The role of bile acids in carcinogenesis

Abstract

Bile acids are soluble derivatives of cholesterol produced in the liver that subsequently undergo bacterial transformation yielding a diverse array of metabolites. The bulk of bile acid synthesis takes place in the liver yielding primary bile acids; however, other tissues have also the capacity to generate bile acids (e.g. ovaries). Hepatic bile acids are then transported to bile and are subsequently released into the intestines. In the large intestine, a fraction of primary bile acids is converted to secondary bile acids by gut bacteria. The majority of the intestinal bile acids undergo reuptake and return to the liver. A small fraction of secondary and primary bile acids remains in the circulation and exert receptor-mediated and pure chemical effects (e.g. acidic bile in oesophageal cancer) on cancer cells. In this review, we assess how changes to bile acid biosynthesis, bile acid flux and local bile acid concentration modulate the behavior of different cancers. Here, we present in-depth the involvement of bile acids in oesophageal, gastric, hepatocellular, pancreatic, colorectal, breast, prostate, ovarian cancer. Previous studies often used bile acids in supraphysiological concentration, sometimes in concentrations 1000 times higher than the highest reported tissue or serum concentrations likely eliciting unspecific effects, a practice that we advocate against in this review. Furthermore, we show that, although bile acids were classically considered as pro-carcinogenic agents (e.g. oesophageal cancer), the dogma that switch, as lower concentrations of bile acids that correspond to their serum or tissue reference concentration possess anticancer activity in a subset of cancers. Differences in the response of cancers to bile acids lie in the differential expression of bile acid receptors between cancers (e.g. FXR vs. TGR5). UDCA, a bile acid that is sold as a generic medication against cholestasis or biliary surge, and its conjugates were identified with almost purely anticancer features suggesting a possibility for drug repurposing. Taken together, bile acids were considered as tumor inducers or tumor promoter molecules; nevertheless, in certain cancers, like breast cancer, bile acids in their reference concentrations may act as tumor suppressors suggesting a Janus-faced nature of bile acids in carcinogenesis.

Background

Bile acids (BAs) belong to cholesterol-derived sterols. Due to the side chain carboxyl group and hydroxylation of their steroid ring they are more polar than cholesterol. They have an amphipatic character for which they are known as natural detergents. Majority of cholesterol is excreted by bile acids that are prone to enterohepatic circulation between the gallbladder and the liver. Cholesterol absorption in the intestine and cholesterol secretion into the bile both require bile salts, which are, together with enterohepatic circulation of BAs, crucial for balancing the plasma cholesterol level [1].

BAs are also signaling molecules. They deorphanized the farnesoid X nuclear receptor (FXR) which is now known as a ligand-inducible transcription factor responsive to BAs [2]. It is important to note that BAs are metabolized in a similar manner as xenobiotics, contributing to the cross-talk between the endogenous and xenobiotic metabolism in the liver through nuclear receptors Pregnane X receptor (PXR), constitutive androstane receptor (CAR) and others [3]. While their synthesis takes place exclusively in the liver, the homeostasis and excretion involve multiple organs and compartments in the body. After discovering their signaling role, BAs have been considered as pro-carcinogenic molecules [4–6]. However, recent studies have provided evidence that in certain cancers, BAs can have antineoplastic features (e.g. breast cancer [7–11]). This novel, context-dependent, dualistic finding prompted us to thoroughly assess the involvement of BAs in carcinogenesis and cancer progression.

Bile acid biosynthesis

The excess of free cholesterol is toxic to cells and needs to be excreted, primarily through conversion to more polar BAs. The introduction of a hydroxyl group in cholesterol reduces the half-life and directs the oxidized molecule to excretion [12]. BA synthesis is thus the main cholesterol detoxification pathway where multiple cytochrome P450 (CYP) enzymes are involved in the classical or alternative pathways (Fig. 1). The two major primary BAs in humans are cholic acid (CA) and chenodeoxycholic acid (CDCA). They are synthesized in the liver and secreted into the gallbladder as glycine or taurine conjugates [13]. The BA composition in mice substantially differs from the humans which has to be taken into account when using mouse as a model for BA related diseases. The mouse Cyp2c70 metabolizes CDCA to more hydrophilic primary muricholic acids (MCAs) [14].

Fig. 1.

Scheme of the classical and alternative bile acids in humans. Only enzymes of the CYP family are listed while the pathway involves enzymes of other protein families. CA and DCA are conjugated and further metabolized in the intestine

The first enzyme of the classical BA synthesis pathway is cholesterol 7α-hydroxylase (CYP7A1), leading to 7α-cholesterol in a rate-limiting reaction step, followed by several enzymatic conversions. This enzyme is prone to the negative feedback regulation by BAs and FXR [2]. Sterol 12α-hydroxylase (CYP8B1) lies at the branching point that leads to CA. Sterol 27-hydroxylase (CYP27A1) is needed for both CA and CDCA. In the alternative pathway, cholesterol is first metabolized by CYP27A1 to form 27-hydroxycholesterol that is a substrate for 25-hydroxycholesterol 7α-hydroxylase (CYP7B1) and later other enzymes [15]. The alternative pathway leads majorly to CDCA. The ratio of CA to CDCA is determined by the expression level of CYP8B1, which transforms a di-hydroxylated BA to tri-hydroxylated BA. The alternative pathway is estimated to account for about 10% of cholesterol conversion [16]. Of importance, there are major differences in individual BA synthesis genes in mouse and in humans which may be due also to different biological roles of human and mouse BA species (reviewed in [15]).

Bacterial metabolism of bile acids, production of secondary bile acids

Hepatocytes secrete BAs to the bile canaliculi. By fusing with each other bile canaliculi form bile ducts, which eventually form the hepatic duct that runs to the gallbladder. The gallbladder empties to the duodenum upon feeding and, hence, releases BAs to the gastrointestinal tract. Primary BAs emulsify dietary fats and activate pancreatic lipases in the small bowel. BAs are then reabsorbed through the enterocytes and get to the liver for reuptake and reuse through the portal circulation. This circle is termed the enterohepatic circulation of BAs. A fraction of the reabsorbed BAs enter the systemic circulation (total BA concentration in the serum is < 5 µM in a healthy individual) and exert hormone-like effects [7, 17–20]. The reference concentrations of the serum, tissue and fecal bile acids are in Tables 1, 2, 3.

Table 1.

Reference serum bile acid levels

	Cohort size, reference	n = 40 [303]		n = 8 [304]		n = 30 [305]		n = 28 [306]		n = 56 (pooled) serum [7]
		Mean	± SEM	Mean	± SD	Mean	± SEM	Mean	± SEM	Mean
Primary bile acids	CA	181.5	83.1	440	651	162.05	40.19	153.68	159.64	287
	GCA	233.0	56.0	85	55	42.55	13.72	72.86	93.69	301
	TCA	179.7	47.0	14	12	2.04	0.63	18.56	29.4	71
	CDCA	256.8	56.3	380	410	1160.64	299.60	654.78	660.43	563
	GCDCA	771.5	111.9	450	210	975.59	205.81	649.19	648.55	931
	TCDCA	120.2	21.8	69	56	7.51	1.74	54.28	69.18	137
Secondary bile acids	DCA	386.7	66.0	320	120	593.27	141.09	402.76	350.11	701
	GDCA	246.2	42.5	104	44	190.78	44.32	156.39	149.88	415
	TDCA	44.9	11.8	21	18	44.06	8.86	24.62	22.68	61
	LCA	12.8	1.8			9.74	1.51	94.95	57.21	31
	GLCA	16.3	4.1	17	20			25.26	15.82	25
	TLCA	23.4	3.6	0,33	0,52	0.46	0.07	22.82	19.29
	UDCA	137.6	25.1	43	27	208.35	32.94	130.83	114.96	147
	GUDCA			76	40	60.92	9.76	128.04	178.12	330
	TUDCA	5.0	1.1	2,7	2,7	1.41	0.30	6.24	5.63

All concentrations are in nM

CA Cholic acid, CDCA Chenodeoxycholic acid, DCA Deoxycholic acid, GCA Glycocholic acid, GCDCA Glycochenodeoxycholic acid, GDCA Glycodeoxycholic acid, GLCA Glycolithocholic acid, GUDCA Glycoursodeoxycholic acid, LCA lithocholic acid, TCA Taurocholic acid, TCDCA Taurochenodeoxycholic acid, TDCA Taurodeoxycholic acid, TLCA Taurolithocholic acid, TUDCA Tauroursodeoxycholic acid, UDCA ursodeoxycholic acid

Table 2.

Reference fecal bile acid levels

	Cohort size, Reference	n = 97 [307]		n = 28 [308]		n = 15 [309]
		Mean µg/mg	± SD	Median nmol/g	Q1; Q3	Median ng/mg of dry feces
Primary bile acids	CA	56.16	255.46	20.19	5.03;1304.28	0.23
	GCA	199.35	317.56	2.23	1.39;3.55
	TCA	4.14	7.82	0.72	0.46;2.11
	CDCA	29.65	102.48	57.16	13.76;1639.92	0.23
	GCDCA			5.17	2.56;10.51
	TCDCA	3.35	10.5	1.41	0.37;3.58
Secondary bile acids	DCA			2159.78	1676.03;3094.08	2.6
	GDCA	110.41	167.88	2.67	1.44;6.83
	TDCA	4.84	12.5	1.75	0.86;6.63
	LCA	548.75	336.88	2339.24	1737.09;2782.40	3.1
	GLCA	0.18	0.18	0.91	0.41;1.28
	TLCA	0.94	4.46	1.03	0.36;2.80
	UDCA			17.21	8.76;33.48	0.1
	GUDCA	0.81	3.88	0.65	0.38;0.87
	TUDCA			0.37	0.07;1.23

CA Cholic acid, CDCA Chenodeoxycholic acid, DCA Deoxycholic acid, GCA Glycocholic acid, GCDCA Glycochenodeoxycholic acid, GDCA Glycodeoxycholic acid, GLCA Glycolithocholic acid, GUDCA Glycoursodeoxycholic acid, LCA lithocholic acid, TCA Taurocholic acid, TCDCA Taurochenodeoxycholic acid, TDCA Taurodeoxycholic acid, TLCA Taurolithocholic acid, TUDCA Tauroursodeoxycholic acid, UDCA ursodeoxycholic acid

Table 3.

Reference tissue bile acid levels

		Gastric juice (µM)		Breast cyst fluid (µM)	Adipose tissue (ng/g)		Liver tissue (nmol/g)		Liver tissue (nmol/g)
		n = 10 [310]		n = 12 [261]	n = 24 [311]		n = 6 [312]		n = 10 [313]
		Mean	± SEM	Min–Max	Median	Min–Max	Mean	± SEM	Mean	± SEM
Primary bile acids	CA	2.38	1.09	3–119 (n = 1, ND)	˂LOD	0–11.4	21.1	13.0	30.4	5.9
	GCA	0.74	0.65		7.5	2.6–33.6
	TCA	0.87	0.1		12.5	4.9–106.9
	CDCA	0.03	0.04	4–305	˂LOD	˂LOD	31.0	16.0	29.8	5.4
	GCDCA	0.55	0.5		15.9	2.2–67.3
	TCDCA	0.57	0.08		2.6	1.0–3.5
Secondary bile acids	DCA	3.78	0.6	17–160 (n = 1, ND)	9.4	0–60.6	6.2	2.3	2.0	0.7
	GDCA	0.39	0.2		14.9	4.8–45.3
	TDCA	5.22	0.02		4.2	1.6–6.0
	LCA	0.12	0.02	9–23 (n = 6, ND)	˂LOD	˂LOD	1.5	0.2	0.7	0.3
	GLCA	0.12	0.007		8.1	2.9–19.0
	TLCA	0.86	0.01		˂LOD	˂LOD
	UDCA	0.02	0.02		˂LOD	˂LOD	2.0	0.8	1.5	0.6
	GUDCA	0.24	0.08		2.0	0–15.9
	TUDCA	3.58	0.002		0.8	0.3–1.9

CA Cholic acid, CDCA Chenodeoxycholic acid, DCA Deoxycholic acid, GCA Glycocholic acid, GCDCA Glycochenodeoxycholic acid, GDCA Glycodeoxycholic acid, GLCA Glycolithocholic acid, GUDCA Glycoursodeoxycholic acid, LCA lithocholic acid, TCA Taurocholic acid, TCDCA Taurochenodeoxycholic acid, TDCA Taurodeoxycholic acid, TLCA Taurolithocholic acid, TUDCA Tauroursodeoxycholic acid, UDCA ursodeoxycholic acid, ND not detected, LOD limit of detection

BAs are very powerful surfactants [21]; therefore, bacteria, mostly in the large bowel, need to protect themselves against being disintegrated by BAs. For example, lipopolysaccharides serve as membrane components in Gram-negative bacteria to passively ward off external toxins or BAs [22]. In addition to that, bacteria have a more sophisticated enzymatic system to cope with BAs termed BA conversion [23].

The hydroxyl groups and the tauryl or glycyl conjugate on BAs are crucial elements of the molecular structure of BAs for their strong surfactant properties. Therefore, the removal, modification or substitution of these molecular elements diminishes the potentially toxic features of primary BAs and renders them largely apolar. The dehydroxylated primary BAs are called secondary BAs and the main site for converting primary BAs to secondary BAs is the large bowel [24]. Secondary BAs can be resorbed to the portal circulation and are transported to the liver, where, however, hydroxylation and conjugation needs to be restored for reuse. The main secondary BAs in humans are lithocholic acid (LCA), deoxycholic acid (DCA) and to a lesser extent, ursodeoxycholic acid (UDCA) [24, 25].

Bile salt hydrolases (BSHs) are responsible for the deconjugation of BAs, namely the removal of glycine or taurine by breaking the C24 N-acyl bond. Glycine and taurine can be fed into the metabolism of bacteria to be used as an energy source [23]. BSH activity is common among the bacteria inhabiting the small and the large intestines [23]; both aerobic [26] and anaerobic bacteria can deconjugate bile salts [27]. Namely, among the Gram-positive bacteria BSH was identified in Clostridium [27–30], Enterococcus [27, 31], Bifidobacterium [27, 32, 33], Lactobacillus [34, 35], Streptococcus [36], Eubacterium [37] and Listeria, among Gram-negative bacteria in Bacteroides [30, 38, 39], while among archea Methanobrevibacter smithii and Methanosphera stadmanae [40].

The substituents on the gonane core of BAs can be also modified, the term “secondary BA” typically stands for the removal of 7α or 7β-hydroxyl groups from primary BAs. Clostridiales and Eubacteria were shown to play a major role in dehydroxylation [23, 41–45], although other genre or species were also implicated (e.g. Bacteroidetes, Escherichia) [7, 38, 44, 46, 47]. Although BA deconjugation and dehydroxylation are different processes, they may be linked through regulatory circuits [30]. Other reactions of BAs involve oxidation, and epimerization that can be linked to intestinal Firmicutes (Clostridium, Eubacterium, and Ruminococcus), Bacteroides and Escherichia [23, 36, 37, 41, 42, 44, 45, 48]. Bacterial enzymes involved in secondary BA production are assembled in the BA inducible (bai) operon [24]. Collectively, BA transformation renders secondary BAs hydrophobic and BAs loose their ability to act as detergents or toxins to bacteria. Moreover, these changes are vital in fine-tuning the affinity of BAs to BA receptors.

Interactions between BAs and gut microbiota are bidirectional. Microbiota can transform primary BAs and, hence, modulate the composition of the BA pool [49, 50]. Inversely, BAs can influence the composition of the microbiome as well [51–56] and facilitate bacterial translocation to tissues [57], further underlining that notion BAs act as potent drivers of the early intestinal microbiota maturation [58]. Oncobiosis (dysbiosis associated with cancers) [59] can alter the secondary BA pool that may contribute to carcinogenic effects [4, 5, 7, 18]. It is of note that several other non-BA bacterial metabolites are known that play role in carcinogenesis [60–64].

Bile acid transporters

The enterohepatic circulation of BAs depends on BA transporters in the gastrointestinal system. Almost 90% of BAs are involved in circulation due to efficient active transport [65]. Different uptake and efflux BAs transporters are present in the hepatic and intestinal cells (Fig. 2). After BAs are synthesized in the liver they are transported into the bile mainly by the ATP-dependent cassette transporter (BSEP) [65], but also minor transporters, the multidrug resistance-associated protein 2 (MRP2, ABCC2) and the multidrug resistance protein 1 (MDR1, ABCB1) [65]. From the intestinal lumen, BAs are uptaken into the intestinal cells by the major apical sodium-dependent bile acid transporter (SLC10A2, ASBT), which transports BAs also across the canalicular membrane in cholangiocytes and renal tubule apical membrane from glomerular filtrate [66]. BAs are then effluxed into the portal circulation by two Solute Carrier Family members, SLC51A or OSTα and SLC51B or OSTβ. The bile acids are then taken back up into hepatocytes by the major transporter the solute carrier family 10 (SLC10A1, NTCP), [65].

Fig. 2.

A scheme of enterohepatic and systemic circulation of bile acids and the transporters in different human cells. Transporters are coloured according to which part of the circulation they belong to. Blue are efflux and influx transporters, which transport BAs in portal circulation. Grey are efflux transporters, which contribute to bile export into bile and faeces. Green are transporters, which are responsible for BA transport into the systemic circulation. Yellow are transporters involved in the efflux of BAs into urine. ASBT/SLC10A2 sodium-dependent bile acid transporter, BSEP/ABCB11 ATP-dependent cassette transporter, MRP2/ABCC2 multidrug resistance-associated protein 2, MRP3/ABCC3 multidrug resistance-associated protein 3, MRP4/ABCC4 multidrug resistance-associated protein 4, OATP1A2/SLCO1A2 Solute Carrier Organic Anion Transporter Family Member 1A2, OATP1B/SLCO1B Solute Carrier Organic Anion Transporter Family, SLC51A/B or OSTα/β Solute Carrier Family members, SLC10A2/ASBT sodium-dependent bile acid transporter

BAs can enter the systemic circulation via export across the hepatic sinusoidal membrane by OSTα/OSTβ, the multidrug resistance-associated protein 3 (MRP3, ABCC3) and the multidrug resistance-associated protein 4 (MRP4, ABCC4) [67]. The MRP transporters have a role in reducing hepatic BA concentration in cholestatic conditions. MRP3 and MRP4 are also present in cholangiocytes, where they efflux BAs to portal circulation and are part of the cholehepatic shunt together with ASBT [66]. Several transporters are expressed in the kidney, where they participate in BA elimination via urine (Fig. 2) [66, 68, 69]. The Solute Carrier Organic Anion Transporter Family, OATP1B1 or SLCO1B1 and OATP1B3 or SLCO1B3 contribute to the systemic clearance of BAs via liver [70]. Other cells also express BA transporters and can, therefore, uptake BAs from the systemic circulation [68, 69, 71].

Bile acids as signaling molecules

In addition to their role in digestion, BAs act as signaling molecules. BAs can activate membrane receptors (Fig. 3), such as G protein-coupled bile acid receptor 1 (GPBAR1, also known as TGR5), sphingosine-1-phosphate receptor 2 (S1PR2), muscarinic receptors (CHRM2 and CHRM3) and nuclear receptors (NRs), such as farnesoid X receptor (FXR, NR1H4), PXR (NR1H2), vitamin D receptor (VDR, NR1H1), CAR (NR1H3) and liver X receptor (LXR, NR1H2-3). Each BA can interact with more than one receptor. Receptors are differentially activated by BAs. For example, FXR is activated by CDCA > DCA > LCA > CA [72], while TGR5 is activated by LCA > DCA > CDCA > CA [73, 74], respectively. VDR and PXR are mainly activated by LCA. BAs mediate immune responses [75], gastrointestinal mucosal barrier function, gestation [76], carcinogenesis [11, 18, 56] and metabolic diseases [20]. The activation of BA receptors may lead to the induction of signaling pathways involved in the regulation of several physiological functions, such as glucose, lipid and energy metabolism, as well as, in cancers. Below, we review the mode of action of BA receptors and highlight those receptor-mediated functions that have a key role in regulating the behavior of cancer cells.

Fig. 3.

The subcellular localization of bile acid receptors. TGR5 G protein-coupled bile acid receptor 1, S1PR2 Sphingosine-1-phosphate receptor 2, CHRM2 Muscarinic receptor-2, CHRM3 Muscarinic receptor-3, FXR Farnesoid X receptor, PXR Pregnane X receptor, CAR Constitutive androstane receptor, VDR Vitamin D receptor, SHP Small heterodimer partner

Cell membrane receptors

G protein-coupled bile acid receptor 1 (GPBAR1, TGR5)

TGR5 is a member of the G protein-coupled receptor superfamily, highly expressed in the epithelium of the gallbladder [77], the intestine [74], the brown adipose tissue and the skeletal muscle [20], as well as in the brain [78]. TGR5 is also expressed in human monocytes/macrophages [73]. TGR5 is not expressed by hepatocytes, while Kupffer cells and liver sinusoidal cells can express the receptor [79].

Secondary BAs LCA and DCA are the most potent, natural ligands for TGR5, but the receptor also responds to CDCA and CA [73, 74] and a set of artificial ligands [80–84] (Table 4). Ligand binding to the TGR5 receptor triggers activation of adenylate cyclase leading to the production of cAMP [73, 74, 85] and the downstream activation of extracellular signal-regulated kinase 1/2 (ERK1/2), protein kinase A (PKA), protein kinase B (AKT), mammalian target of rapamycin complex 1 (mTORC1) and Rho kinase [86–89]. TGR5 activation leads to metabolic changes characterized by energy expenditure and β-oxidation [20, 90]. BA-dependent induction of TGR5 has immunomodulating effects. Most studies point to TGR5-dependent immunosuppression [73, 79, 91–94] partly due to the suppression of the Toll-Like Receptor 4—Nuclear factor-κB (TLR4–NF‐κB) pathway [91, 93, 94]. In line with that, in a murine model of breast cancer, LCA treatment induced the proportions of tumor-infiltrating lymphocytes through TGR5 [7].

Table 4.

Bile acid receptors, their ligands and connected cancers

Receptor	Bile acid ligands	Connected cancers
GPBAR1 (TGR5)	TLCA, LCA, DCA, CDCA, CA	Breast cancer Pancreatic cancer Gastric cancer Colon cancer Oesophageal adenocarcinoma
S1PR2	GCA, TCA, GCDCA, TCDCA, GDCA, TDCA	Cholangiocarcinoma Oesophageal adenocarcinoma
CHRM2, CHRM3	LCT, TLCA	Colon cancer Cholangiocarcinoma
FXR	CDCA, DCA, LCA, CA	Colon cancer Hepatocellular carcinoma Breast cancer Oesophageal adenocarcinoma
PXR	LCA, 3-keto-LCA, CDCA, DCA, CA	Colon cancer Oesophageal adenocarcinoma
CAR	LCA	Breast cancer
VDR	LCA	Colon cancer
LXR α/β	HDCA	Ovarian cancer
SHP	DCA	Hepatocellular carcinoma Breast cancer Gastric cancer

CA Cholic acid, CAR Constititive androstane receptor, CDCA Chenodeoxycholic acid; CHRM2/M3, Muscarinic receptor 2 and 3, DCA Deoxycholic acid, FXR Farnesoid X receptor, GCA Glycocholic acid, GCDCA Glycochenodeoxycholic acid, GDCA Glycodeoxycholic acid, HDCA hyodeoxycholic acid, LCA Lithocholic acid, LCT Lithocholyltaurine, LXR Liver X receptor, PXR Pregnane X receptor, S1PR2 Sphingosine-1-phosphate receptor 2, SHP Small heterodimer partner, TCA Taurocholic acid, TCDCA Taurochenodeoxycholic acid, TDCA Taurodeoxycholic acid, TGR5/GPBAR1 G protein- coupled bile acid receptor 1, TLCA Taurolithocholic acid, VDR Vitamin D receptor

Sphingosine-1-phosphate receptor 2 (S1PR2)

Conjugated BAs activate S1PR2 [95–97] that upregulates the expression of sphingosine kinase 2 (SphK2), which in turn enhances the level of sphingosine-1-phosphate in the nucleus. Elevated nuclear sphingosine-1-phosphate inhibits the function of histone deacetylases resulting in the upregulation of genes encoding nuclear receptors and enzymes involved in lipid and glucose metabolism [98] Similar to TGR5, ligand binding to S1PR2 can activate different downstream signaling pathways, such as ERK, AKT and/or c-Jun N-terminal kinase (JNK1/2) [96, 97, 99, 100]. Glycochenodeoxycholic acid (GCDCA) can trigger apoptosis in hepatocytes through activating S1PR2 [101]. S1PR2 is highly expressed in macrophages [102] and has widespread immunological roles [100, 102, 103].

Muscarinic receptors (CHRM2 and CHRM3)

Taurine conjugated BAs can activate muscarinic receptors, the cholinergic receptor muscarinic 2 and 3 (CHRM2 and CHRM3). CHRMs are overexpressed in colon cancer cells and stimulate cell proliferation and invasion [104, 105]. Taurolithocholic acid (TLCA) induces cholangiocarcinoma cell growth via muscarinic acetylcholine receptor and EGFR (epithelial growth factor receptor)/ERK1/2 signaling [106].

Nuclear receptors

Farnesoid X receptor (FXR, NR1H4)

FXR is a member of the nuclear hormone receptor superfamily. There are two FXR genes, encoding FXRα and FXRβ of which only FXRα is expressed, FXRβ is present as a non-expressed pseudogene in humans. The FXR receptor heterodimerizes with retinoid X receptor (RXR) and binds to FXR response elements (FXREs) within the regulatory regions of its target genes [107]. BAs are physiological ligands for FXR (with decreasing affinity: CDCA, DCA, LCA, CA) [72]. FXR is expressed mainly in the liver, intestine, kidney and adrenal glands [107].

FXRα controls BA synthesis, transport and detoxification. The activation of FXR receptor by BAs reduces the expression of Cyp7a1 and Cyp8b1, key enzymes of BA biosynthesis pathway. In the liver, FXRα induces the transcription of its target gene encoding small heterodimer partner (SHP, NR5O2), an orphan nuclear hormone receptor (see in detail later) that lacks a DNA binding domain and acts as a transcriptional repressor [108]. SHP inhibits the expression of Cyp7a1 through the inhibition of the interaction with liver receptor homolog-1 (LRH-1, NR5A2) [109]. In addition to LRH-1, SHP also prevents the function of hepatocyte nuclear factor-4α (HNF4α), a positive regulator of Cyp7a1 and Cyp8b1 [110]. In the intestine, FXRα induces the expression of fibroblast growth factor 19 (FGF19) in humans and its mouse homolog fibroblast growth factor 15 (FGF15). The secreted growth factor via portal blood reaches the liver where it binds to its receptor, fibroblast growth factor receptor 4 (FGFR4) and induces JNK and ERK pathways and causes repression of Cyp7a1, thus reducing BA synthesis [111]. In addition to Cyp7a1, Cyp8b1 is also repressed by FXRα via SHP-dependent mechanism involving HNF4α [110].

FXRα is also a key regulator of BA transport by influencing the expression of BA transporters. FXRα activation suppresses BA reuptake to hepatocytes through repressing the expression of NTCP via SHP dependent mechanism [112]. At the same time, FXRα facilitates the efflux of BAs from hepatocytes into bile by enhancing the expression of BSEP and into the systemic circulation via OSTα/β transporter [113]. FXR also upregulates MRP2, which promotes BA secretion into the gallbladder. Finally, FXRα activates the expression of intestinal BA-binding protein (I-BABP) in the ileum which promotes transport of BAs from enterocytes into portal blood [114] whereas limits enterocyte uptake of BAs by reducing ASBT expression. FXRα increases the expression of enzymes involved in the detoxification of BAs, such as cholesterol 25-hydroxylase or cytochrome P450 family 3 subfamily A4 (CYP3A4) [115], dehydroepiandrosterone-sulfotransferase (SULT) 2a1 [116] and uridine 5′-diphosphate-glucuronosyltransferase 2B4 (UGT2B4) [117]. Many studies have reported the relationship between FXR and inflammation. NF-kB activation suppressed FXR-mediated gene expression, indicating that there is a negative crosstalk between the FXR and NF-kB signaling [118].

Pregnane X receptor (PXR, NR1I2)

In humans, PXR is mainly expressed in the liver and intestine [119]. Among BAs, the most potent ligand of PXR is LCA, and the oxidized, 3-keto form of LCA. PXR acts as a xenobiotic sensor and regulates the expression of genes involved in the detoxification and metabolism of BAs [120]. Upon ligand binding, PXR binds to the promoter of its target gene as a heterodimer with RXR. Activation of PXR induces the uptake of xenobiotics, their modification by phase I enzymes (CYPs, including CYP3A, CYP2B, CYP2C), conjugation by phase II enzymes, such as glutathione S-transferases, UDP-glucuronosyl-transferases (UGTs) and sulfotransferases, and finally elimination by phase III drug transporters including MDR1, MRP2 and organic anion-transporting polypeptide (OATP2) [120]. The activation of PXR prevents cholesterol gallstone disease by regulating BA biosynthesis and transport [121] and protects the liver against LCA-induced toxicity [122–125]. PXR activation disrupts the interaction between HNF4α and peroxisome proliferator-activated receptor gamma coactivator 1 alpha (PGC-1α, PPARGC1A), which is required for the activation of CYP7A1 gene expression, thus reducing the expression of CYP7A1 and inhibiting the synthesis of BAs [126]. PXR activation is anti-inflammatory [127–129]. PXR activation facilitates lipogenesis, suppressing β-oxidation and ketogenesis and gluconeogenesis [130–132]. Furthermore, PXR through HNF4 and PGC-1α modulates the expression of CYP7A1 [133].

Constitutive androstane receptor (CAR, NR1I3)

CAR is the closest relative to the PXR and is expressed primarily in the liver. First studies identified that CAR has constitutive transcriptional activity in the absence of its ligand [134]. Later, it was reported that the constitutive transcriptional activity of CAR is reversed by androstane metabolites, which are inverse agonists [135]. CAR can be activated by direct ligand binding and indirect activation [136]. In the absence of ligand binding, CAR forms a heterodimer with RXR and transactivates its target genes [137]. CAR recruits coactivators in the nucleus, such as steroid receptor coactivator 1 (SRC-1, NC0A1) and PGC-1 [138]. Similar to PXR, CAR controls the expression of drug-metabolizing enzymes and transporters, thereby supporting the detoxification of xenobiotics [120, 139]. In contrast to PXR, it remains unclear whether BAs can function as natural ligands for CAR; nevertheless, there are reports underscoring the involvement of CAR in BA signaling [11].

Vitamin D receptor (VDR, NR1I1)

In humans, VDR is highly expressed in the kidney, intestine, bone as well as in hepatocytes but expressed at low levels in other tissues [140–142]. LCA is a potent endogenous VDR ligand [143, 144]; hence, VDR can act as an intestinal BA sensor. VDR activation induces expression of CYP3A that metabolizes LCA [143, 145]. In addition, VDR induces the expression of SULT2A1, MRP3 and ASBT to stimulate BA sulfonation, excretion and transport [146–148]. The activated VDR plays a role in the inhibition of BA synthesis via suppression of CYP7A1, thus protecting liver cells during cholestasis [140].

VDR can function as a nuclear receptor and a membrane-bounded receptor. Upon ligand binding, VDR translocates into the nucleus, where it binds to DNA response elements as a heterodimer with RXR to mediate gene transcription. Plasma membrane-associated VDR receptor activates several signaling cascades to inhibit CYP7A1 transcription [142, 149]. It has been shown that the activation of membrane VDR signaling by LCA in the liver activates MEK1/2ERK1/2 pathway, which stimulates nuclear VDR/RXRα heterodimer recruitment of corepressors to inhibit CYP7A1 gene transcription [150]. In biliary epithelial cells, bile salts (CDCA, UDCA) stimulate the expression of cathelicidin, an antimicrobial peptide, via VDR and FXR to control innate immunity [151]. The possible role of VDR in regulating immunity and the role of VDR in different cancer cells and diseases is reviewed in detail elsewhere [152].

Liver X receptor (LXR, NR1H2-3)

LXRs are activated by naturally occurring cholesterol metabolites such as oxysterols and bind to DNA as heterodimers with the RXR [153]. LXRα (NR1H3) and LXRβ (NR1H2) share a high structural homology [154]. LXRβ is ubiquitously expressed, while LXRα is primarily expressed in the liver, the adipose tissue, the intestine and macrophages. Upon ligand activation LXRs regulate gene expression via binding to LXR response elements in the promoter regions of the target genes. LXRα promotes the conversion of cholesterol into BAs through the induction of CYP7A1 expression in the liver. LXRs enhance the efflux of cholesterol from cells [155] and have an anti-inflammatory response in the adipose tissue and macrophages [156]. Hyodeoxycholic acid (HDCA), a naturally occurring secondary BA generated by bacterial C-6 hydroxylation of LCA, is a weak LXRα agonist [157].

Small heterodimer partner (SHP, NR5O2)

SHP is a unique nuclear receptor that contains a ligand-binding domain but lacks the conserved DNA-binding domain. SHP acts as a transcriptional corepressor regulating different metabolic processes, including lipid, glucose, energy homeostasis and BA synthesis via interaction with multiple transcription factors and nuclear receptors (reviewed in [158]). BAs or FGF19 signaling enhances posttranslational modifications of SHP, which modulates the regulatory function of SHP protein [159, 160]. SHP acts as an inhibitory regulator in Hedgehog/Gli signaling pathway [161].

Effects of bile acids in cancers

The role of BAs was implicated in a wide variety of neoplasias (Fig. 4, Tables 5, 6, 7). When assessing the effects of BAs, one has to keep in mind that the concentrations applied in the experiments need to correspond to the reference concentrations in serum or the compartment in question (e.g. parts of the gastrointestinal tract). However, several reports are using substantially higher concentrations than the reference. These studies need to be considered as ones using “therapeutic” concentrations. In the forthcoming chapters, we will review those neoplasias where BAs were implicated in pathogenesis.

Fig. 4.

Different roles of bile acids and bile acids receptors in a wide variety of cancers. Some BAs have opposite effects, which depend on the cell line, BA concentration and other treatment conditions. The crossed circle symbol marks the tumor suppressor effects and the arrow marks the tumor promoter effects. CA Cholic acid, CAR Constititive androstane receptor, CDCA Chenodeoxycholic acid, CHRM2/M3 Muscarinic receptor 2 and 3, DC Deoxycholate, DCA Deoxycholic acid, FXR Farnesoid X receptor, GCDA Glycochenodeoxycholate acid, GCDC Glycochenodeoxycholate, GDC Glycodeoxycholate, GDCA Glycodeoxycholic acid, GLCA Glycolithocholic acid, GUDCA Glycoursodeoxycholic acid, LCA Lithocholic acid, PXR Pregnane X receptor, S1PR2 Sphingosine-1-phosphate receptor 2, SHP Small heterodimer partner, TCA Taurocholic acid, TCDC Taurochenodeoxycholate, TCDCA Taurochenodeoxycholic acid, TDC Taurodeoxycholate, TDCA Taurodeoxycholic acid, TGR5/GPBAR1 G protein- coupled bile acid receptor 1, TLC Taurolithocholate, TLCA Taurolithocholic acid, TUDCA Tauroursodeoxycholic acid, UDCA Ursodeoxycholic acid, VDR Vitamin D receptor

Table 5.

Tumor suppressive effects of UDCA, TUDCA and GUDCA in cancers

Cancer type	Cell models	Concentration	Effects	Ref
Glioblastoma	A172, LN229	400–800 µM	UDCA inhibits cell viability, induces ROS production and endoplasmic reticulum stress, synergizes with proteasome inhibitor Bortezomib	[314]
Neuroblastoma	SH-SY5Y	100 µM	TUDCA protects against mitochondrial damage, cell death and ROS generation via mitophagy	[315]
Pancreatic cancer	HPAC, Capan1	0.2 mM	UDCA reduces intracellular ROS level and Prx2 expression, as well as suppresses EMT and stem cell formation	[227]
Prostate cancer	DU145	0–200 µg/ml	UDCA inhibits cell growth and induces apoptosis via extrinsic and intrinsic pathways	[274]
Melanoma	M14, A375	0–300 µg/ml	UDCA inhibits cell proliferation and induces apoptosis via ROS-triggered mitochondrial-associated pathway	[316]
Hepatocellular carcinoma (HCC)	Huh-BAT, HepG2	750 µM	UDCA has a synergistic effect on the antitumor activity of sorafenib in HCC cells via activation of ERK and dephosphorylation of STAT3	[195]
	HepG2, BEL7402	0.1–1 mM	UDCA inhibits proliferation and induces apoptosis of HCC cell lines by blocking cell cycle and regulating the expression of Bax/Bcl-2 genes. UDCA suppresses growth of BEL7402 cells in vivo	[196] [317]
	HepG2	0.25–1 mM	UDCA induces apoptosis via regulating of Bax to Bcl-2 ratio, the expressions of Smac and Livin, and caspase-3 expression and activity	[197]
	Huh-Bat, SNU761, SNU475	200 µM	UDCA suppresses cell growth and induces DLC1 tumor suppressor protein expression by inhibiting proteasomal DLC1 degradation in an ubiquitin-independent manner	[198]
	HepG2, SK-Hep1, SNU-423, Hep3B	100 µM	UDCA switches oxaliplatin-induced necrosis to apoptosis via inhibition of ROS production and activation of the p53-caspase 8 pathway	[199]
Oral Squamous Carcinoma	HSC-3	100–400 µg/ml	UDCA induces apoptosis via caspase activation	[318]
Leukemia	T leukemia cell line (Jurkat cell)	100 µg/ml	TUDCA and UDCA induce a delay in cell cycle progression	[319]
Gastric cancer	MKN‑74	200 µM	UDCA suppresses chenodeoxycholic acid-induced PGE2 production and tumor invasiveness without affecting the COX-2 expression	[320]
	SNU601, SNU638	0.25–1 mM	UDCA induces apoptosis, which is mediated by lipid raft-dependent death receptor 5 (DR5) expression and activation	[321]
	SNU601	0.6–1 mM	UDCA induces apoptosis via MEK(MAPK)/ERK pathway. DCA-mediated ERK activation exerts an antiapoptotic activity in this cell line	[322]
	SNU601	0.5–1 mM	UDCA induces apoptosis via CD95/Fas death receptor, downregulates ATG5 level and prevents autophagic pathway	[323]
Oesophageal cancer / Barett’s esophagus	BAR-T, BAR-10 T	125–250 µM	UDCA increases antioxidant expression and prevents DCA-induced DNA damage and NF-κB activation	[324]
	SKGT-4, OE33	300 µM	UDCA inhibits DCA-induced NF-κB, AP-1 activation and COX-2 upregulation	[325]
	BE CP-A	0.1–0.2 mM	GUDCA has cytoprotective role by inhibiting oxidative stress	[326]
Colon cancer	HCT116	500 µM	UDCA inhibits DCA-induced apoptosis via modulation of EGFR/Raf-1/ERK signaling	[246]
	HCT116	500 µM	UDCA suppresses DCA-induced apoptosis by stimulating AKT-dependent survival signaling	[327]
	HCT116	500 µM	UDCA protects colon cancer cells from apoptosis induced by DCA by inhibiting apoptosome formation independently of the survival signals mediated by the PI3K, MAPK, or cAMP pathways	[328]
	HCT116	400 µM	UDCA inhibits cell proliferation by suppressing the expression of c-Myc protein and cell cycle regulatory molecules	[329]
	HT29, HCT116	0.2 mM	UDCA inhibits cell proliferation by regulating ROS production, induces activation of ERK1/2, and inhibits formation of colon cancer stem-like cell	[244]
	HCT116	300 µM	UDCA inhibits interleukin β1 and blocks DCA-induced NF-κB and AP-1 activation	[330]
	HT-29	250 µM	UDCA suppresses cell growth, which is enhanced in the presence of caveolin; UDCA promotes endocytosis and degradation of EGFR receptor	[331]
	HCT116, COLO 205	50 µg/ml	TUDCA suppresses NF-κB signaling and ameliorates colitis-associated tumorigenesis	[332]
Cholangiocarcinoma	Mz-ChA-1	0.2–200 µM	TUDCA inhibits cell growth via a signal-transduction pathway involving MAPK p42/44 and PKCα	[333]

AKT AKT Serine/Threonine Kinase 1, AP-1 activator protein-1, ATG5 Autophagy Related 5, BIRC7/Livin baculoviral IAP repeat-containing protein 7, Bax Bcl-2-associated X protein, Bcl-2 B-cell lymphoma 2, cAMP Cyclic adenosine monophosphate, c-Myc Myc-Related translation/localization regulatory factor, COX2 cyclooxygenase-2, DCA Deoxycholic acid, Dlc1 Deleted in Liver Cancer 1, DR5 death receptor 5, EGFR epithelial growth factor receptor, EMT epithelial–mesenchymal transition, ERK extracellular signal-regulated kinase, FAS/CD95 Fas Cell Surface Death Receptor, GUDCA Glycoursodeoxycholic acid, HCC hepatocellular carcinoma, MAPK mitogen-activated protein kinase, NF-κB nuclear factor κappa-light-chain-enhancer of activated B cells, PGE2 prostaglandin E2, PI3K Phosphatidylinositol 3-kinase, PKCα protein kinase C α, Prx2 peroxiredoxin II, RAF1 Raf-1 Proto-Oncogene, Serine/Threonine Kinase, ROS reactive oxygen species, Smac second mitochondria-derived activator of caspase, STAT3 signal transducer and activator of transcription 3, TUDCA Tauroursodeoxycholic acid, UDCA Ursodeoxycholic acid

Table 6.

Antitumor effects of bile acids other than UDCA in cancers

Cancer types	Cell lines	Concentration of bile acids	Effects of bile acids	Refs.
Breast cancer	MCF7, MDA-MB-231	LCA (50–200 µM)	LCA induces TGR5 expression and exhibits anti-proliferative and pro-apoptotic effects. LCA inhibits lipogenesis and reduces ERα expression in MCF7 cells	[10]
	MCF7, 4T1	LCA (0.3 µM)	LCA inhibits cell proliferation, EMT transition, VEGF production and induces antitumor immune response and elicits changes in metabolism through TGR5 receptor	[7]
	MCF7, 4T1	LCA (0.3 µM)	LCA induces NRF2/NFE2L2 dependent oxidative/nitrosative stress via TGR5/CAR receptors	[11]
	MCF7	CDCA (50 µM)	CDCA activates FXR receptor and inhibites Tamoxifen-resistant breast cancer cells proliferation and EGF-induced growth through downregulation of HER2 expression	[268]
	MCF7, MDA-MB-231	CDCA (30 µM)	CDCA induces cell death via activation of FXR	[334]
Colon cancer / Colorectal carcinoma	Caco-2, HT29C19A	LCA (20 µM)	LCA activates VDR to block inflammatory signals in colon cells	[335]
	HCT116	LCA (150–400 µM)	LCA activates p53 and promotes apoptosis by its bindig to MDM4 and MDM2, key negative regulators of p53	[336]
	HCT116	DCA, CDCA (500 µM)	DCA and CDCA induce apoptosis	[337]
	HCT116	DCA (200–250 µM)	DCA induces apoptosis via AP-1 and C/EBP mediated GADD153 expression	[338]
	HCT116	DCA (0.05–0.3 mM)	DCA in physiologically relevant dose inhibits cell growth and induces apoptosis	[242]
Gallbladder cancer (GBC)	NOZ, GBC-SD, EGH1	DCA (50–200 µM)	DCA functions as a tumor suppressive factor in GBC by interfering with miR-92b-3p maturation	[339]
Gastric cancer	SGC7901	DCA (0.1–0.3 mM)	DCA induces apoptosis via the mitochondrial-dependent pathway	[186]
	BGC-823	DCA (0.3 mM)	DCA inhibits the growth of gastric cancer cells via p53 mediated pathway	[185]
	SNU-216, MKN45	DCA (200 µM)	DCA induces MUC2 expression and inhibits tumor invasion and migration	[340]
Hepatocellular carcinoma (HCC)	HEPG2, L02	CDCA (10–50 µM)	CDCA reduces the expression of inflammation mediators, inhibits STAT3 phophorylation and increases expression of SOCS3 via FXR	[193]
	HepG2, Huh7, mouse hepatoma Hepa 1–6	CDCA (50–100 µM)	CDCA induces tumor suppressor N-Myc downstream regulated gene 2 (NDRG2) expression through FXR receptor	[194]
Neuroblastoma (NB)	SK-n-MCIXC, BE(2)-m17, SK-n-SH, Lan-1	LCA (100 µM)	LCA selectively kills the NB cell lines while sparing normal neuronal cells. LCA triggers intrinsic and extrinsic pathways of apoptosis	[8]
Ovarian cancer	OVCAR3	CDCA, DCA (10 µM)	CDCA and DCA upregulate BRCA1 and downregulate ER1 gene expression, which are important implications for disease penetrance and chemoprevention strategies in carriers of BRCA1 mutations	[281]
	A2780	CDCA, DCA (200–400 mM)	CDCA and DCA have significant cytotoxic activity via induction of apoptosis	[279]
Prostate cancer	LNCaP, PC-3	LCA (25–75 µM)	LCA inhibits the proliferation of cancer cells and induces apoptosis	[273]
	PC-3, DU145	LCA (3–50 µM)	LCA decreases cell viability, induces apoptosis as well as induces endoplasmic reticulum stress, autophagy and mitochondrial dysfunction	[9]
	LNCaP, DU145	CDCA (50 µM)	Activation of FXR by CDCA inhibits cell proliferation and lipid accumulation via SREBF pathway	[270]
	LNCaP	CDCA (5 µM)	FXR activation by CDCA inhibits cell growth via upregulation of PTEN	[271]

AP-1 activator protein-1, BRCA1 breast cancer type 1 susceptibility protein, CA Cholic acid, CAR constitutive androstane receptor, CDCA Chenodeoxycholic acid, C/EBP CCAAT/enhancer-binding protein beta, DCA Deoxycholic acid, EGF epidermal growth factor, EMT epithelial–mesenchymal transition, ER estrogen receptor, FXR Farnesoid X receptor, GADD153 growth arrest- and DNA damage-inducible gene 153, GBC Gallbladder cancer, GCDC Glycochenodeoxycholate, GDC Glycodeoxycholate, HER2 human epidermal growth factor receptor 2, LCA Lithocholic acid, MDM2 Mouse double minute 2, MDM4 Double Minute 4, MUC2 mucin 2, NB Neuroblastoma, NDRG2 N-Myc downstream regulated gene 2, NRF2 nuclear factor erythroid 2-related factor 2, NFE2L2 PTEN, phosphatase and tensin homolog, SOCS3 suppressor of cytokine signaling 3, SREBF sterol regulatory element-binding factor, STAT3 signal transducer and activator of transcription 3, TCA Taurocholic acid, TCDC Taurochenodeoxycholate, TDC Taurodeoxycholate, TGR5 G protein-coupled bile acid receptor 1, VEGF vascular endothelial growth factor, VDR vitamin D receptor

Table 7.

Tumor promoter effects of bile acids in cancers

Cancer types	Cell lines	Concentration of bile acids	Effects of bile acids	Refs.
Breast cancer	4T1	DC (100 µM)	DC promotes survival of breast cancer cells by elevating FLK-1 (KDR) and decreasing ceramide-mediated apoptosis of breast cancer progenitor cells	[341]
Cholangiocarcinoma	THLE-3	CDCA (100 µM) LCA (100 µM)	CDCA and LCA induce Snail and reduce E-cadherin expression and facilitate invasion and migration	[188]
	KMBC	TCDC, DC, GCDC (200 µM)	BAs participate in progression of cholangiosarcoma by activating EGFR and inducing COX-2 expression via MAPK cascade	[342]
	human: HuCCT1, CCLP1, SG231, rat: BDE1, BDEspTDEH10	TCA (100 µM)	TCA promotes cholangiosarcoma cell invasion via activation of S1PR2. TCA induces invasive growth of cells, upregulate COX2 expression and PGE2 production through S1PR2 receptor	[96] [95]
	RMCCA-1	TLCA	TLCA induces cell growth through muscarinic acetylcholine receptor (mAChR) and EGFR/ERK1/2 signaling pathways	[106]
Colon cancer / Colorectal carcinoma	HT29, SW620	LCA (30 µM)	LCA induces expression of urokinase-type plasminogen activator receptor (uPAR) and enhances cell invasiveness via ERK1/2 and AP-1 pathway	[343]
	H508, SNU-C4	LCT (300 µM)	LCT interacts with M3 muscarinic receptor and increases cell growth	[105]
	HCT-8/E11, SRC transformed PCmsrc cells	LCA, CDCA, DCA (10 µM)	BAs stimulate cellular invasion, which was dependent on several signaling pathways, such as RhoA, Rac1, PI3K, PKC, MAPK, COX2 and FXR receptor	[344]
	Normal human colonic epithelial cells (HCoEpiC)	LCA, DCA (100 µM)	BAs promote colon cancer by inducing cancer stemness in colonic epithelial cells via modulating CHRM3 and Wnt/β-catenin signaling	[238]
	CaCo-2	LCA (26.6 µM)	LCA increases cell invasion through promoting matrix metalloproteinase 2 (MMP-2) secretion	[345]
	HCT116, HT29	LCA (20 µM), DCA (150 µM)	BAs promote colon carcinogenesis via regulation of Nur77-mediated cell proliferation and apoptosis	[190]
	HCT116	LCA (30 µM)	LCA induces IL-8 expression by activating Erk1/2 MAPK and suppressing STAT3 Metformin inhibits LCA induced IL-8 upregulation in HCT116 cells by suppressing ROS production and NF-kB activity	[346] [347]
	SNU-C4, H508	GLCA, GDCA, (50–300 µM), DCA (300–1000 µM)	BAs induce colon cancer cell proliferation which is CHRM3-dependent and is mediated by transactivation of EGFR	[348]
	HCT116	DC (0.3–0.5 mM)	DC induces mitochondrial oxidative stress and activates NF-kB in cancer cells through multiple mechanisms involving NAD(P)H oxidase, Na+ /K+ -ATPase, CYP, Ca2+ and the terminal mitochondrial respiratory complex IV	[349]
	HT-29	DCA (250 µM)	DCA promotes colorectal tumorigenesis through activation of EGFR-MAPK pathway and induction of calcium signaling	[350]
	HT-29, Caco-2, HCA7, HCT116	DCA (300 µM)	DCA activates COX-2 signaling and mediates proliferation and invasiveness of colorectal epithelial cancer cells	[351]
	HCT-116, HCA-7	DCA (300 µM)	DCA activates EGFR, MAPK and STAT3 signaling and induces tumorigenicity. DCA-induced activation of cellular signaling is mediated by the TGR5	[226]
	SW480, LoVo	DCA (5–50 µM)	DCA activates β-catenin signaling and promotes colon cancer cell growth and invasiveness	[352]
	HCT116, DLD-1, SW620	DCA (100–200 µM)	DCA induces upregulation of EPHA2 in colon cancer cells, which is due to activation of ERK 1/2 cascade, and is p53-independent	[353]
	Caco-2	DCA (20 µM)	DCA stimulates colon cancer-cell migration via PKC	[354]
	Caco-2, HT-29	DC  < 20 µM  > 100 µM	Low-dose (< 20 µM) DC stimulates colon cancer cell proliferation, while high dose (> 100 µM) induces apoptosis in colon cancer cells	[355]
	HCT116	DCA (250 µM)	DCA stimulates pro-apoptotic and anti-apoptotic signaling pathways; sensitivity to DCA induces apoptosis can be modulated by the ERK/MAP kinase	[356]
	HCT116	DCA (200 µM)	DCA suppresses p53 by stimulating proteasome-mediated degradation of p53. DCA suppression of p53 is mediated by stimulating the ERK signaling pathway	[357]
	HM3	DCA (200 µM)	DCA upregulates MUC2 transcription via multiple pathways involving activation of EGFR/PKC/Ras/Raf-1/MEK1/ERK/CREB, PI3/Akt/IKKB/NF-κB and p38/MSK1/CREB while DCA induced MUC2 transcription is inhibited by JNK/c-Jun/AP-1 pathway	[358]
	HT-29	DCA (50–500 µM)	DCA induces oxidative stress and upregulates Thioredoxin reductase (TR) mRNA	[359]
	HT-29	DCA (50–200 µM)	DCA activates anti-apoptotic effect of NF-κB and induces IL-8 expression	[360]
	murine model	/	DCA and tauro-β-muricholic acid have major role in promoting cancer stem cell proliferation	[361]
Endometrial cancer	Ishikawa	CDCA (5 µM)	CDCA enhances cyclin D1 expression and promotes cancer cell proliferation through TGR5-dependent CREB signaling activation	[362]
Gastric cancer	Normal human gastric epithelial cell: GES-1	CDCA, DCA (200 µM)	BAs upregulate CDX2 and MUC2 expression via activation of FXR/NF-κB signaling pathway	[176]
	Normal human gastric epithelial cell: GES-1 gastric carcinoma cell lines (AGS, MKN45, BGC823, AZ521, N87, KATO III, SGC7901)	DCA (200 µM)	DCA activates TGR5-ERK1/2 pathway following induction of HNF4α expression, which further promotes metaplasia markers expression through direct regulation of KLF4 and CDX2	[181]
	AGS	DCA (50 µM)	DCA activates ERK1/2, MAPK and causes a TGR5-dependent trans-phosphorylation of the EGFR	[182]
	MKN74, MKN45	TLCA, TDCA (100 µM)	Activation of TGR5 by BAs promotes EMT process	[183]
	MKN45, AGS	DCA (100 µM)	DCA enhances COX-2 expression via CDX1 and SHP	[178]
	MKN28, MGC803, SGC7901	DCA, CDCA (100 µM)	BAs under acidic conditions increase TERT expression by activation of c-MYC transcription	[179]
Hepatocellular carcinoma (HCC)	HuH-7, Hep3B	CDCA (100 µM)	CDCA induces EMT phenotypes in HCC cells via FXR	[189]
	Huh7, Hep3B and mouse primary hepatocytes (MPH)	LCA (20 µM), DCA (150 µM)	BAs promote liver carcinogenesis via regulation of Nur77-mediated cell proliferation and apoptosis	[190]
	Huh-BAT, SNU-761, SNU-475	DCA (100 µM)	DCA induces ER stress accelerated apoptosis in NTCP-positive HCC cells under hypoxic conditions, while DCA induces COX-2-dependent IL-8 overexpression in NTCP-negative human HCC cells mediated by NFκB	[191]
	SMMC7721, Huh7	GCDC (200 µM)	GCDC promotes HCC invasion and migration by AMPK/mTOR dependent autophagy activation	[363]
	HepG2, BeL-7402, Huh7	GCDA (100 µM)	GCDA contributes to the development of HCC and chemoresistance by inducing MCL1 phosphorylation at T163 via ERK1/2, which stabilizes MCL1 protein to enhance its antiapoptotic function	[364]
	HepG2, Bel7402, QGY7703, SMMC7721, Huh7	GCDA (100 µM)	GCDA induces survival and chemoresistance of liver cancer cells through activation of BCL-2 by phosphorylation	[365]
	LX2, Huh7	DCA (20–80 µM)	DCA causes HSC senescence by modulating malignant behavior of HCC	[192]
	HepG2	TCDCA (100 µM)	TCDCA promotes liver cancer via downregulation of the expression of tumor suppressor gene CEBPα	[366]
	Hep3B	LCA, CDCA (100 µM)	BAs increase cancer invasiveness in human hepatocellular carcinoma and cholangiocarcinoma through repressing E-cadherin and inducing Snail expression	[188]
Hypopharyngeal squamous cell carcinoma	FaDu cells	CA (100 µM), CDCA (100 µM), DCA (100 µM), LCA (20 µM)	BAs induce EMT markers TGFβ1 and MMP-9 in vitro	[367]
Non-small cell lung cancer (NSCLC)	H1975, H1299, PC-9, A549	DCA (20–40 µM)	DCA increases cell migration and invasion through a TGR5-dependent way. TGR5 promotes NSCLC cell proliferaton and migration via JAK2/STAT3 pathway	[368]
Oesophageal adenocarcinoma (EAC) / Barett’s esophagus	HET-1A	DCA (300 µM), CDCA (300 µM), LCA (25 µM)	BAs activate the unfolded protein response and induce Golgi fragmentation via a src-kinase dependant mechanism contributing to cancer progression in the oesophagus	[369]
	SEG-1, BE3 CPC-A, CPC-C	CDCA (100–300 µM)	CDCA induces activation of IKKβ/TSC1/mTOR pathway leading to enhanced EAC cell proliferation	[370]
	OE-33, SK-GT-4	CDCA (100 µM)	CDCA stimulates the development of human esophageal cancer by promoting angiogenesis via the COX2 pathway	[371]
	HET-1A, QH	DCA (100–300 µM)	DCA promotes development of gastroesophageal reflux disease and Barrett’s oesophagus by modulating integrin-αν trafficking	[372]
	OE19, OE33	DCA (100, 300 µM)	DCA inhibits Notch signaling pathway with induction of CDX2 gene expression contributing to the formation of Barrett’s oesophagus	[373]
	OE19	DCA (300 µM)	DCA shows carcinogenic effects via upregulation of COX2, CDX2 and downregulation of DNA repair enzymes (MUTYH, OGG1)	[374]
	OE-19, OE-33	TCA (100 µM)	TCA promotes invasive growth of EAC cells via S1PR2	[165]
	OE19	DCA (50–300 µM)	DCA promotes the progression of EAC by inducing inflammation	[375]
	HET-1A, CP-A, CP-C, OE33	DCA (0.2 mM)	DCA increases Beclin-1/BECN1 expression and autophagy but chronic exposure to BAs leads to decreased Beclin-1/BECN1 expression and autophagy resistance	[376]
	BAR-T	DCA (250 µM)	DCA induces ROS/RNS production, which causes genotoxic injury, and simultaneously induces activation of the NF-κB pathway, which enables cells with DNA damage to resist apoptosis	[377]a
	OE33, KYSE-30	DCA (100–200 µM)	DCA is genotoxic to oesophageal cells at neutral and acid pH through the induction of ROS	[378]
		DCA ≥ 100 µM	DCA induces DNA damage and NF-kB activation (at doses of 100 uM and higher in oesophageal OE33 cells)	[379]
	SEG-1, SKGT-4, CP-A	CDCA, DCA (100 µM, 200 µM)	BAs induce CREB and AP-1-dependent COX2 expression in Barrett’s oesophagus and EAC through ROS-mediated activation of PI3K/AKT and ERK1/2	[380]
	Het-1A, SEG-1, HKESC-1, HKESC-2	DCA (100–1000 µM)	DCA upregulates both intestinal differentiation factor CDX2 and goblet cell-specific gene MUC2 in normal esophageal and cancer cell lines suggesting the involvement of DCA in the pathogenesis of Barrett esophagus	[381]
	SEG-1 cells	DCA (50–300 µM)	DCA induces MUC2 overexpression by activation of NF-kB transcription through a process involving PKC-dependent but not PKA, independent of activation of MAP kinase	[382]
	SKGT-4	DCA (300 µM)	DCA induces COX2 expression via Erk1/2, p38-MAPK and AP-1-dependent mechanisms	[383]
	OE33 cells	DCA (250 µM)	DCA promotes the expression of KLF4 and OCT4 via IL-6/STAT3 signaling pathway. DCA has a malignancy-inducing effect on the transformation of EAC stem cells	[384]
	BAR-T, OA, FLO	TDCA (10−11 M)	TDCA induces cell proliferation through the upregulation of NOX5-S expression and ROS production mediated by activation of the TGR5 receptor	[164]
	OE33, FLO-1, Esc2	DCA (100 µM)	DCA enhances the aggressive phenotype of EAC cells with concomitant metabolic changes occurring via downregulation of UCP2	[385]
Pancreatic cancer	T3M4, HPAF, Capan-1	DCA, CDCA (5–100 µM)	BAs increase the tumorigenic potential of pancreatic cancer cells by inducing FXR/FAK/c-Jun axis to upregulate MUC4 expression	[386]
	BxPC-3, AsPC-1, Capan-2	DCA (300 µM)	DCA activates EGFR, MAPK and STAT3 signaling and induces tumorigenicity. DCA-induced activation of cellular signaling is mediated by the TGR5	[226]

AKT Serine/Threonine Kinase 1, AMPK AMP-activated protein kinase, AP-1 activator protein-1, BA bile acid, Bcl-2 B-cell lymphoma 2, Beclin-1/BECN1 Coiled-Coil Myosin-Like BCL2-Interacting Protein, CDCA chenodeoxycholic acid, CDX1 Caudal Type Homeobox, CDX2 Caudal Type Homeobox 2, CEBPα CCAAT/enhancer-binding protein alpha, CHRM3 Muscarinic Acetylcholine Receptor M3, COX2 cyclooxygenase-2, CREB cAMP response element-binding protein, DC Deoxycholate, DCA Deoxycholic acid, EAC Oesophageal adenocarcinoma, EGFR epithelial growth factor receptor, EMT epithelial-mesenchymal transition, EPHA2 EPH Receptor A2, ERK extracellular signal-regulated kinase, FAK/PTK2 focal adhesion kinase, FLK1/KDR Fetal liver kinase 1/Kinase Insert Domain receptor, FXR farnesoid X receptor, GCDA Glycochenodeoxycholate acid, GCDC Glycochenodeoxycholate, GDCA Glycodeoxycholic acid, GLCA Glycolithocholic acid, HCC hepatocellular carcinoma, HNF4α hepatocyte nuclear factor-4α, HSC hepatic stellate cells, IKKβ/IKBKB Inhibitor Of Nuclear Factor Kappa B Kinase Subunit Beta, IL1 interleukin 1, IL6 interleukin 6, IL8/CXCL8 interleukin 8, JAK2 Janus kinase 2, JNK c-Jun N-terminal kinase, JUN Jun Proto-oncogene, AP-1 Transcription Factor Subunit, KLF4 Kruppel Like Factor 4, LCA Lithocholic acid, LCT Lithocholyltaurine, mAChR muscarinic acetylcholine receptor, MAPK/MEK mitogen-activated protein kinase, MCL1 Induced myeloid leukemia cell differentiation protein, MMP2 matrix metalloproteinase 2, MMP9 matrix metalloproteinase-9, MSK1/RPS6KA5 Nuclear Mitogen- And Stress-Activated Protein Kinase 1, mTOR mammalian/mechanistic target of Rapamycin, MUC2 Mucin 2, MUC4 Mucin 4, MUTYH MutY DNA Glycosylase, MYC Myc Proto-Oncogene Protein, NF-κB nuclear factor κB, NOX5 NADPH Oxidase 5, NR4A1/Nur77/TR3/NGFIB Nuclear receptor subfamily 4 group A member 1, NSCLC non-small cell lung cancer, NTCP/SLC10A1 sodium/taurocholate cotransporting polypeptide, OCT4/POU5F1 Octamer-Binding Transcription Factor, OGG1 8-Oxoguanine DNA Glycosylase, p38/MAPK14 p38 MAP Kinase, PGE2 prostaglandin E2, PI3K Phosphatidylinositol 3-kinase, PKA protein kinase A, PKC protein kinase C, Rac1 Rac Family Small GTPase 1, Raf1 Proto-Oncogene, Serine/Threonine Kinase, RhoA Ras Homolog Family Member A, RNS reactive nitrogen species, ROS reactive oxygen species, S1PR2 sphingosine 1-phosphate receptor 2, SHP Small heterodimer partner, STAT signal transducer and activator of transcription, TCA Taurocholic acid, TCDC Taurochenodeoxycholate, TCDCA Taurochenodeoxycholic acid, TDCA Taurodeoxycholic acid, TERT Telomerase Reverse Transcriptase, TGF-β1 Transforming growth factor β-1, TGR5/GPBAR1 G-protein-coupled bile acid receptor/Takeda-G-protein-receptor-5, TLCA Taurolithocholic acid, TSC1 TSC Complex Subunit 1, TXNRD1 Thioredoxin reductase 1, UCP2 uncoupling protein-2, uPAR/PLAUR urokinase-type plasminogen activator receptor, WNT wingless-type MMTV integration site family

Oesophageal carcinoma

The development of Barrett’s esophagus (BE) and its progression to oesophageal adenocarcinoma (EAC) are linked to gastroesophageal reflux disease (GERD). Conjugated BAs, mainly taurocholic acid (TCA) and glycocholic acid (GCA) are the main BA constituents in GERD refluxate [162]. Conjugated BA levels in the refluxate from patients with advanced BE or EAC are significantly higher than from patients with benign BE [163]. Conjugated BAs, as TCA or taurodeoxycholic acid (TDCA), promote EAC progression [164, 165] (Table 7). Unconjugated BAs, including DCA and CDCA, induce oxidative stress, DNA damage and inflammation contributing to EAC carcinogenesis, while UDCA protects against DCA-induced injury (Tables 5 and 7).

Apparently, numerous BA receptors as TGR5, S1PR2, FXR and VDR are activated in EAC cells in response to BAs in the refluxate [164–167]. In good agreement with that, the inhibition of the FXR receptor suppresses tumor cell viability in vitro and reduced tumor formation in nude mouse xenografts [168]. Furthermore, TGR5 is highly expressed in the EAC and precancerous lesions and is associated with worse overall survival [169] suggesting that these observations can be translated to the human situation.

Acidic bile acids bring about oxidative stress, TDCA can induce NADPH Oxidase 5 (NOX5) through TGR5 [164]. Furthermore, bile acids can induce inflammation through FXR activation [170] and the EGFR–STAT3 (signal transducer and activator of transcription 3)—Apurinic/Apyrimidinic Endodeoxyribonuclease 1 (APE1) pathway [171]. Acidic bile salts can also induce epithelial–mesenchymal transition (EMT) through vascular endothelial growth factor (VEGF) signaling in Barrett's cells [172]. Interestingly, the activation of the EGFR-DNA-PKs (DNA-dependent protein kinase) pathway by insulin-like growth factor binding protein 2 (IGFBP2) protects EAC cells against acidic bile salt-induced DNA damage [173].

Gastric cancer

Carcinogenesis in gastric cancer is a sequential process that includes chronic superficial gastritis, intestinal metaplasia (IM), atrophic gastritis, intramucosal carcinoma, dysplasia and invasive neoplasia [174]. IM is considered a risk factor for gastric tumorigenesis. The concentrations of BAs in gastric juice positively correlate with the degree of intestinal metaplasia [175] and BAs serve a critical multipronged role in the induction of intestinal metaplasia. BAs can enhance caudal-related homeobox family 2 (CDX2) and mucin 2 (MUC2) expression via FXR/NF-κB signaling [176, 177] and cyclooxygenase-2 (COX-2) expression via induction of SHP [178], all promoting gastric intestinal metaplasia. Acidic bile salts can induce telomerase activity in a c-Myc-dependent fashion [179, 180], while DCA can induce the metaplastic phenotype of gastric cancer cells [181] (see Tables 6 and 7). TGR5 is a key factor in BA-induced gastric metaplasia via HNF4α [181], EGFR and mitogen-activated protein kinase (MAPK) [182] activation and promotes EMT in gastric carcinoma cells [183]. TGR5 is overexpressed in gastrointestinal adenocarcinomas, and moderate to strong TGR5 staining is associated with decreased patient survival [184]. Nevertheless, there anticarcinogenic effects of bile acids in gastric cancer, as UDCA (Table 5) or DCA in supraphysiological concentrations [185, 186] or 23(S)-mCDCA [187].

Hepatocellular carcinoma (HCC)

Several studies have shown that more hydrophobic BAs as LCA, DCA and CDCA, are the main promoters of liver cancer and can contribute to the development of HCC (see in Table 7) [188–192]. Nevertheless, CDCA (> 100 µM) [193, 194], UDCA and Tauroursodeoxycholic acid (TUDCA) inhibit HCC cell growth and induce apoptosis [195–199] (see in Tables 5 and 6). Deregulation of BA homeostasis marked by the expression of hepatic BA transporters (BSEP, OSTα/β, MRP2, MDR2-3, NTCP) is diminished leading to increased hepatic BA sequestration and inflammation and reduced FXR signaling [200–203] in liver cirrhosis and nonalcoholic steatohepatitis that are risk factors for the development of HCC. In good agreement with that, metabolomics identified long-term elevated serum BAs in HCC patients [204] and children (< 5 years of age) with bile salt export pump deficiency developed HCC [205].

FXR activity is a major inhibitor of HCC carcinogenesis. Whole-body FXR-deficient mice spontaneously develop liver tumors [206, 207] in which the activation of the Wnt/β-catenin signaling pathway and oxidative stress were identified as the major drivers [208–210]. Nevertheless, liver-specific FXR deficiency in mice does not induce spontaneous liver tumorigenesis, but may only serve as a tumor initiator [211]. Due to their amphipathic nature, BAs can disrupt the plasma membrane and activate protein kinase C (PKC) and phospholipase A2 (PLA2) inducing the p38-MAPK-p53-NFκB pathway [212, 213]. Inflammation can suppress FXR activity that contributes to bile acid accumulation and carcinogenesis [185, 193, 194, 214].

Interestingly, senescence-associated secretory phenotype has crucial role in promoting obesity-associated HCC development in mice. Administration of high-fat diet to mice induces alterations in the gut microbiota and increases the levels of DCA. Increased DCA level promotes SASP phenotype in hepatic stellate cells (HSCs), which in turn secretes various tumor-promoting factors in the liver, thus facilitating HCC development in mice exposed to chemical carcinogen [6]. SHP has a pleiotropic role in HCC, regulates cell proliferation [215], apoptosis [216], epigenetic changes [217] and inflammation [200, 218], which are associated with the antitumor role of SHP in the development of liver cancer.

Pancreatic adenocarcinoma

BAs are involved in the induction and development of pancreatic adenocarcinoma at multiple stages. Gallstone formation can block bile flow and, therefore, can induce and sustain pancreatitis [219], a risk factor for pancreatic adenocarcinoma [220–222]. In fact, several BA species showed a drastic increase in pancreatic adenocarcinoma patients [223]. Treatment of pre-malignant pancreas ductal cells with bile induced carcinogenic transformation [224, 225]. In pancreatic adenocarcinoma cells BAs decrease susceptibility to apoptosis, boost cell cycle progression, the expression of inflammatory mediators and cellular movement, and, in high concentrations, may perturb biomembranes (Table 7) [220, 226]. UDCA, similar to its previously discussed beneficial properties, prevents EMT in pancreatic adenocarcinoma cell lines and, therefore, has antineoplastic properties (Table 5) [227].

Colorectal carcinoma (CRC)

The western diet has tumor promoting activity associated with elevated concentrations of colonic BA (mainly LCA and DCA) and increased fecal BA levels, as detected in samples from CRC patients [228]. In animals, a high-fat diet stimulates bile discharge and results in elevated BA levels in the colon [229]. Moreover, cholecystectomy, through prolonging BA exposure of the intestinal mucosa, has been suggested as a risk factor for the development of CRC [230].

BAs induce genetic instability marked by genomic instability and DNA damage via oxidative stress, defects in mitotic checkpoints, cell cycle arrest, improper chromosome alignment and multipolar division [231, 232]. Genomic instability caused by BAs is coupled with apoptosis resistance due to the degradation of p53 and the inhibition of caspase-3 activity [233]. Furthermore, secondary BAs perturb cell membranes and modulate signaling cascades [234, 235]. These all lead to colonic cell hyperproliferation, survival and invasion [236, 237].

The disruptive effect of BAs on colon epithelium evokes a compensatory cell renewal mechanism by inducing colonic epithelial cells to become cancer stem cells (CSCs) through β-catenin signaling (Table 7) [238]. In the CRC rodent model, both LCA and DCA have tumor promoter role on colonic crypt cells in the early stages of colon carcinogenesis [239]; however, it is important to note that BAs are suggested as tumor promoters, but not as mutagenic agents, since they can not induce tumor formation without a carcinogen/mutagen or a genetic alteration [240, 241]. It should be noted that DCA in low concentrations (0.05–0.3 mM) inhibit colonic cell proliferation via cell cycle block and apoptosis pathways (Table 6) [242].

UDCA can reduce the concentration of toxic BA in stool and blood [243] and has shown to protect against CRC by inhibiting CSC and CRC cell formation and proliferation [244, 245], oncogenic signaling pathways [246], as well as, inducing tumor surveillance [247] (Table 5). Moreover, UDCA can reduces CRC recurrence [248], as well as the risk to develop CRC in patients with pre-cancerous conditions, as colitis [249] or primary biliary cirrhosis [250].

Sustained inflammation was implicated in the pathogenesis of colorectal cancer due to barrier breach, and bacterial translocation leading to inflammation and neoplastic transformation of colonic epithelial cells [251–253]. TGR5 activation by UDCA and LCA may also exert anti-inflammatory responses through TLR4 activation or by reducing pro-inflammatory cytokine production in the colon that can decrease the frequency of developing CRC [254]. BAs can change the gut microbial community [255, 256], suggesting that BAs may also interfere with bacterial translocation.

Breast cancer

The BAs in the breast are of gut origin [257, 258]. Hepatic production of BA is reduced in breast cancer patients as marked by decreasing levels of serum and fecal BAs [7, 259]. Furthermore, bacterial conversion of BAs to secondary BAs is also suppressed, which is the most dominant in in situ and stage I patients [7]. The serum bile acid composition of breast cancer and benign breast disease patients is different; specifically, breast cancer patients had higher serum chenodeoxycholic acid levels and lower dihydroxy tauro-conjugated BA (Tdi-1) and sulfated dihydroxy glyco-conjugated bile acids (Gdi-S-1) [260]. Total fecal bile acid levels are lower in breast cancer patients as compared to controls [259]. LCA concentrations in the breast can be higher than the serum levels [261] (Table 6). Reports showed increased DCA levels in the serum [262] and the breast cyst fluid [263] of breast cancer patients.

LCA is an inhibitor of breast cancer cell proliferation (Table 6) [7, 258, 264]. However, the reports on DCA and UDCA are contradictory [7, 258, 262–264] in physiological concentrations, LCA tunes cancer cell metabolism towards a more oxidative state (through AMP-activated protein kinase (AMPK), PGC-1β and NRF1/NFE2L1) and induces mild oxidative stress through reducing NRF2 (nuclear factor erythroid 2-related factor 2, NFE2L2) expression and inducing Inducible nitric oxide synthase (iNOS) that reverts EMT, reduces VEGF expression, induces antitumor immunity and changes to cancer metabolism that culminates in reduced metastasis formation [7, 11]. In supraphysiological concentrations (> 1 µM) LCA inhibits fatty acid biosynthesis [10] and induces cell death [8–10, 265, 266]. LCA does not exert antiproliferative effects in its tissue reference concentrations on non-transformed primary fibroblasts [7]. LCA exerts its antineoplastic effects through the TGR5 [7] (Table 6).

CDCA in supraphysiological concentrations induces MDRs through FXR [265] and modulates estrogen and progesterone receptor-mediated gene transcription [267]. Furthermore, CDCA inhibits tamoxifen-resistant breast cancer cell proliferation through the activation of the FXR receptor [268] (Table 6). In contrast to that, a report by Journe and colleagues [269] showed that FXR activation has a positive correlation with estrogen receptor expression and luminal characteristics, as well as supported cancer cell proliferation.

Prostate cancer

Among the BAs LCA, UDCA and CDCA exerted antiproliferative effects in prostate cancer. Activation of FXR by CDCA inhibits proliferation of prostate cancer cells, reduces lipid anabolism via inhibiting Sterol Regulatory Element Binding Transcription Factor 1 (SREBF1) [270] and induces the expression of the tumor suppressor phosphatase and tensin homolog (PTEN) [271] (Table 6). Interestingly, FXR signaling also controls androgen metabolism in prostate cancer cells, its activation reduces the expression of UDP-glucuronosyltransferase (UGT) 2B15 and UGT2B17 within cells and causes a reduction of androgen glucuronidation [272]. Similar to CDCA, LCA has antiproliferative effects in prostate cancer and induces apoptosis, endoplasmic reticulum stress, autophagy and mitochondrial dysfunction [9, 273] (see Table 6). UDCA induces death receptor-mediated apoptosis in human prostate cancer cells [274] (Table 5).

Ovarian cancer

In the serum of ovarian cancer patients, 3b-hydroxy-5-cholenoic acid, GUDCA, DCA and TCDCA levels decreased [275, 276]; importantly, taurochenodeoxycholic acid levels decreased in early-stage epithelial ovarian cancer [276]. Zhou and colleagues have shown that sulfolithocholylglycine and TCA showed changes in the serum of ovarian cancer patients [277]. Changes to the BA pool are so characteristic that Guan and colleagues suggested [278] a set of 12 BAs, including glycolithocholic acid, to be used as markers to separate healthy controls from ovarian cancer patients.

The available studies assessed the effects of BAs at supraphysiological concentrations. These concentrations of BAs are cytotoxic and induce apoptosis likely due to changes to membrane damage [279, 280] that is unlikely at physiological concentrations of BAs [7]. DCA can modulate the expression of breast cancer type 1 susceptibility protein (BRCA1) and the estrogen receptor and, through these, can control drug sensitivity of ovarian cancer cells (Table 6) [281]. Furthermore, cholylglycinate interferes with the transport of cisplatin [282] and TCDC sensitizes ovarian carcinoma cells to doxorubicin and Mitomycin [280].

LXR [283–285], PXR [286], VDR [287–296] or CAR [297, 298] activation was shown to exert protective features against ovarian cancer, similar to BA-elicited effects suggesting that BAs may have a more profound role in protecting against ovarian cancer. These protective effects involved the suppression of proliferation [283, 284, 286], invasion [291], EMT [288], de novo fatty acid biosynthesis [295], the proportions of the cancer stem cell population [289], and the improvement of the efficacy of chemotherapy [285, 297, 298] culminating in better patient survival [292, 293]. Conflicting with these observation on report provided evidence that under certain conditions PXR may support proliferation [299]. BAs can influence the expression and the activity of multiple PARP enzymes [300]; therefore, it is likely that BAs could modulate the efficacy of PARP inhibition that is a novel modality in the chemotherapy of ovarian cancer.

Conclusions

Primary and secondary BAs are long-standing players in carcinogenesis. Although these molecules were considered as initiators of neoplasias, recent advances have shown that the pro- or anticarcinogenic activity of BAs varies among neoplasias [301], most probably due to differences in the expression of BA receptors, transporters and cell-specific differences in the outcome of receptor activation. Key pathways activated in neoplasias by BAs are regulated by nuclear receptors, FXR, CAR, SHP, PXR, LXR and VDR and other membrane receptors such as S1PR2, TGR5, CHRM2 and CHRM3. They activate numerous downstream signaling pathways such as EGFR, STAT3, MAPK, HNF4α, NF-κB, TLR4, SOCS3 and β-catenin just to name some. Furthermore, BAs regulate all aspects of tumor development and progression, the EMT, invasion, metabolism, apoptosis, proliferation, senescence, immune environment and response to chemotherapy.

The effect of BAs on neoplasias also depends on the concentrations used in the studies. While in certain models BAs in low concentration have anti-cancer effects, in superphysiological concentrations BAs have pro-cancer effects. This phenomenon is related to their amphipathic structure and the activation of additional off-target pathways not tiggered at physiological concentration. At high concentrations, BAs may perturb membranes and activate signaling pathways that sense disturbance of membranes, such as PLA2 and PKC. At high concentrations, they are also toxic and activate the detoxifying pathways, which regulate the activity of transporters of steroid hormones and chemotherapeutics. Therefore, we would urge the community to carry out studies where the concentrations of BAs correspond to the reference concentrations established for the tissue or, as a proxy, to the serum reference concentrations. As a continuation of that, in the case of UDCA the therapeutic serum concentrations can also be used as a guide. These data are summarized in Table 1. Such studies would be invaluable to understand the (patho)physiological roles of BAs and would give a good frame for the therapeutic applicability.

Along the same lines, it is apparent that BAs can be considered as possible treatment options in certain cancers. Foremost, UDCA, that is a therapeutically available drug, has beneficial effects in multiple neoplasias (e.g. [227, 248, 302], Table 5) pointing towards the possibility for repurposing UDCA. The picture for other BAs is hazier due to frequent contradictions making it hard to outline applicability. However, before the application of BAs in neoplasias we would need to decipher the cross-talk between BAs and drug metabolism, the effect on drug efficacy and drug availability, and discover the possible adverse effects of BAs, that is currently largely missing. Moreover, it is tempting to consider the manipulation of the intestinal microbiome to affect the levels of selected secondary bile acids in humans. Finally, the modulators of BA receptors should be considered as therapeutic options as well. Given the emerging evidence on the potential anti-cancer effects of BAs, further studies are vital in order to develop novel therapeutic strategies using BAs.

Search strategy and selection criteria

References to this review were identified through the prior knowledge of the authors that was complemented by systematic search of PubMed by using the combinations “Prostate cancer AND (bile acid)”, “Gastric cancer AND (bile acid)”, “Hepatocellular carcinoma AND (bile acid)”, “Oesophageal cancer AND (bile acid)”, “(bile acid) receptors AND cancer”, “(bile acid) receptors AND prostate cancer”, “(bile acid) receptors AND gastric cancer”, “(bile acid) receptors AND hepatocellular carcinoma”, “(bile acid) receptors AND oesophageal cancer”, "(bile acid) AND ABC AND transporter", "(bile acid) AND SLC AND transporter", "(bile acid) AND SLCO AND transporter", "(bile acid) AND transport AND review", “Farnesoid X receptor (FXR) AND the cancer types assessed in the study”, “Pregnane X receptor (PXR) AND the cancer types assessed in the study”, “Constitutive androstane receptor (CAR) AND the cancer types assessed in the study”, “Vitamin D receptor (VDR) AND the cancer types assessed in the study” “Liver X receptor (LXR) AND the cancer types assessed in the study”, “Small heterodimer partner (SHP) AND the cancer types assessed in the study”. Articles published in English were included with no restriction on publication date. All references were checked at Pub Peer, two papers were flagged ([215] and [156]), but when reviewing the reports we decided that the issues raised do not impact on the main message and kept the references.

Abbreviations

AKT

Serine/threonine kinase 1

AMPK

AMP-activated protein kinase

AP-1

Activator protein-1

APE1

Apurinic/apyrimidinic endodeoxyribonuclease 1

ATG5

Autophagy related 5

BA

Bile acids

Bai

Bile acid inducible operon

Bax

Bcl-2-associated X protein

Bcl-2

B-cell lymphoma 2

BE

Barrett’s esophagus

Beclin-1/BECN1

Coiled-coil myosin-like BCL2-interacting protein

BIRC7/Livin

Baculoviral IAP repeat-containing protein 7

BSEP/ABCB11

ATP-dependent cassette transporter

BSH

Bile salt hydrolases

BRCA1

Breast cancer type 1 susceptibility protein

CA

Cholic acid

cAMP

Cyclic adenosine monophosphate

CAR/NR1H3

Constitutive androstane receptor

CDCA

Chenodeoxycholic acid

CDX1/2

Caudal type homeobox 1/2

C/EBPα

CCAAT/enhancer-binding protein alpha

CHRM2/3

Muscarinic receptor 2/3

c-Myc

Myc-related translation/localization regulatory factor

COX2

Cyclooxygenase-2

CRC

Colorectal carcinoma

CREB

CAMP response element-binding protein

CSC

Cancer stem cells

CYP

Cytochrome P450

CYP7A1

Cholesterol 7α-hydroxylase

CYP7B1

25-Hydroxycholesterol 7α-hydroxylase

CYP8B1

Sterol 12α-hydroxylase

CYP27A1

Sterol 27-hydroxylase

CYP3A4

Cytochrome P450 family 3 subfamily

DC

Deoxycholate

DCA

Deoxycholic acid

Dlc1

Deleted in Liver Cancer 1

DNA-PK

DNA-dependent protein kinase

DR5

Death receptor 5

EAC

Oesophageal adenocarcinoma

EGF

Epidermal growth factor

EGFR

Epithelial growth factor receptor

EMT

Epithelial–mesenchymal transition

EPHA2

EPH Receptor A2

ER

Estrogen receptor

ERK

Extracellular signal-regulated kinase

FAK/PTK2

Focal adhesion kinase

FAS

Fas Cell Surface Death Receptor

FGF19

Fibroblast growth factor 19

FGF15

Fibroblast growth factor 15

FGFR4

Fibroblast growth factor receptor 4

FLK1/KDR

Fetal liver kinase 1/Kinase Insert Domain receptor

FXR/ NR1H4

Farnesoid X receptor

FXREs

FXR response elements

GADD153

Growth arrest- and DNA damage-inducible gene 153

GBC

Gallbladder cancer

GERD

Gastroesophageal reflux disease

GCA

Glycocholic acid

GCDCA

Glycochenodeoxycholic acid

GCDA

Glycochenodeoxycholate acid

GCDC

Glycochenodeoxycholate

GDC

Glycodeoxycholate

GDCA

Glycodeoxycholic acid

GLCA

Glycolithocholic acid

GPBAR1/TGR5

G-protein-coupled bile acid receptor/Takeda-G-protein-receptor-5

GUDCA

Glycoursodeoxycholic acid

HCC

Hepatocellular carcinoma

HDCA

Hyodeoxycholic acid

HER2

Human epidermal growth factor receptor 2

HNF4α

Hepatocyte nuclear factor-4α

HSC

Hepatic stellate cells

I-BABP

Intestinal BA-binding protein

IGFBP2

Insulin-like growth factor binding protein 2

IKKβ/IKBKB

Inhibitor Of Nuclear Factor Kappa B Kinase Subunit Beta

IL1

Interleukin 1

IL6

Interleukin 6

IL8/CXCL8

Interleukin 8

iNOS

Inducible nitric oxide synthase

JAK2

Janus kinase 2

JNK

C-Jun N-terminal kinase

JUN

Jun Proto-Oncogene AP-1 Transcription Factor Subunit

KLF4

Kruppel Like Factor 4

LBD

Ligand-binding domain

LCA

Lithocholic acid

LCT

Lithocholyltaurine

LOD

Limit of detection

LRH-1/NR5A2

Liver receptor homolog-1

LXRα/β/NR1H3-2

Liver X receptor

mAChR

Muscarinic acetylcholine receptor

MAPK/MEK

Mitogen-activated protein kinase

MCA

Muricholic acid

MCL1

Induced myeloid leukemia cell differentiation protein

MDM2

Mouse double minute 2

MDM4

Double Minute 4

MDR1/ ABCB1

Multidrug resistance protein 1

MMP2

Matrix metalloproteinase 2

MMP9

Matrix metalloproteinase 9

MRP2/ABCC2

Multidrug resistance-associated protein 2

MRP3/ABCC3

Multidrug resistance-associated protein 3

MRP4/ABCC4

Multidrug resistance-associated protein 4

MSK1/RPS6KA5

Nuclear mitogen- and stress-activated protein kinase 1

mTOR

Mammalian target of rapamycin

mTORC1

Mammalian target of rapamycin complex 1

MUC2

Mucin 2

MUC4

Mucin 4

MUTYH

MutY DNA Glycosylase

MYC

Myc proto-oncogene protein

NB

Neuroblastoma

NDRG2

N-Myc downstream regulated gene 2

ND

Not detected

NF-κB

Nuclear factor κappa-light-chain-enhancer of activated B cells

NOX5

NADPH Oxidase 5

NR

Nuclear receptor

NRF2/NFE2L2

Nuclear factor erythroid 2-related factor 2

NR4A1/Nur77/TR3/NGFIB

Nuclear receptor subfamily 4 group A member 1

NSCLC

Non-small cell lung cancer

NTCP/SLC10A1

Sodium/taurocholate cotransporting polypeptide

OATP1A2/SLCO1A2

Solute carrier organic anion transporter family member 1A2

OATP1B/SLCO1B

Solute carrier organic anion transporter family

OATP2

Organic anion-transporting polypeptide

OCT4/POU5F1

Octamer-binding transcription factor

OGG1

8-Oxoguanine DNA glycosylase

PGC-1α

Peroxisome proliferator-activated receptor gamma coactivator 1 alpha

PGE2

Prostaglandin E2

PI3K

Phosphatidylinositol 3-kinase

PKA

Protein kinase A

PKC

Protein kinase C

PLA2

Phospholipase A2

Prx2

Peroxiredoxin II

PXR/ NR1H2

Pregnane X receptor

PTEN

Phosphatase and tensin homolog

p38/MAPK14

P38 MAP kinase

Rac1

Rac family small GTPase 1

Raf1

Proto-oncogene, serine/threonine kinase

RhoA

Ras homolog family member A

RNS

Reactive nitrogen species

ROS

Reactive oxygen species

RXR

Retinoid X receptor

S1PR2

Sphingosine-1-phosphate receptor 2

SHP/ NR5O2

Small heterodimer partner

SLC10A1/NTCP

Solute carrier family 10

SLC10A2/ASBT

Sodium-dependent bile acid transporter

SLC51A/B or OSTα/β

Solute carrier family members

SRC-1/NC0A1

Steroid receptor coactivator 1

Smac

Second mitochondria-derived activator of caspase

SOCS3

Suppressor of cytokine signaling 3

SphK2

Sphingosine kinase 2

SRC-1/NC0A1

Steroid receptor coactivator 1

SREBF

Sterol regulatory element-binding factor

STAT3

Signal transducer and activator of transcription 3

SULT

Sulfotransferase

TCA

Taurocholic acid

TCDC

Taurochenodeoxycholate

TCDCA

Taurochenodeoxycholic acid

TDC

Taurodeoxycholate

TDCA

Taurodeoxycholic acid

TERT

Telomerase Reverse Transcriptase

TGF-β1

Transforming growth factor β-1

TLC

Taurolithocholate

TLCA

Taurolithocholic acid

TLR4

Toll-Like Receptor 4

TSC1

TSC Complex Subunit 1

TUDCA

Tauroursodeoxycholic acid

UCP2

Uncoupling protein-2

UDCA

Ursodeoxycholic acid

UGT

UDP-glucuronosyl-transferase

UGT2B4

Uridine 5′-diphosphate-glucuronosyltransferase 2B4

uPAR/PLAUR

Urokinase-type plasminogen activator receptor

VDR/NR1H1

Vitamin D receptor

VEGF

Vascular endothelial growth factor

WNT

Wingless-type MMTV integration site family

Author contributions

Writing and revising the manuscript: TR, DR, TK, PK, AS, PB, EM. Visualization: TR, AS.

Funding

Open access funding provided by University of Debrecen. Our work was supported by grants from the NKFIH (K123975, FK128387, DE-ÚNKP-21–5-DE-462, ÚNKP-21–3-I-DE-105). Edit Mikó was supported by the Bolyai fellowship of the Hungarian Academy of Sciences. “Project no. TKP2021-EGA-19 and TKP2021-EGA-20 has been implemented with the support provided from the National Research, Development and Innovation Fund of Hungary, financed under the TKP2021-EGA funding scheme.” PB was supported by a grant from the Hungarian Academy of Sciences (POST-COVID2021-33). Our work was supported by the Slovenian Research Agency programme grant P1-0390.

Availability of supporting data

Not applicable.

Declarations

Conflict of interests

The authors declare no conflict of interest.

Ethical approval and Consent to participate

Not applicable.

Consent for publication

All authors aggreed on the publication of the current version of manuscript.