Journal of Chemistry

Journal of Chemistry / 2019 / Article

Research Article | Open Access

Volume 2019 |Article ID 1279036 | https://doi.org/10.1155/2019/1279036

Karoline Klumpp, Frauke Lange, Alexandra S. Muscher-Banse, Nadine Schnepel, Kathrin Hansen, Adrian L. Lifschitz, Laura Mate, Mirja R. Wilkens, "Administration of Vitamin D Metabolites Affects RNA Expression of Xenobiotic Metabolising Enzymes and Function of ABC Transporters in Rats", Journal of Chemistry, vol. 2019, Article ID 1279036, 11 pages, 2019. https://doi.org/10.1155/2019/1279036

Administration of Vitamin D Metabolites Affects RNA Expression of Xenobiotic Metabolising Enzymes and Function of ABC Transporters in Rats

Academic Editor: Ciriaco Carru
Received06 Jun 2019
Accepted13 Sep 2019
Published09 Oct 2019

Abstract

From studies on different species and in cell culture systems, it has been suggested that vitamin D metabolites might affect the metabolism and elimination of xenobiotics. Although most studies performed on rodents and cell cultures report an upregulation of respective enzymes and transporters, data from the literature are inconsistent. Especially results obtained with sheep differ from these observations. As vitamin D metabolites are widely used as feed additives or therapeutics in livestock animals, we aimed to assess whether these differences indicate species-specific responses or occurred due to the very high dosages used in the rodent studies. Therefore, we applied treatment protocols to rats that had been used previously in sheep or cattle. Forty-eight female rats were divided into three treatment and corresponding placebo groups: (1) a single intraperitoneal injection of 1,25-(OH)2D3 or placebo 12 h before sacrifice; (2) daily supplementation with 25-OHD3 by oral gavage or placebo for 10 days; and (3) a single intramuscular injection of vitamin D3 10 days before sacrifice. In contrast to a previous study using sheep, treatment of rats with 1,25-dihydroxyvitamin D3 did not result in an upregulation of cytochrome P450 3A isoenzymes (CYP3A), but a decrease was found in hepatic and intestinal expressions. In addition, a downregulation of P-glycoprotein (P-gp) and breast cancer resistance protein was found in the brain. Taken together, the stimulating effects of vitamin D metabolites on the expression of genes involved in the metabolism and elimination of xenobiotics reported previously for rodents and sheep could not be reproduced. In contrast, we even observed a negative impact on the expression of CYP3A enzymes and their most important regulator, the pregnane X receptor. Most interestingly, we could demonstrate an effect of treatment with 25-hydroxyvitamin D3 and vitamin D3 on the functional activity of ileal P-glycoprotein (P-gp) using the Ussing chamber technique.

1. Introduction

Due to public interest on the potential beneficial effects not only on calcium homeostasis and bone metabolism but also on the possible prevention of diabetes, cancer, inflammatory bowel diseases, etc., vitamin D supplementation has become a common practice in many countries in recent years [1, 2]. However, as many products are sold over the counter, the dosages are often not critically determined by medical professionals. In livestock including high yielding dairy cows, high doses of vitamin D are used as a feed additive and for treatment of imbalances of mineral homeostasis [35].

Many xenobiotica are substrates of cytochrome P450 (CYP) 3A4, an enzyme that is involved in the phase I metabolism of approximately 50% of all therapeutics used in humans [6]. Absorption and excretion rates of a broad range of endogenous and exogenous hydrophobic molecules are substantially determined by the efflux transporter P-glycoprotein (P-gp). As several compounds can inhibit or induce its activity, P-gp plays a crucial role in numerous drug-drug interactions [7]. It was shown that vitamin D metabolites can be substrates of both CYP3A4 and P-gp [8, 9].

Interestingly, oral supplementation with vitamin D and UV exposure affecting endogenous synthesis of vitamin D has been reported to be associated with changes in plasma concentrations of certain therapeutics. In humans, dosage-dependent plasma concentrations of tacrolimus and sirolimus were found to be decreased in summer [10]. Both immunosuppressants are substrates of CYP 3A4 [6] and eliminated by P-gp [11]. In addition, it could be demonstrated that patients medicated with atorvastatin, a drug that is also metabolized by CYP3A4, showed lower plasma concentrations when the treatment was combined with oral vitamin D supplementation [12]. In contrast, such an interaction could not be detected in a study on intestinal absorption of the P-gp substrate digoxin [13], and the results of studies investigating these potential drug-drug interactions in cell culture systems and rodents are inconsistent too.

Human intestinal cells (Caco-2 and LS180) only express the CYP3A4 isoenzyme if 1,25-dihydroxyvitamin D3 (1,25-(OH)2D3) is added to the medium, probably mediated via the vitamin D receptor (VDR). Likewise, primary human hepatocytes respond in the same way to such a treatment although this is not found in all hepatic cell lines. It has been suggested that VDR might bind to xenobiotic-responsive elements in certain CYP promoters [1416]. An upregulation of P-gp induced by hydroxylated vitamin D metabolites as well as an increased functional activity could also be found in Caco-2 cells [17].

In rats, the isoforms CYP3A1/23, CYP3A2, CYP3A9, CYP3A18, and CYP3A62 are expressed with CYP3A9 and CYP3A62 being the most important isoforms in the intestine [1820]. Administration of 1,25-(OH)2D3 and the vitamin D analog 19nor-1,25-(OH)2D3 resulted in a transient increase in intestinal RNA expression of CYP3A9 [21]. In contrast, repeated administration had no effect on CYP3A9 intestinal RNA expression, but the expression of CYP3A1/23 and CYP3A proteins was increased [22, 23] as well as renal RNA expression of CYP3A9 [24]. In sheep, the administration of 1,25-(OH)2D3 led to a pronounced stimulation of both renal and intestinal CYP3A24 [25], the ovine gene orthologous to human CYP3A4 [26]. Expression and activity of intestinal P-gp were not altered in 1,25-(OH)2D3-treated rats [27], while in sheep, hepatic and intestinal expressions were even slightly decreased after oral supplementation with 25-hydroxyvitamin D (25-OHD3) [25]. Results on hepatic P-gp expression in rats were inconsistent with different dosages [22], whereas in the kidney and brain of mice, expression and activity of P-gp were stimulated [28].

To investigate whether the observed discrepancies are species differences or are the result of the very high dosages used repeatedly in rodents, we applied treatment protocols to rats that had been used before in sheep or cattle: 0.5 μg 1,25-(OH)2D3 per kg body weight (BW) intravenously 12 hours before sacrifice, 6 μg 25-hydroxyvitamin D3 (25-OHD3) per kg BW per os daily for 10 days, and 300 μg vitamin D3 per kg BW intramuscularly once 10 days before sacrifice. After sampling, we investigated RNA expression of genes involved in calcium absorption and vitamin D metabolism: VDR, pregnane X receptor (PXR), different CYP3A enzymes, P-gp, and breast cancer resistance protein (BCRP) as well as the functional activity of ileal P-gp.

2. Materials and Methods

2.1. Animals, Treatments, and Sampling

The protocols of the animal treatment were approved by the Lower Saxony State Office for Consumer Protection and Food Safety (33.12-42502-04-15/1995) and their conduct supervised by the Animal Welfare Commissioner of the University of Veterinary Medicine Hannover in accordance with the German Animal Welfare Law.

In the current study, 48 female Sprague Dawley rats aged 8 to 11 weeks (body weight 10 days before sacrifice: 220 ± 7.0 g) were kept on a standard chow (ssniff Spezialdiäten GmbH, Soest, Germany) fed ad libitum and maintained under a 12 : 12-hour light and dark cycle. The animals were divided into three treatment and corresponding placebo groups: (1) a single intraperitoneal injection of 1,25-(OH)2D3 (N = 9, 0.5 μg/kg body weight, Decostriol®, mibe GmbH Arzneimittel, Brehna, Germany) or placebo (N = 7) 12 h before sacrifice; (2) daily supplementation with 25-OHD3 by oral gavage (N = 8, 6 μg/kg body weight, Dedrogyl®, Desma GmbH, Mainz-Kastel, Germany, diluted with tap water to a total volume of 1 ml) or placebo (N = 8, 1 ml of tap water with addition of propylene glycole, the nonpharmacological compound of Dedrogyl®) for 10 days; and (3) a single intramuscular injection of vitamin D3 (N = 8, 300 μg/kg body weight, D3-Vicotrat®, Heyl Chemisch-pharmazeutische Fabrik GmbH & Co. KG, Berlin, Germany) or placebo (N = 8) 10 days before sacrifice.

The animals were anesthetized by exposure to carbon dioxide and sacrificed immediately by exsanguination via cardiac puncture. Serum samples were prepared and stored at −20°C. Tissues for the isolation of RNA were collected within 10 min postmortem and rinsed with ice-cold saline (0.9%). The small intestinal epithelia (proximal jejunum and distal jejunum/ileum, the latter one refers to the segment directly proximal from that used for the Ussing chamber experiments) was scraped from the underlying submucosal and muscle layers with a glass slide. The tissues were frozen in liquid nitrogen and stored at −80°C until analysis. For the Ussing chamber experiments, the ileum was opened along the mesenteric line, rinsed with ice-cold 0.9% (w/v) saline, and kept in ice-cold buffer solution (113.6 mM NaCl, 5.4 mM KCl, 1.2 mM CaCl2, 1.2 mM MgCl2, 0.2 mM HCl, 0.6 mM NaH2PO4, 2.4 mM Na2HPO4, 21.0 mM NaHCO3, 10 mM glucose, and 19.8 mM mannitol) aerated with carbogen. Serosal and muscle layers were peeled off carefully using forceps, and the epithelia were mounted in the chambers within 30 min after sacrifice.

2.2. Plasma Analyses

Serum was analyzed for total calcium colorimetrically by the o-cresolphthalein complexone method [29]. Intra- and interassay coefficients in our laboratory are 5.09% and 6.88%. A commercial ELISA (25(OH)-Vitamin D direct day ELISA®, Immundiagnostik AG, Bensheim, Germany) was used to determine serum 25-OHD concentrations. Intra- and interassay coefficients in our laboratory and sensitivities are 10.1%, 13.4%, and 6.08 ng/ml. According to the manufacturer, cross-reactivity with other vitamin D metabolites compared to 25-OHD3 is 67.8% for 25-OHD2 and 100% for 24,25-(OH)2D3.

Measurement of serum concentrations of 1,25-(OH)2D was carried out by a commercial diagnostic laboratory using a competitive ELISA following solvent extraction (1,25-(OH)2-Vitamin D ELISA®, Immundiagnostik AG, Bensheim, Germany). Intra- and interassay coefficients and sensitivities documented and provided by the laboratory are 6.69%, 9.00%, and 4.80 pg/ml. Cross-reactivity with 1,25-(OH)2D2 compared to 1,25-(OH)2D3 is declared to be 41%.

2.3. Quantification of RNA Expression

Total RNA was isolated using the RNeasy plus Mini Kit (Qiagen, Hilden, Germany) with genomic DNA eliminator spin columns in accordance with the manufacturer’s protocol. Concentration and quality of the RNA were determined by UV absorbance, and 200 ng was reverse transcribed using random hexamer primers and TaqMan-reverse-transcription reagents (Applied Biosystems, Darmstadt, Germany).

RNA expression of β-actin, TRPV6 (transient receptor potential vanilloid type 6), CaBP-D9K (calbindin-D9K), PMCA1b (plasma membrane calcium ATPase 1b), CYP27B1 (cytochrome P450 27B1, 1α-hydroxylase), CYP24A1 (24-hydroxylase), VDR (vitamin D receptor) and PXR (pregnane X receptor), CYP3A9, CYP3A18, CYP3A62, MDR1a, and MDR1b (ABCB1, P-gp, P-glycoprotein), and BCRP (ABCG2, breast cancer resistance protein) was determined using SYBR Green® PCR assays. Specific primers (Table 1) were purchased from Life Technologies (Darmstadt, Germany). Reaction mixtures (20 μl) contained KAPA SYBR FAST Universal Master Mix (PEQLAB Biotechnologie GmbH, Erlangen, Germany), specific primers (200 nM), and 16 ng reverse transcribed RNA. PCR products were amplified (95°C, 3 min; 40 cycles of 95°C, 10 s; and 60°C, 30 s) and detected on a real-time PCR cycler (CFX96TM, Bio-Rad, Munich, Germany). The thermal profile for melt curve determination began with an incubation of 10 min at 55°C with a gradual increase in temperature (0.5°C/10 s) to 95°C.


Gene and sourceSequenceProduct size

GAPDH
NM_017008.4
for 5′-TTGTCAGCAATGCATCCTGC-3′
rev 5′-CGGCATGTCAGATCCACAAC-3′
Probe: 5′-6FAM-TGGCCCCTCTGGAAAGCTGTGGCG-BBQ
307
β-actin
[30]
for 5′-AAGTCCCTCACCCTCCCAAAAG-3′
rev 5′-AAGCAATGCTGTCACCTTCCC-3′
97
BRCP
XM_006236573.3
for 5′-AGTCCGGAAAACAGCTGAGA-3′
rev 5′-CAAGATGACGTTGTGATGGG-3′
235
CaBP-D9K
NM_012521.2
for 5′-TGAGCGCTAAGAAATCTCCCG-3′
rev 5′-GCTGGGGAACTCTGACTGAAT-3′
125
CYP3A9
NM_147206.2
for 5′-CCTGGCTGCTCCTGGTTATC-3′
rev 5′-AAAGGTTTGGGCCCAGGAAT-3′
100
CYP3A18
NM_145782.1
for 5′-CTACGGTGATGGCATGTGGA-3′
rev 5′-CATTGGCCCAAAACACCGAC-3′
178
CYP3A62
NM_001024232.1
for 5′-TCTTGCATACCGCCATGGAT-3′
rev 5′-AAAGCTCCGACGGTTTGTGA-3′
175
CYP24A1
NM_201635.2
for 5′-CTCGGACCCTTGACAAACCA-3′
rev 5′-CCGAATGGGAGATGAGCGAA-3′
184
CYP27B1
NM_053763.1
for 5′-TACCCCTGCTAAAGGCTGTGA-3′
rev 5′-GAGTTGGGTTCCCGAAACTGG-3′
181
MDR1a
NM_133401.1
for 5′-TCTGGCGGCCATTATCCAT-3′
rev 5′-TCATACTACGGTTGTTTCCTACATTTG-3′
101
MDR1b
NM_012623.2
for 5′-TGAATCCCAAAGTGACACTGGT-3′
rev 5′-ATACTTCTGCGAATTGATCTCCTTATT-3′
87
PMCA1b
NM_053311.1
for 5′-AATGCTTTCCAGAGTGGAGGT-3′
rev 5′-TCGGATACCCCACAGGAGT-3′
148
PXR
NM_052980.2
for 5′-GCGTCATCAACTTCGCCAAA-3′
rev 5′-TTCTGGAAGCCGCCATTAGG-3′
193
TRPV6
NM_053686.1
for 5′-GAGCACAGGTTGTGGCTACT-3′
rev 5′-TCCACCCTCAAGAACCAGCG-3′
122
VDR
[24]
for 5′-ACAGTCTGAGGCCCAAGCTA-3′
rev 5′-TCCCTGAAGTCAGCGTAGGT-3′
103

Expression of GAPDH (glyceraldehyde 3-phosphate dehydrogenase) was determined using gene-specific TaqMan® primers and probes (TIB Molbiol GmbH, Berlin, Germany). Reaction mixtures (20 μl) contained TaqMan® Universal PCR Master Mix (Thermo Fisher, Darmstadt, Germany), 50 pM specific primers, 25 pM specific probe, and 16 ng reverse-transcribed RNA. PCR products were amplified as follows: 50°C, 2 min; 95°C, 10 min; 40 cycles of 95°C, 15 s; and 60°C, 1 min.

Absolute copy numbers were determined using calibration curves generated with cloned PCR fragment standards as described elsewhere [31]. Efficiency of the PCR assays tested in advance for dilutions of cDNA and cloned standard ranged from 85 to 105%. Specificity of the amplicons was verified using NCBI Blast (http://blast.ncbi.nlm.nih.gov/Blast.cgi). Parallel PCR assays for each gene target were performed with cDNA samples, genomic standards, and a no-template control with water. Expression of target genes was normalized using the expression of GAPDH or β-actin as stable expressed reference genes during treatments. Each series of experiments was carried out twice.

2.4. Using Chamber Experiments

For each ileum, six pieces of tissue were mounted between the two halves of incubation chambers with an exposed area of 0.50 cm2. Thereby, the Ussing chambers were separated in a serosal and a mucosal compartment each connected to circulation reservoirs filled with respective buffer solutions (113.6 mM NaCl, 5.4 mM KCl, 1.2 mM CaCl2, 1.2 mM MgCl2, 0.2 mM HCl, 0.6 mM NaH2PO4, 2.4 mM Na2HPO4, 21.0 mM NaHCO3, 10 mM glucose, and 19.8 mM mannitol) which were maintained at 38°C by water jackets and continuously stirred and aerated with carbogen by a gas lift system. A computer-controlled voltage clamp device (Mussler Scientific Instruments, Aachen, Germany) was used to determine tissue conductance (Gt) and transepithelial potential difference (PDt) with reference to the mucosal side. All experiments were carried out under open-circuit current conditions.

Activity of P-gp was determined by the use of rhodamine-123 (Sigma-Aldrich Chemie GmbH, Schnelldorf, Germany) that was added to a final concentration of 26 μM either to the serosal (four chambers per animal) or to the mucosal side of the tissue (two chambers per animal). Two of the four chambers with the serosal side as donor compartment were additionally provided with 100 μM verapamil (Sigma-Aldrich Chemie GmbH, Schnelldorf, Germany) to inhibit P-gp-mediated transport of rhodamine-123. After an equilibration period of 30 min, six samples of 400 μl each were taken at intervals of 30 min and this volume was immediately replaced by 400 μl of the respective buffer solution. The concentration of rhodamine-123 in the acceptor compartment was measured at 485 nm (extinction) and 520 nm (emission), calculated by interpolation from a standard curve and corrected cumulatively for the previously removed samples (Infinite M200, Tecan GmbH, Crailsheim, Germany). The secretory response of the intestinal segments to forskolin (10 μM, added to the serosal side, Sigma-Aldrich Chemie GmbH, Schnelldorf, Germany) represented by the increase in PDt served as a parameter to survey the viability of the epithelium at the end of the experiments.

2.5. Statistical Analyses and Presentation of Data

As all approaches included a placebo treatment administered through the same route, results on RNA expression were compared by Student’s t test for unpaired observations for each treatment versus the respective control (; ; ). Data are presented in relation to the corresponding control group. A second-order polynomial model could be calculated for rhodamine-123 net increase over time. In addition, results were compared by 2-way ANOVA for repeated measures (time, treatment, and interaction) followed by Bonferroni’s posttest. All statistical analyses including the linear regression analyses were done using GraphPad Prism Version 6.00 (GraphPad Software, San Diego, California, USA).

3. Results

3.1. Body Weight and Serum Parameters

All animals were clinically healthy during the study. Body weight and serum parameters at sacrifice are presented in Table 2. Body weight was not affected. Treatment with 1,25-(OH)2D3 resulted in significantly greater serum concentrations of 1,25-(OH)2D3 () and total calcium (), while administration of 25-OHD3 and vitamin D3 only increased serum concentrations of 25-OHD3 (; ).


1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

Body weight (g)254 ± 7.74
(241 ± 6.17)
263 ± 4.62
(258 ± 10.2)
246 ± 6.10
(247 ± 7.30)
25-OHD3(ng/ml)32.0 ± 4.02
(23.1 ± 3.88)
87.9 ± 12.0
(25.6 ± 1.80)
154.2 ± 14.2
(31.5 ± 4.73)
1,25-(OH)2D3 (pg/ml)237.6 ± 21.2
(37.4 ± 7.61)
27.0 ± 3.32
(39.3 ± 7.37)
27.1 ± 1.78
(30.9 ± 3.51)
Total calcium (mM)2.85 ± 0.03
(2.68 ± 0.03)
2.71 ± 0.02
(2.70 ± 0.03)
2.64 ± 0.03
(2.69 ± 0.03)

Mean ± SEM of respective control groups are given in brackets; asterisks indicate significant differences between treatment and control groups; , .
3.2. RNA Expression

RNA expression of genes involved in vitamin D metabolism, transepithelial calcium transport, metabolism, and elimination of xenobiotics as well as nuclear receptors is given in Tables 37.


1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

TRPV60.879 ± 0.142
(1 ± 0.08)
1.187 ± 0.267
(1 ± 0.148)
1.741 ± 0.938
(1 ± 0.161)
CaBP-D9K4.773 ± 0.418
(1 ± 0.231)
0.469 ± 0.185
(1 ± 0.342)
0.437 ± 0.076
(1 ± 0.480)
PMCA1b0.790 ± 0.082
(1 ± 0.0731)´
1.054 ± 0.156
(1 ± 0.061)
1.019 ± 0.286
(1 ± 0.283)
VDR1.118 ± 0.107
(1 ± 0.254)
1.489 ± 0.362
(1 ± 0.148)
2.630 ± 1.682
(1 ± 0.113)
PXR1.350 ± 0.165
(1 ± 0.150)
1.430 ± 0.271
(1 ± 0.122)
0.958 ± 0.087
(1 ± 0.080)
CYP3A90.756 ± 0.130
(1 ± 0.148)
1.219 ± 0.125
(1 ± 0.207)
1.056 ± 0.219
(1 ± 0.162)
CYP3A180.936 ± 0.108
(1 ± 0.169)
1.339 ± 0.162
(1 ± 0.091)
1.226 ± 0.203
(1 ± 0.095)
CYP3A620.907 ± 0.130
(1 ± 0.123)
1.163 ± 0.139
(1 ± 0.120)
1.049 ± 0.198
(1 ± 0.144)
MDR1a1.154 ± 0.150
(1 ± 0.252)
1.723 ± 0.393
(1 ± 0.151)
1.174 ± 0.168
(1 ± 0.193)

Means ± SEM of respective control groups set to 1 are given in brackets; asterisks indicate significant differences between treatment and control groups; .

1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

VDR0.976 ± 0.061
(1 ± 0.073)
0.732 ± 0.060
(1 ± 0.350)
1.027 ± 0.068
(1 ± 0.089)
PXR0.991 ± 0.083
(1 ± 0.128)
1.163 ± 0.083
(1 ± 0.131)
1.178 ± 0.105
(1 ± 0.086)
CYP3A90.607 ± 0.088
(1 ± 0.055)
1.546 ± 0.222
(1 ± 0.185)
1.096 ± 0.162
(1 ± 0.170)
CYP3A180.763 ± 0.126
(1 ± 0.082)
1.061 ± 0.113
(1 ± 0.160)
1.381 ± 0.239
(1 ± 0.170)
CYP3A620.775 ± 0.082
(1 ± 0.064)
1.302 ± 0.105
(1 ± 0.146)
0.838 ± 0.074
(1 ± 0.138)
MDR1a1.089 ± 0.071
(1 ± 0.074)
1.299 ± 0.191
(1 ± 0.159)
1.058 ± 0.160
(1 ± 0.242)

Mean ± SEM of respective control groups set to 1 are given in brackets; asterisks indicate significant differences between treatment and control groups; .

1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

VDR1.488 ± 0.135
(1 ± 0.066)
0.833 ± 0.076
(1 ± 0.072)
0.775 ± 0.075
(1 ± 0.089)
PXR0.804 ± 0.063
(1 ± 0.048)
0.905 ± 0.082
(1 ± 0.075)
0.729 ± 0.092
(1 ± 0.068)
CYP24A132.28 ± 5.041
(1 ± 0.276)
1.292 ± 0.464
(1 ± 0.464)
1.958 ± 0.530
(1 ± 0.202)
CYP27B10.187 ± 0.026
(1 ± 0.152)
1.034 ± 0.264
(1 ± 0.368)
0.429 ± 0.104
(1 ± 0.558)
MDR1a1.240 ± 0.078
(1 ± 0.082)
1.295 ± 0.142
(1 ± 0.147)
0.653 ± 0.065
(1 ± 0.345)
MDR1b0.915 ± 0.147
(1 ± 0.253)
1.227 ± 0.366
(1 ± 0.205)
1.193 ± 0.291
(1 ± 0.157)

Means ± SEM of respective control groups set to 1 are given in brackets; asterisks indicate significant differences between treatment and control groups; , .

1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

VDR1.398 ± 0.198
(1 ± 0.092)
1.014 ± 0.204
(1 ± 0.184)
1.000 ± 0.190
(1 ± 0.198)
PXR0.666 ± 0.096
(1 ± 0.120)
0.889 ± 0.137
(1 ± 0.211)
0.950 ± 0.094
(1 ± 0.161)
CYP3A91.157 ± 0.235
(1 ± 0.196)
0.983 ± 0.064
(1 ± 0.122)
1.223 ± 0.119
(1 ± 0.104)
CYP3A180.661 ± 0.094
(1 ± 0.097)
0.789 ± 0.071
(1 ± 0.118)
1.115 ± 0.175
(1 ± 0.074)
CYP3A621.087 ± 0.183
(1 ± 0.084)
0.875 ± 0.089
(1 ± 0.135)
1.166 ± 0.119
(1 ± 0.062)
MDR1a0.828 ± 0.099
(1 ± 0.139)
0.946 ± 0.107
(1 ± 0.102)
1.218 ± 0.149
(1 ± 0.158)
MDR1b1.398 ± 0.254
(1 ± 0.222)
0.813 ± 0.097
(1 ± 0.230)
1.437 ± 0.256
(1 ± 0.152)

Means ± SEM of respective control groups set to 1 are given in brackets; asterisks indicate significant differences between treatment and control groups; .

1,25-(OH)2D3
(0.5 μg/kg body weight, administered intraperitoneally once, 12 h before sacrifice)
25-OHD3
(6 μg/kg body weight, administered daily by oral gavage for 10 days)
Vitamin D3
(300 μg/kg body weight, administered intramuscularly, once 10 days before sacrifice)

VDR0.853 ± 0.051
(1 ± 0.193)
0.983 ± 0.054
(1 ± 0.111)
0.950 ± 0.073
(1 ± 0.106)
PXR2.128 ± 0.992#
(1 ± 0.216)
1.045 ± 0.045
(1 ± 0.115)
1.710 ± 0.656
(1 ± 0.168)
BCRP0.703 ± 0.072
(1 ± 0.071)
1.145 ± 0.107
(1 ± 0.125)
1.371 ± 0.183
(1 ± 0.095)
MDR1a0.719 ± 0.052
(1 ± 0.065)
0.971 ± 0.066
(1 ± 0.070)
1.045 ± 0.084
(1 ± 0.068)
MDR1b0.975 ± 0.109
(1 ± 0.209)
1.027 ± 0.162
(1 ± 0.171)
1.187 ± 0.170
(1 ± 0.137)

Means ± SEM of respective control groups set to 1 are given in brackets; asterisks indicate significant differences between treatment and control groups; #P = 0.053, , and .

Only intraperitoneal administration of 1,25-(OH)2D3 resulted in a significant downregulation of the renal CYP27B1 (, Table 5), while the renal CYP24A1 (, Table 5), renal VDR (, Table 5), and the intestinal calcium transport protein CaBPD9K were significantly upregulated (, Table 3). In addition, the treatment increased the RNA expression of PXR in the brain by trend (, Table 7) and decreased the RNA expression of hepatic PXR (, Table 6) and CYP3A18 (, Table 6), renal PXR (, Table 5), and intestinal CYP3A9 (, Table 4). RNA expression of both efflux transporters investigated, MDR1a and BCRP, and was significantly decreased in the brain (; , Table 7).

While intramuscular treatment with vitamin D3 only exerted a decreasing effect on renal PXR (, Table 5), oral supplementation with 25-OHD3 did not affect any of the genes investigated.

Regression analyses revealed linear correlations between the expression of PXR and CYP3A18 (y = 2.220 ± 0.391 x–0.022 ± 0.011, r2: 0.47, ) and MDR1a (y = 1.290 ± 0.121 x–0.007 ± 0.003, r2: 0.75, ) in the proximal jejunum in all groups except for rats treated with 0.5 μg/kg body weight 12 h before sacrifice (Figure 1).

3.3. Ileal P-gp Activity

While no effect was found in animals treated with 1,25-(OH)2D3 12 hours before sacrifice (data not shown), rats treated with 25-OHD3 or vitamin D3 showed a more pronounced inhibition of probably P-gp-mediated secretion of rhodamine-123 after addition of verapamil to the mucosal compartment of the Ussing chamber (). Analysis of rhodamine-123 net increase over time revealed a second-order polynomial model (y = b0 + b1 · x + b2 · x2, Figure 2) that differed between placebo and treatment groups for the animals that had received 25-OHD3 (b0: 1.36 ± 6.96 and 1.04 ± 8.85, b1: −0.118 ± 0.218 and −0.019 ± 0.278, b2: 0.0031 ± 0.0014 and 0.0041 ± 0.0018, ) as well as for those treated with vitamin D3 (b0: 0.78 ± 4.89 and 0.93 ± 6.05, b1: −0.056 ± 0.153 and 0.053 ± 0.190, b2: 0.0028 ± 0.0010 and 0.0036 ± 0.0012, ). When compared with 2-way ANOVA for repeated measures followed by Bonferroni’s posttest, significant effects could be confirmed for the factors time () and interaction of time and treatment () for the 25-OHD3-group with significant differences between the concentrations determined after 150 min of incubation (). For animals treated with vitamin D3, significant effects could be confirmed for the factors time (), treatment (), and interaction of time and treatment () with significant differences between the concentrations determined after 120 min () and 150 min of incubation ().

4. Discussion

Vitamin D responsive elements have been shown in the promotor regions of human MDR1 and CYP3A4 genes as well as in that of the rat CYP3A9 gene [21, 32, 33]. In contrast to some results previously obtained in rats and sheep treated with 1,25-(OH)2D3 [25, 28], neither isoenzymes belonging to the CYP3A family investigated nor MDR1a/b was upregulated by intraperitoneal administration of 1,25-(OH)2D3 in the present study. It should be noted that, in most previous studies with rodents, 1,25-(OH)2D3 was administered repeatedly or at higher doses. Our serum analysis data and that of RNA expression of genes involved in vitamin D metabolism and calcium transport indicate clearly that the vitamin D metabolites were administered correctly and absorbed efficiently. However, from the results on CYP24A1 and CYP27B1 expression, it might be concluded that rats are generally less sensitive to 25-OHD3 than sheep [25].

In addition, the different response in comparison to sheep could be explained by species-dependent induction of CYP3A enzymes. The predominant regulator of CYP3A enzymes is PXR [34]. The human PXR has been shown to bind hydroxylated vitamin D metabolites [35]. In contrast to other members of the nuclear receptor family, a comparison of the PXR sequences from different mammalian species showed that the proteins share less than 80% amino acid identity in their ligand binding domain (LBD) [36]. The striking differences in the LBD are assumed to be responsible for the selectivity in ligand binding and thus for the differences observed in respect to the induction profiles. For example, rifampicin, but not dexamethasone, induces CYP3A expression in human liver cells, while rat liver cells respond to dexamethasone but not to rifampicin [37]. As differences in the activity of enzymatic biotransformation could be found even between sheep and goats [38] or when different cattle breeds were compared [39], results on pharmacokinetics cannot be easily extrapolated from one species or breed to another.

The observation that none of the intestinal CYP3A enzymes investigated was upregulated with the 1,25-(OH)2D3-treatment is in line with results from Xu et al., who found a selective induction of CYP3A1/23, the isoform that was not addressed here [23]. However, interestingly, hepatic CYP3A18 as well as intestinal CYP3A9 RNA expression were both downregulated in the present study. This contrasts with a report of Khan et al. [40], where no effect of 1,25-(OH)2D3 on rat intestinal and hepatic CYP3A9 could be found, although the same treatment induced an upregulation of CYP3A4 in human tissues. In the present study, a reduction in PXR expression could be shown in the liver and the kidney with 1,25-(OH)2D3-treatment and also in the kidney with vitamin D3-treatment, but the same 1,25-(OH)2D3-protocol stimulated renal PXR expression in sheep [25]. Although other important nuclear receptors like the constitutive androstane receptor and the liver X receptor were not included in this study, these results further underline the relevance of species-specific mechanisms of CYP3A induction. At least for the liver, the response of CYP3A18 expression observed in our rats might be mediated by the decreased expression of PXR that could affect the activation by endogenous ligands [40]. PXR expression has been shown to correlate with CYP3A expression in humans [41]. In the present study, such a correlation with PXR could only be found for the expression of CYP3A18 and MDR1a in the proximal jejunum. Interestingly, no linear relationship could be revealed for rats treated with 1,25-(OH)2D3 (Figure 1). This observation might indicate an interference of the treatment with regulatory pathways involving PXR.

The effect of the treatment with 25-OHD3 and vitamin D3 on intestinal activity of P-gp only became apparent after inhibition of P-gp with verapamil. In both treated groups, the inhibition seemed to last longer than in the respective control groups (Figure 2). The use of rhodamine-123 as a P-gp-substrate and verapamil as a P-gp-inhibitor is well established [4244]. However, a significant efflux of rhodamine-123 mediated by other transport proteins, such as multidrug-related-proteins (MRPs), has to be considered [45, 46]. In the present study, the contribution of other transporters to the net increase of rhodamine-123 in the mucosal compartment has not been investigated. Besides a variation in the abundance of efflux transporters in the animals treated with vitamin D metabolites, alterations in the expression pattern or activity of CYP3A enzymes might explain the different responses to the inhibition of P-gp. Verapamil itself is metabolized by intestinal CYP3A enzymes [47]. Although we could not find any alterations in the RNA expression of the CYP3A isoenzymes investigated, it might be speculated that administration of 25-OHD3 and vitamin D3 led to a change in the relative activity of the different isoforms of CYP3A enzymes resulting in a slower metabolism of the applied inhibitor.

On the other hand, the observed effect might be a direct effect of vitamin D metabolites on P-gp function. Inhibition of P-gp cannot only occur by influencing its expression but also by alteration of the ATPase activity or competition for binding sites. Although verapamil competes with other substrates for the P-gp binding sites, it also increases its ATPase activity [48]. Progesterone and desoxycorticosterone diminish this stimulating effect of verapamil in a dose-dependent manner [49]. Recently, it could be demonstrated that 25-OHD3 and vitamin D3 decrease the verapamil-induced ATPase activity of P-gp in membranes of Sf9 insect cells overexpressing human P-gp too, while under basal conditions, only vitamin D3 exerted a slight effect [8]. This is in line with our observation that significant effects could be found for rhodamine-123 transport only after addition of verapamil.

In brain tissues, we investigated P-gp and BCRP because these transporters share a broad range of substrates and BCRP is upregulated in the blood-brain barrier of MDR1a k.o. mice [50, 51]. In contrast to Durk et al. [52], we did not find an upregulation but rather a significant downregulation of MDR1a and BCRP with the 1,25-(OH)2D3 treatment. Given that our treatment induced expression and activity of CYP24A1, it can be assumed that as a side-effect there was an increase in vitamin D metabolites hydroxylated at carbon 24. In fish and chickens, 24,25-(OH)2D3 has been demonstrated to exert opposite effects to 1,25-(OH)2D3, e.g., a decrease in calcium absorption [53, 54]. Whether such negative impacts of vitamin metabolites hydroxylated at carbon 24 could also play a role in the regulation of nonclassical vitamin D responsive genes has not yet been investigated. But if there were such an effect, it could probably be overcome by the much higher and/or repeatedly administered dosage of 1,25-(OH)2D3 in these reported studies. Another explanation could be an interaction between VDR, PXR, and the estrogen receptor or respective estrogen responsive elements in certain promoters. BCRP is downregulated in brain tissues by 17β-estradiol [55]. At least in breast cancer cells, 1,25-(OH)2D3 interacts with estrogen-responsive elements [56]. In addition, metabolic pathways induced by the upregulation of PXR could affect the tissue concentration of estrogens [57, 58].

In summary, our results show that the stimulating effects of vitamin D metabolites on the expression of genes involved in the metabolism and elimination of xenobiotics previously reported for rats and cell culture systems and, in case of CYP3A also in sheep, could not be reproduced using the treatment protocol applied here. However, alterations of P-gp activity as well as an impact on the expression of some CYP3A isoenzymes and the transcription factor PXR cannot be excluded.

Data Availability

The data used to support this study are included within the article.

Conflicts of Interest

The authors have declared no conflicts of interest.

Acknowledgments

This research was partly supported by the H. Wilhelm Schaumann Foundation. This publication was supported by the Deutsche Forschungsgemeinschaft and University of Veterinary Medicine Hannover, Foundation within the funding programme Open Access Publishing.

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