BioMed Research International

BioMed Research International / 2019 / Article

Research Article | Open Access

Volume 2019 |Article ID 4508048 | 11 pages | https://doi.org/10.1155/2019/4508048

Sulfatases, in Particular Sulf1, Are Important for the Integrity of the Glomerular Filtration Barrier in Zebrafish

Academic Editor: Ravi K. R. Marreddy
Received17 May 2019
Accepted27 Jun 2019
Published22 Jul 2019

Abstract

The 6-O-endosulfatases (sulfs) are important enzymatic components involved in the regulation of heparan sulfate by altering the sulfatation pattern. Specifically in the kidney, sulfs have been implicated in the glomerular podocyte-endothelial cell crosstalk and in the preservation of the glomerular filtration barrier (GFB) in different mouse models. Since it has been shown that in zebrafish larvae, Sulf1, Sulf2a, and Sulf2b are expressed in the pronephric kidney we set out to establish if a reduction in sulf expression leads to GFB dysfunction. Here, we show that a reduced sulf expression following morpholino (MO) induced knockdown in zebrafish larvae promotes damage to the GFB leading to renal plasma protein loss from the circulation. Moreover, a combined knockdown of Sulf1, Sulf2a, and Sulf2b is associated with severe morphologic changes including narrowing of the fenestration between glomerular endothelial cells as well as thickening of the glomerular basement membrane and podocyte foot process effacement, suggesting that glomerular damage is an underlying cause of the circulatory protein loss observed after MO injection. Additionally, we show that a decrease in sulf expression reduces the bioavailability of VegfA in the glomerulus of the pronephros, which may contribute to the structural changes observed in the glomeruli of morphant fish. Furthermore, consistent with previous results, knockdown of the sulfs is associated with arteriovenous malformations in particular in the tail region of the larvae. Overall, taken together our results suggest that 6-O-endosulfatases are important in the preservation of GFB integrity and a reduction in their expression levels induces phenotypic changes that are indicative of renal protein loss.

1. Introduction

The 6-O-endosulfatase enzymes (sulfs) are key regulators of heparan sulfate (HS) exerting their modulating function through the modification of the sulfatation pattern by selectively removing 6-O-sulfate of HS predominantly in the highly sulfated domains [14]. The interaction between HS and vascular endothelial growth factor (VEGF) is mediated directly through the sulfs on the basis of the degree of 6-O-sulfatation on HS polysaccharide chains [59]. The regulatory function of the sulfs on growth factor signaling including VEGFA-associated pathways is mediated directly in the extracellular matrix (ECM) or at the cell surface [9]. In a previous study using HUVECs, siRNA induced knockdown of hSULF1 abrogated arterial marker expression in response to VEGFA stimulation [9]. Furthermore, zebrafish larvae with a reduced sulf1 mRNA expression had arterial malformations including arteriovenous shunts [9]. Given that these malformations were prevented by coinjection of ectopic vegfa165 mRNA, these findings support the hypothesis that Sulf1 expression is necessary for Vegf mediated angiogenesis [9].

Analogous to mouse glomeruli which express both Sulf1 and Sulf2 [1, 3], zebrafish express three homologs of the sulfs: Sulf1, Sulf2a, and Sulf2b, in the pronephric ducts [10]. However, the sulf pronephros expression pattern appears to be dynamic since not all sulf homologs are present in parallel during pronephros development [10].

It has been established in mouse models that endothelial cell morphology and function are influenced by the paracrine mechanisms of podocytes, specifically signaling to the endothelium via the podocyte-derived VEGFA which binds to its receptors, namely, VEGFR1 (Flt1) and VEGFR2 (Flk1) [1113]. Schumacher et al. demonstrated that VEGF signaling was reduced in Sulf1−/−; Sulf2−/− mice, indicating that both sulfatases regulate the VEGF-mediated crosstalk between podocytes and endothelial cells [13].

In a model of diabetic kidney disease using streptozotocin (STZ) in mice, typical characteristics of diabetic nephropathy including mesangial matrix accumulation and foot process effacement were present in Sulf1−/−; Sulf2−/− mice; however, WT mice having received the same STZ-treatment displayed neither mesangial matrix accumulation nor podocyte injury [1]. Takashima et al. attributed the mesangial hypercellularity and matrix expansion to the reduction of glomerular VEGF signaling in Sulf1−/−; Sulf2−/− mice, since mesangial proliferation occurs after depletion of podocyte-derived VEGF [1, 11, 12].

To further evaluate the potential role of sulf1 in proteinuric kidney disease, we used the currently published zebrafish nephrosis model using puromycin aminonucleoside (PAN) via treatment in the fish water [14]. PAN, as previously published in a rat model, causes a specific toxic injury to podocytes resembling human minimal change disease or FSGS including foot process effacement, disruption of the actin cytoskeleton, and expression changes of slit diaphragm associated proteins [14, 15].

In this study, we demonstrate that sulfatases, in particular Sulf1, are pivotal players in maintaining the integrity of the glomerular filtration barrier in zebrafish. The lack of sulfatase expression reduces the glomerular presence of Vegfa in the zebrafish pronephros and the injection of Vegfa 165 zebrafish protein can partially prevent injury to the glomerular filtration barrier after . Therefore, this study provides evidence for the relevance and potential mechanisms for the role of sulfatases, in particular Sulf1, in the regulation of glomerular integrity in zebrafish.

2. Materials and Methods

2.1. Morpholino and Protein Injection

Injections of sulf1 splice acceptor [9], sulf2a ATG blocking, sulf2b splice donor, and scrambled-control morpholinos (Gene Tools, Philomath, OR) or Vegfa 165 recombinant zebrafish protein (R&D Systems, Minneapolis, MN) into fertilized zebrafish eggs were carried out at the 1- to 2-cell stage, as previously described [16, 17]. MOs were ordered from Gene Tools (Philomath, OR) and were diluted 1:1 in injection buffer (20mmol/L HEPES, 200 mmol/L KCl, and 0.75% phenol red).

2.2. Electron Microscopy

Zebrafish larvae were fixed at 96 hpf in solution D and embedded in EPON (recipe/protocol from EMS, Hatfield, PA). Further preparation of the zebrafish embryos for TEM was carried out as stated in previously published protocols [18]. Imaging was done using a Morgagni TEM (FEI, Eindhoven, NL), operated at 80 kV.

2.3. Measurement of the Fluorescence Intensity in the Zebrafish Retinal Vessel Plexus

As a method to evaluate the integrity of the GFB, we measured a GFP-tagged vitamin D binding protein derived from Tg(l-fabp:eGFP-DBP) zebrafish in the retinal vessel plexus of the zebrafish larvae at 96 hpf, as previously described [16]. The maximum fluorescence intensity of gray-scale images of the retinal vessels was measured. The subsequent analysis was carried out with ImageJ (Version 1.48v, National Institutes of Health, Bethesda, MD) and reported in arbitrary units (AU).

2.4. PAN Model

Zebrafish eggs were collected within 30 min of spawning followed by injection with the respective morpholino or the scrambled controls as described above. Prior to treatment, the chorions were removed from the embryos manually with forceps. As described previously [14], at 46 hpf, zebrafish were treated with either 2 mg/ml or 8 mg/ml PAN, which was added into the fish medium with 1% DMSO. Until 96 hpf, zebrafish were kept in the PAN containing medium followed by the fluorescence intensity measurement in the retinal vessel plexus. DMSO added to the fish medium in the appropriate concentration served as control.

2.5. qPCR of Zebrafish Larvae

Purification of total RNAs from zebrafish larvae was done with RNeasy Plus Mini Kit (QIAGEN, Venlo, Netherlands) according to the manufacture’s protocol. Reverse transcription of 1μg RNA was done using Oligo(dT)primer (Promega, Madison, WI, USA), and Random primers (Promega, Madison, WI, USA) that were incubated at 70°C for 10 min followed by retrotranscription in M-MLV RT buffer (Promega, Madison, WI, USA), with dNTPs (Roche, Mannheim, Germany), and M-MLV reverse transcriptase (Promega, Madison, WI, USA) at 42°C for 90 min and at 70°C for 10 min. Sybr green-based qPCR was performed using the TaKaRa SYBR Premix Ex Taq™ II.

2.6. Zebrafish Immunofluorescence Staining on Paraffin Sections

Zebrafish larvae were fixed in 2% paraformaldehyde (PFA), dehydrated in ascending concentrations of ethanol (30%, 50%, 70%, 80%, 90%, and 100%) and transferred to 100% SUB-X (Leica Biosystems, Nussloch, Germany) for 4 hours before embedding in paraffin for 4 hours. After embedding in paraffin, 4 μm sections were cut on a rotational microtome (Leica RM 2245). The sections were deparaffinized in Histo-Clear tissue clearing agent for 3 x 5 min and rehydrated in a descending ethanol series (100%, 96%, 70%, 50%, and finally A. dest.). For antigen retrieval, the slides were treated with trypsin (Merck KGaA, Darmstadt, Germany) at 37°C for 8 min. After blocking, 1:25 rabbit monoclonal anti-VEGFA (Abcam, Cambridge, UK) antibody was incubated for 1 h at room temperature. Donkey anti-Rabbit IgG (H+L) antibody, Alexa Fluor 488 (Thermo Fisher Scientific, MA, USA) was used as secondary antibody for 1 h at room temperature in a 1:500 dilution. Rhodamine Wheat Germ Agglutinin (WGA) (Vector Laboratories, CA, USA) in a 1:2000 dilution was also used. Nuclei staining was performed with DAPI present in the Immunoselect Antifading Mounting Medium (Dianova, Hamburg, Germany). Images were taken with a 10x and a 63x objective on a Leica DMI6000 B microscope (Leica Biosystems, Nussloch, Germany).

2.7. Dextran Microinjection and In Vivo Confocal Imaging of the Vasculature

Tricaine (Sigma-Aldrich, Munich, Germany) was used at a concentration of 0.1–0.5% (in E3 solution) to anesthetize fish prior to microinjection and confocal microscopy. 4.6 nl of the dextran (2000kDa) labeled with tetramethylrhodamine (Invitrogen, San Diego, CA) dissolved in PBS (5mg/ml) was injected into the cardinal vein. Following the dextran injection, confocal imaging of age and size matched embryos was carried out at 48 and 72 hpf. For this, the embryos were mounted and single color z series were acquired on an Olympus Fluoview FV1000 confocal laser scanning microscope system (Olympus, Tokyo, Japan).

2.8. Statistics

The statistical analysis of data was performed using GraphPad Prism 7 software. Error bars correspond to SEM. We used one way ANOVA followed by Tukey’s multiple comparisons test or student’s t test to compare the results of each single test group. A P value of ≤0.05 was considered statistically significant. p≤0.05, p≤0.01, p≤0.001, p≤0.0001.

2.9. Animal Ethics

All animal work was performed according to the NIH Guideline for the Care and Use of Laboratory Animals. The animal protocol was approved by the MDI Biological Laboratory IACUC #17-03 and is in line with the MDIBL international assurance # D16-00341.

3. Results

3.1. Knockdown of Sulf1, Sulf2a, and Sulf2b Causes Arteriovenous Malformations

Circulatory defects as a result of reduced Sulf1 in zebrafish have been previously shown by Gorsi et al. [9]. Therefore in order to further characterize the vascular defects in larvae with reduced sulfatase expression, we performed a MO-induced knockdown of Sulf1, Sulf2a, and Sulf2b and evaluated vascular integrity following 2000 kDa dextran injection at 48 hpf in WT zebrafish or mcherry-flk expression at 72 hpf in Tg(flk:mcherry) larvae. Sulf1 morphant embryos exhibit impaired blood circulation in the tail, and an aberrant connection between caudal artery and caudal vein is present in the majority of larvae at both 48 and 72 hpf (Figures 1(a)B and 1(b)B). Sulf2a morphant larvae display a more variable phenotype and show mild to more severe disruptions in the caudal artery but also in the intersegmental vasculature of the tail at both 48 and 72 hpf (Figures 1(a)C and 1(b)C). Sulf2b morphant larvae also exhibit an impaired vascular integrity in the tail regions showing a reduced blood circulation. Analog to the Sulf2a morphants, induces damage to the intersegmental vasculature (Figures 1(a)D and 1(b)D). Scrambled morpholino injected CTRL larvae neither display an impairment of the venous or arterial blood vessels in the tail region at time point 48 nor 72 hpf (Figures 1(a)A and 1(b)A).

3.2. Knockdown of Sulf1, Sulf2a, and Sulf2b Leads to Circulatory Protein Loss, Pericardial Effusion, and Yolk Sac Edema Indicative of Renal Protein Loss

MO-induced downregulation of either Sulf1, Sulf2a, or Sulf2b causes a significant decrease in the maximum fluorescence intensity of circulating eGFP-DBP in the retinal vessel plexus of Tg(l-fabp:eGFP-DBP) larvae at 96 hpf (Figure 2(a)). A combined knockdown of the sulfs however did not further reduce the maximum fluorescence intensity in the retinal vessel plexus (Figure 2(a)). The scrambled MO injected zebrafish neither displayed a reduction of the fluorescence in comparison with noninjected zebrafish nor did they show phenotypic traits indicative of renal protein loss including pericardial effusion or yolk sac edema (Figures 2(a) and 2(b)). On the contrary, , , and larvae exhibit marked pericardial effusion and moderate yolk sac edema in addition to a mild curvature of the tail at 96 hpf (Figure 2(b)). In order to determine if there is a compensatory effect of sulf expression following MO-knockdown, morphant larvae were collected at 96 hpf and mRNA levels were assessed by qPCR. Both Sulf2a and Sulf2b mRNA show an increase after (Figure 2(c)); and Sulf1 expression is also elevated following ; however it seems that this upregulation is not sufficient to impede the development of a renal phenotype. Additionally, did not lead to a compensatory increase of either Sulf1 or Sulf2a (Figure 2(c)).

3.3. Combined Knockdown of Sulf1, Sulf2a, and Sulf2b Using TEM Reveals Loss of Glomerular Endothelial Fenestration, Thickening of the GBM, and Podocyte Foot Process Effacement

Ultrastructural analysis of the larval glomerulus by TEM showed that scrambled MO injection in Tg(l-fabp:eGFP-DBP) transgene zebrafish (CTRL) did not induce injury to the glomerular filtration barrier (Figure 3). However, caused a partial reduction of the glomerular endothelial fenestration in addition to focal podocyte foot process effacement. The knockdown of Sulf2a showed similar effects since partial foot process effacement was present. The impact of the on the endothelium was more distinct, as shown by a marked reduction in the fenestration of the endothelial cells (Figure 3). However, the most striking signs of glomerular function impairment were detected in the Sulf1, Sulf2a, and Sulf2b combined knockdown larvae. Focal thickening of the GBM was visible and fenestration of the endothelium was strongly diminished while the foot processes of the podocytes appeared focally effaced (Figure 3). These phenotypic changes indicate that a reduction in the expression of all three sulfs further impairs the morphology of the glomerulus when compared to a single .

3.4. Knockdown of Sulf1, Sulf2a, and Sulf2b Leads to Loss of Vegfa Protein Expression in the Larval Zebrafish Glomerulus

Previous work by Gorsi et al. showed that Sulf1 regulates the differentiation of the vasculature in zebrafish in a Vegfa dependent manner [9]. Since the reduction of sulfatase expression causes circulatory protein loss (Figure 2(a)), we wanted to examine whether Vegfa expression in the glomerular region of the pronephros is affected at 96 hpf after MO-induced , , and . In order to assess this, we detected the presence of Vegfa in zebrafish glomeruli after MO-knockdown; analysis of the anatomical structures was carried out by costaining with the lectin WGA which aids in the detection of membranous glycoproteins. The glomeruli of control-MO injected larvae show a strong Vegfa protein expression (Figure 4(a)). In contrast, however, knockdown of Sulf1, Sulf2a, and Sulf2b all shows a striking reduction on Vegfa expression in the larval glomerulus (Figures 4(b)4(d)). Overall these data show that Vegfa expression in the zebrafish glomerulus is dependent on the presence of the sulfatases.

3.5. Knockdown of Sulf1 Induced Circulatory Protein Loss Can Be Partially Prevented by Coinjection of Vegfa 165 Recombinant Protein

Given that Gorsi et al. were able to show that induces arteriovenous malformations in zebrafish larvae which were prevented by the coinjection of Vegfa165 and that Sulf1−/−; Sulf2−/− mice have reduced VEGF signaling [1, 9, 13], we aimed to determine whether ectopic Vegfa 165 could restore the leaky GFB in Tg(l-fabp:eGFP-DBP) larvae with reduced sulfatase expression. As stated above, diminished glomerular Vegfa expression was detected in , , and (Figure 4). Additionally, induced knockdown of the sulfatases caused a reduction in the eGFP-DBP fusion protein detected in the retinal vessel plexus, which was partially prevented in zebrafish using 100 ng/μl of Vegfa 165 recombinant zebrafish protein (Figure 5), while 1 ng/μl did not prevent fusion protein loss (Figure S1). In and larvae, the coinjection of Vegfa 165 did marginally increase the amount of circulating fluorescent protein; however this did not reach a statistical significance. This indicates that solely restoring the Vegfa presence by ectopic supplementation is not sufficient to correct the circulatory protein loss (Figures 5 and S1). Vegfa 165 injection alone did not induce a reduction of eGFP-DBP neither at 100 nor at 1ng/μl (Figures 5 and S1).

3.6. Coinjection of Vegfa165 Recombinant Zebrafish Protein Partially Prevents Yolk Sac Edema and Pericardial Effusion in Sulf1 Morphants But Not in Sulf2a and Sulf2b Morphants

To determine phenotype changes indicative of renal protein loss, we evaluated each larva at 96 hpf regarding pericardial effusion and yolk sac edema. Depending on the severity of edema and pericardial effusion, a normal appearance was scored as a P1 while most severe edema and pericardial effusion was scored as P4. Furthermore, the amount of dead fish at 96 hpf was determined. Analog to the evaluation of the eGFP-DBP in the retinal vessel plexus, ectopic Vegfa 165 expression was associated neither with edema or pericardial effusion nor with a higher mortality at 96 hpf in comparison with scrambled MO (CTRL) injected Tg(l-fabp:eGFP-DBP) fish (Figure 6(a)). The coinjection of Vegfa 165 in zebrafish did not reduce death at 96 hpf but decreased the number of larvae displaying a severe edema P4 phenotype (Figure 6(b)). Since the coinjection of Vegfa 165 did not correct the phenotype to the degree of the CTRL, only a partial prevention of edema and pericardial effusion can be attributed to ectopic Vegfa administration (Figure 6(b)). A minor reduction in the death rate at 96 hpf and a reduction of P4 larvae was detected in larvae that were coinjected with Vegfa 165 (Figure 6(b)). Vegfa 165 ectopic supplementation in fish led to a minor reduction in mortality and decreased the amount of P4 larvae at 96 hpf but did not correct the phenotype to a level comparable to the CTRL larvae (Figure 6(c)). In larvae, the coinjection of Vegfa 165 did not reduce death but slightly lowered the amount of P4 and P3 larvae (Figure 6(d)). Overall, the ectopic expression of Vegfa 165 recombinant protein only showed a tendency to slightly improve the phenotype of all sulf morphant larvae.

3.7. Knockdown of Sulf1 Induces Additional Circulatory Protein Loss in the PAN Nephrosis Model

The PAN nephrosis model is an established model in rats and zebrafish [14, 15]. PAN itself damages podocytes morphologically resembling minimal change glomerulonephritis or FSGS [15]. To determine whether reduction of sulf1 expression could function as modulator to increase the susceptibility for an impaired GFB, we used the previously published PAN nephrosis model in zebrafish larvae [14]. with a reduced MO concentration (15 μM) was not sufficient to reduce the maximum fluorescence intensity on its own, but PAN treated Tg(l-fabp:eGFP-DBP) larvae at 96 hpf showed a reduced fluorescence intensity indicating circulatory eGFP-DBP fusion protein loss (Figure 7). This implies that a reduction in Sulf1 expression may contribute to the destabilization glomerular architecture making the podocytes more susceptible to injury, as previously suggested [1].

4. Discussion

In this study we show that sulfs not only are of relevance for the development of the vasculature of zebrafish, but also play a pivotal role in the maintenance of the glomerular filtration barrier. Not only is Knockdown of Sulf1, Sulf2a, and Sulf2b causative of eGFP-DBP fusion protein loss of Tg(l-fabp:eGFP-DBP) larvae indicative of proteinuria, but also it may function as a second hit to the GFB in the PAN nephrosis model. However, since fusion protein loss cannot solely be attributed to leakage of the glomerular filtration barrier, and edema as well as pericardial effusion being rather unspecific, an ultrastructural analysis using transmission electron microcopy is necessary to determine if the protein loss occurs as a result of an impaired GFB. Electron micrographs of the glomeruli of a single sulf knockdown has shown moderate narrowing of the fenestrae between glomerular endothelial cells while mild phenotypic changes were present in the podocyte foot processes. In spite of not inducing further fusion protein loss, the sulf triple knockdown larvae compared to a single knockdown of the sulfs showed a more severe injury in particular to the endothelial cells and a more distinct thickening of the GBM in comparison with the single knockdown larvae. These phenotypic changes indicate that the fusion protein loss from the circulation occurs as a result of the impaired GFB. Furthermore, reduced Sulf1 and Sulf2a expression in zebrafish larvae was associated with a slight compensatory increase in mRNA expression of the other sulfs. These findings support the hypothesis that a combined sulf knockdown may promote a more severe glomerular impairment phenotype. Our results are consistent with previously reported ultrastructural analysis of murine kidneys which has shown that Sulf1−/−; Sulf2−/− mice present with manifold indicators of glomerular disease including thickening of the GBM, an increase of the subendothelial space while fenestrae between endothelial cells are either narrow or completely lost, and podocyte foot processes appeared effaced [1, 13]. Since the ultrastructural phenotype of Sulf-deficient mice partly resembles the glomerular injury caused by impaired VEGF signaling in humans, other groups have also aimed to investigate the role played by VEGF signaling in Sulf1−/−; Sulf2−/− mice [1, 13, 19, 20]. Here we show that in zebrafish, reduced sulf expression results in impaired Vegfa expression in the glomerulus which may be a contributing factor leading to proteinuria. Ectopic administration of Vegfa 165 also led to a partial prevention of the eGFP-DBP fusion protein loss in zebrafish larvae and showed a tendency to reduce protein loss in larvae. However, given that podocytes produce high amounts and, therefore, are responsible for maintaining the bioavailability of Vegfa for endothelial cells, even unspecific damage to the podocyte itself may reduce Vegfa signaling to endothelial cells. As an example, it has been shown that endothelial cells have significantly fewer fenestrations as a result of podocyte cell ablation induced by the use of a nitroreductase (NTR)/metronidazole (MTZ) model [18, 21, 22]. As proposed by Schumacher et al., reduction of VEGF binding to heparan sulfate may induce paracrine VEGF signaling in the glomerular endothelium [13], while a decrease in VEGFA may be causative for the narrowing of the fenestrae of the endothelial cells as demonstrated in a murine VEGFA conditional knockout model [20]. In conclusion, our results support the concept that sulfs are highly relevant for maintaining the glomerular filtration barrier and mediate this function in a VegfA dependent manner. Furthermore, our data are the first to characterize the glomerular function of the sulfs adding more insight to glomerular endothelial cell crosstalk using a zebrafish model system.

Data Availability

The datasets generated and analyzed during the current study are available from the corresponding author on reasonable request.

Conflicts of Interest

The authors declare they have no competing interests.

Authors’ Contributions

Heiko Schenk designed the experiments, performed the experiments, prepared the figures, and wrote the manuscript. Anna Masseli performed the experiments and prepared the figures. Patricia Schroder performed the experiments. Patricia Bolaños-Palmieri performed the experiments and corrected the manuscript. Michaela Beese performed the experiments. Jan Hegermann performed the experiments. Jan Hinrich Bräsen corrected the manuscript. Hermann Haller designed experiments and corrected the manuscript. Heiko Schenk and Anna Masseli have equal contribution.

Acknowledgments

We want to thank Lynne Staggs for her great technical support. Additionally, we want to thank Mario Schiffer and Ahmed Kotb for their critical comments. Furthermore, Tg(l-fabp:eGFP-DBP) zebrafish were gifts from J. Xie and B. Anand-Apte, Cleveland Clinic, Cleveland, OH. The research reported in this publication was supported by Institutional Development Awards (IDeA) from the National Institute of General Medical Sciences of the National Institutes of Health (P20GM0103423 and P20GM104318).

Supplementary Materials

Figure S1: Measurement of the maximum fluorescence intensity (AU) in the retinal vessel plexus at 96 hpf. Zebrafish embryos were injected in the yolk sac at the 1-2 cell stage with either a scrambled control (CTRL) or with sulf1 MO, sulf2a MO, or sulf2b MO and coinjected with Vegfa 165 protein. MO-induced , , and induced maximum fluorescence intensity reduction indicative of eGFP-DBP loss; however, coinjection of Vegfa 165 1 ng/μl did not prevent fusion protein loss. Primers: Primer sequences for zebrafish: hprt forward: 5’ACCAAACACTATGCGGCTG3’ and reverse: 5’GTGTCCACCCATGTCCTTCA3’. sulf1 forward: 5’AACCCACGATACAGACCTCG3’ and reverse: 5’CCCCCTCAAACTCGACTGAC3’ sulf2a forward: 5’ATTGTGAACCCACAGCGTCT3’ and reverse: 5’TTCAGTTTCTTCTTTGTGAGTGCT3’ sulf2b forward: 5’GACACCATGAGGTGCCAGAG3’ and reverse: 5’TAAAACTGTGACCCGCGACG3’. Morpholinos: sulf1: GTAGTCCTGGTAGTGGTAGAATAAT sulf2a: CCATGACCTTAACCAGTGCTCCACC sulf2b: TTCAGTCTAATTCACCTTCTCCACA CTRL scrambled: CCTCCTACCTCAGTTACAATTTATA. (Supplementary Materials)

References

  1. Y. Takashima, K. Keino-Masu, H. Yashiro et al., “Heparan sulfate 6- O -endosulfatases, Sulf1 and Sulf2, regulate glomerular integrity by modulating growth factor signaling,” American Journal of Physiology-Renal Physiology, vol. 310, no. 5, pp. F395–F408, 2016. View at: Publisher Site | Google Scholar
  2. W. C. Lamanna, M. Frese, M. Balleininger, and T. Dierks, “Sulf loss influences N-, 2-O-, and 6-O-sulfation of multiple heparan sulfate proteoglycans and modulates fibroblast growth factor signaling,” The Journal of Biological Chemistry, vol. 283, no. 41, pp. 27724–27735, 2008. View at: Publisher Site | Google Scholar
  3. S. Nagamine, M. Tamba, H. Ishimine et al., “Organ-specific sulfation patterns of heparan sulfate generated by extracellular sulfatases Sulf1 and Sulf2 in mice,” The Journal of Biological Chemistry, vol. 287, no. 12, pp. 9579–9590, 2012. View at: Publisher Site | Google Scholar
  4. S. Wang, X. Ai, S. D. Freeman et al., “QSulf1, a heparan sulfate 6-O-endosulfatase, inhibits fibroblast growth factor signaling in mesoderm induction and angiogenesis,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 101, no. 14, pp. 4833–4838, 2004. View at: Publisher Site | Google Scholar
  5. C. Ruhrberg, H. Gerhardt, M. Golding et al., “DT: Spatially restricted patterning cues provided by heparin-binding VEGF-A control blood vessel branching morphogenesis,” Genes & Development, vol. 16, pp. 2684–2698, 2002. View at: Google Scholar
  6. E. Chen, S. E. Stringer, M. A. Rusch, S. B. Selleck, and S. C. Ekker, “A unique role for 6-O sulfation modification in zebrafish vascular development,” Developmental Biology, vol. 284, no. 2, pp. 364–376, 2005. View at: Publisher Site | Google Scholar
  7. S. Ashikari-Hada, H. Habuchi, Y. Kariya, and K. Kimata, “Heparin regulates vascular endothelial growth factor165-dependent mitogenic activity, tube formation, and its receptor phosphorylation of human endothelial cells. Comparison of the effects of heparin and modified heparins,” The Journal of Biological Chemistry, vol. 280, no. 36, pp. 31508–31515, 2005. View at: Publisher Site | Google Scholar
  8. L. Jakobsson, J. Kreuger, K. Holmborn et al., “Heparan sulfate in trans potentiates VEGFR-mediated angiogenesis,” Developmental Cell, vol. 10, no. 5, pp. 625–634, 2006. View at: Publisher Site | Google Scholar
  9. B. Gorsi, F. Liu, X. Ma et al., “The heparan sulfate editing enzyme Sulf1 plays a novel role in zebrafish VegfA mediated arterial venous identity,” Angiogenesis, vol. 17, no. 1, pp. 77–91, 2014. View at: Publisher Site | Google Scholar
  10. B. Gorsi, S. Whelan, and S. E. Stringer, “Dynamic expression patterns of 6-O endosulfatases during zebrafish development suggest a subfunctionalisation event for sulf2,” Developmental Dynamics, vol. 239, no. 12, pp. 3312–3323, 2010. View at: Publisher Site | Google Scholar
  11. V. Eremina, M. Sood, J. Haigh et al., “Glomerular-specific alterations of VEGF-A expression lead to distinct congenital and acquired renal diseases,” The Journal of Clinical Investigation, vol. 111, no. 5, pp. 707–716, 2003. View at: Publisher Site | Google Scholar
  12. V. Eremina, S. Cui, H. Gerber et al., “Vascular endothelial growth factor A signaling in the podocyte-endothelial compartment is required for mesangial cell migration and survival,” Journal of the American Society of Nephrology, vol. 17, no. 3, pp. 724–735, 2006. View at: Publisher Site | Google Scholar
  13. V. A. Schumacher, U. Schlötzer-Schrehardt, S. A. Karumanchi et al., “WT1-dependent sulfatase expression maintains the normal glomerular filtration barrier,” Journal of the American Society of Nephrology, vol. 22, no. 7, pp. 1286–1296, 2011. View at: Publisher Site | Google Scholar
  14. J. Müller-Deile, H. Schenk, P. Niggemann et al., “Mutation of microphthalmia-associated transcription factor (mitf) in zebrafish sensitizes for glomerulopathy,” Biology Open, vol. 8, no. 3, 2019. View at: Google Scholar
  15. N. Guan, J. Ding, J. Deng, J. Zhang, and J. Yang, “Key molecular events in puromycin aminonucleoside nephrosis rats,” Pathology International, vol. 54, no. 9, pp. 703–711, 2004. View at: Publisher Site | Google Scholar
  16. N. Hanke, L. Staggs, P. Schroder et al., ““Zebrafishing” for novel genes relevant to the glomerular filtration barrier,” BioMed Research International, vol. 2013, Article ID 658270, 12 pages, 2013. View at: Publisher Site | Google Scholar
  17. H. Schenk, J. Müller-Deile, M. Kinast, and M. Schiffer, “Disease modeling in genetic kidney diseases: zebrafish,” Cell and Tissue Research, vol. 369, no. 1, pp. 127–141, 2017. View at: Publisher Site | Google Scholar
  18. J. Müller-Deile, H. Schenk, P. Schroder et al., “Circulating factors cause proteinuria in parabiotic zebrafish,” Kidney International, 2019. View at: Publisher Site | Google Scholar
  19. K. Uchimura, M. Morimoto-Tomita, A. Bistrup et al., “HSulf-2, an extracellular endoglucosamine-6-sulfatase, selectively mobilizes heparin-bound growth factors and chemokines: effects on VEGF, FGF-1, and SDF-1,” BMC Biochemistry, vol. 7, 2006. View at: Google Scholar
  20. V. Eremina, J. A. Jefferson, J. Kowalewska et al., “VEGF inhibition and renal thrombotic microangiopathy,” The New England Journal of Medicine, vol. 358, no. 11, pp. 1129–1136, 2008. View at: Publisher Site | Google Scholar
  21. W. Zhou and F. Hildebrandt, “Inducible podocyte injury and proteinuria in transgenic zebrafish,” Journal of the American Society of Nephrology, vol. 23, no. 6, pp. 1039–1047, 2012. View at: Publisher Site | Google Scholar
  22. F. Siegerist, A. Blumenthal, W. Zhou, K. Endlich, and N. Endlich, “Acute podocyte injury is not a stimulus for podocytes to migrate along the glomerular basement membrane in zebrafish larvae,” Scientific Reports, vol. 7, no. 1, Article ID 43655, 2017. View at: Publisher Site | Google Scholar

Copyright © 2019 Heiko Schenk et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.


More related articles

563 Views | 242 Downloads | 0 Citations
 PDF  Download Citation  Citation
 Download other formatsMore
 Order printed copiesOrder

Related articles

We are committed to sharing findings related to COVID-19 as quickly and safely as possible. Any author submitting a COVID-19 paper should notify us at help@hindawi.com to ensure their research is fast-tracked and made available on a preprint server as soon as possible. We will be providing unlimited waivers of publication charges for accepted articles related to COVID-19. Sign up here as a reviewer to help fast-track new submissions.