Runx3 is a key modulator during the epithelial-mesenchymal transition of alveolar type II cells in animal models of BPD

Abstract

Bronchopulmonary dysplasia (BPD) is a major challenge for premature infants; however, the underlying mechanisms remain unclear. We previously reported that epithelial-mesenchymal transition (EMT) in alveolar type II (AT2) epithelial cells influences the normal alveolar development process. In this study, we wished to examine whether Runx3 is an important factor for BPD by regulating EMT in AT2 cells. In vivo, animal models of BPD were established by placing newborn rats in hyperoxia tanks. Lung tissue and isolated AT2 cells were collected on different days following exposure to oxygen. The pathological changes in lung tissue, alveolar development and Runx3 expression were then investigated. In vitro, RLE-6TN cells were divided into 5 groups as follows: the control, Runx3, siRunx3, transforming growth factor-β1 (TGF-β1) and Runx3 + TGF-β1 groups, and the biomarkers of EMT were investigated. In the newborn rat model of BPD, Runx3 protein and mRNA levels in both lung tissue and BPD-derived AT2 cells were significantly lower than those in the control group. The correlation between Runx3 protein expression and pulmonary development indicators was analyzed; Runx3 expression positively correlated with the radial alveolar count (RAC) and the percentage of smooth muscle actin-positive secondary septa, but negatively correlated with alveolar wall thickness. EMT was observed in the RLE-6TN cells in which the Runx3 gene was knocked down and follwoing TGF-β1-induced EMT stimulation; however, TGF-β1 failed to induce EMT in the RLE-6TN cells overexpressing Runx3. On the whole, our data indicte that low Runx3 levels may promote EMT, while high Runx3 levels inhibit TGF-β1-induced EMT. Therefore, we predict that low levels of Runx3 in BPD lung tissue may promote EMT in AT2 cells, thus affecting alveolar development.

Introduction

Bronchopulmonary dysplasia (BPD), also known as chronic lung disease (CLD), occurs primarily in premature infants. BPD has a higher morbidity in premature infants with a lower birth weight and fetal age (1). In premature infants with a birth weight <1,250 g, almost 97% also present with BPD (2). The major pathological changes associated with BPD are alveolar simplification, abnormal angiogenesis and various degrees of pulmonary fibrosis (3), which result from both injury and repair mechanisms. Alveolar simplification directly influences the effective alveolar ventilation area, as well as respiratory function. Alveolar type II (AT2) epithelial cells play an important role in the formation of alveoli during pulmonary development. AT2 cells can differentiate into alveolar type I (AT1) epithelial cells and can promote the formation of alveolar structure and the air-blood barrier, promoting normal alveolar development (4). During the normal repair process that occurs in response to pulmonary epithelial injury, AT2 cells differentiate into AT1 cells and proliferate to rebuild the air-blood barrier (5). The normal differentiation of AT2 cells into AT1 cells is essential for normal alveolar development and repair function. Previously (6), we provided evidence of epithelial-mesenchymal transition (EMT) in AT2 cells isolated from rat lung tissue from BPD model systems; we hypothesized that the development of EMT may influence both normal development, as well as the repair processes of alveoli. However, the mechanisms by which EMT occurs in BPD remain poorly understood. In this study, we explored the factors which regulate the development of EMT in AT2 cells in the context of BPD.

Runx3 is a runt domain transcription factor; its expression is closely associated with several diseases and is also a key regulator of gene expression during lung vasculogenesis (7–9). The majority of recent studies on Runx3 have focused on the role of the transcription factor in cancer metastasis; these studies have found that low levels of Runx3 can promote EMT (10), contribute to cancer metastasis (11) and can even be used as an early predictor of cancer development (12). Increased Runx3 expression in cancer cells may inhibit the production of cancer stem cells and reduce the occurrence of tumors (13). In addition, Runx3 exhibits a spatiotemporal expression during embryonic development (14) and also plays a role in pulmonary development. Lee et al (15) studied lung tissue from Runx3^−/− mice. They found that, compared with wild-type mice, Runx3^−/− mice exhibited abnormal alveolar remodeling and alveolar dysplasia 1 day after birth; in addition, they observed the co-expression of surfactant protein B (SPB), an alveolar epithelial marker and Clara cell 10 kDa protein (CC10), a bronchiolar epithelial marker in the bronchiolar epithelial cells of Runx3^−/− mice, indicating the decreased differentiation of epithelial cells. Recently, Lee et al (16) confirmed the presence of abnormal EMT in the lungs of Runx3^−/− mice.

BPD is a result of the disruption of the normal pulmonary development process; Runx3 is an important factor in such a process and can affect EMT. Our previous study (6) confirmed the presence of EMT in lung tissues of newborn rats with BPD. In this study, we wished to determine whether the decreased expression of Runx3 in BPD-affected lung tissue promotes EMT in AT2 cells, and may thus influence the normal pulmonary development process and contribute to the occurrence of BPD. Therefore, we measured Runx3 expression in lung tissues and isolated AT2 cells from the tissue of rats with BPD, and observed the effects of abnormal Runx3 expression on the occurrence of EMT in the RLE-6TN cell line in vitro. We also analyzed the correlation between Runx3 protein expression in lung tissues and pulmonary development indicators in vivo.

Materials and methods

Animal models and lung tissue preparation

Animal models of BMD were established as previously described (17). Pregnant Wistar rats with a body weight of 200–220 g were purchased from the Experimental Animal Center of China Medical University. Each pregnant Wistar rat was fed independently and gave birth naturally at 22 days of gestation. Newborn rats were randomly allocated to either the BPD model group (n=80) or the control group (n=80) within 12 h after birth. Newborn rats in the BPD model group were placed in a plexiglass oxygen tank and subjected to 95% oxygen inhalation for 1 to 21 days; an oxygen analyzer was used to continuously monitor the oxygen concentration. The tank was opened for 10 min and nursing rat dams were switched every 24 h between the hyperoxia and normoxia tanks to avoid oxygen toxicity. Newborn rats in the control group inhaled fresh air as opposed to hyperbaric oxygen; however, all other experimental conditions and control factors were the same as those for the BPD model group. Eight animals were euthanized and lung tissue was collected at each time-point (1, 3, 7, 14 and 21 days). The left lungs were fixed in 4% paraformaldehyde for hematoxylin and eosin (H&E) staining and immunofluorescence assay. The right lungs were preserved in liquid nitrogen for mRNA detection and western blot analysis. All animal procedures were evaluated and approved by the Experimental Animal Ethics Committee of China Medical University, Shenyang, China.

AT2 cell isolation and purification

Another 8 animals were euthanized and AT2 cells were isolated at each time-point (1, 3, 7, 14 and 21 days), respectively in each group. AT2 epithelial cells were isolated from the newborn rat lungs as previously described (6). The isolated AT2 cells were frozen at −80°C for real-time PCR and western blot analysis.

RLE-6TN cultures and groups

RLE-6TN cells constitute a cell line derived from rat AT2 cells that was purchased from the American Type Culture Collection (ATCC; Manassas, VA, USA). The Runx3 expression plasmid and the double-stranded siRNAs against rat Runx3 were synthesized by Shanghai Genebank Co. Lipophilic transfection reagent (Lipofectamine 2000; Invitrogen Life Technologies, Carlsbad, CA, USA) was used. Human transforming growth factor-β1 (TGF-β1)-mammalian was purchased from PeproTech, Inc. (Rocky Hill, NJ, USA).

The cells were grown on 6-well plates in Dulbecco's modified Eagle's medium (DMEM), nutrient mixture F-12 Ham supplemented with 10% fetal bovine serum (FBS), 40 mmol/l HEPES at 37°C in a humidified 5% CO₂ atmosphere (18). The cells were divided into 5 groups according to the different interventional methods as follows: the control group (untransfected RLE-6TN cell monolayer), the Runx3 group (transfected with Runx3 overexpression plasmid for 72 h), the siRunx3 group (Runx3-deficient RLE-6TN cell monolayer transfected with siRNA of Runx3 for 72 h), the TGF-β1 group (2.5 ng/ml TGF-β1 was used to treat the RLE-6TN cell monolayer followed by culture for 48 h), the Runx3 + TGF-β1 group (transfected with Runx3 overexpression plasmid for 24 h, and then 2.5 ng/ml TGF-β1 was used followed by culture for the next 48 h).

Generation of Runx3-overexpressing RLE-6TN cells

The pFlag-control and pFlag-Runx3 expression plasmids were both purchased from Genechem (Shanghai, China). Transfection with the pFlag-control and the pFlag-Runx3 plasmids into the RLE-6TN cells was carried out using Lipofectamine 2000 transfection reagent (Invitrogen Life Technologies) following the manufacturer's instructions. At 72 h after transfection, western blot analysis and real-time PCR were used, respectively for the analysis of protein and mRNA analysis. For immunofluorescence experiments, the cells were seeded on 22 mm round coverslips.

Silencing by small interfering RNA (siRNA)

Logarithmically growing RLE-6TN cells were seeded at a density of 10⁵ cells and transfected with siRNA against Runx3 using Lipofectamine (Invitrogen Life Technologies) following the manufacturer's instructions. At 72 h after transfection, lysates were prepared and analyzed by SDS-PAGE and immunoblotting, anhd real-time PCR was used for the analysis of mRNA expression. Immunofluorescence experiments were also carried out.

Stimulation of RLE-6TN cells with TGF-β1

Confluent cultures (70%) of RLE-6TN cells were maintained in serum-free medium for 24 h. The cells were stimulated with 2.5 ng/ml (100 pmol/l) TGF-β1 for the next 48 h. The collected cells after stimulation were use for mRNA detection, immunofluorescence and western blot analysis.

Runx3-overexpressing RLE-6TN cells stimulated with TGF-β1

Transfection of the pFlag-Runx3 plasmids into the RLE-6TN cells was carried out as mentioned above. Twenty-four hours later, the cells were stimulated with 2.5 ng/ml TGF-β1 for the next 48 h. The collected cells were stored at −80°C for mRNA detection and western blot analysis. For immunofluorescence experiments, the cells were seeded on 22 mm round coverslips. For ultrastructural analysis by transmission electron microscopy (TEM), the collected cells from the 5 different groups were fixed in 2.5% glutaraldehyde.

Validation of Runx3 plasmid transfection and siRNA interference effects

In order to validate the effects of Runx3 plasmid transfection and siRNA interference, we collected RLE-6TN cells at 48 and 72 h post-transfection and measured Runx3 protein and mRNA expression using western blot analysis and real-time PCR.

Analysis of Runx3 in lung tissues and isolated AT2 cells

Runx3 protein expression in lung tissues and AT2 cells was analyzed by western blot analysis. Total protein extracted from the right lung tissue or isolated AT2 cells was quantified using the BCA protein assay kit (Pierce Biotechnology. Rockford, IL, USA). Equivalent amounts of protein were separated using 10% SDS-PAGE gels and transferred onto polyvinylidene difluoride (PVDF) membranes (Millipore Billerica, MA, USA). The membranes were incubated for 1 h in 10% normal donkey serum to block non-specific binding. Next, the membranes were incubated, respectively with primary antibodies against Runx3 (1:1,000, ab49117) and β-actin (1:1,000, mouse monoclonal [ACTN05 (C4)] to actin; ab3280) (both from Abcam, Hong Kong, China) diluted in phosphate-buffered saline (PBS) incubated overnight at 4°C. The following day, after being washed in Tris-buffered saline with 1% Tween-20 (TBST), the membranes were incubated for 2 h in horseradish peroxidase-conjugated secondary antibodies (cat. nos. 31466 and 31430; Thermo Fisher Scientific, Waltham, MA, USA), then imaged by enhanced chemiluminescence reagents. ImageJ software was used to analyze the optical density of protein bands and then normalized to that of β-actin.

Real-time PCR was used to examine Runx3 mRNA expression. Total RNA was extracted from right lung lobes or isolated AT2 cells using TRIzol reagent and frozen at −80°C (Invitrogen Life Technologies, Camarillo, CA, USA) according to the manufacturer's instructions. A total of 1 µg RNA from each sample was reverse-transcribed into cDNA using SuperScript III according the manufacturer's instructions (SuperScript III; Invitrogen Life Technologies). Real-time PCR was performed on a LightCycler (7500 Fast Real-Time PCR system; Applied Biosystems, Foster City, CA, USA) using appropriate primers designed by Primer Premier 5.0 software (Premier Biosoft International, Palo Alto, CA, USA; Table I). The amplification reaction was carried as follows: 95°C for 30 sec (95°C for 5 sec, 60°C for 34 sec) 40 cycles. The relative level of mRNA expression was calculated following normalization to β-actin.

Table I.

Primers design for real-time PCR.

Names	Primer sequences	Distribution	AT (°C)	Product size (bp)	Extension time (sec)
Runx3	F: 5′-GCAACGCTTCCGCTGTCA-3′	NM_130425	60	215	34
	R: 5′-GGCTTTGGTCTGGTCCTCTATC-3′	368–582
SPC	F: 5′-GCCAGTTTCGCATTCC-3′	NM_017342	60	282	34
	R: 5′-GCTTATAGGCGGTCAGG-3′	76–357
α-SMA	F: 5′-CTTGCTAACGGAGGCG-3′	BC158550	60	160	34
	R: 5′-TCCAGAGTCCAGCACAATA-3′	366–525
E-cad	F: 5′-ACAGTCAAACGGCATCTAA-3′	NM_031334	60	190	34
	R: 5′-GGTGAAAGCTGGGAAAC-3′	388–577
N-cad	F: 5′-GACCCAGAAGATGATGTAAG-3′	NM_031333.1	60	171	34
	R: 5′-CTCAGCGTGGATAGGC-3′	2617–2787
β-actin	R: 5′-CGTGCGTGACATTAAAGAG-3′	NM_031144	60	132	34
	F: 5′-TTGCCGATAGTGATGACCT-3′	702–833

F, forward; R, reverse; SPC, surfactant protein C; α-SMA, α-smooth muscle actin; E-cad, E-cadherin; N-cad, N-cadherin.

Analysis of surfactant protein C (SPC), α-smooth muscle actin (α-SMA), E-cadherin (E-cad) and N-cadherin (N-cad) levels in RLE-6TN cells

The expression levels of proteins involved in EMT (SPC, SMA, E-cad and N-cad) in RLE-6TN cells were analyzed by western blot analysis as mentioned above. The antibody concentrations were as follows: SPC (1:100, goat polyclonal antibody; sc-7706; Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA), α-SMA (1:500, mouse monoclonal to α-SMA; ab7817; Abcam), E-cad (1:1,000, rabbit polyclonal to E-cad; GTX100443, GeneTex, Irvine, CA, USA), N-cad (1:1,000, mouse monoclonal to N-cad; ab98952; Abcam) or β-actin (1:1,000, mouse monoclonal [ACTN05 (C4)] to actin; ab3280; Abcam). ImageJ software was used to analyze the optical density of the protein bands and then normalized to that of β-actin.

The mRNA expression of SPC, α-SMA, E-cad, N-cad in the RLE-6TN cells was analyzed by real-time PCR as mentioned above. The primers and amplification conditions are shown in Table I. The relative level of mRNA expression was calculated following normalization to β-actin.

Double-label immunofluorescence assay for RLE-6TN cells

The RLE-6TN cells were cultured, respectively on glass slides in the 5 groups, fixed with 4% paraformaldehyde and permeabilized with 0.5% Triton X-100, then washed 3 times with PBS. The sections were subsequently incubated in 5% FBS for 30 min for antigen blocking. The slides were then incubated with a mixture of two primary antibodies [anti-SPC (1:100 diluted, goat poly-clonal antibody; sc-7706; Santa Cruz Biotechnology, Inc.) and α-SMA (1:100 diluted, mouse monoclonal to α-SMA; ab7817; Abcam)] at −4°C overnight. Normal goat IgG (sc-2028) or normal mouse IgG (sc-2025) (both from Santa Cruz Biotechnology, Inc.) was used respectively in place of the primary antibodies in the negative control samples. The slides were then washed 3 times with PBS and then incubated with a mixture of two secondary antibodies [anti-mouse antibody (Alexa Fluor-488, green fluorescence) and anti-goat antibody (Alexa Fluor-594, red fluorescence)] at 37°C for 60 min. Subsequently, the sections were further washed with PBS 3 times and then subjected to DAPI (1:2,000; Sigma-Aldrich, St. Louis, MO, USA) nuclear staining for 5 min. After washing thoroughly with PBS, images of the sections were acquired using a fluorescence microscope at x400 magnification.

TEM

The RLE-6TN cells collected, respectively from the 5 different groups were fixed in PBS solution (pH 7.4) containing 2.5% glutaraldehyde for 2 h, washed with PBS 3 times, post-fixed in 1% osmium tetroxide for 2 h, washed with distilled water 3 times, dehydrated with gradient ethanol and acetone, and immersed in Epon 812 overnight; the lung tissue blocks were then embedded in Epon 812 and cut into ultrathin sections (60 nm). The ultrathin sections were double-stained with uranyl acetate and aluminum citrate and cellular morphology was observed under a transmission electron microscope (Hitachi H-7650; Hitachi Co., Tokyo, Japan).

Pathology and morphometry

The left lung tissues were fixed in 4% paraformaldehyde for 24 h, dehydrated with gradient ethanol, vitrified with xylene, embedded in paraffin, cut into sections (5 µm) and stained with H&E (G1120; Solarbio Life Sciences, Beijing, China). Morphological changes were assessed using an optical microscope (x40 magnification). Ten fields were randomly selected for analysis from each section to evaluate the development of pulmonary alveoli. The radial alveolar count (RAC) developed by Emery and Mithal (19) was determined. Scion Image software (Scion Corp., Frederick, MD, USA) was used to measure alveolar wall thickness (20). Immunofluorescence assay for α-SMA in lung tissues was carried out according to our previously described methods (6). The number of branch points per millimeter squared and surface density of secondary septa were calculated by computer-assisted image analysis as previously described (21), and the percentage of SMA-positive secondary septa was calculated. Each section was evaluated by two independent pathologists who were blinded to the experimental design.

Statistical analysis

We used SPSS 11.5 software (SPSS, Inc., Chicago, IL, USA) for statistical analysis. Values are presented as the means ± standard deviation (SD); an independent-sample t-test was used to compare differences between 2 groups. One-way analysis of variance (ANOVA) was used to determine the significant difference among multiple groups. Pearson's test was applied for correlation analyses. Statistical significance was assessed at P<0.05. A P-value <0.05 was considered to indicate a statistically significant difference.

Results

Protein and mRNA expression of Runx3 in lung tissues and isolated AT2 cells

On days 1 and 3, the protein expression level of Runx3 in lung tissue did not differ significantly between the 2 groups. On day 7, Runx3 protein expression in the control group remained high, while Runx3 protein expression progressively decreased in the BPD group. On days 7, 14 and 21, the protein expression level of Runx3 in the control group was significantly higher than that in the BPD group (P<0.01) (Fig. 1A and C). Similarly, no significant difference in Runx3 mRNA expression was observed between the 2 groups on days 1 or 3, while the Runx3 mRNA expression level was significantly higher in the control group than in the BPD group on days 7, 14 and 21 (P<0.01) (Fig. 1D).

Figure 1.

Runx3 expression in lung tissues and isolated AT2 cells. (A and C) The protein expression and (D) mRNA level of Runx3 from lung tissues in the control group was significantly higher than that in THE bronchopulmonary dysplasia (BPD) group ON days 7, 14 and 21. (B and E) The protein expression and (F) mRNA level of Runx3 from isolated AT2 cells in the control group was also significantly higher than that in THE BPD group ON days 7, 14 and 21. Values are presented as THE means ± SD; ^*P<0.05, ^**P<0.01 vs. control group. D, refers to the control group; H, to the BPD group, and the digit for the number of days after birth.

In the AT2 cells isolated from primary rats at different time points, no significant differences in both Runx3 protein and mRNA expression were observed between the 2 groups on days 1 and 3. On day 7 and at later time points, the Runx3 protein expression level in the control group was markedly higher than that in the BPD group (P<0.01) (Fig. 1B and E). On days 7, 14 and 21, the Runx3 mRNA expression level in the control group was significantly greater than that in the BPD group (P<0.01) (Fig. 1F).

Effects of ectopic Runx3 expression and siRNA interference

At 48 h following transfection with the Runx3 plasmid, the increased mRNA expression of Runx3 was observed; Runx3 mRNA expression was higher at both 48 and 72 h post-transfection as compared to time 0 (P<0.01) (Fig. 2B). Similarly, the Runx3 protein expression level increased beginning at 48 h post-transfection and it was also significantly higher at 48 and 72 h post-transfection as compared to time 0 (P<0.01) (Fig. 2A and C). At 48 h following transfection of the cells with siRNA, Runx3 mRNA expression was decreased; Runx3 mRNA expression 24, 48 and 72 h post-siRNA transfection was lower than that at time 0 (P<0.01) (Fig. 2B). Similarly, the Runx3 protein expression level began to decrease beginning at 48 h post-siRNA transfection and it remained lower at 48 and 72 h post-transfection than at time 0 (P<0.01) (Fig. 2A and C).

Figure 2.

Effects of ectopic Runx3 expression and siRNA interference. (A–C) Protein and mRNA expression of Runx3 were increased at both 48 and 72 h post-transfection as compared to time 0. Runx3 mRNA and protein expression 24, 48 and 72 h post-siRNA transfection were lower than that at time 0. Values are presented as the means ± SD; ^**P<0.01 vs. time 0.

Expression of SPC, SMA, E-cad, N-cad in RLE-6TN cells

The protein expression of SPC, α-SMA, E-cad and N-cad in the 5 RLE-6TN cell groups was measured. The protein expression levels of the mesenchymal cell markers, α-SMA and N-cad, in the TGF-β1 and siRunx3 groups were significantly higher than those in the control group (P<0.01; Fig. 3A and B), while the protein expression levels of the epithelial cell markers, SPC and E-cad, were significantly lower than those in the control group (P<0.01; Fig. 3A and B). No significant differences in either the epithelial or the mesenchymal cell markers were found between the Runx3 overexpression group or the Runx3 + TGF-β1 group and the control group (Fig. 3A and B). Similarly, the mRNA expression levels of α-SMA and N-cad in the TGF-β1 group and siRunx3 group were significantly higher than those in the control group (P<0.01; Fig. 3C), while the mRNA expression levels of SPC and E-cad were significantly lower than those in control group (P<0.01; Fig. 3C). No significant differences in either the epithelial cell markers or the mesenchymal cell markers were found between the Runx3 overexpression group or the Runx3 + TGF-β1 group and the control group (Fig. 3C).

Figure 3.

(A–C) Expression of surfactant protein C (SPC), α-smooth muscle actin (α-SMA), E-cadherin (E-cad) and N-cadherin (N-cad) in RLE-6TN cells. The control group (untransfected RLE-6TN cell monolayer), Runx3 group (transfected with Runx3 overexpression plasmid for 72 h), siRunx3 group (Runx3 deficient RLE-6TN cell monolayer transfected with siRNA of Runx3 for 72 h), transforming growth factor-β1 (TGF-β1) group (2.5 ng/ml TGF-β1 was used to treat the RLE-6TN cell monolayer followed by culture for 48 h), Runx3 + TGF-β1 group (transfected by Runx3 overexpression plasmid for 24 h, then 2.5 ng/ml TGF-β1 was used and cultured for the next 48 h). Values are presented as the means ± SD; ^**P<0.01 vs. control group.

Double-label immunofluorescence assay

SPC is a specific marker of AT2 cells, while α-SMA is a marker of mesenchymal cells; their co-expression suggests EMT occurrence in RLE-6TN cells. Using two-color immunofluorescence staining we found that in both the control group and the Runx3 group, SPC was expressed in the cytoplasm (red fluorescence), while the expression of α-SMA was not detectable (green fluorescence). In the TGF-β1 group and the siRunx3 group, SPC expression was not observed, yet α-SMA expression was detectable in the cytoplasm. However, in the Runx3 + TGF-β1 group, a large amount of SPC expression and a trace amount of α-SMA expression were found (Fig. 4).

Figure 4.

Double-label immunofluorescence assay in RLE-6TN cells. Surfactant protein C (SPC), red fluorescence; α-smooth muscle actin (α-SMA), green fluorescence; nucleus, blue fluorescence. In both the control and the Runx3 groups, SPC was expressed in the cytoplasm. In the transforming growth factor-β1 (TGF-β1) group and the siRunx3 group, α-SMA expression was detectable in the cytoplasm. In the Runx3 + TGF-β1 group, a large amount of SPC expression and a trace amount of α-SMA expression were found.

Ultrastructural evidence of EMT in RLE-6TN cells

We observed the ultrastructure changes of the 5 RLE-6TN groups by TEM. The normal ultrastructure of RLE-6TN cells (microvilli on cell surface and lamellar bodies in the cells) was observed in the control group, the Runx3 group and the Runx3 + TGF-β1 group (Fig. 5A). However, in the TGF-β1 group and the siRunx3 group, there were a large number of sparse actin microfilaments and some fasciculated actin microfilaments in the cytoplasm of the RLE-6TN cells (Fig. 5B and C).

Figure 5.

Ultrastructure in RLE-6TN cells. (A) Normal ultrastructure of RLE-6TN cells, microvilli (Mv) on cell surface and lamellar bodies (LB) in the cells can be seen in the control group, the Runx3 group and the Runx3 + TGF-β1 group. All 3 groups are shown here in one image, as they all showed a normal ultrastructure of alveolar type 2 epithelial cells. (B and C) A large number of sparse actin microfilaments (white arrows) and some fasciculated actin microfilaments (black arrows) in the cytoplasm in the TGF-β1 group and the siRunx3 group.

Comparison of pulmonary development indicators

The sections were stained with H&E. Morphological changes were assessed using an optical microscope (x40 magnification; Fig. 6). On days 1 and 3, there was no significant difference in the RAC between the 2 groups; however, on days 7, 14 and 21, the RAC of the control group was significantly greater than that of the BPD group (P<0.01; Fig. 7A). On days 7, 14 and 21, the alveolar wall thickness in the BPD group was significantly greater than that in control group (P<0.01; Fig. 7B). On days 1 and 3, α-SMA expression in the lung tissues did not differ significantly between the 2 groups; α-SMA was primarily expressed at the top of secondary septa in the control group samples, but was expressed in the pulmonary mesenchyma in the BPD samples beginning on day 7. On days 7, 14 and 21 the percentage of α-SMA-positive secondary septa in the control group was markedly higher than that in the BPD group (Figs. 7C and 8).

Figure 6.

Pathology of bronchopulmonary dysplasia (BPD). From day 7, the number of alveoli and alveolar septa was significantly increased, the alveolar septa continued thinning and the number of alveoli increased in control group, while there was a decreased number of alveoli and increased alveolar wall thickness in tissues from the BPD model group.

Figure 7.

Comparison of radial alveolar count (RAC), alveolar wall thickness, the percentage of α-smooth muscle actin-positive (α-SMA⁺) secondary septa between the two groups. (A) The RAC of the control group was significantly greater than that of the bronchopulmonary dysplasia (BPD) on days 7, 14 and 21. (B) The alveolar wall thickness in the BPD group was significantly greater than that in control group on days 7, 14 and 21. (C) The percentage of α-SMA⁺ secondary septa in the control group was markedly higher than that in the BPD group on days 7, 14 and 21. ^**P<0.01 vs. control group.

Figure 8.

Immunofluorescence staining of α-smooth muscle actin (α-SMA). α-SMA (white arrows) was primarily expressed at the top of secondary septa in control group samples yet expressed in the pulmonary mesenchyma in bronchopulmonary dysplasia (BPD) samples beginning on day 7.

Analysis of the correlation between Runx3 protein expression in lung tissue and pulmonary development indicators

In the control group, the RAC gradually increased in direct correlation with the increase in Runx3 protein expression; Spearman correlation analysis revealed that Runx3 protein expression positively correlated with RAC (r=0.925, P<0.01; Fig. 9A). In the BPD group, Runx3 protein expression and RAC both decreased gradually over time; Runx3 protein expression positively correlated with RAC (r=0.427, P<0.01; Fig. 9B). In the control group, the alveolar wall became thinner with time and Spearman correlation analysis indicated that Runx3 protein expression negatively correlated with alveolar wall thickness (r=−0.95, P<0.01; Fig. 9C); by contrast, in the BPD group, the alveolar wall became thicker over time although Runx3 protein expression remained negatively correlated with alveolar wall thickness (r=−0.96, P<0.01; Fig. 9D). In the control group, Runx3 protein expression positively correlated with the percentage of α-SMA-positive secondary septa (r=−0.832, P<0.01; Fig. 9E), while in the BPD group, both Runx3 protein expression and the percentage of α-SMA-positive secondary septa in lung tissue gradually decreased over time. Spearman correlation analysis indicated that Runx3 protein expression positively correlated with the percentage of α-SMA-positive secondary septa within the BPD group (r=−0.914, P<0.01; Fig. 9F).

Figure 9.

Correlation between Runx3 protein and pulmonary development indicators. (A and B) Runx3 protein expression positively correlated with the radial alveolar count (RAC). (C and D) Runx3 protein expression negatively correlated with alveolar wall thickness. (E and F) Runx3 protein expression positively correlated with the percentage of α-smooth muscle actin-positive (α-SMA⁺) secondary septa.

Discussion

In mammals, the Runx family of transcription factors includes three genes: Runx1, 2 and 3. Each member contains a highly conserved runt domain and their gene products are similar in structure; however, each member has different biological functions and demonstrates tissue-specific expression. All Runx family members play an important role in the normal development of the body, as well as the tumor formation (22). Runx1 participates in hematopoiesis; for example, the development of leukemia is often associated with a change in the expression of Runx1 (23). Runx2 is associated with osteoporosis; changes in Runx2 expression are associated with cleidocranial dysplasia (24) and osteosarcoma (25). Runx3 is the smallest member of the Runx family and acts to inhibit tumor formation (26). Human Runx3 is located at chromosome 1p36.1 (27). Human Runx3 is 67 kb long and contains two promoters (P1 and P2) and 6 exons. Runx3 gene transcription is mainly controlled by P2 which is located at the front of exon 2 and surrounded by an obvious CpG island with a GC content of ~64% (28).

The Runx3 gene plays a regulatory role in pulmonary development (16), but also affects the occurrence of EMT (29). At E15.5d, the protein expression of Runx3 has been shown to be low in wild-type fetal rats, while at E17.5d, Runx3 protein expression in bronchioles and alveoli increases gradually until the maturation phase (15). In this study, we demonstrated that Runx3 expression in control newborn rat lung tissue was significantly increased between 7 and 21 days after birth; by contrast, Runx3 expression in newborn rat tissue from the BPD group was significantly lower than that in the control group. These data indicate that Runx3 expression in lung tissues was downregulated in the BPD group, perhaps due the abnormal pulmonary development present in this group. The suppressed Runx3 expression may also hinder normal pulmonary development of newborn rats with BPD. In order to further study Runx3 expression in AT2 cells, we isolated AT2 cells from lung tissue in two rat groups with different day ages and then measured the mRNA and protein expression of Runx3 in AT2 cells. We found that the protein and mRNA expression levels of Runx3 in BPD group were markedly lower than those in the control group on days 7, 14 and 21. Previously, we confirmed that EMT occurred in AT2 cells within the BPD group beginning at day 7 (6). Consistent with the above timeline, a decrease in Runx3 expression in AT2 cells within the BPD group also appeared beginning at day 7. Taking these data together with the finding in our previous study that Runx3 can inhibit the EMT process, we hypothesized that a low level of Runx3 in AT2 cells of BPD lung tissues may be associated with the occurrence of EMT.

EMT is a common biological phenomenon defined as the differentiation of epithelial cells into mesenchymal cells (30). During the development of EMT, the levels of epithelial cell markers (e.g., E-cadherin and occludin) gradually decrease (31), while those of mesenchymal cell markers (e.g., N-cadherin and α-SMA) (32,33) progressively increase. In order to verify the regulatory effect of Runx3 on EMT in AT2 cells, we purchased a rat alveolar type II epithelial cell line (RLE-6TN) (ATCC) for Runx3 plasmid transfection and siRNA interference to observe the effects of changes in Runx3 expression on EMT. In addition, we stimulated the RLE-6TN cell line with TGF-β1 to induce EMT and overexpressed Runx3 in RLE-6TN cells in combination with TGF-β1 to observe the effects of Runx3 on TGF-β1-induced EMT. TGF-β1 is a common stimulator used to induce EMT in epithelial cells (34). We also used it to induce EMT in RLE-6TN cells, which was characterized by a decrease in the expression of epithelial cell markers (SPC and E-cad) and an increase in the expression of mesenchymal cell markers (N-cad and α-SMA). In the present study, we found the decreased expression of SPC (an AT2 marker) and E-cad (an epithelial cell marker) and the increased expression of N-cad and α-SMA (mesenchymal cell markers) in Runx3-silent RLE-6TN cells, indicating the development of EMT. Thus, we can conclude that a decrease in Runx3 expression can directly promote the occurrence of EMT. It has been shown that a high level of TGF-β1 is present in BPD lung tissue (35). The pathological changes present in the lungs of transgenic mice overexpressing TGF-β1 are similar to those observed in BPD, which suggests that high levels of TGF-β1 can contribute to the occurrence of BPD (36). We hypothesize that high levels of TGF-β1 may be related to EMT occurrence in AT2 cells from BPD-affected lung tissue. EMT was directly induced using TGF-β1 in RLE-6TN cells cultured under normal conditions, while it was not induced by stimulating Runx3-overexpressing RLE-6TN cells with TGF-β1; specifically, epithelial cell markers were still highly expressed in the Runx3 + TGF-β1 group. This indicates that a high level of Runx3 can suppress TGF-β1-induced EMT.

Epithelial cells and mesenchymal cells have different morphologies and subcellular structures. Specific changes in subcellular structure are found during EMT in renal tubular epithelial cells (37,38); based on these findings, we hypothesized that there may also be a similar change in AT2 cells experiencing EMT. Using TEM, we observed normal ultrastructure of AT2 cells within the control group, the Runx3 overexpression group, and the Runx3 + TGF-β1 group (microvilli on cell surface and characteristic lamellar bodies in the cytoplasm). By contrast, we observed a larger number of sparse, fasciculated actin microfilaments, but no characteristic lamellar bodies in AT2 cells within the Runx3 gene knockdown group and TGF-β1 stimulation group; these data indicate that AT2 cells completely transform into mesenchymal cells via EMT. The above-mentioned findings were confirmed at the ultrastructure level as well. Therefore, we conclude that a low level of Runx3 can directly promote the occurrence of EMT, while a high level of Runx3 has an inhibitory effect on EMT.

Runx3 can directly regulate the EMT process in AT2 cells; furthermore, EMT in AT2 cells of lung tissues may influence the normal development of alveoli. In order to evaluate the association between Runx3 and alveolar development, we performed a correlation analysis of Runx3 protein expression and pulmonary development indicators at the level of lung tissue. RAC, alveolar wall thickness (39), and the percentage of α-SMA-positive secondary septa (20) are the most important indicators of alveolar development. Correlation analysis revealed that Runx3 expression positively correlated with RAC and the percentage of α-SMA-positive secondary septa, but negatively correlated with alveolar wall thickness. This study also demonstrated that in the lung tissues of the normal control group, α-SMA was mainly expressed at the top of secondary septa and the percentage of α-SMA-positive secondary septa was increased significantly from day 7 to 21 after birth. In our previous study, we found that α-SMA protein expression was sharply increased in the BPD group beginning at day 7 after birth, which was significantly greater than that in the control group (6). In this study, using immunofluorescence staining, we found that α-SMA was distributed mainly in pulmonary mesenchyma and rarely in the top of secondary septa in BPD tissues, which is similar to the α-SMA expression results obtained in a premature baboon model of BPD (40). These findings suggest that the correct localization of myofibroblasts is essential for normal pulmonary development and that increased myofibroblasts in the mesenchyma may promote the remodeling of lung tissues in BPD models.

Our study confirmed that Runx3 expression was decreased in the lung tissues of rats with BPD in vivo, that Runx3 expression closely correlated with pulmonary development indicators in vivo, and that Runx3 can promote EMT in AT2 cells in vitro. Therefore, we infer that a low level of Runx3 in lung tissues may contribute to EMT occurrence in AT2 cells and thus influence the normal pulmonary development and promote the occurrence of BPD. The following factors are considered to be associated with the decreased expression of Runx3: methylation of its promoter region (41), histone modification (42), micro-RNA regulation (43), cytoplasmic allotopic expression (44,45) and hemizygote absence (46). Further investigation into the mechanisms by which Runx3 deficiency promtes BPD is necessary and may suggest therapeutic options for the treatment of neonatal BPD.

In conclusion, this study demonstrated that Runx3 expression was decreased in BPD-affected lung tissue, and the lower Runx3, at least in part, impaired normal lung development and contributed to BPD by inducing EMT in AT2 cells. However, the mechanisms underlying the decreased expression of Runx3 in BPD warrant further investigation.

Abbreviations

BPD

bronchopulmonary dysplasia

EMT

epithelial-mesenchymal transition

AT2 cells

alveolar type II epithelial cells

RAC

radial alveolar count

α-SMA

α-smooth muscle actin

CLD

chronic lung disease

AT1 cells

alveolar type I epithelial cells

SPC

surfactant protein C

E-cad

E-cadherin

N-cad

N-cadherin

TEM

transmission electron microscope