scholar

  12. Mark V. Boekschoten
    View author publications

    You can also search for this author in PubMed Google Scholar

  13. Fiona C. McGillicuddy
    View author publications

    You can also search for this author in PubMed Google Scholar

  14. Darcy Kahn
    View author publications

    You can also search for this author in PubMed Google Scholar

  15. Phyllis Nicol
    View author publications

    You can also search for this author in PubMed Google Scholar

  16. Jonas Benzler
    View author publications

    You can also search for this author in PubMed Google Scholar

  17. Claus-Dieter Mayer
    View author publications

    You can also search for this author in PubMed Google Scholar

  18. Janice E. Drew
    View author publications

    You can also search for this author in PubMed Google Scholar

  19. Helen M. Roche
    View author publications

    You can also search for this author in PubMed Google Scholar

  20. Michael Muller
    View author publications

    You can also search for this author in PubMed Google Scholar

  21. Ruben Nogueiras
    View author publications

    You can also search for this author in PubMed Google Scholar

  22. Carlos Dieguez
    View author publications

    You can also search for this author in PubMed Google Scholar

  23. Alexander Tups
    View author publications

    You can also search for this author in PubMed Google Scholar

  24. Lynda M. Williams
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

DS, CG, ACM, E-MB, CK, FHM, BP, MVB, FCM, DK, PN and JB carried out the experimental work. DS, BdR FMC, C-DM, JD, HMR, MM, RN, CD, AT and LMW were responsible for the experimental design and data analysis and wrote the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Lynda M. Williams.

Ethics declarations

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Sergi, D., Campbell, F.M., Grant, C. et al. SerpinA3N is a novel hypothalamic gene upregulated by a high-fat diet and leptin in mice. Genes Nutr 13, 28 (2018). https://doi.org/10.1186/s12263-018-0619-1

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12263-018-0619-1

Keywords

  • SerpinA3N
  • Hypothalamus
  • High-fat diet
  • Leptin

Genes & Nutrition

ISSN: 1865-3499

Contact us