Oxytocin sets the stage for childbirth by initiating uterine contractions, lactation and maternal bonding behaviours. Mice lacking secreted oxcytocin (Oxt−/−, Cd38−/−) or its receptor (Oxtr−/−) fail to nurture. Normal maternal behaviour is restored by peripheral oxcytocin replacement in Oxt−/− and Cd38−/−, but not Oxtr−/− mice, implying that circulating oxcytocin crosses the blood-brain barrier. Exogenous oxcytocin also has behavioural effects in humans. However, circulating polypeptides are typically excluded from the brain. We show that oxcytocin is transported into the brain by receptor for advanced glycation end-products (RAGE) on brain capillary endothelial cells. The increases in oxcytocin in the brain which follow exogenous administration are lost in Ager−/− male mice lacking RAGE, and behaviours characteristic to abnormalities in oxcytocin signalling are recapitulated in Ager−/− mice, including deficits in maternal bonding and hyperactivity. Our findings show that RAGE-mediated transport is critical to the behavioural actions of oxcytocin associated with parenting and social bonding.
Oxytocin mediates both physiological and psychosocial events surrounding mammalian birth, including uterine contractions, initiation of lactation, and maternal bonding1,2. Oxytocin produced by oxytocinergic neurons in hypothalamic paraventricular and supraoptic nuclei (PVN, SON) has both central and peripheral actions, the latter through posterior pituitary release into the circulation1,2,3,4,5,6. Systemic loss of either oxytocin or oxytocin receptors (Oxt−/− and Oxtr−/−) disrupts maternal nurturing behaviours in mice7,8. This is restored by administration of exogenous oxytocin in Oxt−/− but not Oxtr−/− mice, suggesting that peripheral oxytocin has central effects. Mice lacking CD38, a cyclic ADP ribose synthetase and hydrolase necessary for secretion of oxytocin, also display this characteristic behavioural phenotype, which is also reversed following administration of exogenous oxytocin5,9. Exogenous oxytocin in humans also appears to have behavioural effects, particularly in such social deficit-related psychiatric disorders as autism and schizophrenia9,10,11,12,13. Numerous clinical trials are determining the psychopharmacological effects of peripherally administered oxytocin in a variety of conditions14,15. The potential for peripherally administered oxytocin to act centrally is supported by measures of it in the brain. Oxytocin concentrations are maximal in human or primate cerebrospinal fluid (CSF) and mammalian hippocampus and amygdala within 10–60 min of peripheral administration16,17,18,19. Because many peripheral peptides and proteins do not pass freely into the central nervous system (CNS)20,21, we hypothesised a specialised uptake mechanism for oxytocin to cross the blood-brain barrier (BBB) and gain access to the CNS.
RAGE, a member of the immunoglobulin superfamily of pattern recognition receptors, is not known to be related to oxytocin or oxytocin signalling22,23,24,25,26,27,28,29,30,31,32,33. Full-length, membrane bound RAGE (mRAGE) is present on many cell types. Endogenous soluble RAGE (esRAGE), the product of an alternatively spliced mRNA, is found in the circulation as it lacks a membrane-spanning domain29,34. A second soluble form, ectodomain-shed RAGE (sRAGE), is a proteolytic product of mRAGE28,30. The three RAGE forms bind various ligands with similar affinities, including multiple advanced glycation end-products (AGEs) and amyloid β peptide31,32,33,34,35,36,37.
Here, our findings show that the expression of RAGE on capillary endothelial cells of the blood-brain barrier (BBB) is both necessary and sufficient for the transport of oxytocin into the brain. The increases in oxytocin in the brain which follow exogenous administration are lost in RAGE knockout male mice (Ager−/− mice lacking the mouse receptor for AGEs gene). Behaviours characteristic to abnormalities in oxytocin signalling are recapitulated in Ager−/− mice, including deficits in maternal bonding and hyperactivity, and both transport and behavioural deficits are restored in Ager−/− mice following transgenic, endothelial cell expression of RAGE. These findings indicate that RAGE-mediated transport can explain the degree of brain oxytocin recruitment previously reported at the molecular level, and demonstrate that oxytocin is critical to the behavioural actions of oxytocin associated with parenting and social bonding.
Survival of Ager gene null (Ager−/−) pups is often low due to maternal neglect, with even mild maternal stress leading to dramatic reductions in offspring survival (Fig. 1a). This is clearly a maternal deficit, as newborn Ager−/− pups transferred to wild-type (WT) post-partum mothers are nurtured and survive at near normal frequencies. By contrast, normal offspring of WT mothers do poorly when transferred to post-partum Ager−/− mothers (Fig. 1b). Offspring neglect in the absence of gross anatomic or histological defects is a behavioural deficit reminiscent of the characteristic disorders seen with loss of oxytocin function, as in Oxt−/−, Oxtr−/− or Cd38−/− mice5,7,8,9,38,39,40. Survival rates for Ager−/− pups fostered by WT mothers were lower than for WT offspring raised by their WT mothers, and survival rates for WT pups transferred to Ager−/− mothers tend to be higher than for Ager−/− offspring raised by their Ager−/− mothers (Fig. 1a, b). This too is seen in Oxt−/−, Oxtr−/−, or Cd38−/− mice and attributable to intrauterine and peripartum effects of loss of oxytocin function occurring prior to the exchange of offspring. We therefore hypothesised potential interactions between oxytocin and RAGE signalling pathways.
Multiple methods were used to demonstrate direct binding of oxytocin and RAGE. Surface plasmon resonance methods showed concentration-dependent oxytocin binding to immobilised recombinant esRAGE, with an apparent dissociation constant (KD) of 179 nM (Fig. 1c). Oxytocin-RAGE binding was further confirmed using plate assays where either oxytocin or esRAGE was immobilised, and esRAGE or oxytocin was in solution, respectively (Fig. 1d, e).
Endogenous oxytocin and soluble RAGE also associate in human circulation. Using gel permeation chromatography to separate serum proteins based on molecular size, oxytocin immunoreactivity co-eluted with soluble RAGE (Supplementary Figure 1a). Larger amounts of free oxytocin eluted later, as the molar amount of oxytocin in blood exceeds that of soluble RAGE. Endogenous oxytocin in human serum (30 pmol/50 ml) also co-eluted with soluble RAGE following isolation by anti-RAGE antibody affinity chromatography (Supplementary Figure 1b). Mass spectrometry was employed for further structural identification. In this case, we used immobilised esRAGE to isolate oxytocin from 50 ml human serum, and repeated the procedure after adding a synthetic oxytocin standard (100 ng) (Supplementary Figure 1c). Analyses of the eluted fractions by liquid chromatography-tandem mass spectrometry (LC-MS/MS) showed that endogenous oxytocin in human serum is structurally indistinguishable from the synthetic oxytocin standard, as they eluted at identical times (Supplementary Figure 1d) and have identical parent ions (M+H+ 1008.2). Mass spectrometry of the eluted material from the immobilised esRAGE did not identify structurally related peptides such as arginine-vasopressin which may cross-react in immunoassays.
Oxytocin binding to soluble RAGE suggests it also binds membrane RAGE, but oxytocin neither stimulates a RAGE-dependent NF-κB reporter nor inhibits reporter induction by AGEs, a ligand that activates the NF-κB reporter22,27 (Supplementary Figure 2a). Furthermore, oxytocin did not activate NF-κB-independent Rac1 or Cdc42 signalling, which are also suggested to function downstream of RAGE24,41,42 (Supplementary Figures 2b and 2c). Therefore, while oxytocin binds soluble and presumably membrane RAGE, it neither induces nor inhibits intracellular signals reported for RAGE ligands. Moreover, oxytocin binding to soluble RAGE was weakly or non-specifically inhibited by potential RAGE ligands: S100B, AGEs, amyloid β or high-mobility group B1 (HMGB1)24,35,42 (Supplementary Figures 3a–d).
To further explore potential oxytocin-RAGE binding modes, we subdivided extracellular RAGE into its V, C1 and C2 domains. S100B, AGEs, amyloid β, and HMGB1 all bind the RAGE V domain24,28. Oxytocin binding to soluble RAGE was blocked by addition of recombinant V domain, marginally inhibited by C1 domain, and not blocked by C2 domain (Supplementary Figure 3e), suggesting that oxytocin binds the V domain, but at a distinct site from S100B, AGEs, amyloid β or HMGB142,43.
Oxytocin transport across the BBB
In vitro model systems are used to predict the ability of compounds to cross into the CNS and exert central effects44,45. We used one such system constructed using primary cultures of monkey brain capillary endothelial cells (EC) coupled with rat pericytes and astrocytes to assess requirements46 for endothelial RAGE in the transport of oxytocin (Fig. 2a). Endothelial transport of oxytocin was dose-dependent (Fig. 2b) and of a similar rate to transport of centrally acting drugs46. RAGE was either left at endogenous levels or reduced in the ECs by shRNA knockdown (Fig. 2c). The integrity of the in vitro primate “BBB” was unaffected by RAGE knockdown, assessed by high transendothelial electrical resistance (TEER) (Fig. 2d). Notably, oxytocin transport was reduced selectively in the blood-to-brain direction following RAGE knockdown (Fig. 2b). Reverse transport was much less efficient (Fig. 2e), and according to calculated apparent permeability (Papp) measures, inconsequential (Fig. 2f).
Immunohistochemical analyses showed RAGE in vascular patterns limited to CD31 (platelet endothelial cell adhesion molecule)-positive endothelial cells23, which are the components of the BBB, of the hippocampus and choroid plexus of WT (Fig. 3a, b) but not of Ager−/− mice (Supplementary Figure 4a). We also performed confocal microscopic analyses to observe RAGE expression in the circumventricular organs (CVOs) of the brain, referred to as ‘windows of the brain’, and found that RAGE expression was clearly observable in the endothelial cells of the neurohypophysis (Supplementary Figure 4b), but barely in those of the sensory CVOs, including the organum vasculosum of the lamina terminalis, subfornical organ, and area postrema. Further analysis revealed co-localisation of RAGE with cavelolin-1, a marker of plasma membrane invaginations (caveolae), in endothelial cells and the choroid plexus in WT mice (Supplementary Figure 4c), suggesting a role of RAGE in the oxytocin transfer (trafficking) through caveolae-associated endocytosis and transcytosis (Supplementary Figure 4d). By contrast, oxytocin receptors, which could theoretically act as oxytocin transporters, were not co-localised with endothelial cells in numerous sections of 5 brain regions of Venus mice expressing a fluorescent oxytocin receptor reporter47 (Supplementary Figures 4e and f).
RAGE-dependent transport of oxytocin across the BBB
Oxytocin concentrations in blood and CSF were assessed following a subcutaneous injection of oxytocin (30 ng/mouse; approximately 1.1 μg/kg of body weight). Steady-state levels in blood (~20 pg/ml) increased rapidly, peaking within 10 min after injection and returning to baseline by 1–2 h in both WT and Ager−/− male mice (Supplementary Figure 5a). By contrast, levels of oxytocin in CSF from the cisterna magna of WT mice increased more gradually to maxima at 1–2 h before returning to baseline at 4 h (Fig. 4a). Despite equivalently high serum levels following injection of identical amounts of oxytocin (Supplementary Figure 5a), concentrations in the CSF of Ager−/− mice remained at baseline levels (Fig. 4a).
In separate experiments we cannulated the third ventricles of WT and Ager−/− mice and withdrew CSF for oxytocin measurements. Following subcutaneous injection, oxytocin increased in third ventricle CSF of WT but not Ager−/− male mice (Fig. 4b and Supplementary Figure 5b). Microperfusion methods showed that oxytocin also increased in relevant regions of the brain, including the amygdala and PVN of the hypothalamus, of WT but not Ager−/− male mice following subcutaneous, intravenous or intranasal administration of oxytocin but not saline carrier (Fig. 4c, d and Supplementary Figure 5c). The direct CSF measures (Fig. 4a, b) and microperfusion results (Fig. 4c, d) confirm that oxytocin in the blood is transported across the BBB as suggested by Landgraf and his collegues16,17,20 and to our knowledge, show for the first time that endothelial RAGE is required for oxytocin transport into the CNS.
Because this is such an important point, we further investigated oxytocin transport following selective transgenic (Tg) expression of RAGE in endothelial cells of both WT and Ager−/− mice using an Flk-1 promoter26,41. Protein expression in both lines was equivalent to the amount of endogenous endothelial RAGE in WT mice (WT = 1, WT + Tg~2, KO + Tg~1). CSF concentrations were measured following subcutaneous injections of oxytocin. Tg expression in Ager−/− mice increased oxytocin in CSF to the WT concentration, whereas Tg expression in WT mice minimally affected CSF oxytocin concentrations (Fig. 4e and Supplementary Figure 5d). Stable isotope-labelled oxytocin was used to more accurately assess transport into the CSF. Following subcutaneous injection, [13C,15N]oxytocin was undetectable in CSF of Ager−/− male mice, whereas amounts in the CSF of WT or KO + Tg mice were equivalent (Fig. 4f and Supplementary Figure 5e). Although oxytocin has been found to produce sex-specific effects48,49,50, RAGE-mediated oxytocin transport was also observed in female WT-mice (Fig. 4g). These results demonstrated that RAGE is both necessary and sufficient for oxytocin transport into the brain in both male and female mice.
Endothelial RAGE is upregulated in brain capillaries after bilateral common carotid artery occlusion (BCCAO)23. Using this method we found a ~2-fold increase in capillary RAGE (Fig. 5a, b). We predicted this would also promote oxytocin transport. As a control, we showed this procedure does not cause fluorescein to leak into the CSF (Fig. 5c), suggesting there is not a generalised increase in vascular permeability. Nevertheless, exogenous oxytocin increased in the CSF of WT but not Ager−/− male mice after bilateral carotid occlusion (Fig. 5d and Supplementary Figure 5f).
c-Fos as CNS actions of oxytocin
The classical studies of Numan showed c-Fos positive neurons are activated during the acquisition of postpartum maternal behaviours51. We utilised the nuclear translocation of c-Fos as a readout for the neuronal actions of oxytocin52, which are now known to activate c-Fos positive neurons51,52,53. Numbers of c-Fos positive nuclei increased after subcutaneous oxytocin administration in four distinct regions of the brain, the bed nucleus of the stria terminalis (BNST), medial preoptic area (mPOA), centre of the anterior hypothalamic area (AHC) and ventral portion of the intermediate lateral septal nucleus (ILS) (Fig. 6a, b). This is dependent on both oxytocin and RAGE, as there are no effects in Ager−/− male mice or when vehicle control was administered (Fig. 6b).
Loss of maternal nurturing and social interactive behaviours in Cd38−/− mice have been restored following peripheral administration of oxytocin, consistent with transport of peripherally administered exogenous oxytocin into brain5. We would not expect this to reverse the maternal bonding deficit in RAGE-null Ager−/− mice, as endothelial RAGE appears to be required for CNS entry of peripheral oxytocin. Survival of Ager−/− pups is often low due to maternal neglect, with even mild maternal stress leading to dramatic reductions in offspring survival (Fig. 7a). However, our findings predict that restoration of endothelial RAGE in Ager−/− mice would reverse the behavioural phenotypes. There was a substantial rescue of the Ager−/− phenotype, as 63.4% of the transgenic Ager−/− (KO + Tg) offspring survived, compared to only 10.5% survival for the non-transgenic Ager−/− (KO) offspring (P < 0.001) (Fig. 7a). Litters contained both transgenic Ager−/− and non-transgenic Ager−/− offspring, and all offspring were raised by their respective birth mothers. In addition, offspring survival rate was lower in endothelial RAGE-deficient (EC-KO) mothers (P < 0.001; Fig. 7b).
Social behaviour in RAGE knockout mice
Clinical studies have linked autism and Asperger’s disorders and attention-deficit/hyperactivity disorders to oxytocin deficiency7,8,54, and the potential use of exogenous oxytocin to treat these conditions is being assessed in clinical trials10,11,54,55,56,57. Ager−/− male mice are also known to be hyperactive, with greater speeds and distances travelled during both light-dark transition and open field tests58. These have been suggested to be potential mouse equivalents of human anxiety properties. We therefore reasoned that the hyperactivity seen in Ager−/− male mice might also be related to a deficiency in transport of peripheral oxytocin into the CNS, and administered exogenous oxytocin to WT and Ager−/− male mice. Normal activity levels of WT mice were unaffected following administration of either subcutaneous or intraventricular oxytocin (Fig. 7c, d). By contrast, the elevated distances travelled and average movement speeds of Ager−/− mice in light-dark transition tests were normalised after intraventricular but not subcutaneous administration of oxytocin. Concordantly, intraventricular but not nasal administration of oxytocin normalised distances travelled by Ager−/− mice in open field tests (Fig. 7e). These findings provide psychopharmacological support for the importance of vascular RAGE-dependent transport of peripheral oxytocin into the brain, which appears to be necessary for the development and maintenance of normal social behaviours.
Consistent with effects on maternal behaviour, mouse RAGE gene ablation (Ager−/−) mice leads to maternal neglect and dramatically decreased offspring survival. This phenotype is reminiscent of mice lacking oxytocin (Oxt−/−) or with deficiencies in oxytocin secretion (Cd38−/−) or action (Oxtr−/−)5,38,39. Notably, OT release from the hypothalamus was not affected by the RAGE-deficiency (Supplementary Figure 6). Supporting a primary role for oxytocin transport by endothelial RAGE, selective transgenic expression of RAGE in the endothelium of Ager−/− mice rescued the maternal behaviour deficit. The potential for RAGE to serve as an oxytocin transporter is further supported by results from our biochemical binding studies, the in vitro BBB model system, where unidirectional blood to brain transport was seen, and by measurements of oxytocin in various regions of the CNS of WT and Ager−/− male mice before and after peripheral administration of oxytocin. Oxytocin concentrations were consistently elevated in the third ventricle and cysterna as well as amygdala and PVN of WT but not Ager−/− mice. c-Fos activation in the mPOA and BNST is a classical maternal behavioural response8,51, which was also recapitulated by exogenous oxytocin administration in WT but not Ager−/− mice. These observations of peripheral oxytocin effectiveness indicate that hypothalamic oxytocin in Ager−/− mice was not sufficient to induce maternal behaviour, suggesting the importance of central release of oxytocin stimulated by circulating oxytocin59.
The affinity of oxytocin binding to the oxytocin receptor has often been estimated to be KD ~100 nM, although a high affinity form with KD ~1 nM has also been reported60. Therefore our estimated KD ~180 nM for binding between RAGE and oxytocin seems biologically reasonable. Under normal physiological conditions the primary effects of oxytocin are peripheral, and the endothelial RAGE transport system would not be engaged. However, during childbirth when both peripheral and central actions of oxytocin are needed, blood concentrations increase dramatically, which may saturate peripheral receptor occupancy and promote transport across the BBB. Levels of oxytocin in the periphery are lower than those in the CSF, in humans16,61,62, providing a concentration gradient for what appears to be a transport mechanism: this point of view depends on the methods of oxytocin measurements in blood, because a recent report has shown much higher blood OT levels than previously thought using a robust nanoLC-MS platform63. Endothelial RAGE signalling is not required for the central actions of oxytocin, much like the short form of the leptin receptor64. It remains unclear how oxytocin is transported by RAGE on the capillary endothelium. It is most likely that a vesicular trafficking system, involving endocytosis and transcytosis, a transcellular transportation across endothelial cells, is involved in oxytocin transportation mediated by RAGE carrier proteins65 (Supplementary Figure 4d).
Anterograde transport of oxytocin produced in the PVN and SON of the hypothalamus leads to its accumulation in axon terminals of the posterior pituitary, where it is released into the systemic circulation. Surges in the release and circulating concentrations of oxytocin occurring during childbirth activate oxytocin receptors in the reproductive organs1,4, including the uterus where oxytocin stimulates cervical dilation and uterine contractions and the mammary glands to stimulate lactation. Peripheral oxytocin may also act centrally to initiate maternal bonding behaviours5,8. Pharmacological studies clearly show that exogenous oxytocin has behavioural effects5,8,9,10,11,12,24,66, which further demonstrates that peripheral oxytocin can act centrally17,18. However, this has been a point of much debate and dissension13,15,55,67, as polypeptides typically do not cross the BBB without specific transport mechanisms20,45, and mechanisms for oxytocin transport were unknown. Findings presented here show that membrane-associated RAGE on endothelial cells and potentially elsewhere in the CNS binds to and transports peripheral oxytocin into the brain, as recently shown16,17,18,19,66.
It has been reported that intranasally administered oxytocin may be transported to the olfactory nerve via olfactory sensory neurons located in the mucous layer, or may reach the trigeminal nerve via trigeminal ganglion cell fibres, which are also located close to the surface of the nasal cavity67,68. Unfortunately, current experiments do not provide any evidence for such transport mechanisms. However, capillaries are dense in the mucus membrane, and thus the oxytocin can easily enter into the blood stream17,68,69. Once nasally applied oxytocin is conveyed by the blood stream, RAGE in the cerebral micro-vessels will transport oxytocin into the brain. RAGE transport seems to be responsible for the brain uptake of oxytocin nasally delivered oxytocin as treatment for human ASD patients or administration of megadoses of pitocin during labour, which can potentially affect maternal and foetal/newborn behaviour. Instead of direct nasal transport bypassing the BBB, one of the main mechanism may be uptake from the blood via RAGE, because rapid increases in plasma oxytocin concentrations have been reported16; on the other hand, one study reported only a small increase in men70.
It has been reported that approximately 0.002% of the peripherally applied amount of oxytocin (5 μg) reaches the CNS at 10 min after subcutaneous or intraperitoneal administration in rats71, while the bioavailability is approximately 2% in rats, as measured by LC/MS after administration of 500 μg oxytocin in rats72. Rault et al. reported a bioavailability of 0.001% of i.n. application of 50 μg oxytocin in female pigs18. With an intracarotid artery bolus injection of 125I-labelled or 3H-labelled oxytocin, it was estimated that 1–2% of the oxytocin peptide accumulated on the BBB in rats20. In our study, the estimated availability of oxytocin in the CNF was 0.2%, after subcutaneous administration of 30 ng oxytocin in mice, which was a much lower amount of oxytocin than used in previous studies. The findings on oxytocin reaching the CNS were inconsistent among studies; this may be due to differences in treatment protocols, species, and detection methods. Further studies are required to determine the exact bioavailability.
The neural circuitry responsible for the peripartum acquisition of maternal bonding behaviours in rodents and mammals more generally is increasingly understood. Classical mapping studies revealed roles for the mPOA and adjacent vBNST51,52,53,73,74. Lesions in the mPOA identified important roles for dopaminergic neurons projecting to the ventral tegmental area (VTA) involved in reward and reinforcement learning51,53. Serotonergic signalling is also critical for the acquisition of maternal behaviour, as demonstrated by Pet1−/− mice with diminished serotonin synthesis in the CNS75. The loss of maternal bonding by Pet1−/− mice has been attributed to deficits in the mPOA and BNST, which are innervated by serotonergic neurons. oxytocin receptors expressed in the mPOA and BNST are also critical for normal maternal behaviour, which raises important questions about sites of oxytocin expression and mechanisms of oxytocin supply. Our findings suggest that peripheral oxytocin is transported by RAGE into the CNS to activate oxytocin receptors directly.
Finally, there is precedence for RAGE to serve as a peptide transporter across the BBB. For example, RAGE has been shown to transport amyloid β peptide across the BBB, which promotes Alzheimer disease-like symptoms in susceptible mice. RAGE has also been implicated in the pathogenesis of diabetes complications. Since both of these are deleterious, pathological effects, RAGE is being targeted for inhibition in drug discovery efforts35. By contrast, our findings demonstrate that RAGE is required for normal physiological functioning of oxytocin, which may also be inhibited by these drug discovery strategies. Parental bonding and nurturing and numerous other socially interactive behaviours are promoted by oxytocin and may either be missing in its absence or replaced by aggressive or anti-social behaviours.
Mass spectrometry of the eluted material from the immobilised esRAGE in human serum did not identify arginine-vasopressin; additionally, RAGE did not transport it in an in vitro blood–brain barrier (BBB) assay system (Supplementary Figure 7). In conclusion, the contribution of peripheral oxytocin to centrally-mediated behavioural actions has long been predicted76, and may now be understood and studied more precisely in view of the RAGE-mediated transport mechanism reported here. This transport mechanism is not gender-specific, but equally function in male and female mice (Fig. 4g).
Oxytocin was obtained from the Peptide Institute (Osaka, Japan). Liquid chromatography mass spectrometer (LC-MS)-grade water, acetonitrile (ACN), formic acid, trifluroacetic acid (TFA), and trichloroacetic acid (TCA) were purchased from Wako Chemicals (Tokyo, Japan). Stably-labelled oxytocin [13C,15N]oxytocin was synthesised using [13C5,15N1]-Pro7 and [13C6,15N1]-Leu8 (Scrum Co. Ltd., Tokyo, Japan), as described previously73.
RAGE knockout (Ager−/−, deletion of the mouse gene of the receptor for AGE, Ager)41 and wild type (WT, RAGE+/+) mice (C57BL/6J) were produced by crossbreeding heterozygous mutant mice27. Endothelial RAGE-transgenic (Tg) mice26 were crossbred with Ager−/− mice to yield endothelial RAGE-Tg Ager−/− mice (KO + Tg). Both male and female mice were maintained under standard cage conditions (24 °C; 12-h light/dark cycle, lights on at 8:45 a.m.) with sawdust bedding, and food and water ad libitum. Breeding pairs were maintained in separate cages. Offspring were weaned at 21 days of age and housed in same-sex sibling pairs. For monitoring offspring survival, pregnant WT and Ager−/− mice were transferred to a new environment (clean cages) 1 day before delivery. The offspring were either kept with biological mothers or caged with postpartum mothers of the alternative genotype. All animal experiments were approved by the Committee on Animal Experimentation of Kanazawa University and performed in accordance with the Fundamental Guidelines for Proper Conduct of Animal Experiment and Related Activities in Academic Research Institutions under the jurisdiction of the Ministry of Education, Culture, Sports, Science and Technology of Japan.
Polypeptides were separated using a Superdex 75 pg HiLoad 26/600 column (GE Healthcare Japan, Tokyo) eluted at 1.0 ml/min with 5 mM ammonium acetate pH 7.8. Human serum (12 ml) preincubated with 48 ng oxytocin was separated and an enzyme immunosorbent assay (EIA) was used to identify OT in eluting fractions. Anti-RAGE monoclonal antibody (1.0 mg) or purified esRAGE (0.5 mg) were coupled to NHS-activated HiTrap (GE Healthcare). Sera samples (50 ml) from healthy consenting adults were applied to the HiTrap-anti-RAGE column equilibrated with 50 mM Tris–HCl (pH 7.4) and 0.15 M NaCl. Alternatively, the low molecular weight (<3000, Amicon Ultracel3K) fraction of human serum (50 ml) was applied to the HiTrap-esRAGE column previously equilibrated with phosphate-buffered saline (PBS). After washing the bound proteins were eluted with 100 mM glycine-HCl buffer (pH 2.5) for HiTrap-anti-RAGE or 10 mM Tris–HCl (pH 7.4) and 2.0 M NaCl for HiTrap-esRAGE and the eluates were analysed by EIA or LC-MS/MS and Western blotting.
Surface plasmon resonance assay
Isolated human esRAGE was immobilised to BIAcore CM5 research grade sensor chips with the amine coupling kit to a density of ~5000 response units (RU)27,32,41. Oxytocin binding kinetics to the immobilised esRAGE was analysed using a BIAcore 2000 system (GE Healthcare Japan)27,32,41 and mobile phase 10 mM HEPES (pH 7.4), 0.15 M NaCl, 3 mM EDTA and 0.005% (V/V) surfactant P-20 at 25 °C and 20 μl/min. The sensor chips were regenerated with 10 mM NaOH and 0.5% SDS (W/V).
Plate binding and competition assay
Oxytocin binding to RAGE and competition by RAGE ligands were assayed with oxytocin-coated 96-well plates, human esRAGE, and horseradish peroxidase (HRP)-conjugated anti-human RAGE antibody27. Oxytocin (100 μl, indicated concentrations) was immobilised in 96-well microtitre plates, 1 μg/ml esRAGE was added, and bound esRAGE was detected immunochemically using covalently coupled 〈RAGE antibody- horseradish peroxidise-catalysed oxidation of tetramethylbenzidine. RAGE ligands were S100B (Sigma-Aldrich, St. Louis, MO, USA)30, AGE-BSA (glyceraldehyde-derived AGE-BSA)27,32,41, amyloid β 1-42 (Sigma-Aldrich), and high-mobility group box 1 (HMGB1, Sigma-Aldrich)42.
C6 rat glioma cells expressing RAGE and stably transformed with NF-κB promoter-driven luciferase constructs27,41 were incubated for 24 h in Dulbecco’s modified eagle’s medium (DMEM) supplemented with 0.1% foetal bovine serum (FBS) prior to 4 h stimulation with OT, S100B or AGE-BSA (glyceraldehyde-derived AGE-BSA)32,41. The luciferase activities were assayed with a Luciferase Assay System (Promega, Madison, MI, USA).
High MW proteins in diluted mouse plasma were precipitated with 2% TCA; supernatants obtained after centrifugation were analysed by LC-MS/MS. Mouse CSF samples diluted 1:5 with PBS (25 μl) were analysed directly. Human plasma samples (50 ml) spiked with 100 ng of oxytocin and 75 ng of [13C,15N]oxytocin were concentrated using immobilised esRAGE affinity chromatography. The eluting 1.0 ml fractions (Fig. 1h) were analysed by LC-MS/MS. The 25 μl samples were separated using a ZORBAX 300SB-C8 column (2.1 × 150 mm, 5 μm; CA, USA) eluted with a linear gradient of 0.1% (v/v) formic acid and acetonitrile (0–30%) at 0.3 ml/min and 50 °C. Eluted proteins were detected in the multiple reaction monitoring (MRM) mode of the MS/MS system (Shimazu UFLC, Kyoto, Japan; AB Sciex 4000 QTRAP, Framingham, MA, USA; positive ion electrospray (ESI) mode (capillary voltage 5 kV); desolvation voltage (75 V); curtain gas (nitrogen, 12 l/h, 65 psi and 600 °C); nitrogen gas pressure (65 psi), and collision voltage (30 V). Oxytocin MRM transition ions and fragment types were m/z: 1008.2 → 723.2 (b6); and [13C,15N]oxytocin: m/z: 1021.2 → 723.2 (b6)73. Data were acquired and processed with AB Sciex Analyst Version 1.4.1.
Blood-brain barrier (BBB) model
For the in vitro BBB model (MBT-24H, PharmaCo-Cell Co., Nagasaki, Japan), rat brain pericytes (1.5 × 104 cells/cm2) and rat astrocytes (1.5 × 104 cells/cm2) were seeded on the bottom of the collagen-coated polyester membranes of Transwell inserts (Corning Life Sciences, MA, USA). After 16 h the cells firmly adherent, monkey brain vascular endothelial cells (1.5 × 105 cells/cm2) were then seeded on the upper side of the inserts in 24-well culture plates. The in vitro BBB models were established within 4 days of seeding the cells according to the manufacturer’s instructions46. Trans-endothelial electrical resistance (TEER), which primarily reflects the flux of sodium ions through the cell layers in the culture conditions, was measured with an epithelial-volt-ohm metre and an Endohm-6 chamber electrodes (World Precision Instruments, Sarasota, FL, USA). The TEERs of the coated, cell-free filters were subtracted from the measured TEER values of the models and shown as Ω cm2. The apparent permeability constants (Papp) between luminal and abluminal chambers were calculated from the distribution ratios46. Endothelial expression was silenced using RAGE shRNA and the pSilencer 3.0-H1 vector (Ambion, Austin, TX, USA)41.
Isolated brain endothelial cells were washed and resuspended in staining buffer (PBS containing 2% FCS) containing FcBlock (BD Biosciences, San Jose, CA, USA). The cells were incubated with polyclonal rabbit anti-RAGE antibody or isotype IgG (15 min at 4 °C in the dark)27 followed by anti-rabbit IgG-FITC (eBioscience, San Diego, CA, UAS), and analysed by FACS AriaII (BD Biosciences) and FlowJo software (Tree Star, Inc., Ashland, OR, USA).
The hippocampus and choroid plexus were cut into 10-μm-thick sections by using a cryostat. The sections were blocked in PBS containing 0.3% TritonX-100 and 3% BSA for 1 h at room temperature, and incubated at 4 °C overnight with primary polyclonal rabbit anti-RAGE antibody (1:1000), anti-CD31 or anti-Caveolin 1 antibodies (Millipore, Billerica, MA, USA; 1:500) and 4′,6-diamidino-2-phenylindole (DAPI, Dojindo; Kumamoto, Japan, 1:2000) as previously described20. The sections were subsequently washed with 0.3% TritonX-100 in PBS and incubated with Alexa Fluor 488 (1:200, Invitrogen Molecular Probes) and Cy3-labled-IgG (1:100, Jackson ImmunoResearch Laboratories, PA) for 1 h at room temperature. Imaging was performed with a Nikon EZ-C1 laser confocal microscope (Tokyo, Japan).
Sampling of the cerebrospinal fluid (CSF) and blood
CSF was collected according to the protocol for sampling CSF from mice without detectable plasma contamination77,78. Under ketamine anaesthesia (100 mg/kg intraperitoneally), the occipital skull was exposed, and the dura mater of the cisterna magna appeared as a glistening and clear reverse triangle through which the medulla oblongata, a major blood vessel (arteria dorsalis spinalis), and CSF space were visible. A capillary tube was inserted into the cisterna magna through the dura mater, blood-free CSF samples were collected with a 32G needle and immediately frozen with dry ice prior to storage at −80 °C. After CSF collections, blood samples were obtained by cardiac puncture from the mice under continuous ketamine anaesthesia.
For microperfusion probe implantation79, the male mice were with a subcutaneous injections of ketamine. The heads of anesthetised mice were fixed in a stereotactic frame (Narishige, Tokyo, Japan) and a 1 mm hole was drilled in the skull. The intact dura intact was then punctured to create defined opening of the meninges. Using the stereotactic frame, a healing dummy was slowly inserted into the three brain positions80. The probe was fixed to the skull by using two anchor screws and biocompatible dental cement. All surgical procedures were completed within 30 min. A healing dummy was used to provide mechanical stability during the implantation and the healing period of 2 weeks80. The microperfusion probe (a 4-mm length of the coaxial tube, 2.5 mm in diameter) consisting of a 20 G fluorinated ethylene propylene guide cannula was replaced before sampling with an inflow/outflow tubing on the day of the experiments80. This tubing was connected to two glass Hamilton microsyringes placed in syringe pumps (Eicom, Osaka, Japan). Microperfusate was pumped into the probe at a flow rate of 2 µl/min, and the samples were withdrawn at the same flow rate. Sampling was conducted for 2 h. Both microprobes were perfused without sampling for 60 min before the first 30-min microperfusates from the amygdala, PVN, and prefrontal cortex were collected. The microperfusates were mixed under sterile conditions and consisted of 154 mM NaCl, 2.2 mM CaCl2, 5.6 mM KCl, 2.3 mM NaHCO3, and 0.15% BSA (pH 7.4)80. Beginning immediately after the nasal application, 4 additional microperfusates were taken at 30-min intervals. After the termination of the experiments, the brains were removed and snap-frozen to obtain 40-μm cryo-cut stained brain slices later for the histological verification of the perfusion site.
Administration of oxytocin
Synthetic oxytocin (1000 ng/ml × 20 μl) was administered nasally; the solution was applied bilaterally on the rhinarium, which is the area referred to as the glaberous skin around the nostrils, using a pipette), intravenously (100 ng/ml × 30 μl) through the tail vein, or subcutaneously (100 ng/ml × 0.3 ml) into the shoulder skin. [13C,15N]oxytocin (100 μg/ml × 0.3 ml) was subcutaneously injected.
Enzyme immunoassay for oxytocin
Oxytocin immunoreactivity levels in serum and CSF were quantified by using an oxytocin EIA kit (Enzo Life Sciences, NY, USA, formerly Assays Designs, MI, USA), following the manufacturer’s manual. The CSF samples (5 μl) were thawed and diluted 1:20 in assay buffer77. CSF samples were assayed without protein extraction due to the low protein concentration in the CSF. The plasma samples (100 μl) were thawed on ice and assayed with protein extraction5,77, whereas an additional extraction step may have resulted in lower than actual oxytocin levels. Each sample volume was so small, the CSF was assayed without extraction, though unextracted samples result in binding of complexes of oxytocin stuck to interacting proteins. The oxytocin assay had two linear ranges, which covers a lower concentration range from a few to 30 pg/ml, and a higher concentration range between 50 and 1000 pg/ml. The inter-assay and intra-assay coefficients of variation were less than 15%.
Oxytocin release from the hypothalamus
WT and Ager−/− male mice were anaesthetised with pentobarbital sodium (50 mg/kg). The entire bilateral hypothalami were obtained and placed separately in different wells of a 12-well plate with 0.4 ml normal Locke’s solution (pH 7.25) containing 140 mM NaCl, 5 mM KCl, 1.2 mM MgCl2, 2.2 mM CaCl2, 10 mM glucose, 10 mM HEPES, and 0.01% BSA, in a 35 °C water bath. The incubation medium was replaced 10 times every 3 min, as described80. Beginning at the 11th replacement, the temperature was shifted to 38.5 °C. From the 13th–15th replacements, cyclic ADP-ribose (a final concentration of 100 μM, Sigma) was added into the Locke’s medium at 38.5 °C. Aliquots from the 8th replacement were preserved at −80 °C for assaying the oxytocin concentrations released from the hypothalamus.
Light-dark transition test
The light-dark transition was used to examine the anxiolytic-like or anxiogenic-like activity of the mice as previously described81. The light-dark test chamber (200 mm × 600 mm × 200 mm) consisted of two dividing rooms: a small dark (2 lux) safe compartment (one-third, 200 mm × 200 mm × 200 mm—dark box) and a large brightly illuminated (250 lux) aversive compartment (two-thirds, 400 mm × 200 mm × 200 mm—light box). The mice were placed into the light arena and were allowed to move freely between the two chambers for 600 s. Each male mouse was placed in the centre of the light chamber, and the mouse was allowed to run freely between the two chambers for 10 min. The trial was recorded for 10 min by using the ANY-maze video system (Stoelting Co., Wood Dale, IL, USA). Latency to enter (defined by all four paws entering), time spent, entries, and distances travelled in the light chamber were recorded. A recovery test was performed following subcutaneous injection of oxytocin (100 ng/ml × 0.3 ml) or intraventricular application of oxytocin (100 ng/ml) for 10 min at 2 μl/min, through implanted cannulae, as described above.
Open field test
The open field test is meant to assess anxious behaviour80. It uses a wooden box (60 × 60 × 20 cm) covered with polypropylene and having an outlined centre space (30 × 30 cm). Animal are in the box for 10 min, and their movements into the centre are digitally recorded and analysed using ANY-maze software. This test is based on the idea that mice naturally prefer to be near protective walls rather than being exposed to potential dangers in open spaces. Test chambers are cleaned after each trial.
Cerebral ischaemia model
WT and Ager−/− male mice (8 to 12-weeks-old and weighing 20–30 g) were used for the experiments. The animals were anaesthetised with 2.0% halothane and maintained with 0.5% halothane through a facemask. Brain ischaemia was induced via bilateral occlusion of the common carotid arteries (BCCAO) for 15 min using microvascular clips as described previously23. Laser-Doppler flowmetry was used to measure cerebral cortical microperfusion (3 mm lateral to bregma). In our experimental model, the mice that exhibited <15% of the baseline control microperfusion during the first minute of occlusion were used in subsequent experiments. Rectal temperature was maintained at 36.5–37.5 °C by using a heat lamp and a blanket until the mice were completely alert. The control animals underwent a sham-operation that was identical with the exception of the occlusion. To quantify accumulative BBB leakages, 200 µl of sodium fluorescein (Sigma-Aldrich) at a concentration of 6 mg/ml in PBS was injected via the venous sinus of retro-orbital in the mice. Sodium fluorescein (MW 376.3) is a fluorescent tracer that does not cross an intact BBB. Sixty minutes later, the CSF and blood were collected according to the protocol for sampling of CSF and blood from mice80. The fluorescence of CSF and serum were measured at 460 nm at an excitation wavelength of 355 nm by using a Fluoroscan Ascent FL luminometer (Labsystems. Wilmington, DE, USA). Results are presented as relative fluorescence units (CSF value/serum value) (%).
The c-Fos immunohistochemistry was performed as previously described53. Briefly, anesthetized male mice were intracardially perfused with cold PBS followed by a cold 4% paraformaldehyde (PFA) in PBS. The brains were removed and post-fixed in a 4% PFA solution overnight at 4 °C. Brain regions were cut into 2–4 large blocks. The blocks were sliced on a microtome into 20-μm-thick sections. The sections were pre-incubated in blocking solution (3% bovine serum albumin and 0.3% Triton X-100 in PBS) for 1 h, then incubated with an anti-c-Fos antibody (sc-52, 1:200; Santa Cruz Biotechnology, Santa Cruz, CA, USA) in the blocking solution for 12 h at 4 °C. After three washes with washing buffer, the sections were incubated with goat anti-rabbit IgG antibody coupled with Alexa Fluor 488 (Invitrogen, Carlsbad, CA, USA) in the blocking solution for 1 h at room temperature. The images were obtained by using an Olympus IX71 inverted microscope equipped with a cooled CCD camera (Cool SNAP HQ2; Roper Scientific, Tucson, AZ, USA). The number of c-Fos immuno-positive nuclei in each brain section were recorded and analysed using Metamorph software (Molecular Devices, Downingtown, PA, USA).
The immunogold staining method was applied to the amygdala as previously described5. Briefly, after 10 min of oxytocin (100 ng/ml × 0.3 ml) injection, wild type (WT, Ager+/+) and Ager−/− mice were perfused with a mixture containing 2% paraformaldehyde and 2% glutaraldehyde solution in 0.1 M phosphate buffer (pH 7.2). The tissue blocks were then fixed by immersion for 4 h at 4 °C in the same solution and washed for 1 h with 0.1 M phosphate buffer (pH 7.2). After washing, the tissue blocks were dehydrated and embedded in LR-White resin (London Resin Co.). Ultrathin sections were mounted on nickel grids. The sections were washed with PBS, incubated in a blocking solution of 1% bovine serum albumin (BSA) and 0.05% sodium azide (NaN3) in PBS for 15 min, and then exposed with anti-oxytocin polyclonal antibody (1:5000, Chemicon International, Inc. USA) overnight at 4 °C. After washing twice with PBS, the sections were incubated with 5 nm gold-conjugated goat anti-rabbit secondary antibody (1:100, Sigma, USA) in a solution containing 0.1% BSA in PBS for 4 h at room temperature. The sections were washed with PBS and then with distilled water. After washing, the sections were stained with uranyl acetate and analysed under a transmission electron microscope (Joel, Tokyo Japan) by using an 80-kV accelerating voltage.
P values were calculated by using two-tailed Student’s t-test for pair wise comparisons, and one-way or two-way analysis of variance (ANOVA) followed by Bonferroni’s or Tukey’s test for multiple comparisons, unless otherwise stated. The Kaplan–Meier survival analysis was performed to compare survival curves between the different groups of mice. A P-value of < 0.05 was considered statistically significant. Data are expressed as mean ± SEM. Statistical data with F vales are shown in Supplementary Table 1.
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
The data that support the findings in this study are available from the corresponding author upon reasonable request. The source data of each figure are presented as a Supplementary Data 1.
Brunton, P. J. & Russell, J. A. The expectant brain: adapting for motherhood. Nat. Rev. Neurosci. 9, 11–25 (2008).
Dulac, C., O’Connell, L. A. & Wu, Z. Neural control of maternal and paternal behaviors. Science 345, 765–770 (2014).
Carter, C. S. Oxytocin and human evolution. Curr. Top. Behav. Neurosci. 35, 291–319 (2018).
Castel, M., Gainer, H. & Dellmann, H. D Neuronal secretory systems. Int. Rev. Cytol. 88, 303–459 (1984).
Jin, D. et al. CD38 is critical for social behaviour by regulating oxytocin secretion. Nature 446, 41–45 (2007).
Leng, G., Pineda, R., Sabatier, N. & Ludwig, M. 60 Years of neuroendocrinology: the posterior pituitary, from Geoffrey Harris to our present understanding. J. Endocrinol. 226, T173–T185 (2015).
Insel, T. R. The challenge of translation in social neuroscience: a review of oxytocin, vasopressin, and affiliative behavior. Neuron 65, 768–779 (2010).
Rilling, J. K. & Young, L. J. The biology of mammalian parenting and its effect on offspring social development. Science 345, 771–776 (2014).
Higashida, H., Yokoyama, S., Kikuchi, M. & Munesue, T. CD38 and its role in oxytocin secretion and social behavior. Horm. Behav. 61, 351–358 (2012).
Insel, T. R. Translating oxytocin neuroscience to the clinic: A National Institute of Mental Health Perspective. Biol. Psychiatry 79, 153–154 (2016).
Guastella, A. J. et al. Intranasal oxytocin improves emotion recognition for youth with autism spectrum disorders. Biol. Psychiatry 67, 692–694 (2010).
Gordon, I. et al. Intranasal oxytocin enhances connectivity in the neural circuitry supporting social motivation and social perception in children with autism. Sci. Rep. 6, 35054 (2016).
Feifel, D., Shilling, P. D. & MacDonald, K. A review of oxytocin’s effects on the positive, negative, and cognitive domains of schizophrenia. Biol. Psychiatry 79, 222–233 (2016).
Zik, J. B. & Roberts, D. L. The many faces of oxytocin: implications for psychiatry. Psychiatry Res. 226, 31–37 (2015).
Bethlehem, R. A., Baron-Cohen, S., van Honk, J., Auyeung, B. & d Bos, P. A. The oxytocin paradox. Front. Behav. Neurosci. 8, 48 (2014).
Striepens, N. et al. Elevated cerebrospinal fluid and blood concentrations of oxytocin following its intranasal administration in humans. Sci. Rep. 3, 3440 (2013).
Neumann, I. D., Maloumby, R., Beiderbeck, D. I., Lukas, M. & Landgraf, R. Increased brain and plasma oxytocin after nasal and peripheral administration in rats and mice. Psychoneuroendocrinology 38, 1985–1993 (2013).
Rault, J. L. Effects of positive and negative human contacts and intranasal oxytocin on cerebrospinal fluid oxytocin. Psychoneuroendocrinology 69, 60–66 (2016).
Lefevre, A. A comparison of methods to measure central and peripheral oxytocin concentrations in human and non-human primates. Sci. Rep. 7, 17222 (2017).
Ermisch, A. et al. On the blood-brain barrier to peptides: accumulation of labelled vasopressin, DesGlyNH2-vasopressin and oxytocin by brain regions. Endocrinol. Exp. 19, 29–37 (1985).
Pardridge, W. M. Drug transport across the blood-brain barrier. J. Cereb. Blood Flow Metab. 32, 1959–1972 (2012).
Senatus, L. M. & Schmidt, A. M. The AGE-RAGE axis: implications for age-associated arterial diseases. Front. Genet. 8, 187 (2017).
Kamide, T. et al. RAGE mediates vascular injury and inflammation after global cerebral ischemia. Neurochem. Int. 60, 220–228 (2012).
Manigrasso, M. B., Juranek, J., Ramasamy, R. & Schmidt, A. M. Unlocking the biology of RAGE in diabetic microvascular complications. Trends Endocrinol. Metab. 25, 15–22 (2014).
Takuma, K. et al. RAGE-mediated signaling contributes to intraneuronal transport of amyloid-beta and neuronal dysfunction. Proc. Natl Acad. Sci. USA 106, 20021–20026 (2009).
Yamamoto, Y. et al. Development and prevention of advanced diabetic nephropathy in RAGE-overexpressing mice. J. Clin. Invest. 108, 261–268 (2001).
Yamamoto, Y. et al. Septic shock is associated with receptor for advanced glycation end products ligation of LPS. J. Immunol. 186, 3248–3257 (2011).
Yamamoto, Y. & Yamamoto, H. RAGE-mediated inflammation, type 2 diabetes, and diabetic vascular complication. Front. Endocrinol. 4, 105 (2013).
Yonekura, H. et al. Novel splice variants of the receptor for advanced glycation end-products expressed in human vascular endothelial cells and pericytes, and their putative roles in diabetes-induced vascular injury. Biochem. J. 370, 1097–1109 (2003).
Motoyoshi, S. et al. cAMP ameliorates inflammation by modulation of macrophage receptor for advanced glycation end-products. Biochem. J. 463, 75–82 (2014).
Mackic, J. B. et al. Human blood-brain barrier receptors for Alzheimer’s amyloid-beta 1- 40. Asymmetrical binding, endocytosis, and transcytosis at the apical side of brain microvascular endothelial cell monolayer. J. Clin. Invest. 102, 734–743 (1998).
Yamamoto, Y. et al. Short-chain aldehyde-derived ligands for RAGE and their actions on endothelial cells. Diabetes Res. Clin. Pract. 77, S30–S40 (2007).
Matsumoto, K. et al. Immunohistochemical analysis of transporters related to clearance of amyloid-β peptides through blood-cerebrospinal fluid barrier in human brain. Histochem. Cell. Biol. 144, 597–611 (2015).
Deane, R. et al. RAGE mediates amyloid-beta peptide transport across the blood-brain barrier and accumulation in brain. Nat. Med. 9, 907–913 (2003).
Deane, R. et al. A multimodal RAGE-specific inhibitor reduces amyloid β-mediated brain disorder in a mouse model of Alzheimer disease. J. Clin. Invest. 122, 1377–1392 (2012).
Saito, R., Araki, S., Yamamoto, Y. & Kusuhara, K. Elevated endogenous secretory receptor for advanced glycation end products (esRAGE) levels are associated with circulating soluble RAGE levels in diabetic children. J. Pediatr. Endocrinol. Metab. 30, 63–69 (2017).
Gasparotto, J. et al. Receptor for advanced glycation end products mediates sepsis-triggered amyloid-β accumulation, Tau phosphorylation, and cognitive impairment. J. Biol. Chem. 293, 226–244 (2018).
Takayanagi, Y. et al. Pervasive social deficits, but normal parturition, in oxytocin receptor-deficient mice. Proc. Natl Acad. Sci. USA 102, 16096–16101 (2005).
Ferguson, J. N. et al. Social amnesia in mice lacking the oxytocin gene. Nat. Genet. 25, 284–288 (2000).
Modi, M. E. & Young, L. J. The oxytocin system in drug discovery for autism: animal models and novel therapeutic strategies. Horm. Behav. 61, 340–350 (2012).
Myint, K. M. et al. RAGE control of diabetic nephropathy in a mouse model: effects of RAGE gene disruption and administration of low-molecular weight heparin. Diabetes 55, 2510–2522 (2006).
Takeuchi, A. et al. Low molecular weight heparin suppresses receptor for advanced glycation end products-mediated expression of malignant phenotype in human fibrosarcoma cells. Cancer Sci. 104, 740–749 (2013).
Xue, J. et al. Change in the molecular dimension of a RAGE-ligand complex triggers RAGE signaling. Structure 24, 1509–1522 (2016).
Pollak, T. A. et al. The blood-brain barrier in psychosis. Lancet Psychiatry 5, 79–92 (2018).
Lundquist, S. et al. Prediction of drug transport through the blood-brain barrier in vivo: a comparison between two in vitro cell models. Pharm. Res. 19, 976–981 (2002).
Nakagawa, S. et al. Pericytes from brain microvessels strengthen the barrier integrity in primary cultures of rat brain endothelial cells. Cell. Mol. Neurobiol. 27, 687–694 (2007).
Yoshida, M. et al. Evidence that oxytocin exerts anxiolytic effects via oxytocin receptor expressed in serotonergic neurons in mice. J. Neurosci. 29, 2259–2271 (2009).
Rilling, J. K. et al. Sex differences in the neural and behavioral response to intranasal oxytocin and vasopressin during human social interaction. Psychoneuroendocrinology 39, 237–248 (2014).
Scheele, D. et al. Opposing effects of oxytocin on moral judgment in males and females. Hum. Brain Mapp. 35, 6067–6076 (2014).
Steinman, M. Q. et al. Sex-specific effects of stress on oxytocin neurons correspond with responses to intranasal oxytocin. Biol. Psychiatry 80, 406–414 (2016).
Numan, M. & Numan, M. J. Projection sites of medial preoptic area and ventral bed nucleus of the stria terminalis neurons that express Fos during maternal behavior in female rats. J. Neuroendocrinol. 9, 369–384 (1997).
Martinez, L. A., Levy, M. J. & Petrulis, A. Endogenous oxytocin is necessary for preferential Fos expression to male odors in the bed nucleus of the stria terminalis in female Syrian hamsters. Horm. Behav. 64, 653–664 (2013).
Zhong, J. et al. c-Fos expression in the paternal mouse brain induced by communicative interaction with maternal mates. Mol. Brain 7, 66 (2014).
Feldman, R. et al. Sensitive parenting is associated with plasma oxytocin and polymorphisms in the OXTR and CD38 genes. Biol. Psychiatry 72, 175–181 (2012).
Politte, L. C., Henry, C. A. & McDougle, C. J. Psychopharmacological interventions in autism spectrum disorder. Harv. Rev. Psychiatry 22, 76–92 (2014).
Cai, Q., Feng, L. & Yap, K. Z. Systematic review and meta-analysis of reported adverse events of long-term intranasal oxytocin treatment for autism spectrum disorder. Psychiatry Clin. Neurosci. 72, 140–151 (2018).
Munesue, T. et al. Oxytocin for male subjects with autism spectrum disorder and comorbid intellectual disabilities: a randomized pilot study. Front. Psychiatry 7, 2 (2016).
Sakatani, S. et al. Deletion of RAGE causes hyperactivity and increased sensitivity to auditory stimuli in mice. PLoS One 4, e8309 (2009).
Zhang, G. & Cai, D. Circadian intervention of obesity development via resting-stage feeding manipulation or oxytocin treatment. Am. J. Physiol. Endocrinol. Metab. 301, E1004–E1012 (2011).
Gimpl, G. & Fahrenholz, F. The oxytocin receptor system: structure, function, and regulation. Physiol. Rev. 81, 629–683 (2001).
Kagerbauer, S. M. et al. Plasma oxytocin and vasopressin do not predict neuropeptide concentrations in human cerebrospinal fluid. J. Neuroendocrinol. 25, 668–673 (2013).
Martin, J. et al. Vasopressin and oxytocin in CSF and plasma of patients with aneurysmal subarachnoid haemorrhage. Neuropeptides 48, 91–96 (2014).
Brandtzaeg, O. K. et al. Proteomics tools reveal startlingly high amounts of oxytocin in plasma and serum. Sci. Rep. 6, 31693 (2016).
Hileman, S. M., Pierroz, D. D. & Flier, J. S. Leptin, nutrition, and reproduction: timing is everything. J. Clin. Endocrinol. Metab. 85, 804–847 (2000).
Abbott, N. J., Patabendige, A. A., Dolman, D. E., Yusof, S. R. & Begley, D. J. Structure and function of the blood-brain barrier. Neurobiol. Dis. 37, 13–25 (2010).
Neumann, I. D. & Landgraf, R. Balance of brain oxytocin and vasopressin: implications for anxiety, depression, and social behaviors. Trends Neurosci. 35, 649–659 (2012).
Leng, G. & Ludwig, M. Intranasal oxytocin: myths and delusions. Biol. Psychiatry 79, 243–250 (2016).
Dal Monte, O., Noble, P. L., Turchi, J., Cummins, A. & Averbeck, B. B. CSF and blood oxytocin concentration changes following intranasal delivery in macaque. PLoS One 29, e103677 (2014).
Temesi, A., Thuróczy, J., Balogh, L. & Miklósi, Á. Increased serum and urinary oxytocin concentrations after nasal administration in beagle dogs. Front. Vet. Sci. 4, 147 (2017).
Quintana, D. S. et al. Saliva oxytocin measures do not reflect peripheral plasma concentrations after intranasal oxytocin administration in men. Horm. Behav. 102, 85–92 (2018).
Mens, W. B., Laczi, F., Tonnaer, J. A., de Kloet, E. R. & van Wimersma Greidanus, T. B. Vasopressin and oxytocin content in cerebrospinal fluid and in various brain areas after administration of histamine and pentylenetetrazol. Pharmacol. Biochem. Behav. 19, 587–591 (1983).
Tanaka, A. et al. Delivery of oxytocin to the brain for the treatment of autism spectrum disorder by nasal application. Mol. Pharm. 15, 1105–1111 (2018).
Higashida, H. et al. Intestinal transepithelial permeability of oxytocin into the blood is dependent on the receptor for advanced glycation end products in mice. Sci. Rep. 7, 7883 (2017).
Bridges, R. S. Neuroendocrine regulation of maternal behavior. Front. Neuroendocrinol. 36, 178–196 (2015).
Liu, C. et al. Pet-1 is required across different stages of life to regulate serotonergic function. Nat. Neurosci. 13, 1190–1198 (2010).
Landgraf, R., Ermisch, A. & Hess, J. Indications for a brain uptake of labelled vasopressin and ocytocin and the problem of the blood-brain barrier. Endokrinologie 73, 77–81 (1979).
Lopatina, O. et al. H. Communication impairment in ultrasonic vocal repertoire during the suckling period of Cd157 knockout mice: transient improvement by oxytocin. Front. Neurosci. 11, 266 (2017).
Liu, L. & Duff, K. A technique for serial collection of cerebrospinal fluid from the cisterna magna in mouse. J. Vis. Exp. 21, pii: 960 (2008).
Paxinos, G. & Franklin, K. B. J. The Mouse Brain in Stereotaxic Coordinates. 2. (Academic Press, San Diego, 2001).
Zhong., J. et al. Cyclic ADP-ribose and heat regulate oxytocin release via CD38 and TRPM2 in the hypothalamus during social or psychological stress in mice. Front. Neurosci. 10, 304 (2016).
Cherepanov, S. M. et al. Effects of three lipidated oxytocin analogs on behavioral deficits in CD38 knockout mice. Brain Sci. 7, 10 (2017).
We acknowledge financial supports from Kanazawa University SAKIGAKE project 2018 and the Strategic Research Programme for Brain Sciences from the Ministry of Education, Culture, Sports, Science and Technology, Japan. We thank for Grants-in-Aid for Scientific Research (24590375, 25461335 and 18K06889) and the Programme for Fostering Globally Talented Researchers from Japan Society for Promotion of Sciences (S2901).
The authors declare no competing interests.
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Excitation/inhibition imbalance and impaired neurogenesis in neurodevelopmental and neurodegenerative disorders
Reviews in the Neurosciences (2019)
Synthesis of oxytocin derivatives lipidated via a carbonate or carbamate linkage as a long-acting therapeutic agent for social impairment-like behaviors
Bioorganic & Medicinal Chemistry (2019)