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Endothelial-specific depletion of TGF-β signaling affects lymphatic function

Inflammation and Regeneration volume 41, Article number: 35 (2021) Cite this article

Abstract

Background

Transforming growth factor (TGF)-β is a multifunctional cytokine involved in cell differentiation, cell proliferation, and tissue homeostasis. Although TGF-β signaling is essential for maintaining blood vessel functions, little is known about the role of TGF-β in lymphatic homeostasis.

Methods

To delineate the role of TGF-β signaling in lymphatic vessels, TβRIIfl/fl mice were crossed with Prox1-CreERT2 mice to generate TβRIIfl/fl; Prox1-CreERT2 mice. The TβRII gene in the lymphatic endothelial cells (LECs) of the conditional knockout TβRIIiΔLEC mice was selectively deleted using tamoxifen. The effects of TβRII gene deletion on embryonic lymphangiogenesis, postnatal lymphatic structure and drainage function, tumor lymphangiogenesis, and lymphatic tumor metastasis were investigated.

Results

Deficiency of LEC-specific TGF-β signaling in embryos, where lymphangiogenesis is active, caused dorsal edema with dilated lymphatic vessels at E13.5. Postnatal mice in which lymphatic vessels had already been formed displayed dilation and increased bifurcator of lymphatic vessels after tamoxifen administration. Similar dilation was also observed in tumor lymphatic vessels. The drainage of FITC-dextran, which was subcutaneously injected into the soles of the feet of the mice, was reduced in TβRIIiΔLEC mice. Furthermore, Lewis lung carcinoma cells constitutively expressing GFP (LLC-GFP) transplanted into the footpads of the mice showed reduced patellar lymph node metastasis.

Conclusion

These data suggest that TGF-β signaling in LECs maintains the structure of lymphatic vessels and lymphatic homeostasis, in addition to promoting tumor lymphatic metastasis. Therefore, suppression of TGF-β signaling in LECs might be effective in inhibiting cancer metastasis.

Background

Transforming growth factor-β (TGF-β) is a secreted dimeric protein that has pleiotropic effects and plays a key role in many cellular processes during both embryogenesis and tissue homeostasis in adults [1]. Therefore, abnormal TGF-β signaling has also been associated with various diseases, including cancer, fibrotic disorders, and cardiovascular diseases [2] [3]. The TGF-β signaling pathway is initiated through two different serine/threonine kinase receptors: type II (TβRII) and type I (TβRI; also termed activin receptor-like kinase-5 [ALK5]). In canonical TGF-β signaling, the activated receptor complex phosphorylates receptor-regulated Smads (R-Smads; i.e., Smad2 and Smad3) at two serine residues at their C-terminal to permit the phosphorylation of two R-Smads to form ternary complexes with the common partner Smad (Co-Smad), Smad4. The R-Smad/Co-Smad complex then enters the nucleus where it acts as a transcriptional factor to regulate the expression of TGF-β target genes in cell type-specific and context-dependent manners [4].

Lymphatic vessels maintain homeostasis by balancing tissue fluid throughout the body, regulating inflammation via the immune system, forming new lymphatic vessels from preexisting lymphatic vessels upon environmental stimulus, and contributing to tumor metastasis [5]. Lymphatic progenitor cells originate from the venous endothelial cells during embryonic development. The expression of the transcriptional factor Prox-1 is imperative for the development and maintenance of lymphatic endothelial cells (LECs). Prox1, a master regulator of LECs, induces the expression of vascular endothelial growth factor receptor 3 (VEGFR3) in the lymphatic progenitor cells that bud from the cardinal vein. Subsequently, the lymphatic progenitor cells form the lymph sac in a VEGF-C/VEGFR3 dependent manner. The VEGF-C/VEGFR3 pathway plays a central role in spreading the lymphatic network throughout the body [6, 7]. Although the molecular mechanisms that control lymphangiogenesis have been elucidated, little is known about the mechanisms that maintain the plasticity and stability of lymphatic vessels.

Mouse genetic studies regarding the deficiency of TGF-β signaling in fetal LECs have revealed a significant reduction in lymphatic vessel germination and remodeling in the absence of TGF-β [8]. Contrastingly, TGF-β inhibited LEC differentiation through suppression of Prox1 and LYVE-1 expression in cultured LECs. Consistently, the blockage of endogenous TGF-β signaling by a chemical inhibitor enhanced lymphangiogenesis in a mouse model of chronic peritonitis [9]. Thus, the nature of involvement of TGF-β signaling in lymphangiogenesis is still unclear.

In this study, we showed that TGF-β signaling plays a key role in maintaining the structure and function of lymphatic vessels. LEC-specific deletion of the TβRII gene results in dilation of the lymphatic lumen and impaired lymphatic drainage function. When Lewis lung carcinoma cells constitutively expressing green fluorescent protein (LLC-GFP) were implanted into mice lacking the TβRII gene in their LECs, tumor lymphatic vessels were dilated and lymphatic metastasis was suppressed. These results indicate that TGF-β signaling acts as a tumor malignant factor via lymphatic endothelial cells.

Materials and methods

Mice

TβRIIfl/fl mice [10] were crossed with Prox1-CreERT2 mice [11] to generate TβRIIfl/fl; Prox1-CreERT2 mice. Tamoxifen (Tx) (Sigma-Aldrich, St. Louis, MO T5648) dissolved in corn oil (20 mg/mL) was intraperitoneally administrated to mice (40 mg/kg/day) for consecutive 5 days into control (TβRIIfl/fl) mice and TβRIIfl/fl; Prox1-CreERT2 mice, where TβRII gene in LECs is deficient (TβRII iΔLEC). For embryonic analysis, pregnant mice were administrated with Tx (40 mg/kg/day) 10.5 and 11.5 days after mating. Then, mice were sacrificed to analyze embryos at E13.5. The lymphatic structures of adult mouse ear and tail were examined 4 weeks after the first injection of Tx. The mice were housed in the animal facilities of the Laboratory Animal Resource Center at the Tokyo University of Pharmacy and Life Sciences under specific pathogen-free (SPF) conditions at constant temperature and humidity and fed a standard diet. Treatment of the mice was in accordance with the institutional guidelines of the Animal Care and Use Program of the Tokyo University of Pharmacy and Life Sciences (L18-3, L19-18, L20-5).

Establishment LLC cells expressing eGFP

LLC cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM; Nakalai Tesuque, Kyoto, Japan) containing 10% fetal calf serum (FCS; Invitrogen, Carlsbad, CA, USA), 1× MEM nonessential amino acids (NEAA; Sigma-Aldrich) and 100 U/mL penicillin/streptomycin (FUJIFILM Wako, Osaka, Japan) [12]. To obtain the eGFP stable transformants, LLC cells were co-transfected with pEGFP-N1 (GenBank Accession #U55762) and CS-CDF-CG-PRE (RDB04379) including the Zeocin-resistant gene. For selection of stable transformants, LLC cells were maintained in DMEM containing 600 mg/mL of Zeocin (Invitrogen).

In vivo lymphatic drainage of FITC-dextran

Four weeks after Tx administration, male TβRIIfl/fl and TβRII iΔLEC mice (7-12 weeks old) were subcutaneously injected with 50 μl of 10 mg/mL FITC-dextran (MW 2,000,000, Sigma-Aldrich, FD2000S) into their rear footpads. Five minutes later, the transport of FITC-dextran was visualized with MVX10 fluorescence stereomicroscope (Olympus, Tokyo, Japan).

In vivo xenografts

Male TβRIIfl/fl and TβRII iΔLEC mice (7–12 weeks old) were subcutaneously implanted with LLCs (2.5 × 105 cells) in 100 μl of PBS. Tumor volumes (V) were calculated using the following formula: length × width × width × 0.5 [13]. The tumors were surgically removed and embedded into a frozen section compound (Leica). Lymphatic metastasis was measured by the expression of eGFP when LLC-GFP cells implanted into mouse footpad were metastasized. In brief, the legs were clarified with CUBIC 1 week after the LLC-GFP transplantation [14] and tumor metastasis to the popliteal lymph nodes (PLN) was evaluated with the fluorescent stereomicroscope (Olympus).

Immunofluorescence analysis and quantification

Antibodies were obtained from the following sources: Rabbit polyclonal anti-LYVE-1 (ab14917) and anti-Ki-67 (ab15580) antibodies from Abcam (Cambridge, UK); rat monoclonal anti-PECAM-1 (550274) and anti-VE-cadherin (550548) antibodies from BD Transduction Laboratories (Franklin Lakes, NJ); goat anti-VEGFR3 antibody (35917) from R&D systems (Minneapolis, MN). Ear skins from adult mice were dissected, fixed in 4% paraformaldehyde (PFA) in PBS for overnight at 4 °C, and washed three times with PBS. After connective tissues and hairs were removed, the samples were permeabilized in 0.1% Triton X-100 (Sigma-Aldrich) and incubated in blocking reagent (Dako, Glostrup, Denmark) before staining. The tumors and 1 cm from buttock of the tail were surgically removed and embedded into a frozen section compound (Leica). Fresh frozen sections (5 μm) were cut with a CM1850 cryostat (Leica Camera AG, Wetzlar, Germany), mounted on Cryofilm (Leica), and fixed in 100% ethanol and 4% PFA. The films were washed three times with PBS, permeabilized with 0.1% Triton X-100 for 5 min, and blocked with Blocking Reagent for 1 h at 37 °C. First antibodies in Blocking Reagent were added and incubated overnight at 4 °C. The films were washed three times with PBS and then incubated with Alexa488-conjugated donkey anti-rabbit IgG (A21206, Thermo Fisher Scientific, Waltham, MA), Alexa488-conjugated goat anti-rabbit IgG (A11008, Thermo Fisher Scientific), Alexa594-conjugated goat anti-rat IgG (A21208, Thermo Fisher Scientific) antibody, Alexa594-conjugated donkey anti-rat IgG (A21209, Thermo Fisher Scientific) antibody, or Alexa647-conjugated donkey anti-goat IgG (A11058, Thermo Fisher Scientific) at 1:200 for 1 h at room temperature [13]. After the nuclei as needed were stained with 2 μg/mL DAPI (Dojindo Laboratories, Kumamoto, Japan) for 5 min, the samples were washed three times with PBS, and the fluorescence signals were visualized by BZ-9000 fluorescence microscope (Keyence, Osaka, Japan). For mouse ear skin, the LYVE-1-positive area and the number of branches were analyzed with 12 μm2 image from each of the 4 mice used. For tumor sections, the immunostaining-positive area was measured using three independent images at 10x magnification from each mouse (3 control and 6 TβRIIiΔLEC mice). For tail sections, the immunostaining-positive area was measured using one image including tissues around the artery at × 10 magnification from each of the 4 mice. These analyses were carried out using BZ-X analyzer imaging software (Keyence) or ImageJ. The analysis of proliferative lymphatic endothelial cells from each mouse (n = 3) were measured the rate of Ki-67-positive cells from at least 100 VEGFR3-positive LECs per mouse.

RNA isolation and RT-PCR

Total RNA was extracted using a NucleoSpin® RNA Plus kit (Takara Bio Inc., Shiga, Japan). Reverse transcription was performed with a PrimeScript II 1st strand cDNA Synthesis Kit (Takara). qPCR was performed with a KAPA SYBR Fast qPCR kit (Nippon Genetics, Tokyo, Japan). All reactions were carried out on a LightCycler®96 (Roche). Each sample was analyzed in triplicate at least twice for each PCR measurement. Melting curves were checked to ensure specificity. Relative quantification of mRNA expression was calculated using the standard curve method with the GAPDH level. Before qPCR, the DNA fragment amplified using each primer set was detected to be a single band with the correct size by agarose gel electrophoresis. The following primer sets were used to amplify cDNAs; 5′-CAGCCCACCCTCAATACCAG-3′ and 5′-AGAAGGTGTTTGTGGCTGCT-3′ for mouse VEGF-C [15], 5′-TGCAGTGGCAAAGTGGAGATT-3′ and 5′-TGCCGTTGAATTTGCCGT-3′ for mouse GAPDH [16].

Statistical analysis

Numerical results were expressed as means ± standard deviation. Significance was assessed using the unequal variances t test and the chi-square test. Probability values below 0.05 were considered significant.

Results

TGF-β regulates lymphatic network development

In mouse development, the initiation of lymphatic vessel differentiation is observed at embryonic day 10–10.5 (E10–10.5) in the anterior cardinal vein with a subpopulation of endothelial cells expressing LYVE-1, Sox18, Prox1, and VEGFR3 [6] [7, 17]. To verify the effect of TGF-β signal deficiency on active lymphangiogenesis of LECs, Tx was administered to pregnant mice 10.5 and 11.5 days after mating. Next, we analyzed the phenotype of embryos at E13.5 (Fig. 1a). Mild edema and blood clots were found on the back of TβRIIiΔLEC embryos harvested from Tx-treated pregnant mice (Fig. 1b). Therefore, we visualized lymphatic vessels in the skin from their backs using the anti-LYVE-1 antibody (Fig. 1c). Interestingly, lymphatic networks with abnormally dilated lymphatic vessels were observed in the TβRIIiΔLEC embryos. These results are consistent with previous findings in which TGF-β signaling acts as an active regulator of lymphangiogenesis [9].

Fig. 1
figure 1

TβRIIiΔLEC mice exhibit embryonic edema and abnormal lymphatic vessel structure. a Treatment protocol for i.p. administration of tamoxifen (Tx). Pregnant mice were injected with Tx at E10.5 and E11.5, and embryos were analyzed at E13.5. b Gross analysis of TβRIIfl/fl; Prox1-CreERT2 (TβRIIiΔLEC), and littermate control (TβRIIfl/fl) embryos at E13.5. Mild edema (arrowhead) and blood clots (arrows) are observed in TβRIIiΔLEC pups. Scale bar: 1 mm. c. Back skin immunohistochemistry of mice embryos at E13.5 with anti-LYVE-1 (green) and anti-PECAM-1 (red) antibodies. Scale bar: 100 μm

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TβRIIiΔLEC mice injected with Tx showed expanded lymphatic vessel network

The deficiency of TGF-β signaling in lymphatic vessels was studied using the ear skin and tail 4 weeks after postnatal mice were administered with Tx (Fig. 2a). To visualize the lymphatic vessels of the mouse ear [18], the lymphatic capillary maker, LYVE-1 was detected with fluorescence. Remarkable differences in the composition of the lymphatic vessel network were observed between control (TβRIIfl/fl mice treated with Tx) and TβRIIiΔLEC mice (Fig. 2b). In adult TβRIIiΔLEC mice, the lymphatic networks exhibited distorted structures with dilated and narrowed lymphatic vessels compared to the control mice. Their dilated structures were not as remarkable as those seen during embryogenesis. Furthermore, the LYVE-1-positive area (Fig. 2c) and the number of lymphatic branches in TβRIIiΔLEC mice (Fig. 2d) were significantly increased compared to those in the control mice.

Fig. 2
figure 2

Lymphatic vessels increase in TβRIIiΔLEC mice. a. Experimental schedule. Mice were treated with i.p. tamoxifen (40 mg/kg) for five consecutive days and sacrificed at day 22 (3 weeks). The ears shown using the dotted square and the tail shown using the dotted line were analyzed. b Whole-mount LYVE-1 staining of ear skin from control and TβRIIiΔLEC mice. Representable images are shown. Scale bar: 100 μm. c. Image-based analysis of LYVE-1-positive lymphatic vessel area. The average of LYVE-1-positive area in TβRIIiΔLEC mice (n = 4) was significantly higher than that in control mice (n = 4). d Number of branching points of lymphatic vessels. The average of the branching number in TβRIIiΔLEC mice (n = 4) was significantly higher than that in control mice (n = 4). e, f Immunohistostaining of the transverse section of the mice tails with anti-LYVE-1 (green) and anti-PECAM-1 (red) (e)/VE-Cadherin (red) antibodies (f). Sections were counterstained with DAPI (nucleus, blue). Scale bar: 100 μm. g Image-based analysis of LYVE-1-positive lymphatic vessel area of Fig. 2e from control (n = 3) and TβRIIiΔLEC mice (n = 3)

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The transverse sequential sections of mouse tails were stained with antibodies against LYVE-1 and PECAM-1, which is a marker of endothelial cells, or against LYVE-1 and VE-cadherin, which is an endothelial-specific adhesion molecule. There were no differences in the vessel structure stained with anti-PECAM-1 (Fig. 2e) or anti-VE-cadherin antibodies (Fig. 2g) of mouse tails between control and TβRIIiΔLEC mice, whereas the structures of the lymphatic vessels were increased in TβRIIiΔLEC mice compared with the control mice (Fig. 2e). When we measured the area of LYVE-1-positive lymphatic capillary, LYVE-1-positive LECs in TβRIIiΔLEC mice were significantly increased compared to those in the control mice (Fig. 2g). These results suggest that TGF-β signaling might control the number of LYVE-1-positive lymphatic endothelial cells.

TβRIIiΔLEC mice treated with Tx showed expanded lymphatic vessel network

Next, we examined the lymphatic drainage function in TβRIIiΔLEC mice. It is known that any substrate injected into the hind footpad is excreted in the popliteal lymph node (PLN). Thus, we injected FITC-dextran into the footpad of TβRIIiΔLEC mice [19] 4 weeks after the administration of Tx (Fig. 3a). Five minutes later, FITC-dextran was found to be excreted in the PLN and reached the upper limbs of the control mice. On the other hand, less amount of FITC-dextran fluorescence could be observed in the lymphatic vessels upstream of the PLN around the thigh from TβRIIiΔLEC mice (Fig. 3b). FITC-dextran administrated into footpad might not be able to drain into the lymphatic vessels beyond the PLN due to impaired lymphatic function in TβRIIiΔLEC mice. We further explored lymphatic vessel dysfunction in TβRIIiΔLEC mice using a tumor lymphatic metastasis model. When LLC cells that constitutively express eGFP (LLC-GFP) were inoculated into the footpad of the mice 3 weeks after the administration of Tx (Fig. 3a), metastasis to PLN was noted 1 week after the transplantation of LLC cells (Fig. 3c). Metastasis of LLC cells was observed in 85.7% of control mice, whereas it was observed in only 27.3% of TβRIIiΔLEC mice treated with Tx, which significantly reduced compared to the control (P = 0.013; chi-square test) (Fig. 3d). Additionally, immunofluorescence staining was performed to confirm the presence of LLC-GFP cells in PLNs from wild-type mice (Fig. 3e). GFP-positive LLC cells were detected in the PLN stained with an anti-VEGFR3 antibody, demonstrating that lymphatic metastasis took place in the PLN. These results indicated that TGF-β signaling plays a key role in the maintenance of the lymphatic drainage function and that it promotes tumor lymphatic metastasis.

Fig. 3
figure 3

TβRIIiΔLEC mice exhibit decreased lymphatic drainage and tumor lymphatic metastasis. a. The mice were intraperitoneally administered Tx for five consecutive days. Three or 4 weeks later, LLC-GFP or FITC-dextran respectively were subcutaneously injected into their rear footpads independently. b Representative images of lymph flow from the lower extremities to the popliteal lymph node (PLN). (n = 7 mice per genotype) Scale bar: 5 mm. c Representative images of LLC-GFP metastasized to the PLN. Scale bar: 500 μm. d Quantification of metastasis (black) and no metastasis (white) to the PLN. Scale bar: 200 μm. (control; n = 7, TβRIIiΔLEC; n = 11) e Immunohistostaining of the sagittal section of PLN from control mice with anti-VEGFR3 (red) and anti-PECAM-1 (blue) antibodies. Green fluorescence was derived from LLC-GFP. Scale bar: 100 μm

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TβRIIiΔLEC mice treated with Tx showed dilated tumor lymphatic vessels

To investigate whether deletion of the TβRII gene in LECs affects tumor growth, TβRIIiΔLEC mice were treated with tamoxifen consecutively for 5 days before a subcutaneous injection of 2.5 × 105 LLC cells into their dorsal region. Figure 4a shows a comparison of the tumor volume between TβRIIiΔLEC and control mice 2 weeks after injection. There were no differences in tumor growth or tumor weight (Fig. 4b) between the two groups. However, accumulation of tissue fluid around tumors from TβRIIiΔLEC mice could be observed although the gross morphology of tumors between two groups was quite similar (Fig. 4c). Abundant VEGFR3-positive lymphatic vessels were observed in the tumors from TβRIIiΔLEC mice (Fig. 4d).

Fig. 4
figure 4

LEC-specific TβRII deletion does not affect tumor growth. a LLC cells were subcutaneously transplanted into Tx-treated control or TβRIIiΔLEC mice. Tumor size was measured from above the skin at the indicated days. Tumor volumes were calculated using the formula: length × width × width × 0.5. The data presented are the means ± S.D. (n = 6) b Tumor weight 15 days after LLC transplantation. (n = 6) c Appearance of xenografted tumors transplanted into control or TβRIIiΔLEC mice 15 days after LLC transplantation. TβRIIiΔLEC mice had tissue fluid accumulation around tumor (arrows). Representative images are shown. Scale bar: 5 mm. d Immunohistostaining of the tumor sections with anti-PECAM-1 (green) and anti-VEGFR3 (red) antibodies. Sections were counterstained with DAPI (nucleus, blue). Scale bar: 50 μm

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To determine the differences in blood and lymphatic vessel structures between control and TβRIIiΔLEC mice, we analyzed the sections that were stained with anti-PECAM-1 and anti-VEGFR3 antibodies for blood and lymphatic vessel structures, respectively. No differences in PECAM-1-positive area between control and TβRIIiΔLEC mice were observed in blood vessel structures (Fig. 5a), whereas the VEGFR3-positive areas were remarkably reduced in TβRIIiΔLEC mice (Fig. 5b). Additionally, lymphatic lumens in TβRIIiΔLEC mice were larger than those in the control mice (Fig. 5c), indicating upregulation of lymphangiogenesis. Inhibition of TGF-β signaling has been reported to promote lymphangiogenesis and LEC proliferation in the presence of VEGF-C. Therefore, we investigated endothelial cell growth and VEGF-C expression in the tumor tissue. Immunofluorescent staining of tumor tissues showed that Ki-67-positive lymphatic endothelial cells were increased in TβRIIiΔLEC mice (Fig. 5d, e), and the expression level of VEGF-C was significantly increased in the tumor tissue of TβRIIiΔLEC mice compared to the control mice (Fig. 5f). These data indicated that LECs in TβRIIiΔLEC mice might proliferate and form dilated lumens due to lack of TGF-β signaling under the control of VEGF-C.

Fig. 5
figure 5

LEC-specific TβRII deletion potentiates lymphangiogenesis. a–c Image-based analysis of PECAM-1-positive, VEGFR3-positive, or lymphatic lumen areas. There was no significant difference in the average of PECAM-1-positive area between TβRIIiΔLEC (n = 3) and control mice (n = 3) (a). The average of the VEGFR3-positive area (b) and the lymph lumen area surrounded by VEGFR3 (c) in TβRIIiΔLEC mice (n = 3) was significantly higher than that in control mice (n = 3). d Immunohistostaining of the tumor-derived sections used in Fig. 4 with anti-Ki-67 (green), and anti-PECAM-1 (red), and anti-VEGFR3 (purple) antibodies. Scale bar: 50 μm. e Image-based analysis of Ki-67-positive LECs (percentage of Ki-67+ cells/VEGFR3+ cells). f qPCR analysis of tumor tissue from control and TβRIIiΔLEC mice (n = 2 per genotype). Expression levels of VEGF-C gene are depicted as fold induction relative to the expression levels of control mice. The data presented are the means ± S.D. (n = 3)

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Discussion

Lymphangiogenesis is regulated by various cytokines, some of which control angiogenesis, such as vascular endothelial growth factors (VEGFs). TGF-β is not only implicated in angiogenesis and promotes blood vessel maturation [20], but also known to regulate lymphangiogenesis in a context-dependent manner [8, 9]. James et al. showed that LEC-specific deletion of the TβRII gene in embryos caused a marked decrease in lymphatic sprouting and remodeling during mouse development, when they injected Tx into pregnant dams at E12.5 and analyzed embryos at E14.5 [8]. Lymphatic progenitor cells start to bud from the cardinal vein at E10.5, and form lymph sacs at E11.5 [21]. Therefore, we administrated Tx to pregnant dams at E10.5 and E11.5 when the early stage of lymphatic differentiation and then analyzed at E13.5. Although there was not any alteration with respect to lymphatic cell differentiations from venous endothelial cell in embryos from TβRIIiΔLEC mice, we could see dilated lymphatic vessels in their embryos as reported by James et al. (Fig. 1b, c). As previously reported [20], TGF-β signaling might not be involved in the fate determination of LECs to establish lymphatic network formation. However, TGF-β signaling might play an important role in maintenance of the lymphatic vessel structure. In the mouse model for chronic peritonitis, the TGF-β kinase inhibitor increased LYVE-1-positive area [9]. They also showed lymphangiogenesis could be enhanced by VEGF-C secreted from inflammatory macrophages. The tumors from TβRIIiΔLEC mice also increased the area of VEGFR3-positive lymphatic lumen. This phenomenon might be due to the fact that LECs escaping from TGF-β signal proliferate in the presence of VEGF-C from the tumor microenvironment (Fig. 5e) [22]. Since the role of TGF-β signaling in LECs seems to be context-dependent, it would be necessary to analyze the crosstalk of TGF-β signal with other signaling pathways in future.

In this study, we used anti-LYVE-1 and anti-VEGFR3 antibodies to detect LECs (Figs. 1c and 2b, e), although there are several available antibodies that recognize lymphatic vessels. The anti-LYVE-1 antibody is useful to detect lymphatic vessel structures in fetal skin and tissue from adult mice. However, the anti-LYVE-1 antibody is not available in some cases because it can also recognize embryonic hematopoietic stem cells [23] and macrophages [24] in tumor microenvironment. Thus, we used the anti-VEGFR3 antibody in tumor tissues (Figs. 4d and 5d, Supplemental Figure 1). Podoplanin is another lymphatic specific maker [25], but it is also used as a cancer biomarker [26] (Supplementary Figure 1).

Cancer metastasis responsible for the death of patients with cancer is a hallmark of malignant tumors [27] [28]. Since cancer cells metastasize to distant organs through blood and lymphatic vessels, it is very important to understand how tumor angiogenesis and lymphangiogenesis are regulated in the human body. Tumor lymphatic vessels connect primary tumor cells and lymph nodes. Consequently, cancer cells invade the lymph nodes to move to other organs [29]. In the present study, we found that TGF-β signaling is involved in lymphatic drainage, in addition to confirming structural abnormalities of lymphatic vessels by the loss of LEC-specific TGF-β signaling. The quantitative analysis to evaluate the effect of TGF-β on lymphatic flow might be needed [30], but it is interesting that deletion of TGF-β signaling suppressed tumor lymphatic metastasis by reducing lymphatic drainage [31] (Fig. 3). TGF-β is abundant in the tumor microenvironment and enhances motility and metastasis of cancer cells. Our results suggest that the abundant TGF-β may act on lymphatic endothelial cells to promote tumor metastasis. Thus, the inhibition of TGF-β signaling by small compounds, antibodies, Fc-chimeric receptors [32], or RNA interference may block tumor metastasis via lymphatic vessels [33] [34].

Conclusions

LEC-specific TβRII knockout mice showed that TGF-β signaling promotes lymphatic drainage. Furthermore, TGF-β enhances tumor metastasis via lymphatic vessels. Therefore, blockage of TGF-β signaling might inhibit tumor metastasis targeting the lymphatic vessels.

Availability of data and materials

All data generated and/or analyzed during the current stud are available from the corresponding author on reasonable request.

Abbreviations

ALK:

Activin-like kinase

cDNA:

Complementary deoxyribonucleic acid

DMEM:

Dulbecco’s modified Eagle’s medium

GFP:

Green fluorescent protein

FCS:

Fetal calf serum

FITC-dextran:

Fluorescein isothiocyanate-dextran

LLC:

Lewis lung carcinoma

LEC:

Lymphatic endothelial cell

TGF-β:

Transforming growth factor β

VEGF:

Vascular endothelial growth factor

VEGFR:

Vascular endothelial growth factor receptor

References

  1. Morikawa M, Derynck R, Miyazono K. TGF-β and the TGF-β family: context-dependent roles in cell and tissue physiology. Cold Spring Harbor perspectives in biology. 2016;8(5). https://doi.org/10.1101/cshperspect.a021873.

  2. Gordon KJ, Blobe GC. Role of transforming growth factor-beta superfamily signaling pathways in human disease. Biochimica et biophysica acta. 2008;1782(4):197–228. https://doi.org/10.1016/j.bbadis.2008.01.006.

    CAS  Article  PubMed  Google Scholar 

  3. Goumans MJ, Ten Dijke P. TGF-β Signaling in Control of Cardiovascular Function. Cold Spring Harbor perspectives in biology. 2018;10(2). https://doi.org/10.1101/cshperspect.a022210.

  4. David CJ, Massague J. Contextual determinants of TGFbeta action in development, immunity and cancer. Nature reviews Molecular cell biology. 2018;19(7):419–35. https://doi.org/10.1038/s41580-018-0007-0.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  5. Alitalo K, Carmeliet P. Molecular mechanisms of lymphangiogenesis in health and disease. Cancer cell. 2002;1(3):219–27. https://doi.org/10.1016/S1535-6108(02)00051-X.

    CAS  Article  PubMed  Google Scholar 

  6. Escobedo N, Oliver G. Lymphangiogenesis: origin, specification, and cell fate determination. Annual review of cell and developmental biology. 2016;32(1):677–91. https://doi.org/10.1146/annurev-cellbio-111315-124944.

    CAS  Article  PubMed  Google Scholar 

  7. Oliver G, Kipnis J, Randolph GJ, Harvey NL. The lymphatic vasculature in the 21(st) century: novel functional roles in homeostasis and disease. Cell. 2020;182(2):270–96. https://doi.org/10.1016/j.cell.2020.06.039.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  8. James JM, Nalbandian A, Mukouyama YS. TGFβ signaling is required for sprouting lymphangiogenesis during lymphatic network development in the skin. Development (Cambridge, England). 2013;140(18):3903–14.

    CAS  Article  Google Scholar 

  9. Oka M, Iwata C, Suzuki HI, Kiyono K, Morishita Y, Watabe T, et al. Inhibition of endogenous TGF-beta signaling enhances lymphangiogenesis. Blood. 2008;111(9):4571–9. https://doi.org/10.1182/blood-2007-10-120337.

    CAS  Article  PubMed  Google Scholar 

  10. Levéen P, Larsson J, Ehinger M, Cilio CM, Sundler M, Sjöstrand LJ, et al. Induced disruption of the transforming growth factor beta type II receptor gene in mice causes a lethal inflammatory disorder that is transplantable. Blood. 2002;100(2):560–8. https://doi.org/10.1182/blood.V100.2.560.

    Article  PubMed  Google Scholar 

  11. Srinivasan RS, Dillard ME, Lagutin OV, Lin FJ, Tsai S, Tsai MJ, et al. Lineage tracing demonstrates the venous origin of the mammalian lymphatic vasculature. Genes & development. 2007;21(19):2422–32. https://doi.org/10.1101/gad.1588407.

    CAS  Article  Google Scholar 

  12. Furuta C, Miyamoto T, Takagi T, Noguchi Y, Kaneko J, Itoh S, et al. Transforming growth factor-beta signaling enhancement by long-term exposure to hypoxia in a tumor microenvironment composed of Lewis lung carcinoma cells. Cancer science. 2015;106(11):1524–33. https://doi.org/10.1111/cas.12773.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  13. Nagata A, Itoh F, Sasho A, Sugita K, Suzuki R, Hinata H, et al. The evolutionarily conserved deubiquitinase UBH1/UCH-L1 augments DAF7/TGF-β signaling, inhibits dauer larva formation, and enhances lung tumorigenesis. The Journal of biological chemistry. 2020;295(27):9105–20. https://doi.org/10.1074/jbc.RA119.011222.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  14. Susaki EA, Tainaka K, Perrin D, Kishino F, Tawara T, Watanabe TM, et al. Whole-brain imaging with single-cell resolution using chemical cocktails and computational analysis. Cell. 2014;157(3):726–39. https://doi.org/10.1016/j.cell.2014.03.042.

    CAS  Article  PubMed  Google Scholar 

  15. Wuest TR, Carr DJ. VEGF-A expression by HSV-1-infected cells drives corneal lymphangiogenesis. The Journal of experimental medicine. 2010;207(1):101–15. https://doi.org/10.1084/jem.20091385.

    Article  PubMed  PubMed Central  Google Scholar 

  16. Motizuki M, Isogaya K, Miyake K, Ikushima H, Kubota T, Miyazono K, et al. Oligodendrocyte transcription factor 1 (Olig1) is a Smad cofactor involved in cell motility induced by transforming growth factor-β. The Journal of biological chemistry. 2013;288(26):18911–22. https://doi.org/10.1074/jbc.M113.480996.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  17. Yang Y, García-Verdugo JM, Soriano-Navarro M, Srinivasan RS, Scallan JP, Singh MK, et al. Lymphatic endothelial progenitors bud from the cardinal vein and intersomitic vessels in mammalian embryos. Blood. 2012;120(11):2340–8. https://doi.org/10.1182/blood-2012-05-428607.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  18. Ulvmar MH, Mäkinen T. Heterogeneity in the lymphatic vascular system and its origin. Cardiovascular research. 2016;111(4):310–21. https://doi.org/10.1093/cvr/cvw175.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  19. Hirashima M, Sano K, Morisada T, Murakami K, Rossant J, Suda T. Lymphatic vessel assembly is impaired in Aspp1-deficient mouse embryos. Developmental biology. 2008;316(1):149–59. https://doi.org/10.1016/j.ydbio.2008.01.023.

    CAS  Article  PubMed  Google Scholar 

  20. Itoh F, Itoh S, Adachi T, Ichikawa K, Matsumura Y, Takagi T, et al. Smad2/Smad3 in endothelium is indispensable for vascular stability via S1PR1 and N-cadherin expressions. Blood. 2012;119(22):5320–8. https://doi.org/10.1182/blood-2011-12-395772.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  21. Yang Y, Oliver G. Development of the mammalian lymphatic vasculature. The Journal of clinical investigation. 2014;124(3):888–97. https://doi.org/10.1172/JCI71609.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  22. Greten FR, Grivennikov SI. Inflammation and cancer: triggers, mechanisms, and consequences. Immunity. 2019;51(1):27–41. https://doi.org/10.1016/j.immuni.2019.06.025.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  23. Lee LK, Ghorbanian Y, Wang W, Wang Y, Kim YJ, Weissman IL, et al. LYVE1 marks the divergence of yolk sac definitive hemogenic endothelium from the primitive erythroid lineage. Cell reports. 2016;17(9):2286–98. https://doi.org/10.1016/j.celrep.2016.10.080.

    CAS  Article  PubMed  Google Scholar 

  24. Cho CH, Koh YJ, Han J, Sung HK, Jong Lee H, Morisada T, et al. Angiogenic role of LYVE-1-positive macrophages in adipose tissue. Circulation research. 2007;100(4):e47–57. https://doi.org/10.1161/01.RES.0000259564.92792.93.

    CAS  Article  PubMed  Google Scholar 

  25. Breiteneder-Geleff S, Soleiman A, Horvat R, Amann G, Kowalski H, Kerjaschki D. Podoplanin--a specific marker for lymphatic endothelium expressed in angiosarcoma. Verhandlungen der Deutschen Gesellschaft fur Pathologie. 1999;83:270–5.

    CAS  PubMed  Google Scholar 

  26. Krishnan H, Rayes J, Miyashita T, Ishii G, Retzbach EP, Sheehan SA, et al. Podoplanin: an emerging cancer biomarker and therapeutic target. Cancer science. 2018;109(5):1292–9. https://doi.org/10.1111/cas.13580.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  27. Fares J, Fares MY, Khachfe HH, Salhab HA, Fares Y. Molecular principles of metastasis: a hallmark of cancer revisited. Signal transduction and targeted therapy. 2020;5(1):28. https://doi.org/10.1038/s41392-020-0134-x.

    Article  PubMed  PubMed Central  Google Scholar 

  28. Welch DR, Hurst DR. Defining the hallmarks of metastasis. Cancer research. 2019;79(12):3011–27. https://doi.org/10.1158/0008-5472.CAN-19-0458.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  29. Vaahtomeri K, Alitalo K. Lymphatic vessels in tumor dissemination versus immunotherapy. Cancer research. 2020;80(17):3463–5. https://doi.org/10.1158/0008-5472.CAN-20-0156.

    CAS  Article  PubMed  Google Scholar 

  30. Mohanakumar S, Telinius N, Kelly B, Lauridsen H, Boedtkjer D, Pedersen M, et al. Morphology and function of the lymphatic vasculature in patients with a fontan circulation. Circulation Cardiovascular imaging. 2019;12(4):e008074. https://doi.org/10.1161/CIRCIMAGING.118.008074.

    Article  PubMed  Google Scholar 

  31. Pickup M, Novitskiy S, Moses HL. The roles of TGFβ in the tumour microenvironment. Nature reviews Cancer. 2013;13(11):788–99. https://doi.org/10.1038/nrc3603.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  32. Takahashi K, Akatsu Y, Podyma-Inoue KA, Matsumoto T, Takahashi H, Yoshimatsu Y, et al. Targeting all transforming growth factor-β isoforms with an Fc chimeric receptor impairs tumor growth and angiogenesis of oral squamous cell cancer. The Journal of biological chemistry. 2020;295(36):12559–72. https://doi.org/10.1074/jbc.RA120.012492.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  33. Huynh LK, Hipolito CJ, Ten Dijke P. A Perspective on the Development of TGF-β Inhibitors for Cancer Treatment. Biomolecules. 2019;9(11). https://doi.org/10.3390/biom9110743.

  34. Teixeira AF, Ten Dijke P, Zhu HJ. On-target anti-TGF-β therapies are not succeeding in clinical cancer treatments: what are remaining challenges? Frontiers in cell and developmental biology. 2020;8:605. https://doi.org/10.3389/fcell.2020.00605.

    Article  PubMed  PubMed Central  Google Scholar 

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Acknowledgements

We greatly appreciate the following for kindly providing their mice: Dr. Guillermo Oliver for Prox1-CreERT2, and Dr. Stefan Karlsson for TβRIIfl/fl. We thank Mr. T. Seya and Mrs. T. Miyamoto for the technical assistance. We would like to thank Editage (www.editage.com) for English language editing.

Funding

This research was supported by the Japan Society for the Promotion of Science, Grant-in-Aid for Scientific Research (C) (17K08794 and 20K07430 to FI), and the Core-to-Core program “Cooperative International Framework in TGF-β Family Signaling” of the Japan Society for the Promotion of Science (FI, TW and SI).

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Author notes

  1. Kunpei Fukasawa and Kako Hanada contributed equally to this work.

Authors and Affiliations

  1. Laboratory of Cardiovascular Medicine, Tokyo University of Pharmacy and Life Sciences, 1432-1, Horinouchi, Hachioji, Tokyo, 1925-0392, Japan

    Kunpei Fukasawa, Kako Hanada, Kei Ichikawa, Takahiro Takagi & Fumiko Itoh

  2. Laboratory of Stem Cell Regulation, Tokyo University of Pharmacy and Life Sciences, 1432-1, Horinouchi, Hachioji, Tokyo, 1925-0392, Japan

    Kunpei Fukasawa, Kako Hanada & Fumiko Itoh

  3. Division of Pharmacology, Niigata University Graduate School of Medical and Dental Sciences, 1-757 Asahimachi-dori, Chuo-ku, Niigata, 951-8510, Japan

    Masanori Hirashima

  4. Laboratory of Biochemistry, Showa Pharmaceutical University, 3-3165, Higashi-Tamagawagakuen, Machida, Tokyo, 194-8543, Japan

    Susumu Itoh

  5. Department of Biochemistry, Graduate School of Medical and Dental Sciences, Tokyo Medical and Dental University, 1-5-45 Yushima, Bunkyo-ku, Tokyo, 113-8549, Japan

    Testuro Watabe

Authors
  1. Kunpei Fukasawa
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  8. Fumiko Itoh
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Contributions

KF, KH, KI, MH, TT, and FI conducted the in vivo and in vitro experiments and analyzed the data. MH, SI and TW took part in the interpretation of the data and discussion of the paper. FI and SI wrote the manuscript. FI, MH, SI, and TW revised the manuscript. All authors have read and approved the manuscript.

Corresponding author

Correspondence to Fumiko Itoh.

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Ethics approval and consent to participate

All experimental procedures were performed in accordance with the institutional guidelines of the Animal Care and Use Program of the Tokyo University of Pharmacy and Life Sciences (L18-3, L19-18, L20-5).

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The authors declare that they have no competing interests.

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Supplementary Information

Additional file 1: Supplementary Figure 1.

Antibodies that recognize LECs in tumor tissue. LLC cells were subcutaneously transplanted into Tx-treated control TβRIIF/F mice, and 15 days after LLC injection, fresh frozen sections were prepared. Immunohistostaining with anti-podoplanin (PDPN, green), anti-LYVE-1 (red) and anti-VEGFR3 (blue) was performed. Scale bar: 100 μm

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Fukasawa, K., Hanada, K., Ichikawa, K. et al. Endothelial-specific depletion of TGF-β signaling affects lymphatic function. Inflamm Regener 41, 35 (2021). https://doi.org/10.1186/s41232-021-00185-4

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  • DOI: https://doi.org/10.1186/s41232-021-00185-4

Keywords

  • TGF-β
  • Lymphatic vessel
  • Endothelial cell
  • Prox1
  • Tumor metastasis

Inflammation and Regeneration

ISSN: 1880-8190

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