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Review

The Diverse Forms of Lactose Intolerance and the Putative Linkage to Several Cancers

by
Mahdi Amiri
1,*,†,
Lena Diekmann
1,†,
Maren Von Köckritz-Blickwede
1,2 and
Hassan Y. Naim
1,*
1
Department of Physiological Chemistry, University of Veterinary Medicine Hannover, Hannover, Germany
2
The Research Center for Emerging Infections and Zoonosis (RIZ), University of Veterinary Medicine Hannover, Hannover, Germany
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Nutrients 2015, 7(9), 7209-7230; https://0-doi-org.brum.beds.ac.uk/10.3390/nu7095332
Submission received: 15 July 2015 / Revised: 7 August 2015 / Accepted: 21 August 2015 / Published: 28 August 2015
(This article belongs to the Special Issue Lactose Intolerance: Biology, Genetics and Dietary Management)
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Abstract

:
Lactase-phlorizin hydrolase (LPH) is a membrane glycoprotein and the only β-galactosidase of the brush border membrane of the intestinal epithelium. Besides active transcription, expression of the active LPH requires different maturation steps of the polypeptide through the secretory pathway, including N- and O-glycosylation, dimerization and proteolytic cleavage steps. The inability to digest lactose due to insufficient lactase activity results in gastrointestinal symptoms known as lactose intolerance. In this review, we will concentrate on the structural and functional features of LPH protein and summarize the cellular and molecular mechanism required for its maturation and trafficking. Then, different types of lactose intolerance are discussed, and the molecular aspects of lactase persistence/non-persistence phenotypes are investigated. Finally, we will review the literature focusing on the lactase persistence/non-persistence populations as a comparative model in order to determine the protective or adverse effects of milk and dairy foods on the incidence of colorectal, ovarian and prostate cancers.

1. Introduction

The main sources of energy in our daily diet are carbohydrates, like starch, sucrose or lactose. The breakdown of starch molecules requires preliminary digestion by salivary and pancreatic amylases. These endoamylases only cleave α-1,4 glucosidic bonds. The final hydrolysis of di- and oligo-saccharides occurs by disaccharidases, which are located in the brush border membrane of enterocytes in the small intestine [1,2,3]. The three main intestinal disaccharidases are two α-glucosidases, (1) sucrase-isomaltase (SI) and (2) maltase-glucoamylase (MGA), and one β-glycosidase: lactase-phlorizin hydrolase (LPH). While SI is responsible for the cleavage of sucrose, isomaltose and 75%–80% of the hydrolysis of maltose, MGA mostly cleaves maltose. LPH accounts for 95% of lactase activity in the intestinal mucosa and additionally cleaves glycosylceramides [4]. The activities of SI and LPH are highest in the proximal intestine, whereas MGA has its highest activity in the ileum [5].
The hydrolysis of those ingested disaccharides, like lactose, is required for the uptake into the enterocytes. Only the constituent monosaccharides glucose, galactose and fructose are absorbable. The entry into the interior of the enterocytes occurs via carrier molecules. The uptake of glucose and galactose is mediated through the sodium/glucose cotransporter 1 (SGLT1) transporter, while fructose is carried by the GLUT transporter [6].
The defects of intestinal digestion of di- and oligo-saccharides (like congenital sucrase-isomaltase or lactase deficiency) or defects in the absorption of monosaccharides (like congenital glucose-galactose deficiency) lead to fermentative diarrhea, which constitutes the major symptoms associated with malabsorption. Undigested di- or oligo-saccharides or malabsorbed monosaccharides are osmotically-active molecules that lead to an increased flux of water into the gut. In the cecum, fermentation of the unabsorbed carbohydrate molecules occurs by colonic bacteria. This process, in turn, results in the production of H2, CO2 and fatty acids, which induce a further increase of the stool volume. The consequences of those different forms of malabsorption can range from mild to severe malnutrition and eventually death, depending on several factors, like the age of the patient and other exogenous factors.
In the first part of this review, we will discuss the structure, intracellular processing and functional features of the human lactase-phlorizin hydrolase protein, as well as the molecular genetics behind different types of LPH deficiencies. In the second part, a possible association of lactase persistent or lactase non-persistent phenotypes with the incidence of some common types of cancer is reviewed.

2. Molecular Aspects of Human Lactase-Phlorizin Hydrolase Protein

2.1. Structure and Function

LPH is a type I membrane glycoprotein, which is localized at the brush border membrane of enterocytes in the small intestine, where it fulfills its enzymatic digestive function [1,7]. While LPH, the only β-galactosidase in the intestinal lumen, cleaves specifically β-glucosidic linkages between monosaccharides, SI and MGA are α-glucosidases, which are responsible for the cleavage of α-glucosidic linkages [8,9,10]. The hydrolysis of oligo-and di-saccharides is required for the uptake across the brush border membrane to the cell interior and the further transport through the blood stream [11]. A possible digestive interaction has been shown to occur among the three disaccharidases in such a way that a decrease in the lactase activity level results in increased sucrase activity [12].
The lactase gene coding for human LPH is located on chromosome 2, including 49,340 base pairs with 17 exons [13,14]. After transcription and splicing, the mRNA contains 6274 bases and encodes for a polypeptide with 1927 amino acid residues [15]. LPH is a type I membrane glycoproteins that is synthesized as a single-chain precursor molecule in the endoplasmic reticulum (ER). The protein consists of an N-terminal extracellular domain, which comprises four homologues domains revealing 38%–55% identity to each other [15]. This high similarity among the four domains led to the assumption that LPH could have emerged from two subsequent duplications of a prokaryotic β-glycosidase gene [16]. LPH is anchored into the membrane via a membrane anchor built from 19 hydrophobic amino acids and ends with a 26 amino acid-long hydrophilic cytoplasmic domain [15]. The catalytic activities are located in domain III with the phlorizin-hydrolase activity at position Glu1273 and in domain IV with the lactase activity at position Glu1749 [10].

2.2. Biosynthesis and Trafficking

Different mammalian intestinal epithelial cells and different species were used to study the biosynthesis and the processing of LPH [1,17,18,19,20,21]. The primary structure of LPH is highly conserved among different mammalian species, so that human and rabbit LPH sequences have 82.6% identity and 90% similarity, and between human and rat LPH, these values are 77.6% and 86.7%, respectively (based on European Molecular Biology Open Software Suite (EMBOSS) Needle pairwise alignment). The synthesis of LPH starts in the ER, where it is post-translationally modified and then further transported along the secretory pathway. The protein is synthesized as a monomeric pro-LPH molecule with a molecular weight of 215 kDa (Figure 1A) [1]. The first co-translational modification in the ER is N-glycosylation, which plays an indispensable role in the correct folding of the protein [22]. The primary sequence of LPH consists of 15 N-glycosylation sites. Besides the correct folding of the protein, another requirement must be fulfilled in the ER before further transport of the protein. This is the formation of homodimers of two pro-LPH molecules, which is mediated by their transmembrane domains (Figure 1B) [23,24]. It is shown that dimerization is also required for the proper activity of LPH, before further trafficking to the Golgi apparatus [23,24].
In the Golgi apparatus, pro-LPH is complex N- and O-glycosylated, generating a 230-kDa pro-LPH protein [7,17]. It is known that N- and O-glycosylation are very important for correct folding, the transport, as well as the enzymatic activity of the protein [25,26]. Previous studies showed a four-fold increased activity of the N- and O-glycosylated form of LPH compared to the N-glycosylated form, indicating the importance of O-glycosylation for the enzymatic function of this protein [26]. The final post-translational processing of pro-LPH to the mature brush border form requires two proteolytic cleavage steps, which are not necessary for the activation and the transport competence of the protein [17,19]. One cleavage step occurs in the trans-Golgi network leading to the formation of LPHβinitial, where domains I and II, which are together known as the profragment LPHα, are cleaved off at position Arg734/Leu735 (Figure 1C). The profragment LPHα is known to function as an intramolecular chaperone, which is directly involved in the correct folding of LPHβinitial [27]. LPHα is directly degraded after the intracellular cleavage step in the Golgi apparatus and is neither accessorily N-glycosylated, despite its five N-glycosylation sites, nor O-glycosylated [28]. It can be assumed that LPHα builds, due to its high content of hydrophobic amino acids, a compact, rigid and trypsin-resistant structure, which can mask the potential N-glycosylation sites directly after translation. There is no other individual role of LPHα known in the context of the whole protein function or its enzymatic activity [28,29]. LPHβinitial, which extends from Leu735 to Tyr1927, is further sorted to the apical membrane. The final cleavage occurs at the cell surface by pancreatic trypsin at position Arg868/Ala869 (Figure 1D). The remaining so-called LPHβfinal is a 160-kDa mature protein [1,21].
Nutrients 07 05332 g001 1024
Figure 1. Maturation steps of lactase-phlorizin hydrolase (LPH) in the intestinal epithelial cells. (A) The protein is synthesized as a monomeric pro-LPH molecule by translocation in the endoplasmic reticulum (ER). LPH is a type I transmembrane glycoprotein, which consists of a luminal C-terminus, a membrane anchor and an ectodomain with four highly-conserved structural and functional domains and an extracellular N-terminus. In the ER, the polypeptide is N-glycosylated, which is required for the correct folding of the protein; (B) Prior to its exit from the ER, pro-LPH molecules form homodimers, which are required for the acquisition of transport-competence and enzymatic activity; (C) After transport to the Golgi apparatus, pro-LPH is cleaved in the trans-Golgi network, which leads to the removal of LPHα, leaving LPHβinitial. In addition, LPH is further N- and O-glycosylated, which is crucial for the correct folding, and subsequently, for the enzymatic activity of the protein; (D) After proper sorting of the protein to the apical membrane, LPHβinitial is cleaved by pancreatic trypsin in the intestinal lumen to generate the mature form of the protein, called LPHβfinal, consisting only of domains III and IV.
Figure 1. Maturation steps of lactase-phlorizin hydrolase (LPH) in the intestinal epithelial cells. (A) The protein is synthesized as a monomeric pro-LPH molecule by translocation in the endoplasmic reticulum (ER). LPH is a type I transmembrane glycoprotein, which consists of a luminal C-terminus, a membrane anchor and an ectodomain with four highly-conserved structural and functional domains and an extracellular N-terminus. In the ER, the polypeptide is N-glycosylated, which is required for the correct folding of the protein; (B) Prior to its exit from the ER, pro-LPH molecules form homodimers, which are required for the acquisition of transport-competence and enzymatic activity; (C) After transport to the Golgi apparatus, pro-LPH is cleaved in the trans-Golgi network, which leads to the removal of LPHα, leaving LPHβinitial. In addition, LPH is further N- and O-glycosylated, which is crucial for the correct folding, and subsequently, for the enzymatic activity of the protein; (D) After proper sorting of the protein to the apical membrane, LPHβinitial is cleaved by pancreatic trypsin in the intestinal lumen to generate the mature form of the protein, called LPHβfinal, consisting only of domains III and IV.
Nutrients 07 05332 g001
The homologous domain III of LPH is also known to function as an intramolecular chaperone. Elimination of this domain results in a misfolded protein, which is blocked in the ER. Domain III, which contains the phlorizin-hydrolase active site, is a fully-autonomous domain, which can be correctly sorted and transported, when expressed alone [30].
To achieve its physiological function, the hydrolysis of lactose, LPH must be transported to the luminal surface of the epithelial cells. Polarized sorting is often an event that is determined by specific sorting signals or by interacting with cellular components, such as membrane microdomains [31]. The transport to the apical surface of epithelial cells can be mediated via a glycophosphatidyl inositol (GPI) anchor, which associates in the trans-Golgi network with membrane microdomains enriched in glycosphingolipids and cholesterol [32,33]. The correct sorting of sucrase-isomaltase requires the association with lipid rafts, which is mediated by O-glycosylation of the protein [34,35]. The potential role of N-glycans to act as apical sorting signals was first described for the glycoprotein gp80, which is missorted after treatment with N-glycosylation inhibitors [36]. Interestingly, LPH does not associate with conventional lipid rafts, and it is known that N- and O-glycans have no effect on its apical sorting [22,32,37]. Transmembrane domain sequences are also known to be responsible for the apical sorting of different proteins, like, for example, the influenza virus neuraminidase [38]. The presence of the transmembrane region of LPH is one requirement for dimerization and, thus, also for sorting of LPH [39]. Neither the proteolytic cleavage step is implicated in the apical trafficking of LPH nor does the large profragment LPHα contain an apical sorting signal [19,40]. Recent studies strongly suggested that the sorting signals of LPH are located in domain IV, corresponding to the mature cleaved form, LPHfinal [39,41]. It could be demonstrated that deletion of 236 amino acids of domain IV including the catalytic site has almost no influence on the sorting of LPH, while the further deletion of 87 amino acids leads to a missorting of the protein to the basolateral membrane. The region of the signal sequence was localized, but the exact amino acid sequence was not defined until now. It is known that apical membrane proteins are transported in distinct vesicular carriers, called SAVs (SI-associated vesicles) and LAVs (LPH-associated vesicles), when coming from the trans-Golgi network (TGN) [42,43]. Lectin proteins are postulated to serve as the sorting receptors that transiently cluster N-glycosylated proteins into apically-destined domains [44]. Galectin-3 is suggested to play an important role in the apical sorting as a sorting receptor by delivering non-raft-dependent glycoproteins to the lumen of LAVs in a carbohydrate-dependent manner [45].

3. Lactose Intolerance

Insufficient levels of lactase activity in the intestine lead to the inability to digest lactose from dairy products, especially milk. This type of malabsorption is called lactose intolerance and is classified into four different types. The first one is the primary lactase deficiency, also called adult hypolactasia, which appears in adulthood and is caused by the absence of a lactase persistent allele [46]. The second type is the congenital lactase deficiency, which is an autosomal recessive inherited disease that eliminates lactase activity already in infants [47,48]. The third type is the acquired or secondary lactase deficiency and is induced by an injury of the small intestine, e.g., from acute gastroenteritis, chemotherapy or infections with intestinal microbes [49]. Developmental lactase deficiency is the fourth form of lactose intolerance (LI), which occurs in preterm infants. In this type, birth occurs before lactase enzyme is optimally developed at term birth [49,50]. Compared to full-term infants, human fetuses have about 30% lactase activity at 26–34 weeks of gestation, which increases to 70% by 35–38 weeks [51,52]. Therefore, immature infants with less than 34 weeks of gestation suffer from maldigestion of lactose.

4. Adult Type of Hypolactasia

The prevalence of the primary adult type of hypolactasia (ATH) varies from less than 5% to almost 100% between different populations [53], but worldwide, an average of two-thirds of the adult population is affected [54]. The highest prevalence is detected in American Indians and Asians and up to 80% of Blacks, Arabs and Latinos reveal this disorder, while the lowest prevalence is detected in northwestern Europe [54]. Evolutionally, most mammals reach a peak of lactase activity directly after birth during lactation, when milk is the only nutrition. Usually, the lactase activity decreases to 5%–10% compared to the initial level between weaning and before adulthood, associated with changes in the composition of the diet. The persistence of lactase activity is most likely an event due to the “cultural-historical hypothesis”, proposing that diet conditions and natural selection in periods of diet stress are the reason for the permanent ability to digest lactose [55].
The persistence of lactase activity throughout life can be explained by a single autosomal dominant gene, allowing adults to accept high amounts of lactose in the diet [56,57]. Initial genotype/phenotype studies showed that two single nucleotide polymorphisms (SNPs) C/T−13910 and G/A−22018 substitutions in the LCT gene are associated with lactase persistence. Both nucleotide polymorphisms are localized upstream of the lactase gene and influence the LCT promotor [58,59]. While homozygotes with CC and GG stay non-persistent and show non-detectable lactase levels, the homozygotes with either TT or AA are persistent. Heterozygote carriers showed intermediate lactase levels with a wide range of varying symptoms [60]. This phenomenon is explained by in vitro experiments showing the strong binding of the transcription factor octamer-binding protein 1 (Oct-1) to the T−13910 variant, which can enhance the activity of the LCT gene promoter and increase the expression levels of LPH mRNA in the intestinal mucosa [46,61]. Meanwhile, the T−13910 variant seems to be associated with lactase persistent (LP) mostly in individuals of European origin. Later studies on populations from Africa and the Middle East have revealed different SNPs being associated with LP, including the G−13907, C−13913, G−13915, G−14009 and C−14010 variants [62,63,64,65,66]. Similar to the C−13910, C−13913 and G−13915 variants are located in the Oct-1 binding site (Positions −13922 to −13910), while the C−14010 variant is located more upstream in between the Oct-1 and hepatocyte nuclear factor 1-alpha (HNF1α) binding sites. All of these variants are suggested to activate the LCT promoter with a similar cis-acting effect via enhancing the Oct-1 factor binding and inducing chromatin changes in the vicinity of the LCT gene, resulting in the LP phenotype [61,62,64,66].
Besides the C−13910 genotype, studies have shown an association between C−13779 and G−13806 variants and the lactase non-persistent (LNP) phenotype in African and Indian populations [66,67]. However, there are many SNPs identified upstream of the LCT for which no functional characteristics have been reported yet: A−13937, A−14107, T−14091 and C−14176 detected in the South African population [68], T−13801, G−14012 and C−14026 identified in the Indian population [67] and T−14011 identified in Estonian and Indian individuals [69].
The symptoms of ATH patients range from mild symptoms to severe diarrhea and weight loss due to bacterial fermentation of undigested lactose and unabsorbed carbohydrates. Not all patients show these symptoms, although they suffer from the loss of lactase activity. In general, the intensity of the symptoms correlates with the consumed amount of lactose. Some individuals remain clinically unremarkable, because they can tolerate moderate amounts of lactose and lactose-containing nutrition [70]. Symptomatic lactose malabsorbers are presumed to have an additional susceptibility, e.g., for irritable bowel syndrome (IBS) [71,72,73]. It was shown that the bowel transit in patients with IBS is increased, which may also lead to the symptoms of lactose malabsorbers [74].
Nowadays, there are different established approaches available to diagnose lactose intolerance. The simplest and cheapest diagnostic tool is the lactose breath test, where the patient receives a defined amount of lactose. The undigested lactose is fermented by colonic bacteria and can be measured as hydrogen in the breath [75]. Another diagnostic method is the determination of lactase activity measured in small intestine tissue biopsy samples. Measurements below a lactase activity of 8 U/g or 0.7 U/g wet weight are defined to be associated with lactose intolerance [76]. This method is only reliable if the morphology of the mucosa and the enzymatic activities of the other disaccharidases, like MGA and SI, are in a normal range [77]. The latest method to detect lactose-intolerant patients is a genetic test of the C/T−13910 polymorphism [78]. The homozygous genotype CC determines hypolactasia. Nevertheless, it is very important to see the patient as a complex organism and to be sensitive to any additional influencing factors, which may lead to false-negative or false-positive results in the above-described test. The current recommended treatment of lactose-intolerant patients is the reduction of lactose consumption by diminishing lactose-containing products in the diet or to consume low-lactose or lactose-free food. It has been observed that ATH subjects drink less fresh milk compared to the persistent ones. This can affect energy and calcium levels, thereby eventually increasing the risk of osteoporosis [79,80]. The degree of the symptoms appearing is individually variable due to the consumed lactose and the personal lactase activity. People who remain symptomatic during complete lactose absence in the diet might be affected by other diseases, like IBS, celiac disease or bacterial overgrowth in the intestine [81].

5. Congenital Lactase Deficiency

Congenital lactase deficiency (CLD) is a severe and rare autosomal recessive disorder that leads to an elimination of lactase activity from birth onward. Most rationales for this disease are the appearance of truncated proteins as a result of frame shifts or missense mutations in the coding region of LPH [47,82,83]. There are a few cases described where a mutation led to a single amino acid substitution, which interfered with the function of LPH [84,85]. In a study with 32 Finish patients, five different mutations in the coding region of LCT were detected. One of them, called Finmajor, was identified as a homozygous type in 84% of the patients. This mutation (Y1390X) leads to a truncated protein. Two further mutations (S1666fsX1722 and S218fsX224) result in a frame shift and a premature stop codon. The latest two mutations (Q268H and G1363S) generate an amino acid substitution [47,84]. The Finmajor mutation was analyzed by sequence comparison among 556 anonymous blood donors. The highest carrier frequency of 1:35 was found in a little town in Finland [47]. Noticeably, all of the other four mutations could not be detected in any regional subpopulation screening, except the G1363S mutation, which was found in another study in two siblings of Turkish origin in the homozygous state. This study also detected four other mutations, two in an Italian patient and two others in a Finish patient [85]. The G1363S-mutant was analyzed at the protein level, and it was demonstrated that this mutation leads to a misfolded protein that is blocked in the ER [84]. Recent studies have revealed two mutations in LCT in a Japanese infant with CLD, also resulting in a truncated protein [86]. Those two mutants, LPH-Y1473X and LPH-D1796fs, were also analyzed at the protein level and revealed that both proteins are misfolded and ultimately degraded in the ER. Interestingly, no interaction between the wild-type LPH monomer with one of the pathogenic LPH mutants was detectable, and the wild-type LPH generated normal homodimers that are enzymatically active, as well as transport competent [87]. Another new mutation (S1150fs) in LCT was recently found in a Turkish infant, resulting in a truncated protein [88]. Taking these findings under closer consideration, it may be hypothesized that the origin of the genetic background that lead to this severe and rare disease may be located in Finland.
Typical symptoms of a severe CLD start from a few days after birth by the onset of nursing with watery diarrhea, meteorism and malnutrition. Previous studies could show that the microvilli reveal a normal shape, but the analysis of enzymatic activities from small intestinal biopsies indicated very low levels of lactase [61,62]. Life-threatening dehydration and electrolyte loss of newborns requires very rapid treatment. The treatment strategy for those patients is the removal of lactose from the diet and the application of milk substitutes. The severeness of this disease occurs because the symptoms are gastrointestinal problems, which might also arise in the case of other diseases. A recent study revealed that severe osmotic diarrhea due to CLD is elicited by severe mutations in the LPH gene that occur in either a compound heterozygous or homozygous pattern of inheritance [87]. Until now, no genetic test has been available to analyze if the parents of an unborn infant might be carriers of a pathogenic mutation in the gene of LPH.

6. Secondary Lactose Intolerance Caused by Infections

The secondary LI occurs when the small intestine decreases lactase production after an illness, injury or surgery. Among the diseases associated with secondary LI is celiac disease and Crohn’s disease, but also, infections with various microbes, such as viruses, bacteria and parasites, have been described. In the case of intestinal parasites, Giardia infections were associated with a higher proportion of lactose intolerance in patients from Gabon, Central Africa, analyzed by hydrogen breast tests [89]. In 1991, children with vertically-transmitted human immunodeficiency virus (HIV) infection were evaluated for carbohydrate malabsorption using lactose hydrogen breath tests and d-xylose absorption studies and identified 61% of children with carbohydrate malabsorption. Based on these finding, the authors hypothesized that HIV may be directly involved in the development of lactose malabsorption. Interestingly, a specific interaction of LPH and rotavirus protein NSP4 has been described, which is responsible for the rotavirus-mediated secondary LI [90]. Using cultured human intestinal fully-differentiated enterocyte-like Caco-2 cells, the authors showed that lactase enzymatic activity at the brush border membrane (BBM) is significantly decreased in rhesus monkey rotavirus (RRV)-infected cells. This decreased enzyme activity was not associated with Ca2+- and cAMP-dependent signaling events induced by the virus, and furthermore, LPH biosynthesis, stability and protein expression at the BBM was not affected. Instead, the kinetic of lactase enzymatic activity present at the BBM was modified as a result of an inhibitory action of the secreted non-structural rotavirus protein NSP4. NSP4 has pleiotropic functions in viral morphogenesis, as well as pathogenesis [91]. As an example, NSP4 has been shown to alter the F-actin network through the actin-remodeling protein cofilin [92]. Besides viruses and parasites, some bacteria have also been shown to modulate intestinal functions by secreting toxins that lead to the disruption of intestinal epithelial barrier function and subsequent loss of carbohydrate metabolism as, for example, Clostridium difficile or [93] Staphylococcus aureus toxins [94]. Thus, opportunistic bacteria that use intestine as a reservoir, like methicillin-resistant Staphylococcus aureus, may lead to secondary LI-mediated diarrhea during colonization of the host [95,96].
In summary, microbes may use a large variety of sophisticated mechanisms to induce structural and functional lesions at the BBM of human intestinal cells and, thereby, lead to secondary LI. Studying the mechanisms of pathogen-induced damage of epithelial cells might help to develop protective strategies against infection-associated diarrhea.

7. Association of Lactase Persistence and Dairy Consumption with the Incidence of Some Common Cancers

With a concentration of about 5% (w/v), lactose is a major ingredient of the milk of cows, sheep and goats [97]. Lactose intolerance appears when lactase activity in the small intestine is insufficient or absent [84,98,99]. The transit of the mal-digested and unabsorbed lactose to the colon is followed by extra bacterial fermentation and production of gas and short chain fatty acids [100,101,102]. Besides irritable influence, these compounds can highly increase the luminal osmolality and interfere with water absorption in the colon, and therefore, cause substantial watery diarrhea. Hypothetically, 12 g of lactose (from about 250 mL of milk) can hold 800 mL of water after processing in the colon [97].
Almost two third of the world population are lactose intolerant because of ATH with a restricted proportion of milk and dairy products in their diet. Besides lactose, dairy foods are nutritious resources of lipids, protein, vitamins and minerals, particularly calcium [103]. In different physiological abnormalities, where dairy foods exert a protective or adverse effect, a comparison between LI and normal subjects has provided an interesting body of evidence for the assessment of the bioactive function of different dairy ingredients in the establishment of health and disease conditions. Colorectal, ovarian and prostate cancers are the most common cancer types in which a protective or adverse effect of milk and dairy foods has been investigated and discussed for a long time [104,105,106,107].

7.1. Colorectal Cancer

Colorectal cancer is the fourth most commonly diagnosed and the second cause of fatal cancer in the United States [104]. Diet has a direct relationship with incidence and/or progression of colorectal cancer [108,109]. Consumption of milk, but not cheese that contains saturated fat has been shown to reduce the risk of colorectal cancer [110,111]. A similar protective function has been identified for a calcium- and vitamin D-supplemented diet, attributing the anti-cancer effect of milk to these two biologically-active components [112]. In the intestinal epithelial cells, calcium and vitamin D are shown to regulate cell growth and to promote cell differentiation via stimulation of calcium-sensing receptors [106,113]. Furthermore, in the intestinal lumen, calcium can bind and complex fatty acids, as well as secondary bile acids, and thereby, reduce their cytotoxicity, as well as tumorigenic exposure to the epithelium [114].
In line with these findings, studies in Hungarian and Finnish populations have shown an increased risk for colorectal cancer among LNP subjects [115,116]. However, other studies on Italian, British and Spanish populations do not support such an association [115,117,118]. Based on a meta-analysis of different populations, Szilagyi et al. have concluded that the protective effect of dairy food against colorectal cancer is detectable in populations with high or low LNP frequencies, but not in those with significant mixed LNP/LP composition [119,120].
Vitamin D can increase calcium absorption in the intestine [121,122]. Therefore, besides life style and nutritional habits, attitudes and exposure to sunshine should also be considered when the effects of dairy food on colorectal cancer are discussed [123]. Interestingly, LNP has been found to have a direct association with sunshine [124,125]. This might be a suggestive evidence for higher LP frequency in higher attitudes as an evolutionary adaptation in order to uptake more of the required vitamin D through dietary sources, especially dairy foods.

7.2. Ovarian and Prostate Cancers

Besides the alimentary tract and its associated disorders, such as inflammatory bowel syndrome and colorectal cancer, which are directly exposed to and influenced by the components of milk and dairy foods [126], the pathogenesis of some other parts or organs of the body is also thought to be linked with certain biologically-active ingredients in dairy foods [127]. Thus, the different levels of milk consumption between LP and LNP populations have provided a reasonable model to validate the consistency of the hypotheses regarding beneficial or adverse influences of dairy foods in such conditions. However, conflicting results are available in the literature.
On the one hand, lactose and female sex-related hormones, such as estrogens, in cow’s milk are suspected to play a role in the incidence of ovarian cancer in female or prostate cancer in male subjects [110,128]. The hydrolysis of lactose in the intestine by LP individuals results in the liberation and absorption of glucose and galactose. An excess amount of galactose, especially in the imperfect metabolized form of galactose-1-phosphate, is thought to exert a toxic effect on germ cells, particularly on female ovaries [110,129,130]. Trauma to the surface of the ovary and stimulation of the gonadotropin hormones are two suggested mechanisms for the adverse effect of galactose in the pathogenesis of ovarian cancer [131,132].
In a study of 301 subjects with invasive epithelial ovarian cancer, individuals that belong to the highest category of lactose consumption showed a two-fold elevated risk for serous subtypes of ovarian cancer in comparison to individuals that belong to the lowest category. In this study, each 11 g increase in the lactose intake was found to be associated with 20% higher risk for ovarian cancer [133]. Similar studies by Cramer [134] and Meloni et al. [130] have also supported the role of lactose absorption and galactose toxicity in the incidence of ovarian cancer with a higher prevalence for LP women.
On the other side, several publications are found that do not support a correlation of milk consumption with ovarian cancer. One such study is on 327 Finnish, 303 Polish and 152 Swedish subjects genetically determined as LNP versus relevant controls, which did not confirm any role for LP and higher milk intake in the etiology of ovarian cancer [105]. Similarly, another study on 108 Caucasian women from western Washington diagnosed with stage I ovarian cancer in comparison to matched controls did not support any correlation between lactose consumption and ovarian cancer [129].
Interestingly, in a cohort study by Koralek et al., among 31,925 subjects, a higher consumption of total dairy food was significantly associated with a decreased risk for ovarian cancer [135]. The authors demonstrated that calcium intake reduces the risk for ovarian cancer, similar to what was previously discussed for colorectal cancer. In summary, the evidence for the association of milk consumption and increased risk for prostate cancer is multifactorial and controversial. Current studies do not demonstrate a direct link between LP/LNP genotype and the incidence of prostate cancer; however, some studies have suggested an association between the consumption of dairy products and the development of prostate cancer [136,137]. The investigation of fifty-five prostate cancer subjects by Agarwal et al. has determined a lower incidence of LI in these patients in comparison to the general population [138], which is in line with the hypothesis that higher milk intake is a risk factor for prostate cancer [107,139,140]. However, the adverse effect of milk in prostate cancer is considered to be minor and rather suggestive [110,111].
Calcium, insulin-like growth factors, saturated fat and cow’s female hormones are dairy components, and their putative role in prostate cancer is under discussion [141,142]. The estrogens of cow’s milk are proposed to influence the growth of estrogen-sensitive cells in the human body and, thereby, to modulate prostate and ovarian cancers [143,144]. However, it is noteworthy to indicate that in several studies, the levels of biologically-active estrogens in the commercially available milk products have been defined to be far below an effective range to exert such a detrimental effect on consumers [145,146,147,148,149,150,151].

8. Concluding Remarks and Outlook

In the intestinal lumen, lactose from milk and dairy foods is hydrolyzed by LPH to glucose and galactose, which are subsequently absorbed. LPH is a membrane-bound glycoprotein of the intestinal epithelial cells. Insufficient levels of lactase activity in the intestine may result in the occurrence of gastrointestinal symptoms upon consumption of milk and dairy products, known as LI. The most common type of LI affecting more than two-thirds of the world population is the ATH or lactase LNP phenotype. This phenotype is caused by reduced activity of the lactase gene promoter after childhood. In LP individuals, different SNPs at 13–14 kbp upstream of the lactase gene have been identified that regulate chromatin changes to keep the lactase expression persistent during adulthood. Other types of LI are induced by inherited mutations in the coding region of LPH, known as alactasia or secondary LI, as a result of the pathogenic defects of the intestinal tissue, as caused by parasitic, bacterial or viral infections.
Besides lactose, milk and dairy foods are rich in other biologically-active compound, which are thought to exert protective or adverse effects on the incidence of colorectal ovarian or prostate cancers. Evidence from comparative studies on LP and LNP cases are more supportive for a protective or at least non-adverse function of milk and dairy food against colorectal and ovarian cancers. The adverse effects of dairy products on prostate cancer are more suggestive than decisive and are found to be mostly linked to the consumption of low fat milk [136]. Furthermore, probiotics in the non-fermented and fermented milk products are shown to balance the gut microbiota and, thereby, exert an immunomodulatory function, which leads to improved gastrointestinal physiology and helps recovery from many gut-associated disorders, including gastro-enteritis, inflammatory bowel disease and constipation [126,152,153,154].
Therefore, milk and dairy foods are not recommended to be ignored in the daily diet. To overcome lactose intolerance syndromes, LNP individuals can follow strategies, such as reducing the amount and increasing the frequency of dairy consumption, as well as using fermented dairy products, which contain active microbial lactase and have a slower bowel transit [100,155].
There is emerging evidence that attributes the occurrence of IBS to the marginal levels of activity of intestinal disaccharidases [156,157]. The contribution of heterozygote mutations in the LCT gene or the LNP phenotype to the appearance of IBS symptoms is an important topic that needs to be investigated in the future. Lower dairy consumption in LNP individuals is associated with a modified gut microbiota [158]. In these cases, the role of altered gut microbiota in the incidence of different intestinal disorders, including IBS and IBD, is an open interesting question, which needs to be further studied.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Naim, H.Y.; Sterchi, E.E.; Lentze, M.J. Biosynthesis and maturation of lactase-phlorizin hydrolase in the human small intestinal epithelial cells. Biochem. J. 1987, 241, 427–434. [Google Scholar] [CrossRef] [PubMed]
  2. Naim, H.Y.; Sterchi, E.E.; Lentze, M.J. Structure, biosynthesis, and glycosylation of human small intestinal maltase-glucoamylase. J. Biol. Chem. 1988, 263, 19709–19717. [Google Scholar] [PubMed]
  3. Naim, H.Y.; Sterchi, E.E.; Lentze, M.J. Biosynthesis of the human sucrase-isomaltase complex. Differential O-glycosylation of the sucrase subunit correlates with its position within the enzyme complex. J. Biol. Chem. 1988, 263, 7242–7253. [Google Scholar] [PubMed]
  4. Semenza, G. Anchoring and biosynthesis of stalked brush border membrane proteins: Glycosidases and peptidases of enterocytes and renal tubuli. Annu. Rev. Cell. Biol. 1986, 2, 255–313. [Google Scholar] [CrossRef] [PubMed]
  5. Triadou, N.; Bataille, J.; Schmitz, J. Longitudinal study of the human intestinal brush border membrane proteins. Distribution of the main disaccharidases and peptidases. Gastroenterology 1983, 85, 1326–1332. [Google Scholar] [PubMed]
  6. Ferraris, R.P. Dietary and developmental regulation of intestinal sugar transport. Biochem. J. 2001, 360, 265–276. [Google Scholar] [CrossRef] [PubMed]
  7. Hauri, H.P.; Sterchi, E.E.; Bienz, D.; Fransen, J.A.; Marxer, A. Expression and intracellular transport of microvillus membrane hydrolases in human intestinal epithelial cells. J. Cell Biol. 1985, 101, 838–851. [Google Scholar] [CrossRef] [PubMed]
  8. Sim, L.; Willemsma, C.; Mohan, S.; Naim, H.Y.; Pinto, B.M.; Rose, D.R. Structural basis for substrate selectivity in human maltase-glucoamylase and sucrase-isomaltase N-terminal domains. J. Biol. Chem. 2010, 285, 17763–17770. [Google Scholar] [CrossRef] [PubMed]
  9. Amiri, M.; Naim, H.Y. Miglustat-induced intestinal carbohydrate malabsorption is due to the inhibition of α-glucosidases, but not β-galactosidases. J. Inherit. Metab. Dis. 2012, 35, 949–954. [Google Scholar] [CrossRef] [PubMed]
  10. Zecca, L.; Mesonero, J.E.; Stutz, A.; Poiree, J.C.; Giudicelli, J.; Cursio, R.; Gloor, S.M.; Semenza, G. Intestinal lactase-phlorizin hydrolase (LPH): The two catalytic sites; the role of the pancreas in pro-LPH maturation. FEBS. Lett. 1998, 435, 225–228. [Google Scholar] [CrossRef]
  11. Colombo, V.; Lorenz-Meyer, H.; Semenza, G. Small intestinal phlorizin hydrolase: The “β-glycosidase complex”. Biochim. Biophys. Acta. 1973, 327, 412–424. [Google Scholar] [CrossRef]
  12. Sterchi, E.E.; Mills, P.R.; Fransen, J.A.; Hauri, H.P.; Lentze, M.J.; Naim, H.Y.; Ginsel, L.; Bond, J. Biogenesis of intestinal lactase-phlorizin hydrolase in adults with lactose intolerance. Evidence for reduced biosynthesis and slowed-down maturation in enterocytes. J. Clin. Investig. 1990, 86, 1329–1337. [Google Scholar] [CrossRef] [PubMed]
  13. Kruse, T.A.; Bolund, L.; Grzeschik, K.H.; Ropers, H.H.; Sjostrom, H.; Noren, O.; Mantei, N.; Semenza, G. The human lactase-phlorizin hydrolase gene is located on chromosome 2. FEBS. Lett. 1988, 240, 123–126. [Google Scholar] [CrossRef]
  14. Boll, W.; Wagner, P.; Mantei, N. Structure of the chromosomal gene and cdnas coding for lactase-phlorizin hydrolase in humans with adult-type hypolactasia or persistence of lactase. Am. J. Hum. Genet. 1991, 48, 889–902. [Google Scholar] [PubMed]
  15. Mantei, N.; Villa, M.; Enzler, T.; Wacker, H.; Boll, W.; James, P.; Hunziker, W.; Semenza, G. Complete primary structure of human and rabbit lactase-phlorizin hydrolase: Implications for biosynthesis, membrane anchoring and evolution of the enzyme. EMBO. J. 1988, 7, 2705–2713. [Google Scholar] [PubMed]
  16. Wacker, H.; Keller, P.; Falchetto, R.; Legler, G.; Semenza, G. Location of the two catalytic sites in intestinal lactase-phlorizin hydrolase. Comparison with sucrase-isomaltase and with other glycosidases, the membrane anchor of lactase-phlorizin hydrolase. J. Biol. Chem. 1992, 267, 18744–18752. [Google Scholar] [PubMed]
  17. Naim, H.Y.; Lacey, S.W.; Sambrook, J.F.; Gething, M.J. Expression of a full-length cDNA coding for human intestinal lactase-phlorizin hydrolase reveals an uncleaved, enzymatically active, and transport-competent protein. J. Biol. Chem. 1991, 266, 12313–12320. [Google Scholar] [PubMed]
  18. Hauri, H.P.; Sander, B.; Naim, H. Induction of lactase biosynthesis in the human intestinal epithelial cell line Caco-2. Eur. J. Biochem. 1994, 219, 539–546. [Google Scholar] [CrossRef] [PubMed]
  19. Jacob, R.; Brewer, C.; Fransen, J.A.; Naim, H.Y. Transport, function, and sorting of lactase-phlorizin hydrolase in madin-darby canine kidney cells. J. Biol. Chem. 1994, 269, 2712–2721. [Google Scholar] [PubMed]
  20. Buller, H.A.; Montgomery, R.K.; Sasak, W.V.; Grand, R.J. Biosynthesis, glycosylation, and intracellular transport of intestinal lactase-phlorizin hydrolase in rat. J. Biol. Chem. 1987, 262, 17206–17211. [Google Scholar] [PubMed]
  21. Danielsen, E.M.; Skovbjerg, H.; Noren, O.; Sjostrom, H. Biosynthesis of intestinal microvillar proteins intracellular processing of lactase-phlorizin hydrolase. Biochem. Biophys. Res. Commun. 1984, 122, 82–90. [Google Scholar] [CrossRef]
  22. Naim, H.Y. Processing and transport of human small intestinal lactase-phlorizin hydrolase (LPH). Role of N-linked oligosaccharide modification. FEBS. Lett. 1994, 342, 302–307. [Google Scholar] [CrossRef]
  23. Danielsen, E.M. Biosynthesis of intestinal microvillar proteins. Dimerization of aminopeptidase N and lactase-phlorizin hydrolase. Biochemistry 1990, 29, 305–308. [Google Scholar] [CrossRef] [PubMed]
  24. Naim, H.Y.; Naim, H. Dimerization of lactase-phlorizin hydrolase occurs in the endoplasmic reticulum, involves the putative membrane spanning domain and is required for an efficient transport of the enzyme to the cell surface. Eur. J. Cell Biol. 1996, 70, 198–208. [Google Scholar] [PubMed]
  25. Jacob, R.; Weiner, J.R.; Stadge, S.; Naim, H.Y. Additional N-glycosylation and its impact on the folding of intestinal lactase-phlorizin hydrolase. J. Biol. Chem. 2000, 275, 10630–10637. [Google Scholar] [CrossRef] [PubMed]
  26. Naim, H.Y.; Lentze, M.J. Impact of o-glycosylation on the function of human intestinal lactase-phlorizin hydrolase. Characterization of glycoforms varying in enzyme activity and localization of O-glycoside addition. J. Biol. Chem. 1992, 267, 25494–25504. [Google Scholar] [PubMed]
  27. Jacob, R.; Peters, K.; Naim, H.Y. The prosequence of human lactase-phlorizin hydrolase modulates the folding of the mature enzyme. J. Biol. Chem. 2002, 277, 8217–8225. [Google Scholar] [CrossRef] [PubMed]
  28. Naim, H.Y.; Jacob, R.; Naim, H.; Sambrook, J.F.; Gething, M.J. The pro region of human intestinal lactase-phlorizin hydrolase. J. Biol. Chem. 1994, 269, 26933–26943. [Google Scholar] [PubMed]
  29. Naim, H.Y. The pro-region of human intestinal lactase-phlorizin hydrolase is enzymatically inactive towards lactose. Biol. Chem. Hoppe. Seyler. 1995, 376, 255–258. [Google Scholar] [PubMed]
  30. Behrendt, M.; Polaina, J.; Naim, H.Y. Structural hierarchy of regulatory elements in the folding and transport of an intestinal multidomain protein. J. Biol. Chem. 2010, 285, 4143–4152. [Google Scholar] [CrossRef] [PubMed]
  31. Stoops, E.H.; Caplan, M.J. Trafficking to the apical and basolateral membranes in polarized epithelial cells. J. Am. Soc. Nephrol. 2014, 25, 1375–1386. [Google Scholar] [CrossRef] [PubMed]
  32. Danielsen, E.M. Involvement of detergent-insoluble complexes in the intracellular transport of intestinal brush border enzymes. Biochemistry 1995, 34, 1596–1605. [Google Scholar] [CrossRef] [PubMed]
  33. Ikonen, E.; Simons, K. Protein and lipid sorting from the trans-golgi network to the plasma membrane in polarized cells. Semin. Cell. Dev. Biol. 1998, 9, 503–509. [Google Scholar] [CrossRef] [PubMed]
  34. Alfalah, M.; Jacob, R.; Preuss, U.; Zimmer, K.P.; Naim, H.; Naim, H.Y. O-linked glycans mediate apical sorting of human intestinal sucrase-isomaltase through association with lipid rafts. Curr. Biol. 1999, 9, 593–596. [Google Scholar] [CrossRef]
  35. Jacob, R.; Alfalah, M.; Grunberg, J.; Obendorf, M.; Naim, H.Y. Structural determinants required for apical sorting of an intestinal brush-border membrane protein. J. Biol. Chem. 2000, 275, 6566–6572. [Google Scholar] [CrossRef] [PubMed]
  36. Urban, J.; Parczyk, K.; Leutz, A.; Kayne, M.; Kondor-Koch, C. Constitutive apical secretion of an 80-kD sulfated glycoprotein complex in the polarized epithelial Madin-Darby canine kidney cell line. J. Cell. Biol. 1987, 105, 2735–2743. [Google Scholar] [CrossRef] [PubMed]
  37. Jacob, R.; Preuss, U.; Panzer, P.; Alfalah, M.; Quack, S.; Roth, M.G.; Naim, H.; Naim, H.Y. Hierarchy of sorting signals in chimeras of intestinal lactase-phlorizin hydrolase and the influenza virus hemagglutinin. J. Biol. Chem. 1999, 274, 8061–8067. [Google Scholar] [CrossRef] [PubMed]
  38. Kundu, A.; Avalos, R.T.; Sanderson, C.M.; Nayak, D.P. Transmembrane domain of influenza virus neuraminidase, a type ii protein, possesses an apical sorting signal in polarized MDCK cells. J. Virol. 1996, 70, 6508–6515. [Google Scholar] [PubMed]
  39. Panzer, P.; Preuss, U.; Joberty, G.; Naim, H.Y. Protein domains implicated in intracellular transport and sorting of lactase-phlorizin hydrolase. J. Biol. Chem. 1998, 273, 13861–13869. [Google Scholar] [CrossRef] [PubMed]
  40. Grunberg, J.; Luginbuhl, U.; Sterchi, E.E. Proteolytic processing of human intestinal lactase-phlorizin hydrolase precursor is not a prerequisite for correct sorting in madin darby canine kidney (MDCK) cells. FEBS. Lett. 1992, 314, 224–228. [Google Scholar] [CrossRef]
  41. Jacob, R.; Zimmer, K.P.; Naim, H.; Naim, H.Y. The apical sorting of lactase-phlorizin hydrolase implicates sorting sequences found in the mature domain. Eur. J. Cell Biol. 1997, 72, 54–60. [Google Scholar] [PubMed]
  42. Jacob, R.; Naim, H.Y. Apical membrane proteins are transported in distinct vesicular carriers. Curr. Biol. 2001, 11, 1444–1450. [Google Scholar] [CrossRef]
  43. Jacob, R.; Heine, M.; Alfalah, M.; Naim, H.Y. Distinct cytoskeletal tracks direct individual vesicle populations to the apical membrane of epithelial cells. Curr. Biol. 2003, 13, 607–612. [Google Scholar] [CrossRef]
  44. Delacour, D.; Koch, A.; Jacob, R. The role of galectins in protein trafficking. Traffic 2009, 10, 1405–1413. [Google Scholar] [CrossRef] [PubMed]
  45. Delacour, D.; Cramm-Behrens, C.I.; Drobecq, H.; le Bivic, A.; Naim, H.Y.; Jacob, R. Requirement for galectin-3 in apical protein sorting. Curr. Biol. 2006, 16, 408–414. [Google Scholar] [CrossRef] [PubMed]
  46. Kuokkanen, M.; Enattah, N.S.; Oksanen, A.; Savilahti, E.; Orpana, A.; Jarvela, I. Transcriptional regulation of the lactase-phlorizin hydrolase gene by polymorphisms associated with adult-type hypolactasia. Gut 2003, 52, 647–652. [Google Scholar] [CrossRef] [PubMed]
  47. Kuokkanen, M.; Kokkonen, J.; Enattah, N.S.; Ylisaukko-Oja, T.; Komu, H.; Varilo, T.; Peltonen, L.; Savilahti, E.; Jarvela, I. Mutations in the translated region of the lactase gene (LCT) underlie congenital lactase deficiency. Am. J. Hum. Genet. 2006, 78, 339–344. [Google Scholar] [CrossRef] [PubMed]
  48. Robayo-Torres, C.C.; Nichols, B.L. Molecular differentiation of congenital lactase deficiency from adult-type hypolactasia. Nutr. Rev. 2007, 65, 95–98. [Google Scholar] [CrossRef] [PubMed]
  49. Heyman, M.B. Lactose intolerance in infants, children, and adolescents. Pediatrics 2006, 118, 1279–1286. [Google Scholar] [CrossRef] [PubMed]
  50. Lasekan, J.B.; Jacobs, J.; Reisinger, K.S.; Montalto, M.B.; Frantz, M.P.; Blatter, M.M. Lactose-free milk protein-based infant formula: Impact on growth and gastrointestinal tolerance in infants. Clin. Pediatr. (Phila) 2011, 50, 330–337. [Google Scholar] [CrossRef] [PubMed]
  51. Antonowicz, I.; Lebenthal, E. Developmental pattern of small intestinal enterokinase and disaccharidase activities in the human fetus. Gastroenterology 1977, 72, 1299–1303. [Google Scholar] [PubMed]
  52. Erasmus, H.D.; Ludwig-Auser, H.M.; Paterson, P.G.; Sun, D.; Sankaran, K. Enhanced weight gain in preterm infants receiving lactase-treated feeds: A randomized, double-blind, controlled trial. J. Pediatr. 2002, 141, 532–537. [Google Scholar] [CrossRef] [PubMed]
  53. Scrimshaw, N.S. Global and regional consequences of occult hunger. Arch. Latinoam. Nutr. 1994, 44, 75S–84S. [Google Scholar] [PubMed]
  54. Sahi, T. Genetics and epidemiology of adult-type hypolactasia. Scand. J. Gastroenterol. Suppl. 1994, 202, 7–20. [Google Scholar] [CrossRef] [PubMed]
  55. Simoons, F.J. Primary adult lactose intolerance and the milking habit: A problem in biologic and cultural interrelations. Am. J. Dig. Dis. 1970, 15, 695–710. [Google Scholar] [CrossRef] [PubMed]
  56. Sahi, T. Hypolactasia and lactase persistence. Historical review and the terminology. Scand. J. Gastroenterol. Suppl. 1994, 202, 1–6. [Google Scholar] [CrossRef] [PubMed]
  57. Harvey, C.B.; Wang, Y.; Hughes, L.A.; Swallow, D.M.; Thurrell, W.P.; Sams, V.R.; Barton, R.; Lanzon-Miller, S.; Sarner, M. Studies on the expression of intestinal lactase in different individuals. Gut 1995, 36, 28–33. [Google Scholar] [CrossRef] [PubMed]
  58. Enattah, N.S.; Sahi, T.; Savilahti, E.; Terwilliger, J.D.; Peltonen, L.; Jarvela, I. Identification of a variant associated with adult-type hypolactasia. Nat. Genet. 2002, 30, 233–237. [Google Scholar] [CrossRef] [PubMed]
  59. Olds, L.C.; Sibley, E. Lactase persistence DNA variant enhances lactase promoter activity in vitro: Functional role as a cis regulatory element. Hum. Mol. Genet. 2003, 12, 2333–2340. [Google Scholar] [CrossRef] [PubMed]
  60. Matthews, S.B.; Waud, J.P.; Roberts, A.G.; Campbell, A.K. Systemic lactose intolerance: A new perspective on an old problem. Postgrad. Med. J. 2005, 81, 167–173. [Google Scholar] [CrossRef] [PubMed]
  61. Lewinsky, R.H.; Jensen, T.G.; Moller, J.; Stensballe, A.; Olsen, J.; Troelsen, J.T. T-13910 DNA variant associated with lactase persistence interacts with Oct-1 and stimulates lactase promoter activity in vitro. Hum. Mol. Genet. 2005, 14, 3945–3953. [Google Scholar] [CrossRef] [PubMed]
  62. Jensen, T.G.; Liebert, A.; Lewinsky, R.; Swallow, D.M.; Olsen, J.; Troelsen, J.T. The -14010*C variant associated with lactase persistence is located between an Oct-1 and HNF 1α binding site and increases lactase promoter activity. Hum. Genet. 2011, 130, 483–493. [Google Scholar] [CrossRef] [PubMed]
  63. Tishkoff, S.A.; Reed, F.A.; Ranciaro, A.; Voight, B.F.; Babbitt, C.C.; Silverman, J.S.; Powell, K.; Mortensen, H.M.; Hirbo, J.B.; Osman, M.; et al. Convergent adaptation of human lactase persistence in Africa and Europe. Nat. Genet. 2007, 39, 31–40. [Google Scholar] [CrossRef] [PubMed]
  64. Ingram, C.J.; Elamin, M.F.; Mulcare, C.A.; Weale, M.E.; Tarekegn, A.; Raga, T.O.; Bekele, E.; Elamin, F.M.; Thomas, M.G.; Bradman, N.; et al. A novel polymorphism associated with lactose tolerance in Africa: Multiple causes for lactase persistence? Hum. Genet. 2007, 120, 779–788. [Google Scholar] [CrossRef] [PubMed]
  65. Coelho, M.; Sequeira, F.; Luiselli, D.; Beleza, S.; Rocha, J. On the edge of bantu expansions: MtDNA, Y chromosome and lactase persistence genetic variation in southwestern Angola. BMC Evol. Biol. 2009, 9, 80. [Google Scholar] [CrossRef] [PubMed]
  66. Ingram, C.J.; Raga, T.O.; Tarekegn, A.; Browning, S.L.; Elamin, M.F.; Bekele, E.; Thomas, M.G.; Weale, M.E.; Bradman, N.; Swallow, D.M. Multiple rare variants as a cause of a common phenotype: Several different lactase persistence associated alleles in a single ethnic group. J. Mol. Evol. 2009, 69, 579–588. [Google Scholar] [CrossRef] [PubMed]
  67. Gallego Romero, I.; Basu Mallick, C.; Liebert, A.; Crivellaro, F.; Chaubey, G.; Itan, Y.; Metspalu, M.; Eaaswarkhanth, M.; Pitchappan, R.; Villems, R.; et al. Herders of Indian and European cattle share their predominant allele for lactase persistence. Mol. Biol. Evol. 2012, 29, 249–260. [Google Scholar] [CrossRef] [PubMed]
  68. Torniainen, S.; Parker, M.I.; Holmberg, V.; Lahtela, E.; Dandara, C.; Jarvela, I. Screening of variants for lactase persistence/non-persistence in populations from south Africa and Ghana. BMC Genet. 2009, 10, 31. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  69. Friedrich, D.C.; Santos, S.E.; Ribeiro-dos-Santos, A.K.; Hutz, M.H. Several different lactase persistence associated alleles and high diversity of the lactase gene in the admixed Brazilian population. PLoS ONE 2012, 7, e46520. [Google Scholar] [CrossRef] [PubMed]
  70. Vesa, T.H.; Marteau, P.; Korpela, R. Lactose intolerance. J. Am. Coll. Nutr. 2000, 19, 165S–175S. [Google Scholar] [CrossRef] [PubMed]
  71. Malagelada, J.R. Lactose intolerance. N. Engl. J. Med. 1995, 333, 53–54. [Google Scholar] [CrossRef] [PubMed]
  72. Montes, R.; Monge, E. Lactose malabsorption and IBS. Scand. J. Gastroenterol 2004, 39, 1033. [Google Scholar] [CrossRef] [PubMed]
  73. Bolin, T. IBS or intolerance? Aust. Fam. Physician 2009, 38, 962–965. [Google Scholar] [PubMed]
  74. Wackerbauer, R.; Schmidt, T. Symbolic dynamics of jejunal motility in the irritable bowel. Chaos 1999, 9, 805–811. [Google Scholar] [CrossRef] [PubMed]
  75. Arola, H. Diagnosis of hypolactasia and lactose malabsorption. Scand. J. Gastroenterol. Suppl. 1994, 202, 26–35. [Google Scholar] [CrossRef] [PubMed]
  76. Forget, P.; Lombet, J.; Grandfils, C.; Dandrifosse, G.; Geubelle, F. Lactase insufficiency revisited. J. Pediatr. Gastroenterol. Nutr. 1985, 4, 868–872. [Google Scholar] [CrossRef] [PubMed]
  77. Newcomer, A.D.; McGill, D.B. Lactose tolerance tests in adults with normal lactase activity. Gastroenterology 1966, 50, 340–346. [Google Scholar] [PubMed]
  78. Rasinpera, H.; Savilahti, E.; Enattah, N.S.; Kuokkanen, M.; Totterman, N.; Lindahl, H.; Jarvela, I.; Kolho, K.L. A genetic test which can be used to diagnose adult-type hypolactasia in children. Gut 2004, 53, 1571–1576. [Google Scholar] [CrossRef] [PubMed]
  79. Wilt, T.J.; Shaukat, A.; Shamliyan, T.; Taylor, B.C.; MacDonald, R.; Tacklind, J.; Rutks, I.; Schwarzenberg, S.J.; Kane, R.L.; Levitt, M. Lactose intolerance and health. Evid. Rep. Technol. Assess (Full Rep.) 2010, 192, 1–410. [Google Scholar] [PubMed]
  80. Kull, M.; Kallikorm, R.; Lember, M. Impact of molecularly defined hypolactasia, self-perceived milk intolerance and milk consumption on bone mineral density in a population sample in Northern Europe. Scand. J. Gastroenterol. 2009, 44, 415–421. [Google Scholar] [CrossRef] [PubMed]
  81. Suchy, F.J.; Brannon, P.M.; Carpenter, T.O.; Fernandez, J.R.; Gilsanz, V.; Gould, J.B.; Hall, K.; Hui, S.L.; Lupton, J.; Mennella, J.; et al. National institutes of health consensus development conference: Lactose intolerance and health. Ann. Intern. Med. 2010, 152, 792–796. [Google Scholar] [CrossRef] [PubMed]
  82. Lifshitz, F. Congenital lactase deficiency. J. Pediatr. 1966, 69, 229–237. [Google Scholar] [CrossRef]
  83. Savilahti, E.; Launiala, K.; Kuitunen, P. Congenital lactase deficiency. A clinical study on 16 patients. Arch. Dis. Child. 1983, 58, 246–252. [Google Scholar] [CrossRef] [PubMed]
  84. Behrendt, M.; Keiser, M.; Hoch, M.; Naim, H.Y. Impaired trafficking and subcellular localization of a mutant lactase associated with congenital lactase deficiency. Gastroenterology 2009, 136, 2295–2303. [Google Scholar] [CrossRef] [PubMed]
  85. Torniainen, S.; Freddara, R.; Routi, T.; Gijsbers, C.; Catassi, C.; Hoglund, P.; Savilahti, E.; Jarvela, I. Four novel mutations in the lactase gene (LCT) underlying congenital lactase deficiency (CLD). BMC Gastroenterol. 2009, 9, 8. [Google Scholar] [CrossRef] [PubMed]
  86. Uchida, N.; Sakamoto, O.; Irie, M.; Abukawa, D.; Takeyama, J.; Kure, S.; Tsuchiya, S. Two novel mutations in the lactase gene in a Japanese infant with congenital lactase deficiency. Tohoku. J. Exp. Med. 2012, 227, 69–72. [Google Scholar] [CrossRef] [PubMed]
  87. Diekmann, L.; Pfeiffer, K.; Naim, H.Y. Congenital lactose intolerance is triggered by severe mutations on both alleles of the lactase gene. BMC Gastroenterol. 2015, 15, 36. [Google Scholar] [CrossRef] [PubMed]
  88. Fazeli, W.; Kaczmarek, S.; Kirschstein, M.; Santer, R. A novel mutation within the lactase gene (LCT): The first report of congenital lactase deficiency diagnosed in central Europe. BMC Gastroenterol. 2015, 15, 90. [Google Scholar] [CrossRef] [PubMed]
  89. Gendrel, D.; Richard-Lenoble, D.; Kombila, M.; Dupont, C.; Moreno, J.L.; Gendrel, C.; Nardou, M.; Chaussain, M. Influence of intestinal parasitism on lactose absorption in well-nourished African children. Am. J. Trop. Med. Hyg. 1992, 46, 137–140. [Google Scholar] [PubMed]
  90. Beau, I.; Cotte-Laffitte, J.; Geniteau-Legendre, M.; Estes, M.K.; Servin, A.L. An NSP4-dependant mechanism by which rotavirus impairs lactase enzymatic activity in brush border of human enterocyte-like Caco-2 cells. Cell. Microbiol. 2007, 9, 2254–2266. [Google Scholar] [CrossRef] [PubMed]
  91. Ball, J.M.; Mitchell, D.M.; Gibbons, T.F.; Parr, R.D. Rotavirus NSP4: A multifunctional viral enterotoxin. Viral. Immun. 2005, 18, 27–40. [Google Scholar] [CrossRef] [PubMed]
  92. Berkova, Z.; Crawford, S.E.; Blutt, S.E.; Morris, A.P.; Estes, M.K. Expression of rotavirus NSP4 alters the actin network organization through the actin remodeling protein cofilin. J. Virol. 2007, 81, 3545–3553. [Google Scholar] [CrossRef] [PubMed]
  93. Weese, J.S.; Parsons, D.A.; Staempfli, H.R. Association of clostridium difficile with enterocolitis and lactose intolerance in a foal. J. Am. Vet. Med. Assoc. 1999, 214, 229–232. [Google Scholar] [PubMed]
  94. Kwak, Y.K.; Vikstrom, E.; Magnusson, K.E.; Vecsey-Semjen, B.; Colque-Navarro, P.; Mollby, R. The staphylococcus aureus alpha-toxin perturbs the barrier function in Caco-2 epithelial cell monolayers by altering junctional integrity. Infect. Immun. 2012, 80, 1670–1680. [Google Scholar] [CrossRef] [PubMed]
  95. Miko, B.A.; Uhlemann, A.C.; Gelman, A.; Lee, C.J.; Hafer, C.A.; Sullivan, S.B.; Shi, Q.; Miller, M.; Zenilman, J.; Lowy, F.D. High prevalence of colonization with Staphylococcus aureus clone USA 300 at multiple body sites among sexually transmitted disease clinic patients: An unrecognized reservoir. Microbes. Infect. 2012, 14, 1040–1043. [Google Scholar] [CrossRef] [PubMed]
  96. Hess, D.J.; Henry-Stanley, M.J.; Erickson, E.A.; Wells, C.L. Intracellular survival of Staphylococcus aureus within cultured enterocytes. J. Surg. Res. 2003, 114, 42–49. [Google Scholar] [CrossRef]
  97. Michael, L.; Timothy, W.; Aasma, S. Clinical implications of lactose malabsorption versus lactose intolerance. J. Clin. Gastroenterol. 2013, 47, 471. [Google Scholar]
  98. Dallas, M.S. Genetics of lactase persistence and lactose intolerance. Genetics 2003, 37, 197–219. [Google Scholar]
  99. Virginie, A.; Patrick, C.E.; Christiane, L.-A.; Jean-Marc, B.; François, B.; Robert, B.; Daniel, T.; Anne-Marie, D. Lactose malabsorption and colonic fermentations alter host metabolism in rats. Br. J. Nutr. 2013, 110, 625–631. [Google Scholar]
  100. Suarez, F.L.; Savaiano, D.A.; Levitt, M.D. Review article the treatment of lactose intolerance. Aliment. Pharmacol. Ther. 1995, 9, 589–597. [Google Scholar] [CrossRef] [PubMed]
  101. He, T.; Priebe, M.G.; Harmsen, H.J.; Stellaard, F.; Sun, X.; Welling, G.W.; Vonk, R.J. Colonic fermentation may play a role in lactose intolerance in humans. J. Nutr. 2006, 136, 58–63. [Google Scholar] [PubMed]
  102. Benjamin, M.; Daniel, P.; Heiko, F.; Michael, F.; Stephan, R.V.; Mark, F. Lactose malabsorption and intolerance: Pathogenesis, diagnosis and treatment. United Eur. Gastroent. J. 2013, 1, 151–159. [Google Scholar]
  103. Sanchez, B.; GavilÁN, D.; Margolles, A.; Gueimonde, M. Probiotic fermented milks: Present and future. Int. J. Dairy Technol. 2009, 62, 472–483. [Google Scholar] [CrossRef]
  104. Robert, T.G.; Taylor, M.; Sherry, B.; Phyllis, A.W. Cancer statistics, 2000. CA. Cancer. J. Clin. 2000, 50, 7–33. [Google Scholar]
  105. Kuokkanen, M.; Butzow, R.; Rasinpera, H.; Medrek, K.; Nilbert, M.; Malander, S.; Lubinski, J.; Jarvela, I. Lactase persistence and ovarian carcinoma risk in Finland, Poland and Sweden. Int. J. Cancer 2005, 117, 90–94. [Google Scholar] [CrossRef] [PubMed]
  106. Peter, R.H. New insights into calcium, dairy and colon cancer. World J. Gastroenterol. 2008, 14, 4429–4433. [Google Scholar]
  107. Ma, R.W.L.; Chapman, K. A systematic review of the effect of diet in prostate cancer prevention and treatment. J. Hum. Nutr. Diet. 2009, 22, 187–199. [Google Scholar] [CrossRef] [PubMed]
  108. Vargas, A.J.; Thompson, P.A. Diet and nutrient factors in colorectal cancer risk. Nutr. Clin. Pract. 2012, 27, 613–623. [Google Scholar] [CrossRef] [PubMed]
  109. Raúl Baena, R.; Pedro Salinas, H. Diet and cancer: Risk factors and epidemiological evidence. Maturitas 2014, 77, 202208. [Google Scholar]
  110. Rock, C.L. Milk and the risk and progression of cancer. Nestle. Nutr. Workshop Ser. Pediatr. Program 2011, 67, 173–185. [Google Scholar] [PubMed]
  111. Glade, M.J. World Cancer Research Fund/American Institute for Cancer Research. Food, Nutrition, Physical Activity and the Prevention of Cancer: A Global Perspective. Nutrition 2008, 24, 393–398. [Google Scholar] [CrossRef]
  112. Renate, C.H.B.; Renate, M.W.; Jacoba, M.S.R.; Lea, K.; Anne-Claire, B.O.L.; Ettje, F.T.; Doris, S.M.C.; Teresa, N.; Ellen, K. Dietary supplement use and colorectal cancer risk: A systematic review and meta-analyses of prospective cohort studies. Int. J. Cancer 2015, 136, 2388–2401. [Google Scholar]
  113. Van der Meer, R.; Lapré, J.A.; Govers, M.J.; Kleibeuker, J.H. Mechanisms of the intestinal effects of dietary fats and milk products on colon carcinogenesis. Cancer Lett. 1997, 114, 75–83. [Google Scholar] [CrossRef]
  114. Govers, M.J.; Termont, D.S.; Lapré, J.A.; Kleibeuker, J.H.; Vonk, R.J.; van der Meer, R. Calcium in milk products precipitates intestinal fatty acids and secondary bile acids and thus inhibits colonic cytotoxicity in humans. Cancer Res. 1996, 56, 3270–3275. [Google Scholar] [PubMed]
  115. Rasinperä, H.; Forsblom, C.; Enattah, N.S.; Halonen, P.; Salo, K.; Victorzon, M.; Mecklin, J.P.; Järvinen, H.; Enholm, S.; Sellick, G.; et al. The c/c−13910 genotype of adult-type hypolactasia is associated with an increased risk of colorectal cancer in the Finnish population. Gut 2005, 54, 643–647. [Google Scholar] [CrossRef] [PubMed]
  116. Krisztián, B.; Erika, H.; János, P.K.; Henrik, H.; Áron, L.; Péter, L.L.; Bernadett, B.; Barna, B.; Péter, L.; Gábor, S. Effects of the lactase 13910 c/t and calcium-sensor receptor a986s g/t gene polymorphisms on the incidence and recurrence of colorectal cancer in Hungarian population. BMC Cancer 2008, 8, 317. [Google Scholar]
  117. Ada, P.; Enrico, S.; Angela, M.; Annamaria, G.; Rosa, C.; Michele, Q.; Antonio, M.; Mauro, C.; Paolo Usai, S.; Francesco, P. Genotyping of the lactase-phlorizin hydrolase c/t-13910 polymorphism by means of a new rapid denaturing high-performance liquid chromatography-based assay in healthy subjects and colorectal cancer patients. J. Biomol. Screen. 2007, 12, 733–739. [Google Scholar]
  118. Elena, T.; Paola, P.; Elisabetta, B.; Giovanni, C.A.; Gianfranco, T.; Luciana, F.; Mohammad, A.; Francesca, C.; Nicola, L.; Giovanni, S.; et al. Lct-13910c > t polymorphism-associated lactose malabsorption and risk for colorectal cancer in Italy. Dig. Liver Dis. 2010, 42, 741743. [Google Scholar]
  119. Szilagyi, A.; Nathwani, U.; Vinokuroff, C.; Correa, J.A.A.; Shrier, I. Evaluation of relationships among national colorectal cancer mortality rates, genetic lactase non-persistence status, and per capita yearly milk and milk product consumption. Nutr. Cancer 2006, 55, 151–156. [Google Scholar] [CrossRef] [PubMed]
  120. Szilagyi, A.; Nathwani, U.; Vinokuroff, C.; Correa, J.A.A.; Shrier, I. The effect of lactose maldigestion on the relationship between dairy food intake and colorectal cancer: A systematic review. Nutr. Cancer 2006, 55, 141–150. [Google Scholar] [CrossRef] [PubMed]
  121. Martha, L.S.; Carol, S.; Maureen, M.; Khe-Ni, M.; Bette, J.C.; John, D.P.; Roger, W. Associations between vitamin D, vitamin D receptor gene and the androgen receptor gene with colon and rectal cancer. Int. J. Cancer 2006, 118, 3140–3146. [Google Scholar]
  122. Christakos, S.; Dhawan, P.; Porta, A.; Mady, L.J.; Seth, T. Vitamin D and intestinal calcium absorption. Mol. Cell. Endocrinol. 2011, 347, 25–29. [Google Scholar] [CrossRef] [PubMed]
  123. Andrew, S.; Henry, L.; Barry, B.; Xue, X.Q. Latitude, sunshine, and human lactase phenotype distributions may contribute to geographic patterns of modern disease: The inflammatory bowel disease model. Clin. Epidemiol. 2014, 6. [Google Scholar]
  124. George Davey, S.; Debbie, A.L.; Nic, J.T.; Jamil, B.; Matt, K.; Ian, N.M.D.; Shah, E. Lactase persistence-related genetic variant: Population substructure and health outcomes. Eur. J. Hum. Genet. 2008, 17, 357–367. [Google Scholar]
  125. Andrew, S. Determinants of geographic patterns of diseases: Interaction of lactose/lactase status and sunshine exposure. Med. Hypotheses 2010, 75, 466–470. [Google Scholar]
  126. Orel, R.; Trop, T.K. Intestinal microbiota, probiotics and prebiotics in inflammatory bowel disease. World J. Gastroenterol. 2014, 20. [Google Scholar] [CrossRef] [PubMed]
  127. Shiby, V.K.; Mishra, H.N. Fermented milks and milk products as functional foods—A review. Crit. Rev. Food Sci. Nutr. 2013, 53, 482–496. [Google Scholar] [CrossRef] [PubMed]
  128. Peter, W.P. Dairy product consumption and the risk of prostate cancer. Int. Dairy J. 2009, 19, 551–565. [Google Scholar]
  129. Herrinton, L.J.; Weiss, N.S.; Beresford, S.A.; Stanford, J.L.; Wolfla, D.M.; Feng, Z.; Scott, C.R. Lactose and galactose intake and metabolism in relation to the risk of epithelial ovarian cancer. Am. J. Epidemiol. 1995, 141, 407–416. [Google Scholar] [PubMed]
  130. Gian Franco, M.; Carla, C.; Carlo La, V.; Giuseppina, R.; Maria Chiara, M.; Guido, A.; Pier Luigi, C. Lactose absorption in patients with ovarian cancer. Am. J. Epidemiol. 1999, 150, 183–186. [Google Scholar]
  131. Fathalla, M.F. Incessant ovulation—A factor in ovarian neoplasia? Lancet 1971, 2, 163. [Google Scholar] [CrossRef]
  132. Cramer, D.W.; Welch, W.R. Determinants of ovarian cancer risk. II. Inferences regarding pathogenesis. J. Natl. Cancer Inst. 1983, 71, 717–721. [Google Scholar] [PubMed]
  133. Kathleen, M.F.; David, J.H.; Graham, A.C.; Charles, S.F.; Daniel, W.C.; Frank, E.S.; Walter, C.W.; Susan, E.H. A prospective study of dietary lactose and ovarian cancer. Int. J. Cancer 2004, 110, 271–277. [Google Scholar]
  134. Cramer, D.W. Lactase persistence and milk consumption as determinants of ovarian cancer risk. Am. J. Epidemiol. 1989, 130, 904–910. [Google Scholar] [PubMed]
  135. Koralek, D.O.; Bertone-Johnson, E.R.; Leitzmann, M.F.; Sturgeon, S.R.; Lacey, J.V.; Schairer, C.; Schatzkin, A. Relationship between calcium, lactose, vitamin D, and dairy products and ovarian cancer. Nutr. Cancer 2006, 56, 22–30. [Google Scholar] [CrossRef] [PubMed]
  136. Torniainen, S.; Hedelin, M.; Autio, V.; Rasinpera, H.; Balter, K.A.; Klint, A.; Bellocco, R.; Wiklund, F.; Stattin, P.; Ikonen, T.; et al. Lactase persistence, dietary intake of milk, and the risk for prostate cancer in Sweden and Finland. Cancer Epidemiol. Biomarkers Prev. 2007, 16, 956–961. [Google Scholar] [CrossRef] [PubMed]
  137. Ruth, C.T.; Paul, N.A.; Afshan, S.; Naomi, E.A.; Rudolf, K.; Federico, C.; Silke, F.; Anne, T.; Nina Føns, J.; Kim, O.; et al. Genetic variation in the lactase gene, dairy product intake and risk for prostate cancer in the European prospective investigation into cancer and nutrition. Int. J. Cancer 2013, 132, 1901–1910. [Google Scholar]
  138. Mayank mohan, A.; Satyavati, V.R.; Arup kumar, M.; Sunita, M.; Niranjan, K.; Santosh, K.; Naveen chandra, A.; Shrawan kumar, S. Lactose intolerance in prostate cancer patients: Incidence and associated factors. Scand. J. Gastroenterol. 2008, 43, 270276. [Google Scholar]
  139. June, M.C.; Crystal, N.H.; Michael, F.L.; Eric, B.R.; Walter, C.W.; Meir, J.S.; Edward, L.G. Diet after diagnosis and the risk of prostate cancer progression, recurrence, and death (United States). Cancer Causes Control 2005, 17, 199–208. [Google Scholar]
  140. Parodi, A.; Dulbecco, P.; Savarino, E.; Giannini, E.G.; Bodini, G.; Corbo, M.; Isola, L.; De Conca, S.; Marabotto, E.; Savarino, V. Positive glucose breath testing is more prevalent in patients with IBS-like symptoms compared with controls of similar age and gender distribution. J. Clin. Gastroenterol 2009, 43, 962–966. [Google Scholar] [CrossRef] [PubMed]
  141. Davaasambuu, G.; Akio, S. The possible role of female sex hormones in milk from pregnant cows in the development of breast, ovarian and corpus uteri cancers. Med. Hypotheses 2005, 65, 1028–1037. [Google Scholar]
  142. Qin, L.; Xu, J.; Wang, P.; Tong, J.; Hoshi, K. Milk consumption is a risk factor for prostate cancer in western countries: Evidence from cohort studies. Asia Pac. J. Clin. Nutr. 2007, 16, 467–476. [Google Scholar] [PubMed]
  143. Qin, L.Q.; Wang, P.Y.; Takashi, K.; Kazuhiko, H.; Akio, S. Estrogen: One of the risk factors in milk for prostate cancer. Med. Hypotheses 2004, 62, 133–142. [Google Scholar] [CrossRef]
  144. Shi, W.F.; Jeffrey, S.B. Estrogen plays a critical role in AAV2-mediated gene transfer in ovarian cancer. Acta Pharmacol. Sin. 2008, 29, 1440–1450. [Google Scholar] [CrossRef] [PubMed]
  145. Hassan, M.; Peter, S.; Aldert, A.B. Naturally occurring estrogens in processed milk and in raw milk (from gestated cows). J. Agri. Food Chem. 2006, 54, 9785–9791. [Google Scholar]
  146. John, V.; Terry, E.; Penny, K.-E.; Joan, B.; Steven, D.; Robin, S.; Daniel, G.; Roger, C.; Michael, M.; Matthew, L. Survey of retail milk composition as affected by label claims regarding farm-management practices. J. Am. Diet. Assoc. 2008, 108, 1198–1203. [Google Scholar]
  147. Daniel, W.F.; Xia, X.; Timothy, D.V. Quantitative measurement of endogenous estrogen metabolites, risk-factors for development of breast cancer, in commercial milk products by lc-ms/ms. J. Chromatogr. B. Analyt. Technol. Biomed. Life. Sci. 2009, 877, 1327–1334. [Google Scholar]
  148. Pape-Zambito, D.A.; Magliaro, A.L.; Kensinger, R.S. 17β-estradiol and estrone concentrations in plasma and milk during bovine pregnancy. J. Dairy Sci. 2008, 91, 127–135. [Google Scholar] [CrossRef] [PubMed]
  149. Pape-Zambito, D.A.; Roberts, R.F.; Kensinger, R.S. Estrone and 17β-estradiol concentrations in pasteurized-homogenized milk and commercial dairy products. J. Dairy Sci. 2010, 93, 2533–2540. [Google Scholar] [CrossRef] [PubMed]
  150. Furnari, C.; Maroun, D.; Gyawali, S.; Snyder, B.W.; Davis, A.M. Lack of biologically active estrogens in commercial cow milk. J. Dairy Sci. 2012, 95, 9–14. [Google Scholar] [CrossRef] [PubMed]
  151. Peter, W.P. Impact of cows’ milk estrogen on cancer risk. Int. Dairy J. 2012, 22, 314. [Google Scholar]
  152. Arthur, C.O.; Seppo, S.; Erika, I. Probiotics: An overview of beneficial effects. Antonie Van Leeuwenhoek 2002, 82, 279–289. [Google Scholar]
  153. Johnson, I.T. New approaches to the role of diet in the prevention of cancers of the alimentary tract. Mutat. Res. 2004, 551, 9–28. [Google Scholar] [CrossRef] [PubMed]
  154. Lourdes, S.L.; Adrián, H.M.; Hugo, S.G.; Verónica, M.H.; Belinda, V.C.; Aarón, F.G.C. The effects of consuming probiotic fermented milk on the immune system: A review of scientific evidence. Int. J. Dairy Technol. 2015, 68, 153–165. [Google Scholar]
  155. Jarvis, J.K.; Miller, G.D. Overcoming the barrier of lactose intolerance to reduce health disparities. J. Natl. Med. Assoc. 2002, 94, 55–66. [Google Scholar] [PubMed]
  156. Money, M.E.; Camilleri, M. Review: Management of postprandial diarrhea syndrome. Am. J. Med. 2012, 125, 538–544. [Google Scholar] [CrossRef] [PubMed]
  157. Austin, G.L.; Dalton, C.B.; Hu, Y.; Morris, C.B.; Hankins, J.; Weinland, S.R.; Westman, E.C.; Yancy, W.S., Jr.; Drossman, D.A. A very low-carbohydrate diet improves symptoms and quality of life in diarrhea-predominant irritable bowel syndrome. Clin. Gastroenterol. Hepatol. 2009, 7, 706–708. [Google Scholar] [CrossRef] [PubMed]
  158. He, T.; Priebe, M.G.; Zhong, Y.; Huang, C.; Harmsen, H.J.; Raangs, G.C.; Antoine, J.M.; Welling, G.W.; Vonk, R.J. Effects of yogurt and bifidobacteria supplementation on the colonic microbiota in lactose-intolerant subjects. J. Appl. Microbiol. 2008, 104, 595–604. [Google Scholar] [CrossRef] [PubMed]

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Amiri, M.; Diekmann, L.; Von Köckritz-Blickwede, M.; Naim, H.Y. The Diverse Forms of Lactose Intolerance and the Putative Linkage to Several Cancers. Nutrients 2015, 7, 7209-7230. https://0-doi-org.brum.beds.ac.uk/10.3390/nu7095332

AMA Style

Amiri M, Diekmann L, Von Köckritz-Blickwede M, Naim HY. The Diverse Forms of Lactose Intolerance and the Putative Linkage to Several Cancers. Nutrients. 2015; 7(9):7209-7230. https://0-doi-org.brum.beds.ac.uk/10.3390/nu7095332

Chicago/Turabian Style

Amiri, Mahdi, Lena Diekmann, Maren Von Köckritz-Blickwede, and Hassan Y. Naim. 2015. "The Diverse Forms of Lactose Intolerance and the Putative Linkage to Several Cancers" Nutrients 7, no. 9: 7209-7230. https://0-doi-org.brum.beds.ac.uk/10.3390/nu7095332

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