Deletion of MCP-1 Impedes Pathogenesis of Acid Ceramidase Deficiency

Yu, Fabian P. S.; Dworski, Shaalee; Medin, Jeffrey A.

doi:10.1038/s41598-018-20052-6

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Published: 29 January 2018

Deletion of MCP-1 Impedes Pathogenesis of Acid Ceramidase Deficiency

Fabian P. S. Yu^1,4,
Shaalee Dworski¹ &
Jeffrey A. Medin^1,2,3,4,5

Scientific Reports volume 8, Article number: 1808 (2018) Cite this article

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Abstract

Farber Disease (FD) is an ultra-rare Lysosomal Storage Disorder caused by deficient acid ceramidase (ACDase) activity. Patients with ACDase deficiency manifest a spectrum of symptoms including formation of nodules, painful joints, and a hoarse voice. Classic FD patients will develop histiocytes in organs and die in childhood. Monocyte chemotactic protein (MCP-1; CCL2) is significantly elevated in both FD patients and a mouse model we previously generated. Here, to further study MCP-1 in FD, we created an ACDase;MCP-1 double mutant mouse. We show that deletion of MCP-1 reduced leukocytosis, delayed weight loss, and improved lifespan. Reduced inflammation and fibrosis were observed in livers from double mutant animals. Bronchial alveolar lavage fluid analyses revealed a reduction in cellular infiltrates and protein accumulation. Furthermore, reduced sphingolipid accumulation was observed in the lung and liver but not in the brain. The neurological and hematopoietic defects observed in FD mice were maintained. A compensatory cytokine response was found in the double mutants, however, that may contribute to continued signs of inflammation and injury. Taken together, targeting a reduction of MCP-1 opens the door to a better understanding of the mechanistic consequences of ceramide accumulation and may even delay the progression of FD in some organ systems.

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Introduction

The gene ASAH1 encodes acid ceramidase (ACDase, EC 3.5.1.23), a hydrolase that degrades the bioactive lipid ceramide into sphingosine and a free fatty acid¹. Mutations in ASAH1 can result in acid ceramidase deficiency which may manifest as Farber Disease (FD, Farber Lipogranulomatosis, OMIM #22000), a rare inherited Lysosomal Storage Disorder (LSD). While patients who are diagnosed with FD can display a range of symptoms, the cardinal signs are painful joints, formation of subcutaneous nodules, and the development of a hoarse voice that may lead to aphonia. In severe cases, patients may have neurologic involvement, develop hepatosplenomegaly, and fail to thrive, leading to childhood lethality^2,3. We previously generated a mouse model of ACDase-deficiency that has high fidelity with the human disorder⁴. In this model, the P361R mouse mutation (which is orthologous to the human P362R mutation) was knocked in⁵. Mice homozygous for the mutation (Asah1^P361R/P361R) recapitulate the classical form of human FD with a phenotype that includes systemic ceramide accumulation, increased leukocytosis, and enlargement of visceral organs⁴. The mice are much smaller than littermates and progressive macrophage infiltration is present in the pulmonary, hematopoietic, hepatic, and central nervous systems⁴. Large foamy macrophages and associated tissue injury is also commonly observed.

The mouse model of FD that we developed also demonstrates a unique cytokine profile that includes dramatically higher levels of MCP-1 in plasma⁶. Further, we have also recently shown that FD patients have increased levels of monocyte chenoattractant protein (MCP-1), keratinocyte chemoattractant (KC), macrophage inflammatory protein-1α (MIP-1α), and the inflammatory cytokine interferon gamma-induced protein-10 (IP-10)⁶ in their plasma. In the mouse, MCP-1 is the most elevated and its highest concentration is detected at the end of the animal’s life. MCP-1 is a potent chemoattractant that is responsible for the recruitment of monocytes. It is a member of the C-C chemokine subfamily and functions by binding to its G-protein coupled receptor: chemokine receptor 2 (CCR2). Both MCP-1 and CCR2 have been widely studied for their role in monocyte recruitment during infection and for their other roles during inflammation⁷. Expression of MCP-1 can be detected in a variety of cell types, including endothelial, smooth muscle, astrocytic, and microglial cells^8,9. However, the major sources of MCP-1 are monocytes and macrophages¹⁰. Numerous FD case reports have demonstrated that histiocytic infiltration is present in many tissues and that plasma chitotriosidase is significantly elevated^3,11. This inflammatory phenotype is reflected in our Asah1^P361R/P361R mouse, which displays macrophage and neutrophil infiltration in various tissues and organs^4,12. In clinical practice, the management strategy for the treatment of FD focuses largely on managing patient symptoms to date. Bone marrow transplantation (BMT) may be an option for certain Farber patients as might enzyme replacement therapy (ERT)¹³. Several case reports have demonstrated that BMT reduced the number and size of subcutaneous nodules and decreased joint pain in patients with FD^14,15. Along these lines, we previously demonstrated that MCP-1 levels are reduced in FD patient plasma post-BMT⁶. This further suggests that there may be a relationship between MCP-1 and FD symptoms, and supports MCP-1 as a prospective biomarker for FD.

Here, to further understand the role of MCP-1 in FD development and progression, we generated and characterized an Asah1 and MCP-1/CCL2 double deficient mouse (herein called Asah1^P361R/P361R;MCP-1^−/−). In this study, we show that ablation of MCP-1 can impede symptoms of FD. This is an important insight into the pathogenesis of this disorder and opens the door to a whole new line of therapy.

Results

Deletion of MCP-1 improves the course of FD

Asah1^P361R/P361R;MCP-1^+/+ mice demonstrated an expected life span of 7–9 weeks⁴. Asah1^P361R/P361R;MCP-1^−/− mice displayed a significantly increased lifespan to a median age of 13 weeks (Fig. 1A). Asah1^P361R/P361R;MCP-1^−/− mice also weighed more between 5 and 6 weeks of age than Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 1B,C). No differences in body weight were found after 7 weeks of age, however, between Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 1B and D). Asah1^P361R/P361R; MCP-1^+/+ mice also develop a tight skin phenotype that renders them difficult to restrain¹⁶. Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice skin stretch length was found to be significantly different at 5 weeks of age (Fig. 1E). No differences were detected in lifespan, weight, or skin stretch length between Asah1^P361R/P361R; MCP-1^+/− and Asah1^P361R/P361R;MCP-1^+/+ mice (Supplementary Fig. S1), therefore the remainder of this study focused exclusively on homozygous Asah1^P361R/P361R;MCP-1^−/− mice.

Organomegaly is a common phenotype present in classical FD and the Asah1^P361R/P361R;MCP-1^+/+ mouse⁴. Deletion of MCP-1 resulted in a delay in organ weight accumulation when normalized to body weight (Fig. 1). In terms of absolute organ weights, only the thymus showed a significant change in 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice when compared to age-matched controls (Supplementary Fig S2). The weight differences were only revealed when the organ weight was normalized with body weight. The kidney and liver weight as a percentage of total body weight in the Asah1^P361R/P361R;MCP-1^−/− mice were within the normal ranges at 8–9-weeks of age (Fig. 1J,L). There was a decrease in brain, thymus, lung, and spleen weights as a percentage of total body weight when compared to Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 1F,G,I,K). Other than an increase in brain weight as a percentage of body weight (Fig. 1F), there were no other weight increases between 8–9 and 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 1G–L).

Peripheral blood cell counts

Complete blood counts (CBCs) from peripheral blood draws of 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice showed a normalization in circulating red blood cells (RBC) and white blood cells (WBC) compared to 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 2A,B). However, by 11–12 weeks of age the numbers of WBCs in Asah1^P361R/P361R;MCP-1^−/− mice were similar to that of 8–9-week-old Asah1^P361R/P361R; MCP-1^+/+ mice (Fig. 2B). Absolute lymphocyte cell counts were unchanged between genotypes; however, based on the differential cell counts of WBCs, lymphocyte percentages were significantly decreased between controls, Asah1^P361R/P361R;MCP-1^+/+, and Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 2C,D). Increased monocytes, neutrophils, and eosinophils are common in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice⁴. A reduction in monocytes was found in both the absolute and differential cell counts between the 8–9-week-old Asah1^P361R/P361R; MCP-1^+/+ mice and the 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 2E,F). Neutrophils cell counts were not statistically significant between 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ and 8–9 and 11–12 Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 2G,H). Basophil cell counts did not change significantly either (Fig. 2I,J). Absolute eosinophil cell counts were similar to control mice in 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice, but were elevated in 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 2K). However, based on the differential cell counts, the percentage of eosinophils did not differ significantly between any of the genotypes (Fig. 2L).

MCP-1 deletion does not normalize hematopoiesis

We previously reported that the bone marrow of Asah1^P361R/P361R;MCP-1^+/+ mice displayed a dramatic reduction in the pre-B, pro-B, immature-B, and transitional-B cells¹². Fluorescence activated cell sorting (FACS) analysis of cells from the bone marrow of 9-week-old Asah1^P361R/P361R;MCP-1^−/− mice also showed a reduction in B-cell progenitors (Fig. 3A). There were no differences in the various B-cell progenitor populations between 9-week-old Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 3C). H&E staining of 9-week-old Asah1^P361R/P361R;MCP-1^−/− and both 9- and 12-week-old Asah1^P361R/P361R;MCP-1^−/− tibias revealed a pale architecture compared to both Asah^+/+;MCP-1^+/+ and Asah1^+/+;MCP-1^−/− samples. These light H&E areas were stained positive for Mac-2 but not for B220 and CD-3, which demonstrate myeloid lineage-mediated infiltration (Fig. 3B). Similarly, FACS analysis of T-cells from thymic tissue of 9-week-old Asah1^P361R/P361R;MCP-1^−/− mice demonstrated a significant reduction in CD4⁺;CD8⁺ T-cell numbers compared to Asah1^P361R/P361R;MCP-1^+/+ mice with no differences seen between both genotypes in the various T-cell subsets (Fig. 3D and Supplementary Fig S3). Histological analysis performed on thymic tissue obtained from 9-week-old Asah1^P361R/P361R;MCP-1^−/− mice showed pale H&E staining that was additionally characterized by the presence of Mac-2 staining. Tissue injury and macrophage infiltration appear progressive as the staining of tissue from 12 weeks of age Asah1^P361R/P361R;MCP-1^−/− mice became more pale for H&E and more intense for Mac-2 (Supplementary Fig S3). FACS analysis of cells from 9-week-old spleen tissue of Asah1^P361R/P361R; MCP-1^−/− mice showed a significant reduction in CD11b⁺ and Gr1⁺ granulocytes compared to cells from 9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 3E and Supplementary Fig. S4).

The spleen parenchyma in the 9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice is also highly disrupted by the presence of foamy macrophages and demonstrates a reduction in B220⁺ and CD3⁺ cells (Supplementary Fig. S4). This phenotype is present in the 9-week-old Asah1^P361R/P361R;MCP-1^−/− mice but to a lesser extent (Supplementary Fig. S4). However, by 12 weeks of age the phenotype becomes exacerbated and mirrors that typically seen in the spleen of 9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Supplementary Fig. S4). MCP-1 deletion also appears to decrease the rate of tissue destruction in the spleen.

Liver inflammation and injury markers are reduced

Histological analyses (via H&E, Trichrome and IHC staining for Mac-2) demonstrated significant tissue disruption, fibrosis, and macrophage infiltration in liver tissue from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice compared to controls (Fig. 4A–C). The infiltration and fibrosis present in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mouse livers was more pervasive compared to samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− animals (Fig. 4C,D). The formation of large, foamy histiocytes and fibrotic regions increased by 11–12 weeks of age in Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 4E) but not to the extent seen in Asah1^P361R/P361R;MCP-1^+/+ mice. Albumin levels in serum showed a significant decrease in samples from Asah1^P361R/P361R;MCP-1^+/+ mice when compared to those from aged-matched controls (Fig. 4F). Ablation of MCP-1 normalized albumin levels in 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice, which was later lost in 11–12-week-old animals when compared to 8–9-week-old Asah1^+/+;MCP-1^+/+ mice (Fig. 4F). Although a decrease was detected in 11–12-week-old double mutants, there was no significant change when compared to 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 4F). We also measured various enzymes that are associated with liver injury. At 8–9 weeks of age, alkaline phosphatase (ALP) levels were increased in Asah1^P361R/P361R;MCP-1^+/+ mice compared to age-matched controls (Fig. 4G). ALP from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice was not different from age-matched controls, but 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice did display elevated ALP, similar to the levels seen in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 4G). In comparison to control mice, alanine aminotransferase (ALT) was elevated similarly in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice and in both 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 4H). In comparison to control mice, aspartate aminotransferase (AST) levels were elevated in both 8–9 and 11–12-week-old Asah1^P361R/P361R; MCP-1^−/− mouse samples but not to the same extent as that seen in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 4I).

Reduction of pulmonary infiltrates and protein accumulation

Recently we demonstrated that Asah1^P361R/P361R;MCP-1^+/+ mice develop chronic lung injury and inflammation¹⁷. Here we examined the effects of deletion of MCP-1 on those parameters. Micrographs of representative BALF Cytospin slides showed significant cellularity and proteinaceous material in samples from both 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ and 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice in comparison to controls (Fig. 5A–D). That said, samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice demonstrated a reduction in infiltrating cells and a lesser abundance of extracellular protein-stained debris than samples from the 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5D). That latter phenotype became even more pronounced in the 11–12 week Asah1^P361R/P361R;MCP-1^−/− samples (Fig. 5E). This observation was also reflected in BALF supernatant turbidity and protein concentration analyses. At 8–9 weeks of age, BALF turbidity and protein levels from Asah1^P361R/P361R;MCP-1^−/− were significantly lower than in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5F–G). However, by 11–12 weeks of age, BALF turbidity and protein levels from Asah1^P361R/P361R;MCP-1^−/− mice had increased to levels similar to 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5F–G). Quantitation of BALF cells was performed on Kwik-Diff stained Cytospin slides. Total cell counts in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice were not significantly different from samples from age-matched Asah1^P361R/P361R;MCP-1^+/+ mice, but the Asah1^P361R/P361R;MCP-1^+/+ mice did display a significant increase in cell recruitment between 8–9 and 11–12 weeks of age (Fig. 5H). BALF cell differentials from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice revealed an increase in macrophage abundance and reductions in neutrophil, lymphocyte, and percentage of multinucleated macrophages when compared to age-matched Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5I–L). The percentage of total macrophage, neutrophil, and percentage of multinucleated macrophages in the BALF of 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice had normalized to the levels found in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5I–L). Thus, it appears that deletion of MCP-1 may impede cellular recruitment to the lungs. This trend was also observed when an ELISA was performed on BALF supernatant to detect surfactant proteins (SP). There we observed a reduction of detectable SP-B and SP-C in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice. By 11–12 weeks of age SP-B and SP-C in the BALF of Asah1^P361R/P361R;MCP-1^−/− mice were detected at levels similar to 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 5N and O). Interestingly, though elevated in BALF supernatants from all Asah1^P361R/P361R mice, no significant changes were seen in Surfactant Protein (SP) A or D levels with altered MCP-1 expression (Fig. 5M and P).

Brain and behavioral phenotypes persist in MCP-1 deficient mice

Asah1^P361R/P361R;MCP-1^+/+ mice develop significant central nervous system defects including neuroinflammation, demyelination, neurodegeneration, and hydrocephaly. These become progressively more severe as the disease manifests fully¹⁸. To assess the state of neuroinflammation, brain tissues were stained with GFAP and Iba-1 to highlight activated astrocytes and microglia. Brain samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ and both 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice have similar Iba-1 and GFAP staining patterns in the cerebellum, thalamus, and cerebral cortex (Fig. 6A–G). This may indicate that there is no additive effect of inflammation between 8–9 and 11–12 weeks of age in these models. From brain wet-to-dry weight ratios, no changes in brain edema were found between 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ and both 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 6H).

Behavioral phenotypes unchanged in MCP-1 deficient mice

The Asah1^P361R/P361R;MCP-1^+/+ mice replicate behavioral features that are typically present in FD patients¹⁸. Amongst these the Asah1^P361R/P361R;MCP-1^+/+ mice have shown decreased locomotion, decreased exploratory behavior, increased thigmotaxis, and weakness in grip strength and rotarod testing¹⁸. To assess whether MCP-1 ablation may improve behavior parameters, we repeated the grip strength and Rotarod tests. In the grip strength test, both 8–9 and 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− mice displayed significantly decreased ability on both total limb and forelimb strength tests when compared to age-matched control mice (Fig. 6I and J). However, when we normalize for body weight, 8–9 week-old Asah1^P361R/P361R;MCP-1^−/− mice showed no differences in total limb or forelimb strength compared to age-matched controls (Fig. 6K,L). At 11–12 weeks, Asah1^P361R/P361R;MCP-1^−/− mice lost their total limb strength but maintained a hind-limb strength advantage (Fig. K,L). This may suggest that hind-limb weakness occurs prior to forelimb weakness in our model. However, due to their tight skin and our subsequent difficulty in scruffing Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice, we could not reliably obtain hind-limb data. Lastly, the Rotarod test demonstrated that 8–9 and 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− animals displayed a motor and endurance phenotype that largely mirrors what we reported in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice¹⁸ (Fig. 6M). Taken together, there appears to be no improvement in neuroinflammation or brain edema, and little improvement in age-matched motor strength, in the test animals.

Tissue-specific changes in sphingolipid profiles due to MCP-1 deletion

Sphingolipid profiles were measured via liquid chromatography-mass spectrometry (LC-MS) in lipid extracts from liver, lung, and brain tissue lysates from control and test animals. Sphingolipids assayed included ceramides (Cer), ceramide-1-phosphate (C1P), sphingomyelin (SM), monohexosylceramides (MHC), sphingosine (Sph), and sphingosine-1-phosphate (S1P). The most abundant sphingolipid in all three tissues in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice was Cer (Fig. 7A–C and Supplementary Fig S6). The greatest changes in abundance were in the lung, where 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice displayed increased Cer and SM levels compared to control mice, but had a significant reduction in Cer and increased SM when compared to 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 7B). Interestingly, this shift was no longer present in tissues from 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice. When we examined liver tissues, 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice had a reduction in total and C24:1 Cer compared to samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice. By 12 weeks of age, the C24:1 and total Cer content in liver were increased to the same level as that seen in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice. There were no differences between Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice for SM, MHCs, C1P, and S1P for the liver (Fig. 7J,M and Supplementary Figs S5 and S6). Sph in liver was unchanged between Asah1^P361R/P361R;MCP-1^−/− mice and age-matched controls, however a decrease was found when compared to the 11–12-week-old group (Supplementary Fig. S6A).

The greatest changes in Cer levels were seen in the lungs. There we observed a reduction in C24:1, C24:0, and total Cer content in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− animals compared to those from age-matched Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 7E). This relationship is reflected in a significant increase in SM24:1, SM24:0, and total SMs between samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− animals compared to those from age-matched Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 7K). In the lungs, we observed a significant reduction in C24:0 MHCs, total MHCs, C24:0 C1P, and total C1P species but no changes in Sph and S1P between samples from 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− animals compared to those from 9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Supplementary Figs S5 and S6). In brain lysates, there were no observed changes in the sphingolipid species we queried between samples from 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− animals compared to those from 9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice.

Unique Cytokine signature in Asah1^P361R/P361R;MCP-1^−/− double mutants

To access whether the absence of MCP-1 may affect cytokine profiles, a multiplex mouse cytokine panel was queried using serum samples. As we have seen before, MCP-1 levels were found to be dramatically increased in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice⁴. As expected, no MCP-1 was found in serum samples from 8–9 and 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 8A). Interestingly, the levels of monocyte inflammatory protein-1 alpha (MIP-1α) in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice was significantly higher compared to those obtained from age-matched Asah1^P361R/P361R;MCP-1^+/+ mice; these values were even further increased in samples from such mice at 11–12 weeks of age (Fig. 8B). Keratinocyte chemoattractant (KC) concentrations peaked in samples from both 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ and Asah1^P361R/P361R;MCP-1^−/− mice. While KC levels were detected at lower levels in 11–12-week-old samples compared to 8–9-week-old samples in Asah1^P361R/P361R;MCP-1^+/+, they were nonetheless statistically elevated when compared to controls (Fig. 8C). Interferon gamma-induced protein 10 (IP-10) concentrations in serum from 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice were elevated to similar levels as those seen in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice (Fig. 8E). Interestingly, monocyte induced by gamma interferon (MIG), Interleukin (IL) IL-12, and IL1α were not significantly increased in samples from 8–9-week-old Asah1^P361R/P361R; MCP-1^+/+ mice when compared to control mice but were indeed significantly increased in samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− mice (Fig. 4D,F,G). Although not statistically significant, IL1β, and IL13 concentrations displayed a trend towards an increase in 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− samples (Supplementary Fig. S7). No differences were seen for basic fibroblast growth factor (bFGF), IL-4, IL-5, IL-6, IL-10, IL-17, granulocyte macrophage colony-stimulating factor (GM-CSF), interferon gamma (IFNγ), or vascular endothelial growth factor (VEGF) (Supplementary Fig. S7). We further measured MCP-3 and MCP-5 levels by ELISA in mouse serum. Both MCP-3 and MCP-5 levels were significantly elevated in 8–9-week-old Asah1^P361R/P361R; MCP-1^+/+ when compared to age-matched controls (Fig. 8H,I). MCP-3 and MCP-5 levels were also elevated in both 8–9 and 11–12-week-old Asah1^P361R/P361R;MCP-1^−/− mice. No differences in MCP-3 and MCP-5 levels between samples from 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+, 8–9 and 11–12 week-old Asah1^P361R/P361R;MCP-1^−/− mice were observed.

Discussion

The signs and symptoms of FD can manifest along a spectrum. In its moderate form, FD patients will develop arthritis-like symptoms such as joint pain and nodule formation³. In its severe classical form, however, FD patients will often have significant inflammation, neurological complications, and respiratory failure¹. In our FD mouse, widespread inflammation has been reported to affect many organs in the Asah1^P361R/P361R;MCP-1^+/+ mouse^4,12,17. Here we examine multiple parameters of FD manifestations in the context of deletion of a key chemokine (MCP-1) that we identified previously as a biomarker for this disorder⁶. Our analyses of the hematopoietic, hepatic, pulmonary, and neurological systems demonstrates that the severity of MCP-1-mediated inflammation is organ dependent. Our results here further demonstrate that attenuation of MCP-1 in FD mice can affect ceramide accumulation, improve survival, and delay pathology.

The Asah1^P361R/P361;MCP-1^+/+ mouse has impaired hematopoiesis characterized by a decline in pre- and pro-B cell numbers in the bone marrow of aged mice and a reduction of CD4⁺ CD8⁺ T-cells within the thymus of 5-weeks-of-age animals that progressively worsens¹². Despite increased longevity and a delay in weight loss and skin elasticity at 8–9-weeks-of-age, the Asah1^P361R/P361R;MCP-1^−/− mice share a similar hematological profile to the Asah1^P361R/P361R;MCP-1^+/+ mice. Histological analyses revealed tissue damage to the architecture of the bone marrow, thymus, and spleen with 11–12 weeks of age Asah1^P361R/P361R;MCP-1^−/− mice, sharing a profile that is very similar to 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice. Since age-matched Asah1^P361R/P361R;MCP-1^−/− mice show reduced leukocytosis and a reduction in granulocytes in the spleen, it suggests that absence of MCP-1 can slow the rate of macrophage infiltration; this also suggests, however, that the bone marrow and thymus may be more sensitive to inflammation and injury when the sphingolipid balance is perturbed. This phenotype has also been noted in studies on the sphingosine 1-phosphate lyase deficient mouse (SGPL^−/−), where investigators showed impaired B-cell development in the bone marrow, thymic atrophy associated with a reduction in CD4⁺ and CD8⁺ thymocytes, and an increase in thymic ceramide levels^19,20.

Deletion of MCP-1 also leads to improvement in the hepatic system. In comparison to age-matched control animals, there was a reduction in liver injury enzymes, decreased formation of characteristic large foamy macrophages, and less tissue fibrosis in the double mutants. MCP-1 expression within the liver has been shown to play a role in hepatic inflammation and fibrosis in patients with hepatitis C²¹. Similarly, inhibition of MCP-1 with the structured L-enantiomeric RNA oligonucleotide mNOX-E36 (aka Spiegelmer) has shown promise in reducing fibrosis in murine models of chronic liver disease²². Since we also see a reduction in accumulated ceramides, it is possible that, similar to the lungs, an absence of MCP-1 is reducing the rate of recruitment of cells which is reducing the total amounts of ceramide as well as the inflammation-induced injury that we normally observe in Asah1^P361R/P361R;MCP-1^+/+ mice.

Infiltration of immune cells into the lungs and respiratory failure can be a significant problem in FD¹. Recently we have shown that Asah1^P361R/P361R;MCP-1^+/+ mice develop chronic lung injury caused by a combination of inflammation and vascular leakage¹⁷. Here we find that MCP-1 deletion results in significant improvement of lung phenotypes. BALF from Asah1^P361R/P361R;MCP-1^−/− mice revealed both lower protein content and lower cell counts than that from Asah1^P361R/P361R;MCP-1^+/+ mice. In addition, there was a mild reduction in lipo-protein-like material in the BALF, which also correlated with a reduction in various surfactant proteins. Surprisingly, in addition to reduced inflammation in the lungs, we also observed a reduction in all measured sphingolipids in lung tissue lysates (Fig. 8B). One explanation for this may be the reduced recruitment of cells within the lung parenchyma. Another explanation may be the reduced inflammatory cues produced by MCP-1 localized within the lungs; the role of MCP-1 as an instigator of inflammation and as a potential biomarker has been widely reported^23,24. Increased MCP-1 can also be detected in rare diseases like pulmonary alveolar proteinosis, chronic obstructive pulmonary disease, as well as in severe cases of acute lung injury^25,26,27. In addition, use of anti-rat MCP-1 antibodies has shown efficacy in reducing not only the size, but the quantity of glucan-induced pulmonary granulomas vasculitis in rats²⁸. Due to the widespread role of MCP-1 in lung pathology, it is thus possible that in the context of FD, MCP-1-mediated recruitment of inflammatory cells may be more penetrant and pernicious in the lung than other organs in our mouse model.

The brains of Asah1^P361R/P361R;MCP-1^+/+ mice show an accumulation and a shift in the relative abundance of various sphingolipids, the presence of cellular storage bodies in various neuronal cells, signs of inflammation, and elevated MCP-1 levels^4,18. Histological analyses on age-matched brains from Asah1^P361R/P361R;MCP-1^−/− mice also demonstrated significant astrocytosis and large activated microglia (Fig. 6D,E). Though not statistically significant, there also appears to be a trend towards an increase in percentage staining of Iba-1 from 8–9-week-old to 11–12-week-old brains of Asah1^P361R/P361R;MCP-1^−/− mice. Behavioral assays on the Asah1^P361R/P361R;MCP-1^−/− mice demonstrated little change from controls, however we do show a mild improvement in forelimb grip strength force when normalized for body weight (Fig. 6J,L). Together, this demonstrates that deletion in MCP-1 may have a minor effect in delaying the signs of neural inflammation in our Farber mice.

Inhibition of inflammatory cytokines has shown variable results in LSD brain models. For example, in the Hexβ^−/−; Mip-1α^−/− mouse, deletion of Mip-1α led to an improvement in brain pathology²⁹. The opposite outcome was observed when the same cross was performed with the Niemann-Pick Type C (NPC^−/−) mouse model³⁰. Both of those LSD models demonstrate some shared phenotypes; however, in the latter cross the mice experienced a decreased lifespan^29,30. The group that characterized this outcome rationalized that in the context of NPC, it is possible that inflammation in the brain may serve a protective role³⁰. This theme is also shared in the case of globoid cell leukodystrophy (GLD; Krabbe’s disease), which shares some neurological phenotypes with the Farber mouse such as activated microglia/macrophages and demyelination¹⁸. To genetically remove macrophages, one group crossed the GLD Twitcher (twi^−/−) mouse to the macrophage-deficient osteoporotic (CSF-1^op/op) mouse³¹. Double mutants there not only had a shorter lifespan but also manifested an exacerbated neurological phenotype compared to control twi^−/− mice³¹.

Brain sphingolipid profiles of our Asah1^P361R/P361R;MCP-1^−/− mice were largely unchanged compared to Asah1^P361R/P361R;MCP-1^+/+ mice. In our analyses of Sph there was a minor but significant reduction in Sph for both the Asah1^P361R/P361R;MCP-1^+/+, and Asah1^P361R/P361R;MCP-1^−/− groups. This observation deviates somewhat from our previously published results wherein we detected a modest increase in Sph in brain lysates from ACDase deficient mice¹⁸. The variability could be a combination of the different tissue homogenization protocols, lipid extraction methods, internal standards used, instrumentation, and LC/MS protocols as these were processed at different sites. Interestingly this contrasting result may be exclusive to Sph, however, as all other sphingolipids measured in both studies displayed the same trend¹⁸.

Nonetheless, elevated ceramide levels were noted in the brain. Increases in ceramides are also detected in various CNS conditions, such as in multiple sclerosis (MS)³². This study showed that activated astrocytes that were preferably localized to MS-related brain lesions were the main contributors of the increased levels of ceramides detected³². Furthermore, inhibition of the de novo pathway of ceramide synthesis with the S1P analogue FTY720 was able to attenuate reactive phenotype of astrocytes³². Therefore, it is possible that the inflammatory consequences of increased MCP-1 in the brain are masked by the deleterious effects of significant ceramide and sphingolipid accumulation

Our study demonstrated that genetic ablation of MCP-1 allowed Asah1^P361R/P361R mice to survive up to 14 weeks of age. This increased longevity coincided with reduced pathology in the lungs and liver of 8–9-week-old Asah1^P361R/P361R;MCP-1^−/− and age matched controls. By 11–12-weeks of age the disease phenotypes in Asah1^P361R/P361R;MCP-1^−/− mice largely mirrors that of 8–9-week-old Asah1 ^P361R/P361R;MCP-1^+/+ mice. While little to no changes were seen in the hematopoietic and neurological systems, the absence of MCP-1 slowed the deleterious effects of ceramide-induced inflammation. In addition, we found new changes in the cytokine profiles that may, in part, explain the impeded pathology in the Asah1^P361R/P361R;MCP-1^−/− mice.

KC expression was previously found to peak at 7–8 weeks and decline by 9 weeks in Asah1^P361R/P361R;MCP-1^+/+ mice⁶. In this study, deletion of MCP-1 caused a shift where KC was seen to peak at 8–9-weeks and later decrease in 11–12 week samples (Fig. 8C). Further, our data also highlights a possible compensatory accumulation of the cytokines MIP-1α, MIG, IL-12, and IL-1α in the double mutant animals. Along these lines, we previously showed that MIP-1α levels increase by 5 weeks and peaked at 9 weeks of age in Asah1^P361R/P361R;MCP-1^+/+ mice⁶. In this study, we found no statistical significance for MIP-1α in 8–9-week-old Asah1^P361R/P361R;MCP-1^+/+ mice samples. This may in part be due to sample variability in the Asah1^P361R/P361R;MCP-1^+/+ samples. However MIP-1α was elevated and significant in both 8–9 and 11–12-week-old Asah1^P361R/P361;MCP-1^−/− mice samples. MIP-1α, a well-studied chemokine, is known for its roles in macrophage recruitment and inflammatory responses. In fact, other studies of LSDs such as Gaucher disease and Sandhoff’s disease have reported elevations of MIP-1α as part of disease progression in patient and mouse models^29,33. In Gaucher disease, where glucosylceramide accumulates, infiltration of tissues and formation of large foamy macrophages is also widely abundant^34,35. Both MCP-1 and MIP-1α have been found to be elevated in the serum samples of Gaucher patients³⁶. Large foamy macrophages are a shared phenotype present in both Farber and Gaucher disease. Due to this similarity and the tight balance of sphingolipid metabolism, the compensatory accumulation of MIP-1α may yet be another shared sign. While more work is required, it is possible that the inflammation observed in both Farber disease and Gaucher disease manifest similarly.

Here we also report elevations in MIG in the serum of our Asah1^P361R/P361;MCP-1^−/− mice. In contrary, MIG from Asah1^P361R/P361;MCP-1^+/+ mice samples were not found to be statistically significant in this study but appear to show a trend towards an increase, which is also mirrored in FD patient plasma⁶. Similar findings were noted for IL-12. Lastly, IL-1α was elevated in the double mutants. This was unexpected as IL-1α in our previous data was variably expressed in mouse plasma⁶. There is evidence that activation of IL-1 may lead to the accumulation of ceramide and expression of the inflammatory enzyme COX-2 along with prostaglandin E₂ production³⁷. More work will be required to elucidate the roles of these cytokines in FD, however these data together demonstrate the complexity and nuanced cytokine/chemokine regulation that might be involved in the inflammatory response seen in FD.

Analyses of MCP-3 and MCP-5 by ELISA in mouse serum revealed significantly increased levels of these factors in samples from 8–9-week-old Asah1^P361R/P361;MCP-1^+/+ mice. This observation demonstrates that other agonists of CCR2 are also contributors to the inflammatory phenotype seen in ACDase deficiency^38,39. While the MCP-3 and MCP-5 levels were not statistically significant between 8–9 and 11–12-weeks in the Asah1^P361R/P361;MCP-1^−/− mice, there appeared to be a trend towards an increase. The high levels of MCP-3 and MCP-5 would partly explain the continued presence of foamy macrophages in Asah1^P361R/P361;MCP-1^−/− mice. A previous study has shown that MCP-3^−/− mice that were exposed to Listeria monocytogenes infection showed a similar inflammatory phenotype as those of MCP-1^−/− mice⁴⁰. That study demonstrated that both MCP-1 and MCP-3 act in parallel on CCR2 in the context of innate immune defense⁴⁰. This phenomenon may apply in our model as the ablation of MCP-1 alone provided a modest lifespan improvement to Asah1^P361R/P361 mice. Furthermore, another chemokine, MCP-4, which was not measured in this study, has also been shown to be an agonist for CCR2⁴¹. Out of all three chemokines measured, MCP-1 was detected at the highest level in serum samples of Asah1^P361R/P361;MCP-1^+/+ mice, suggesting a dominant role for that factor in macrophage recruitment in ACDase deficiency. While additional work will be required, the discovery of elevated MCP-3 and MCP-5 further underscores the importance of CCR2 signaling in ACDase biology.

MCP-1 is a potent chemo-attractant that has been implicated in exacerbating the pathology of an array of diseases. Genetic crosses between the MCP-1^−/− mouse and other disease models ranging from the Charcot-Marie-Tooth mouse model to the more common atherosclerosis mice models have been previously performed^42,43,44. Results showed that the absence of MCP-1 led to attenuation of neuroinflammation in the case of the Charcot-Marie-Tooth model, and reduction in aortic lesions the atherosclerotic ApoE deficient mouse^42,44.

MCP-1 has also been identified as a therapeutic target for other conditions including kidney and heart disease^45,46. Use of the structured L-enantiomeric RNA oligonucleotide mNOX-E36 (aka Spiegelmer) to inhibit MCP-1 has shown promise in murine models of chronic liver disease²². Similarly another group has shown that use of the MCP-1 inhibitor 2-Methyl-2-[[1-(phenylmethyl)-1H-indazol-3yl]methoxy]propanoic acid (aka Bindarit) can protect mice when induced with acute pancreatitis, and limit proteinuria in rat models of renal disease^47,48.

A heightened inflammatory response is common in many LSDs that involve sphingolipid storage as well as other more common diseases^49,50. In the case of MCP-1 release, one study has showed that C1P can promote MCP-1 release in various cell types via the downstream PI3K/Akt, MEK/ ERK, and p38 pathways⁵¹. Another study has demonstrated that inhibition of de novo synthesized ceramide can lead to IL-6 and MCP-1 secretion from adipocytes in vitro⁵². This observation was also replicated in an experiment wherein obese mice, that were treated with myriocin - a potent inhibitor of the de novo pathway of ceramide synthesis showed a reduction in ceramide levels and MCP-1 mRNA expression⁵³.

Currently the treatment options for FD are limited to anti-inflammatory therapy and, in some patients, BMT. Recombinant acid ceramidase (rhAC) is currently being developed, and has shown great promise as a potential therapy for FD¹³. A recent study showed that treating the ACDase-deficient mice with rhAC significantly improved survival, and reduced MCP-1 with repeated infusions¹³. Still, human studies and clinical approval of this treatment modality are still a ways off. Our study has demonstrated that targeting MCP-1 may delay the course of FD, and contribute to reduced inflammation within the respiratory and visceral systems. While more work will be required, the use of targeted anti-inflammatory treatments in conjunction with substrate reduction therapy, enzyme replacement therapy, or gene therapy may also create a synergistic benefit for FD management^54,55,56,57.

Material and Methods

Animal use, breeding and genotyping

To generate homozygous Asah1^P361R/P361R mice, we crossed Asah1^+/P361R heterozygotes as previously reported⁴. CCL2^tm1Rol (MCP-1^−/−) knockout mice⁵⁸ were purchased from Jackson Laboratory (Bar Harbor, MA). Male MCP-1^−/− mice were crossed to female Asah1^+/P361R mice to generate doubly heterozygous animals (Asah1^+/P361R;MCP-1^+/−). These doubly heterozygous mice were mated with MCP-1^−/− mice to generate Asah1^+/P361R;MCP-1^−/− mice. Subsequently Asah1^+/P361R;MCP-1^−/− mice were mated with each other to generate Asah1^P361R/P361R and MCP-1^−/− homozygous double mutants (Asah1^P361R/P361R;MCP-1^−/−). Genotypes were confirmed via PCR using genomic DNA from ear notches. For MCP-1 genotyping, a set of three primers were used, 5-GCC AGA GGC CAC TTG TGT AG-3, 5-TGA CAG TCC CCA GAG TCA CA-3, and 5-TCA TTG GGA TCA TCT TGC TG-3, yielding a 287 bp product for the wild-type gene and a 179 bp product for the knocked-out gene. To detect the wild-type allele of Asah1, we used the primers 5-CAG AAG GTA TGC GGC ATC GTC ATA C-3 and 5-AGG GCC ATA CAG AGA AAC CCT GTC TC-3, which yielded a 379 bp product. For the Asah1 knock-in allele, we used the primers 5-TCA AGG CTT GAC TTT GGG GCA C-3 and 5-GCT GGA CGT AAA CTC CTC TTC AGA CC-3, which amplifies a 469 bp product from the neomycin resistance cassette. All animal procedures were approved and carried out in strict adherence to the policies of the University Health Network (UHN) Animal Care Committee and the Medical College of Wisconsin (MCW) Institutional Animal Care and Use Committee (IACUC).

Animal data and organ weights

Mice survival was recorded for Kaplan-Meier curves. For organ weight, mice were euthanized with CO₂ gas and immediately weighed. Organs were collected immediately and weighed. Brain edema was determined by brain wet-to-dry weight ratio. Whole brains were weighed to determine wet weight and then were placed in a laboratory oven (Qualtech Industries Denver, CO) to evaporate for 48 hours. Dried samples were weighed to obtain dry weight. Skin stretch was quantified with a digital vernier caliper (Fisher Scientific, Waltham, MA) by measuring the height of the tent formed when scruffing the mouse.

Peripheral blood and serum biochemistry, ELISAs, and cytokine analyses

Peripheral blood was collected by cardiac puncture into EDTA-coated microtainers (BD, Biosciences Canada, Mississauga, Canada). Blood samples were inserted into a Hemavet (Drew Scientific Group, Waterbury CT) for complete blood count (CBC) analyses. For serum separation, mouse blood was collected via cardiac puncture into serum separator SST microtainers (BD Biosciences). Sample tubes were gently inverted and the blood was allowed to clot at room temperature for 30 minutes. Samples were then centrifuged at 1200 g for 10 minutes. The serum portion was immediately collected and stored in −80 °C until use. Mouse cytokine levels were measured on collected serum with the Cytokine-20-Plex mouse panel (Thermo Scientific Pierce, Waltham, MA) following the manufacturer’s instructions. Luminescence was measured on the Luminex 100 instrument (Luminex, Austin, TX). Data with a low bead count (<45 beads) was omitted. Additionally, we measured MCP-3 and MCP-5 in mouse serum with MCP-3 and MCP-5 ELISA kits (Thermo Scientific, Waltham, MA). Serum metabolites and liver enzymes in serum were measured using the VetScan Comprehensive Diagnostic Profile and Mammalian Liver Profile (Abaxis Union City, CA) on the Abaxis VetScan VS2 (Abaxis Union City, CA). An AST ELISA kit (Cloud-Clone Corp. Wuhan China) was used to assay for serum amino aspartate transferase (AST) levels.

BALF turbidity, cytospin and differential

A 20-gauge catheter (BD, Biosciences) was inserted into the trachea of CO₂-euthanized mice and secured. The lungs were flushed three times by gentle washing with 1.0 ml of ice-cold phosphate buffered saline (PBS). BALF was collected in 1.5 ml tubes and centrifuged at 300× g at 4 °C for 10 minutes. The supernatant was removed and stored at −80 °C. BALF supernatant was measured for turbidity on the NanoDrop One (Thermo Scientific Wilmington DE) at OD₆₀₀. Protein concentration of BALF supernatant was measured using a commercially available bicinchoninic acid (BCA) assay kit (Thermo Scientific Pierce, Waltham, MA). Surfactant proteins A, B, C, and D in BALF supernatant were measured using ELISA kits for mouse material (Cloud-Clone Corp. Wuhan, China) as per the manufacturer’s instructions.

For cell analyses, BALF cell pellets were resuspended in 500 µl of PBS and varying dilutions were used to measure total cell counts, which were performed on trypan blue-stained samples on the Countess II FL automated cell counter (Life Technologies, Carlsbad, CA). The remainder of the resuspended cells were diluted in various concentrations to a total volume of 200 µl with PBS and a cytospin was performed with the Shandon CytoSpin III Cytocentrifuge (Thermo Shandon, Waltham, MA) for 5 mins at 300 g. For cell type analyses, cytospins that contained 200,000 cells per slide were stained with the Kwik-Diff kit (Thermo Scientific Pierce, Waltham, MA). Differential cell counts were obtained by averaging counts from 10 non-overlapping zones with a total of 200 cells scored in each zone.

Histopathology and immunohistochemistry

As mentioned above, mice were euthanized by CO₂ inhalation. Cardiac perfusion with ice-cold PBS was performed with a 24 G needle and, following necropsy, organs were immediately fixed in 10% phosphate-buffered formalin for 24–48 hours. Organs were subsequently embedded in paraffin and sectioned at 4 μm. Dissected tibias were decalcified with Cal-Ex II fixative/decalcifier per the manufacturer’s instructions (Fisher Scientific.) prior to embedding and sectioning. For analysis of the hematopoietic system, paraffin-embedded thymus, tibia, and spleen samples were stained with hematoxylin and eosin (H&E). Immunohistochemistry (IHC) was then performed with the following primary antibodies: B220 (BD Biosciences #550286; 1:100), CD3 (Sigma #C7930; 1:1000), and Mac-2 for myeloid cells (Cedarlane #CL8942AP; 1:2000). For liver analyses, tissue sections were stained for H&E and Masson’s trichrome. Liver IHC was performed using the following primary antibodies: anti-mouse neutrophil, clone 7/4 (Cedarlane, Burlington, Canada) and rat anti-mouse Mac-2 (Galectin-3) clone M3/38 (Cedarlane). For brain analyses, tissue sections were stained with H&E and IHC was performed using the following primary antibodies: rabbit anti-ionized, calcium-binding adaptor molecule 1 (Iba-1) (Wako Chemicals USA, Cambridge, MA) and chicken anti-glial fibrillary acidic protein (GFAP) (Aves Lab Inc, Tigard, OR). The following secondary antibodies and kits were then used to detect primary antibodies: rabbit anti-rat IgG, biotinylated (Vector Laboratories, Burlingame, CA); goat anti-rabbit IgG, biotinylated (Vector Laboratories); goat anti-rat IgG, biotinylated (Vector Laboratories); donkey anti-chicken IgG (Jackson ImmunoResearch USA, West Grove PA); donkey anti-rabbit IgG, biotinylated (ImmunoResearch); avidin-biotin/HRP (Vector Laboratories); DAB kit (Vector Laboratories) and Vectastain Elite ABC kit (Vector Laboratories). Histology slides were scanned on the Aperio AT2 histology slide scanner (Leica Biosystems, Buffalo Grove, IL) or NanoZoomer 2.0-HT histology slide scanner (Hamamatsu Photonics, Ichinocho, Japan). Scanned micrographs were analyzed with Aperio ImageScope analysis software (Leica Biosystems, Grove, IL).

Flow cytometry of hematopoietic cells

Flow cytometry was performed on bone marrow, spleen, and thymus samples. For the latter two, cells were forced through a 40 µm nylon cell strainer in PBS with 2% fetal calf serum (FCS). For the bone marrows, cells were collected by flushing femurs and tibias with PBS containing 2% FCS. After RBC lysis, collected cells were washed and resuspended in PBS with 2% FCS and counted on a hemocytometer. For fluorescence-activated cell sorting (FACS) analyses, cells were stained for 30 mins at 4 °C with the following antibodies: CD3 FITC (BioLegend San Diego, CA; 17A2), CD4 PE (BD Biosciences; GK1.5), CD8 APC (BD Biosciences; 53–6.7), CD19 BV605 (Biolegend; 6D5), CD43 APC (Biolegend; S11), IgD e450 (eBiosciences; 11–26 Waltham, MA), IgM PE-Cy-7 (Biolegend; RMM-1), B220 PE (eBiosciences RA3–6B2), Gr-1 FITC (Biolegend RB-6–8C5), Mac1 PE (BD Biosciences; M1/70), and CD11c APC (eBiosciences; N418). FACS analysis was performed on a LSR Fortessa flow cytometer (BD Biosciences) with FACSDiva software (BD Biosciences). Data was analyzed with FlowJo software (Tree Star Inc, Ashland, OR).

Sphingolipid mass spectrometry

Brain, liver, and lung tissue samples were homogenized in 500 µl PBS with the Omni Bead Raptor 24 tissue homogenizer (Omni International, Inc., Kennesaw, GA) using 2.8 mm ceramic beads. Lipids were extracted from 50 µl of tissue lysate with 200 µl isopropanol. Two sets of lipid mass spectrometry analyses were performed. In the first experiment; the following internal standards were used for sphingolipid measurements: ceramide 100 ng (d18:1/ 22:0) d₄ (Medical University of South Carolina (MUSC) Lipidomics Core, Charleston, SC); monohexosylceramide 100 ng (d18:1/17:0) (Avanti Polar Lipids Inc., Alabaster, AL); sphingomyelin, 1000 ng (d18:1/17:0) (Avanti Polar Lipids Inc.); and ceramide-1-phosphate (d18:1/16:0), (d18:1/24:0) and (d18:1/24:1) (Matreya Inc., Pleasant Gap, PA); (Avanti Polar Lipids Inc.)⁵⁹. For the second experiment the following internal standards were used: 100 ng of d₇-Sphingosine (Avanti Polar Lipids Inc.); and 100 ng of d₇-sphingosine-1-phosphate (Avanti Polar Lipids Inc.). Relative quantification (i.e. peak:area ratio) was obtained for the analytes in comparison to those from their corresponding internal standards.

Samples were analyzed on the Shimadzu 20AD HPLC system using reverse-phase C18 HPLC columns (Agilent Co., Santa Clara, CA) and a Leap PAL autosampler coupled to a triple quadrupole mass spectrometer (API-4000: Applied Biosystems, Carlsbad, CA) operated in MRM (multiple reaction mode) at the MUSC Lipidomics Core. Positive-ion ESI mode was used to detect all sphingolipids. Tissue extraction samples were injected in duplicate for data averaging. The Analyst 1.5.1 software was used for data analysis (Applied Biosystems). Data are presented as fold change relative to the averaged sphingolipid values detected in samples from 8–9-week-old Asah1^+/+;MCP-1^+/+ mice.

Quantification and image analysis

For the quantitative evaluation of GFAP and Iba-1 staining in brain samples, five non-overlapping images (20x magnification, 485 µm × 285 µm) for each anatomical region of interest were obtained from scanned micrographs for each slide. Three consecutive brain sections per mouse were stained, scanned, and analyzed. All quantitation was performed with Fiji-ImageJ analysis software (National Institutes of Health, Bethesda, MD).

Behavioral tests

Motor coordination and muscle strength were tested with an accelerating rotating rod (rotarod) and grip strength meter. Circadian rhythms were taken into account; all tests were performed between 8 am and 12 pm. To reduce non-study related variability, all tests were performed with the same apparatus in the same room. For the IITC Rotarod (IITC Inc. Life Science, Woodland Hills CA), mice were placed on the device and subjected to acceleration from 4 rpm to 40 rpm for a total of 5 minutes. The time when the mice fell off - measured from start - was then recorded. Animals were subjected to three trials per day for two consecutive days; with the same individual performing all tests. For the grip strength test, each animal was weighed prior to the trial. Both total-limb grip strength and fore-limb grip strength were measured with a digital grip strength meter (Columbus Instruments, Columbus, OH). For this assay, mice were placed on the metal grid and allowed to grip with either all total limbs or just forelimbs. After confirmation of grip, the mouse tail was pulled posteriorly parallel to the grid at a constant rate until release. The grip strength, measured by Gram-force, was recorded for three consecutive trials and then averaged. The grip strength was expressed as mean grip strength relative to weight Gram-force/gram body weight for both total limbs and forelimbs.

Statistical analyses

Data are expressed as means ± standard error. Survival significance was tested with the log-rank (Mantal-Cox) test comparing pairs of curves. All subsequent data was analyzed with a 1-way ANOVA followed by a Tukey post-test. All statistics were analyzed using GraphPad Prism 5.0 (GraphPad Software Inc, La Jolla, CA). Significant differences are expressed in the figures as *p < 0.05, **p < 0.01, and ***p < 0.001.

References

Levade, T., Sandhoff, K., Schulze, H. & Medin, J. In Scriver’s OMMBID (Online Metabolic and Molecular Bses of Inherited Diseases) eds Valle, D., Beaudet, A. L., Vogelstein, B., Kinzler, K. W., Antonarakis, S. E., Ballabio, A. (McGraw-Hill, New York, 2014).
Ahmad, A., Mazhar, A. U. & Anwar, M. Farber disease: a rare neurodegenerative disorder. J Coll Physicians Surg Pak. 19, 67–68 (2009).
PubMed Google Scholar
Ehlert, K. et al. Farber disease: clinical presentation, pathogenesis and a new approach to treatment. Pediatr Rheumatol Online J. 5, 15 (2007).
Article PubMed PubMed Central Google Scholar
Alayoubi, A. M. et al. Systemic ceramide accumulation leads to severe and varied pathological consequences. EMBO Mol Med. 5, 827–842 (2013).
Article CAS PubMed PubMed Central Google Scholar
Li, C. et al. The human acid ceramidase gene (ASAH): structure, chromosomal location, mutation analysis, and expression. Genomics 62, 223–231 (1999).
Article CAS PubMed Google Scholar
Dworski, S. et al. Acid Ceramidase Deficiency is characterized by a unique plasma cytokine and ceramide profile that is altered by therapy. Biochim Biophys Acta 1863, 386–394 (2017).
Article CAS PubMed Google Scholar
Deshmane, S. L., Kremlev, S., Amini, S. & Sawaya, B. E. Monocyte chemoattractant protein-1 (MCP-1): an overview. J. Interferon Cytokine Res. 29, 313–326 (2009).
Article CAS Google Scholar
Cushing, S. D. et al. Minimally modified low density lipoprotein induces monocyte chemotactic protein 1 in human endothelial cells and smooth muscle cells. Proc. Natl. Acad. Sci. USA 87, 5134–5138 (1990).
Article ADS CAS PubMed PubMed Central Google Scholar
Standiford, T. J. et al. Macrophage inflammatory protein-1 alpha mediates lung leukocyte recruitment, lung capillary leak, and early mortality in murine endotoxemia. J. Immunol. 155, 1515–1524 (1995).
CAS PubMed Google Scholar
Yoshimura, T., Robinson, E. A., Tanaka, S., Appella, E. & Leonard, E. J. Purification and amino acid analysis of two human monocyte chemoattractants produced by phytohemagglutinin-stimulated human blood mononuclear leukocytes. J. Immunol. 142, 1956–1962 (1989).
CAS PubMed Google Scholar
Saygi, S., Haytoglu, Z., Savas, T., Alkan, O. & Erol, I. P78–2554: Farber disease in a child with a novel homozygous c. 92G > T mutation. Eur. J. Paediatr. Neurol. 19, S116 (2015).
Google Scholar
Dworski, S. et al. Markedly perturbed hematopoiesis in acid ceramidase deficient mice. Haematologica. 100, e162–5 (2015).
Article PubMed PubMed Central Google Scholar
He, X. et al. Enzyme replacement therapy for Farber disease: Proof-of-concept studies in cells and mice. BBA Clinc. (2017).
Yeager, A. et al. Bone marrow transplantation for infantile ceramidase deficiency (Farber disease). Bone Marrow Transplant. 26 (2000).
Vormoor, J. et al. Successful hematopoietic stem cell transplantation in Farber disease. J. Pediatr. 144, 132–134 (2004).
Article PubMed Google Scholar
Lopez-Vasquez, L. et al. Acid ceramidase deficiency leads to multiple skin abnormalities in a mouse model of Farber disease. Mol. Genet. Metab. 117, S75–S76 (2016).
Article Google Scholar
Yu, F. P. et al. Chronic lung injury and impaired pulmonary function in a mouse model of acid ceramidase deficiency. Am. J. Physiol. Lung Cell Mol. doi: 10.1152/ajplung.00223.2017. (2017).
Sikora, J. et al. Acid Ceramidase Deficiency in Mice Results in a Broad Range of Central Nervous System Abnormalities. Am. J. Pathol. 187, 864–883 (2017).
Article CAS PubMed Google Scholar
Vogel, P. et al. Incomplete inhibition of sphingosine 1-phosphate lyase modulates immune system function yet prevents early lethality and non-lymphoid lesions. PloS one 4, e4112 (2009).
Article ADS PubMed PubMed Central Google Scholar
Weber, C. et al. Discontinued postnatal thymocyte development in sphingosine 1-phosphate-lyase-deficient mice. J. Immunol. 183, 4292–4301 (2009).
Article CAS PubMed Google Scholar
Mühlbauer, M. et al. A novel MCP-1 gene polymorphism is associated with hepatic MCP-1 expression and severity of HCV-related liver disease. Gastroenterology 125, 1085–1093 (2003).
Article PubMed Google Scholar
Baeck, C. et al. Pharmacological inhibition of the chemokine CCL2 (MCP-1) diminishes liver macrophage infiltration and steatohepatitis in chronic hepatic injury. Gut 61, 416–426 (2012).
Article CAS PubMed Google Scholar
Chiao, Y. A. et al. Multi-analyte profiling reveals matrix metalloproteinase-9 and monocyte chemotactic protein-1 as plasma biomarkers of cardiac aging. Circ. Cardiovasc. Genet. 4, 455–462 (2011).
Article CAS PubMed PubMed Central Google Scholar
Ruhwald, M., Bjerregaard-Andersen, M., Rabna, P., Eugen-Olsen, J. & Ravn, P. IP-10, MCP-1, MCP-2, MCP-3, and IL-1RA hold promise as biomarkers for infection with M. tuberculosis in a whole blood based T-cell assay. BMC research notes 2, 19 (2009).
Article PubMed PubMed Central Google Scholar
Bhatia, M., Zemans, R. L. & Jeyaseelan, S. Role of chemokines in the pathogenesis of acute lung injury. Am. J. Respir. Cell. Mol. Biol. 46, 566–572 (2012).
Article CAS PubMed PubMed Central Google Scholar
Suga, M. et al. Clinical significance of MCP-1 levels in BALF and serum in patients with interstitial lung diseases. Eur. Respir. J. 14, 376–382 (1999).
Article CAS PubMed Google Scholar
Iyonaga, K. et al. Elevated bronchoalveolar concentrations of MCP‐1 in patients with pulmonary alveolar proteinosis. Eur. Respir. J. 14, 383–389 (1999).
Article CAS PubMed Google Scholar
Flory, C. M., Jones, M. L. & Warren, J. S. Pulmonary granuloma formation in the rat is partially dependent on monocyte chemoattractant protein 1. Lab. Invest. 69, 396–404 (1993).
CAS PubMed Google Scholar
Wu, Y. P. & Proia, R. L. Deletion of macrophage-inflammatory protein 1 alpha retards neurodegeneration in Sandhoff disease mice. Proc. Natl. Acad. Sci. USA 101, 8425–8430 (2004).
Article ADS CAS PubMed PubMed Central Google Scholar
Lopez, M. E., Klein, A. D., Hong, J., Dimbil, U. J. & Scott, M. P. Neuronal and epithelial cell rescue resolves chronic systemic inflammation in the lipid storage disorder Niemann-Pick C. Hum. Mol. Genet. 21, 2946–2960 (2012).
Article CAS PubMed PubMed Central Google Scholar
Kondo, Y., Adams, J. M., Vanier, M. T. & Duncan, I. D. Macrophages counteract demyelination in a mouse model of globoid cell leukodystrophy. J. Neurosci. 31, 3610–3624 (2011).
Article CAS PubMed PubMed Central Google Scholar
van Doorn, R. et al. Fingolimod attenuates ceramide-induced blood–brain barrier dysfunction in multiple sclerosis by targeting reactive astrocytes. Acta Neuropathol., 1–14 (2012).
Van Breemen, M. J. et al. Increased plasma macrophage inflammatory protein (MIP)-1α and MIP-1β levels in type 1 Gaucher disease. Biochim. Biophys. Acta 1772, 788–796 (2007).
Article Google Scholar
Jmoudiak, M. & Futerman, A. H. Gaucher disease: pathological mechanisms and modern management. Br. J. Haematol. 129, 178–188 (2005).
Article CAS PubMed Google Scholar
Mistry, P. K. et al. Glucocerebrosidase gene-deficient mouse recapitulates Gaucher disease displaying cellular and molecular dysregulation beyond the macrophage. Proc. Natl. Acad. Sci. USA 107, 19473–19478 (2010).
Article ADS CAS PubMed PubMed Central Google Scholar
Pavlova, E. V. et al. Potential biomarkers of osteonecrosis in Gaucher disease. Blood Cells Mol. Dis. 46, 27–33 (2011).
Article CAS PubMed Google Scholar
Homaidan, F. R., El-Sabban, M. E., Chakroun, I., El-Sibai, M. & Dbaibo, G. S. IL-1 stimulates ceramide accumulation without inducing apoptosis in intestinal epithelial cells. Mediators Inflamm. 11, 39–45 (2002).
Article CAS PubMed PubMed Central Google Scholar
Franci, C., Wong, L. M., Van Damme, J., Proost, P. & Charo, I. F. Monocyte chemoattractant protein-3, but not monocyte chemoattractant protein-2, is a functional ligand of the human monocyte chemoattractant protein-1 receptor. J. Immunol. 154, 6511–6517 (1995).
CAS PubMed Google Scholar
Sarafi, M. N., Garcia-Zepeda, E. A., MacLean, J. A., Charo, I. F. & Luster, A. D. Murine monocyte chemoattractant protein (MCP)-5: a novel CC chemokine that is a structural and functional homologue of human MCP-1. J. Exp. Med. 185, 99–109 (1997).
Article CAS PubMed PubMed Central Google Scholar
Jia, T. et al. Additive roles for MCP-1 and MCP-3 in CCR2-mediated recruitment of inflammatory monocytes during Listeria monocytogenes infection. J. Immunol. 180, 6846–6853 (2008).
Article CAS PubMed PubMed Central Google Scholar
Berkhout, T. A. et al. Cloning, in vitro expression, and functional characterization of a novel human CC chemokine of the monocyte chemotactic protein (MCP) family (MCP-4) that binds and signals through the CC chemokine receptor 2B. J. Biol. Chem. 272, 16404–16413 (1997).
Article CAS PubMed Google Scholar
Groh, J. et al. Attenuation of MCP-1/CCL2 expression ameliorates neuropathy in a mouse model for Charcot–Marie–Tooth 1X. Hum. Mol. Genet. 19, 3530–3543 (2010).
Article CAS PubMed Google Scholar
Kohl, B., Fischer, S., Groh, J., Wessig, C. & Martini, R. MCP-1/CCL2 modifies axon properties in a PMP22-overexpressing mouse model for Charcot-Marie-Tooth 1A neuropathy. Am. J. Pathol. 176, 1390–1399 (2010).
Article CAS PubMed PubMed Central Google Scholar
Dawson, T. C., Kuziel, W. A., Osahar, T. A. & Maeda, N. Absence of CC chemokine receptor-2 reduces atherosclerosis in apolipoprotein E-deficient mice. Atherosclerosis 143, 205–211 (1999).
Article CAS PubMed Google Scholar
Tesch, G. H. MCP-1/CCL2: a new diagnostic marker and therapeutic target for progressive renal injury in diabetic nephropathy. Am. J. Physiol. Renal Physiol. 294, F697–701 (2008).
Article CAS PubMed Google Scholar
Niu, J. & Kolattukudy, P. E. Role of MCP-1 in cardiovascular disease: molecular mechanisms and clinical implications. Clin. Sci. (Lond) 117, 95–109 (2009).
Article CAS Google Scholar
Bhatia, M., Ramnath, R. D., Chevali, L. & Guglielmotti, A. Treatment with bindarit, a blocker of MCP-1 synthesis, protects mice against acute pancreatitis. Am. J. Physiol. Gastrointest. Liver Physiol. 288, G1259–65 (2005).
Article CAS PubMed Google Scholar
Zoja, C. et al. Effects of MCP-1 inhibition by bindarit therapy in a rat model of polycystic kidney disease. Nephron 129, 52–61 (2015).
Article CAS PubMed Google Scholar
El Alwani, M., Wu, B. X., Obeid, L. M. & Hannun, Y. A. Bioactive sphingolipids in the modulation of the inflammatory response. Pharmacol. Ther. 112, 171–183 (2006).
Article CAS PubMed Google Scholar
Maceyka, M. & Spiegel, S. Sphingolipid metabolites in inflammatory disease. Nature 510, 58–67 (2014).
Article ADS CAS PubMed PubMed Central Google Scholar
Arana, L. et al. Ceramide 1-phosphate induces macrophage chemoattractant protein-1 release: involvement in ceramide 1-phosphate-stimulated cell migration. Am. J. Physiol. Endocrinol. Metab. 304, E1213–26 (2013).
Article CAS PubMed Google Scholar
Hamada, Y. et al. Involvement of de novo ceramide synthesis in pro-inflammatory adipokine secretion and adipocyte–macrophage interaction. J. Nutr. Biochem. 25, 1309–1316 (2014).
Article CAS PubMed Google Scholar
Yang, G. et al. Central role of ceramide biosynthesis in body weight regulation, energy metabolism, and the metabolic syndrome. Am. J. Physiol. Endocrinol. Metab. 297, E211–24 (2009).
Article CAS PubMed PubMed Central Google Scholar
Schuchman, E. H. Acid ceramidase and the treatment of ceramide diseases: the expanding role of enzyme replacement therapy. BBA - Molecular Basis of Disease. 1862, 1459–1471 (2016).
Article CAS Google Scholar
Walia, J. S. et al. Autologous Transplantation of Lentivector/Acid Ceramidase–Transduced Hematopoietic Cells in Nonhuman Primates. Hum. Gene Ther. 22, 679–687 (2011).
Article CAS PubMed PubMed Central Google Scholar
Ramsubir, S. et al. In vivo delivery of human acid ceramidase via cord blood transplantation and direct injection of lentivirus as novel treatment approaches for Farber disease. Mol. Genet. Metab. 95, 133–141 (2008).
Article CAS PubMed PubMed Central Google Scholar
Medin, J. A. et al. Retrovirus-mediated correction of the metabolic defect in cultured Farber disease cells. Hum. Gene Ther. 10, 1321–1329 (1999).
Article CAS PubMed Google Scholar
Lu, B. et al. Abnormalities in monocyte recruitment and cytokine expression in monocyte chemoattractant protein 1-deficient mice. J. Exp. Med. 187, 601–608 (1998).
Article CAS PubMed PubMed Central Google Scholar
Bielawski, J. et al. Sphingolipid analysis by high performance liquid chromatography-tandem mass spectrometry (HPLC-MS/MS). Sphingolipids as Signaling and Regulatory Molecules 46–59 (2010).

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Acknowledgements

We thank the staff at The Centre for Phenogenomics (TCP), the Centre for Modeling Human Diseases (CMHD) Pathology core in Toronto, and the Children’s Hospital of Wisconsin (CHW) Children’s Research Institute (CRI) Histology Core for technical assistance with histology and immunohistochemistry services. We also thank the Advanced Optical Microscopy Facility (AOMF) at the University Health Network for providing whole-slide scanning for pathology analysis. We thank the staff at the MCW Neuroscience Research Center Rodent Behavior Core for technical assistance on behavioral assays. Thanks to the Medical University of South Carolina (MUSC) Lipidomics Core for lipidomic services. We also want to express thanks to Dr. Joshua Moreau for technical and flow cytometry assistance. Lastly, the authors would like to thank Dr. Monty McKillop for critical reviewing of this manuscript. These studies were supported by the MACC Fund Endowed Chair awarded to J.A.M. from MCW.

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Authors and Affiliations

Institute of Medical Science, University of Toronto, Toronto, ON, Canada
Fabian P. S. Yu, Shaalee Dworski & Jeffrey A. Medin
Department of Medical Biophysics, University of Toronto, Toronto, ON, Canada
Jeffrey A. Medin
University Health Network, Toronto, ON, Canada
Jeffrey A. Medin
Department of Pediatrics, Medical College of Wisconsin, Milwaukee, WI, USA
Fabian P. S. Yu & Jeffrey A. Medin
Department of Biochemistry, Medical College of Wisconsin, Milwaukee, WI, USA
Jeffrey A. Medin

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Fabian P. S. Yu
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Contributions

J.A.M., and F.P.S.Y. conceived and designed research; F.P.S.Y. and S.D. performed experiments; J.A.M., F.P.S.Y., and S.D. analyzed data; J.A.M, F.P.S.Y., S.D. interpreted results; J.A.M. and F.P.S.Y. drafted the manuscript; J.A.M., F.P.S.Y., and S.D. edited and revised the manuscript; J.A.M., S.D., and F.P.S.Y. approved the final version of manuscript.

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Correspondence to Jeffrey A. Medin.

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Yu, F.P.S., Dworski, S. & Medin, J.A. Deletion of MCP-1 Impedes Pathogenesis of Acid Ceramidase Deficiency. Sci Rep 8, 1808 (2018). https://doi.org/10.1038/s41598-018-20052-6

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Received: 21 September 2017
Accepted: 10 January 2018
Published: 29 January 2018
DOI: https://doi.org/10.1038/s41598-018-20052-6

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